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Understanding Nanocellulose–Water Interactions: Turning a Detriment into an Asset

Laleh Solhi, Valentina Guccini, Katja Heise and 10 more

Chemical Reviews · 2023 · Review · CC BY

doi:10.1021/acs.chemrev.2c00611

Abstract

Modern technology has enabled the isolation of nanocellulose from plant-based fibers, and the current trend focuses on utilizing nanocellulose in a broad range of sustainable materials applications. Water is generally seen as a detrimental component when in contact with nanocellulose-based materials, just like it is harmful for traditional cellulosic materials such as paper or cardboard. However, water is an integral component in plants, and many applications of nanocellulose already accept the presence of water or make use of it. This review gives a comprehensive account of nanocellulose-water interactions and their repercussions in all key areas of contemporary research: fundamental physical chemistry, chemical modification of nanocellulose, materials applications, and analytical methods to map the water interactions and the effect of water on a nanocellulose matrix.

Full text

From PubMed Central, U.S. National Library of Medicine, as current on Oct 21, 2026. Paragraph numbers are ours, so an answer can point at one.

Introduction

The term nanocellulose refers to anisotropic nanoparticles that can be isolated from, in most cases, a processed plant cell wall. While the early accounts of nanocellulose originate from the mid-20th century, the first decade of the 21st century saw process-related advances that enabled a more facile and efficient isolation of nanocellulose for materials construction. This development in nanocellulose preparation and its applications has unleashed an unprecedented scientific interest in cellulose-based materials over the past 15 years.− Although much of the attention has focused on utilizing nanocellulose as a building block in new functional materials, the fundamental progress in cellulose science stemming from nanocellulose research has also been remarkable.−

This review presents a comprehensive, critical coverage of a topic which is dominant in both fundamental aspects and materials applications of nanocellulose: cellulose–water interactions. The presence of water or humidity in cellulose-based materials is often seen as a detriment. Everyone knows what happens to paper when you immerse it in water: it disintegrates and loses its mechanical strength. Nanocellulose is made of much smaller entities than pulp fibers, and because of its high surface area, it takes up more water and the effect is even more drastic. As high strength coupled with low density is one of the main assets of nanocellulose, the strength loss in water is a major issue. In general, water is seen as a nuisance, and the ensuing problems are being tackled with “brute force” such as chemical hydrophobization and the like. Quantification, localization, and influence of water within a cellulose matrix has also been subject to a number of analytical challenges throughout the history, and it continues to be that way.

The purpose of this review is to point out how the presence of water can be beneficial as well as detrimental in nanocellulose-based systems, processes, and materials: isolation, chemical modification, biomedical templates, responsive hydrogels, sensors, smart emulsions, and so forth. Although intuitively utilized since the ancient times, for example, Egyptians exploiting wood swelling in water to seal leaking joints in their boats, the systematic usage of water interactions has started to emerge only within the past few years.

The specific response to water has its roots in the amphiphilic nature of cellulose and its native crystallite structure. The literature on fundamental aspects of cellulose–water interactions spans roughly one century, albeit with a dramatic upsurge during the past decade, fully covered in this review. Understanding the different “types” of bound water and how to measure them, is another crucial step to exploiting nanocellulose–water interactions, and as such, we extensively discuss analytical tools including modeling and experimental approaches to elucidate the relationships between water and nanocellulose.

A number of studies and reviews focus on the interactions of water and other natural polymers such as chitin, and collagen, in the literature. To our knowledge, a comprehensive review on such materials to the extent of the scope of this review has not been published. In addition to presenting fundamentals and characterization, this review focuses on new nanocellulose-based materials which may suffer (but just as well benefit) from the presence of water. We see this as a vital approach in the current research environment where “green” solutions to chemicals and materials are intensively sought after. Accepting (and taking advantage of) the presence of water and the predictability of processing nanocellulose in water is also important when we consider replacing nonaqueous solvents with water in striving toward a more sustainable society. Combined with the comprehensive nature of our approach, spanning fundamentals and analytics, the all-inclusive take on the role of water interactions in nanocellulose production, modification, and applications is what distinguishes this review from other recent reviews that touch on the subject of cellulose–water interactions.,,,−

Overview of the Properties of Water

Water is usually considered as either a solvation agent or a suspension medium in nanocellulose related research, and the complexity of water is often overlooked. To understand nanocellulose–water interactions, it is pivotal to briefly review some of the relevant characteristics and main features of water. To limit the scope of this discussion, we focus on liquid water at moderate temperatures and pressures. For more comprehensive reviews of water and its properties in more extreme conditions, we guide the reader to relevant publications in the field.− The complex behavior of water results from a combination of hydrogen bonding, dissociation behavior, and the complex structural dynamics, influenced by temperature, pressure, and its interaction with the interfaces and other molecules. As we approach this topic, it should be noted that much controversy still exists regarding the detailed mechanisms and dynamics of water behavior at this level. Also, the developments in the simulation of water properties and dynamics− as well as experimental techniques, have been recently reviewed elsewhere.

IUPAC defines a hydrogen bond as “an attractive interaction between a hydrogen atom from a molecule or a molecular fragment X–H in which X is more electronegative than H, and an atom or a group of atoms in the same or a different molecule, in which there is evidence of bond formation”. This definition leaves the mechanism of this attractive interaction purposefully open, as no single physical force can be found to be responsible for the phenomena we observe as hydrogen bonding. Indeed, the hydrogen bond is either described as a sum of several forces such as electrostatic interactions, polarization, induction interactions between multipoles, charge-transfer-induced covalency, or an independent interaction with unidentified origin. The consensus in the scientific community is that there are three-dimensional dynamics and a random network of hydrogen-bonded molecules in liquid water in which the hydrogen bonds are continuously broken and reformed on the time scale of femtoseconds to picoseconds. Thus, there is a broad distribution of possible energies and an indefinitely high number of molecules involved in the hydrogen bonding network of bulk liquid water. This means that assigning a specific, singular, hydrogen bonding energy to a liquid water system would be misleading. Moreover, as water can be both an acceptor and a donor of multiple hydrogen bonds, a distribution of acceptor–donor states exists. The 2 acceptor −2 donor model, resulting in tetrahedral molecular ordering, seems to be the dominant structure on average. Due to the random structuring of hydrogen bonds, a water cluster can be identified as a subgroup of water molecules, which form comparatively stable substructures in the time frame of hydrogen bond formation and dissociation. These water clusters can influence the structuring of hydrogen bonds in the surrounding medium outside the cluster. Although their very existence is not that controversial, the exact structure, lifetime, and effects that clusters have on the surrounding water medium are still under debate. In addition to water clustering, other phenomena characterized by the hydrogen water dynamics include proton hopping (the exchange of protons between neighboring water molecules) and changes in the hydrogen bond structure of water around OH– and H3O+ ions. Fluctuations in hydrogen bond networks are experimentally accessible by computer simulations, albeit some spectroscopic methods also allow for probing of the phenomena occurring on these time scales. For a more detailed discussion on how the various ways the hydrogen bond energy of water has been approximated and investigated we suggest a book chapter by Chaplin and a review by Cisneros et al. for a more technical-oriented approach.

In addition to water structuring in molecular clusters, the hydrogen bond network of water is altered due to interactions with interfaces or other molecules resulting in the reordering of water molecules. Interesting examples of this phenomenon are the structuring of water in the presence of solutes, at the surface of water-dispersed colloids/particles, and even at hydrophobic surfaces. We address the structuring of water around nanocellulosic materials in section 3.1 when the amphiphilic nature of nanocellulose is discussed.

Origin and Basic Crystalline Structure of Cellulose

Cellulose is a semicrystalline polysaccharide composed of β-1,4-linked d-anhydroglucopyranose units (C6H10O5), and it is biosynthesized from glucose through a uridine diphosphate glucose intermediate by all higher-order plants, green algae, as well as some specific marine animals (tunicates) and certain bacteria (namely those belonging to the genera Acetobacter, Rhizobium, Agrobacterium, and Sarcina). Cellulose is the most ubiquitously present natural polymer in both land and marine ecosystems and functions as a highly effective natural carbon sink in terrestrial ecosystems turning over almost 3.6 gigatons of carbon annually. The majority of cellulose is found in higher-order plants, and it typically accounts for 40–50% of the mass of wood material depending on the species of the plant source.

Cellulose biosynthesis is carried out by the cellulose synthase complex or terminal complex (TC), where simultaneously upon their synthesis the cellulose polymer chains are assembled into higher-order structures known as microfibrils, which are the smallest supramolecular units of cellulose in nature. Microfibrils are semicrystalline, slender threads that form the structural scaffold of the plant cell wall. In the native cellulose crystal, sheets formed by hydrogen bonding are stacked on top of each other through interplanar van der Waals forces. Within the sheets, the intramolecular hydrogen bonds in the native cellulose I crystal are between HO(3)–HO(5) and HO(2)–HO(6), whereas the major intermolecular bond forms between HO(3) and HO(6) (Figure 1a for cellulose I and Figure 1b for cellulose II). Overall, the hydrogen bond energy of cellulose ranges from 17 to 30 kJ mol–1, and the intermolecular hydrogen bond energy is approximated to be around 20 kJ mol–1. In cellulose I, for example, the density of hydrogen bonds is approximately 3.7 × 1018 m–2 along the 1(−1)0 crystallographic plane.

The widths and the shapes of the crystal, which determine the width of the microfibril, differ according to the cellulose source. As a rule of thumb, the higher the plant has climbed on the evolutionary ladder, the thinner the crystal. Trees have the thinnest crystals (∼3 nm), while algae have the widest (>20 nm). This observation can be rationalized by taking into account that the crystallinity and order in the higher plant cell walls are optimized to find a perfect balance between strength and flexibility and to ensure the structural integrity of the organism depending on their growth and environmental condition (e.g., wind, water availability).

The number of cellulose chains that make up the cellulose crystallite in a microfibril is dependent on the source of the cellulose, and it is still a matter of debate among the cellulose community. For instance, in the case of wood cellulose, it was traditionally accepted that each TC synthesizes microfibrils consisting of 36 cellulose polymer chains (i.e., a 6 × 6 chain cross-section, Figure 1c). Later, however, Jarvis and co-workers suggested that 24 chains make up the crystal (Figure 1d), and more recently, models for 18 chain crystals have gained ground (Figure 1e). These 24 and 18 chain models appear currently more accepted within crystallographers than the traditional 36 chain model. Regardless of the exact number of chains making up the microfibril, it is important to understand that cellulose in nature exists exclusively in the form of microfibrils and it is never found in nature as single polymer chains or in a fully amorphous form.

Native crystalline cellulose, also referred to as cellulose I, is assembled with the cellulose polymer chains running parallel to one another, and it exists as two different crystal structures (i.e., polymorphs): triclinic Iα or monoclinic Iβ. Primarily, the crystal structure of cellulose is governed by the conformation of the TC, which in turn affects the morphology of the resulting microfibril. Linear TCs, for example, mostly produce Iα rich cellulose and relatively wide microfibrils with high degree of crystallinity, while rosette-shaped TCs produce thin, Iβ-rich cellulose microfibrils., Tsekos et al. showed a rough, but indisputable, correlation between the shape of the TC and the resulting cellulose microfibril. It is important to note, however, that both polymorphs coexist in all cellulose and their ratio varies depending on the cellulose source. Cellulose Iβ is dominant in higher-order plants and tunicate-synthesized cellulose, while cellulose Iα is the main component of celluloses synthesized by algae and bacteria.

Two alternative hypotheses have been proposed to explain the simultaneous presence of the Iα and Iβ forms of cellulose. The first is that cellulose Iα is synthesized by a different type of TC from cellulose Iβ, whereas the second hypothesis is that the different cellulose polyomorphs result from events that occur after the synthesis of the cellulose polymer chains. For example, it has been shown that bending can interconvert the crystalline forms of cellulose I and that their ratio is very sensitive to the angle through which the microfibril is bent.

Besides the native crystalline form, different cellulose polymorphs exist, in which the crystalline structure of cellulose Iα and Iβ have been altered through physicochemical treatments. Cellulose II can be prepared by reorganizing the hydrogen bonding network such that the cellulose chains run antiparallel to each other in the crystal structure using either a mercerization process where cellulose I is swollen in the presence of NaOH or through the regeneration (i.e., solubilization and subsequent recrystallization) of cellulose (Figure 1b). Cellulose I readily converts into cellulose II in an irreversible process, as cellulose II is thermodynamically more stable than cellulose I. A third cellulose polymorph called cellulose III can also be reversibly prepared by exposing cellulose I or II to liquid ammonia or certain diamines. However, cellulose I and II arguably garner the most research interest because of their biological, industrial, and scientific relevance, and cellulose I is overwhelmingly the most dominant polymorph in all nanocellulose constructs.

Cellulose Morphology and the Hierarchical Structure of the Plant Cell Wall

While cellulose microfibrils are predominantly crystalline, there is direct evidence showing that the microfibril structure in higher plants has regions of disordered cellulose distributed along their length (Figure 2)., The length of the crystalline portions between these disordered regions is primarily governed by the source of the cellulosic material, and this is often depicted using the so-called fringed-fibrillar model.,,− For example, the length of the crystalline regions in cotton-derived cellulose is on average 125 nm (i.e., a degree of polymerization (DP) of 250), whereas that of tunicate cellulose can be as high as 3 μm (DP = 6000). The inherent length of the crystalline portions of the cellulose structure is linked to the leveling-off degree of polymerization (LODP), corresponding to the DP at which the cellulose structure become inaccessible for further degradation when exposed to strong mineral acids or oxidizing agents at semidilute concentrations.,

Isolated native cellulose often gives crystallinity index values between 60% and 90% when analyzed by X-ray diffraction or solid-state NMR spectroscopy. However, such values do not directly indicate that, for example, 70% of the cellulose in the microfibrils would be crystalline and the remaining 30% would be disordered or “amorphous”. In comparison to the crystalline regions, the disordered regions are reportedly very short: accounts of 1–2 nm and 3–6 nm have been proposed,, i.e., they are more like defects in the crystallite rather than bulky amorphous regions as they are often schematically depicted in traditional literature. Much of the response of the disordered cellulose in analytics likely comes from the microfibril surface simply because the chains there have higher degrees of freedom. As a result, the systematically higher crystallinity reported for algae or tunicates comes largely from the fact that their microfibrils, and therefore their crystallites, are wider than those in higher plants (i.e., there are fewer surface cellulose chains)., Cellulose sample preparation prior to crystallinity measurements can also affect the degree of crystallinity values obtained, at least within a few percent range. Certainly, the frequency of the disordered regions also plays a role here, but we believe that the crystallite width is a more significant factor.

Furthermore, while nearly all studies assume that the disordered cellulose regions are a part of natural microfibrils, some reports have suggested that these regions of disorder are in fact a result of the processes involved in cellulose isolation. For example, Atalla et al. put forward that native celluloses are irreversibly transformed and develop the semicrystalline character upon isolation at elevated temperatures. These issues are still under debate. Nonetheless, the semicrystalline nature of cellulose is a fact of processed cellulosic materials, such as virtually all nanocellulose types, and it adds to their complexity as areas of high order are less susceptible to chemical and biological attack.

The role of disordered regions in water-induced swelling of cellulosic materials is not straightforward. There is a common consensus that crystalline cellulose is impenetrable by water. However, the disordered regions may be somewhat “accessible”, but they are certainly not “swollen” by water because of their short, defect-like texture. It has never been shown that the length of a microfibril would increase when immersed in water. However, small angle neutron scattering data have shown that a somewhat higher concentration of D2O molecules can be observed in the vicinity of the disordered segments.

Another often misunderstood fundamental issue with cellulose–water interactions is hydrogen bonding. Despite the undisputable importance of hydrogen bonding between water molecules and nanocellulose at the interface in governing the characteristics and properties of cellulose dispersions, we would like to echo the conclusions of Wohlert et al. in their critical review on the general role of hydrogen bonding in nanocellulose structure and properties as a material. They conclude that hydrogen bonding is one interaction among several, and its relative contribution to the nanocellulose properties is highly dependent on the specific conditions and cannot easily be determined by intuition or even by analysis.,

In any case, the combination of the insolubility of cellulose in water with its ability to interact with water are fundamentally important to sustaining its structural integrity. Nature has utilized this feature of cellulose to engineer the incredible structure that is the plant cell wall. The plant cell wall is made up of three distinct regions: (i) the primary cell wall, (ii) the secondary cell wall (made up of three layers), and (iii) the middle lamella. Within the primary and secondary plant cell walls, cellulose microfibrils are further assembled into microfibril bundles and form a composite network structure with the two other main plant cell wall components, namely hemicellulose and lignin (Figure 2).−

Within the plant cell wall, the microfibrils (and their bundles) are orientated depending on which layer of the cell wall they exist in (Figure 2). In the primary cell wall, the microfibrils form very thin oriented layers with different orientations to one another, forming the impression of a random network., On the other hand, the highly aligned microfibrils have a unique microfibril angle in each of the three layers of the secondary cell wall. This level of natural hierarchical engineering provides plants with the necessary flexibility required for growth and swelling in the presence of water while ensuring the plant has sufficient axial stiffness., When discussing the swelling of cellulosic materials in water, one must remember that it is never the individual cellulose microfibril that swells, it is always a scaffold where bulk water clusters between the microfibrils. As a result of axial microfibril orientation in the secondary wall, the plant fibers always swell copiously in a radial direction, but their length of increase when immersed in water is negligible.

Plant fibers are always swollen by water as the major component in their native growth environment, which imparts the plants with necessary flexibility. It was earlier proposed that water is held in a microporous gel of hemicelluloses and lignin distributed as fine platelets within a cellulose skeleton. Yet the water content is strictly controlled by the presence of more hydrophobic lignin in the cell wall. Conventional pulping process including beating and bleaching (delignification) is often undertaken when chemically processing plant fibers to, for example, pulp for paper production. Rheological properties of fiber–water suspensions where water acts as a suspension matrix are of critical importance in many of papermaking process from beating, screening, fractionation, dispersion flow in headbox, sheet forming, and dewatering. In general, delignified fibers make up a strong network because the fibers are able to form inter- and intrahydrogen bonds with each other due to cellulose surface exposure after lignin removal. Two general water transport mechanisms including diffusion and capillary flow were suggested in cellulosic materials. If the fiber network is exposed to water, however, the fibers and the network lose their integrity and mechanical strength because lignin is no longer there to obstruct the water adsorption to cellulose surface due to pore flow accompanied by a surface “hopping” mechanism., A delignified fiber is also prone to irreversible loss of porosity due to drying. Pores between the cellulose microfibrils are filled with water in a swollen state and the pores disappear due to capillary forces as the water is removed. When the fiber is re-exposed to water, the pores reappear but not to the same extent as before drying. This decrease in the swelling capability of a fiber is referred to as hornification, and it has genuine practical implications not only in papermaking and paper recycling but also in nanocellulose production.− Hornification is often (usually without explicit evidence) attributed to “irreversible hydrogen bond formation between neighboring microfibrils upon drying”. To our perception, a more likely reason could be hydrophobic interactions where the hydrophobic sites of the cellulose crystals in microfibrils partially aggregate. Such hydrophobic bonding is less likely to be cleaved by water upon re-exposure than hydrogen bonding. We must acknowledge, however, that several accounts refer to co-crystallization or association of hydrophilic sites as a culprit for hornification, with obvious involvement of (also) hydrogen bonding between the microfibrils., The issue remains unsettled within the community. Hornification or similar phenomena with microfibril aggregation have even been reported to occur in air-dried cotton fibers upon exposure to HCl vapor, a preliminary phase in one type of nanocellulose isolation procedure. Moreover, the loss in swelling capability is not restricted to fully delignified samples and it has also been observed to an extent for lignin-containing samples such as wood and mechanical pulp., The situation is further complicated by the fact that hornification is known to be at least partially reversible with introduction of mechanical force in the system, a process referred to as beating in the papermaking sciences. In addition, the response of the dimensional behavior of paper to relative humidity changes is a reflection of individual cellulose fiber changes in macroscale manner. The torsional response, i.e., twist, in drying of a collapsed fiber is a function of the microfibril angle, the fiber length, and the factional linear shrinkage across the microfibrils, which is closely related to the nanoscale twist of nanocellulose (will be explicitly discussed in section 2.3 and section 4.1). All in all, drying of wood and other native specimen is a more complex affair with a series of structural rearrangements taking place, involving physical deformations such as bending, buckling, or twisting of the fibrous cellulose bundles.−

Types of Nanocellulose

Nanocellulose refers to cellulosic materials which have at least one dimension in the nanoscale. A vast majority of nanocellulose consists of anisotropic nanoparticles with varying aspect ratios although spherical nanocelluloses have also been reported., Nanocellulose, namely cellulose nanofibrils (CNFs), cellulose nanocrystals (CNCs), and bacterial cellulose (BC), have garnered a vast amount of research attention due to their incredible versatility. Their high aspect ratios, high surface area to volume ratios, abundance of surface hydroxy groups, and high strength enable them to be used in a wide variety of potential applications., While all nanocellulose grades exhibit the aforementioned properties, CNFs and BC are distinctly different materials to CNCs, as attested visually in Figure 3.,

CNFs are essentially isolated cellulose microfibrils (Figure 2 and Figure 3a). In consequence, they are flexible and semicrystalline threads, with diameters in the nanoscale (average width of 2–50 nm) but lengths in the micrometer range (1–15 μm)., A series of chemical (e.g., a 2,2,6,6-tetramethylpiperidin-1-yl)oxyl (TEMPO)-mediated oxidation) and/or enzymatic pretreatments (e.g., cellulases), followed by substantial mechanical defibrillation, are necessary to liberate CNFs from their biological matrix, i.e., the plant fiber, given the strong interactions between cellulose microfibrils and the tightly knit hierarchical structure of the cell wall. During the mechanical defibrillation, high shear forces are applied to isolate single CNFs which have dimensions dependent on both the isolation method and the source of the cellulose. The surface charge of CNFs depends on the amount of residual hemicellulose, namely xylan with methylglucuronic acid groups, and the choice of pretreatment. Specifically, the CNFs prepared by TEMPO-mediated oxidation pretreatment (TOCNF) carry very high charge densities, with approximately every second anhydroglucose unit on the surface bearing a carboxylic group when the maximum degree of oxidation is applied. Full details on CNF isolation can be found in the relevant reviews., TEMPO-mediated oxidation is also the only pretreatment method that manages to truly individualize microfibrils into CNFs. With other isolation methods, the CNFs always consist of (at least partially) microfibrillar bundles.

CNCs (sometimes called nanowhiskers) on the other hand, are highly crystalline, rod-shaped nanoparticles, with widths between 3 and 50 nm and lengths ranging from 50 nm to 10 μm (Figure 3b) depending on the cellulose source. The most common source for CNCs is cotton because of the wide availability and relative purity of ordinary laboratory filter paper; the typical widths of cotton CNCs range from 5 to 20 nm and lengths from 50 to 300 nm (with an average at ∼120 nm). Similar to CNFs, CNCs are also prepared using a top-down approach. By contrast, however, CNCs are typically isolated using an acid-catalyzed hydrolysis, which selectively degrades the more reactive disordered regions of the cellulose microfibril and leaves intact the crystalline regions.,− The length (or DP) of CNCs is largely governed by the LODP of their source material (see section 2.2.2 for a description of LODP and Figure 2). The conventional method to isolate CNCs is to perform a hydrolysis reaction in the presence of concentrated sulfuric acid at elevated temperatures, which in addition to hydrolyzing the disordered regions introduces charged sulfate half ester groups on the CNC surface, thus imparting colloidal stability.− Recently, many alternative isolation methods for CNCs have surfaced, based on, e.g., oxidation and esterification, but these approaches often require the additional presence of a strong mineral acid to perform the hydrolysis of disordered regions. A critical factor is that CNCs require some type of a surface charge group to come up with a stable colloidal dispersion in water. While sulfated CNCs are still overwhelmingly the most produced and studied, CNCs stabilized by phosphate, and carboxylate groups,,, have gained ground in recent years. For comprehensive accounts of CNC preparation, the interested reader is referred to recent reviews on the topic.,, One of the distinguishing characteristics of CNC dispersions is that they spontaneously form (lyotropic) chiral nematic liquid crystals, a feature that has spawned a sizable branch of CNC research over the past 30 years.−

The current trend in the literature is to regard BC as the third member of the nanocellulose family because it is produced by various bacterial species from low molecular weight sugars using a bottom-up approach (Figure 3c). BC is directly synthesized as a hydrated nanofiber network, i.e., a hydrogel,, and unlike CNF and CNC preparation, it requires no isolation steps apart from washing away the bacteria and growth culture medium with mild alkali. Although the bottom-up preparation route for BC is distinctly different from the other nanocellulose types, BC is essentially a form of CNF as it consists of semicrystalline, flexible threads. In contrast to plant-based CNFs, BC nanofibers are like flat ribbons, that is, their cross-sectional dimensions are rectangular: ca. 7 nm high and 20–140 nm wide. After rinsing off the bacteria, BC is also the purest form of nanocellulose without remnants of hemicellulose or lignin and virtually without any charge. The chemical purity is among the reasons why BC has been popular, particularly in biomedical applications.

Both CNCs and CNFs show a longitudinal twist with a right-handed chirality, which ultimately originates from the crystalline structure of cellulose., Molecular dynamics (MD) simulations have established the twist in molecular cellulose as well as in cellulose I crystal., Combining computational and experimental data, Conley et al. quantified a twist of 800 nm period for wood-based CNC. As the CNCs from typical sources like wood, cotton, or ramie have lengths spanning 50–300 nm, the long periodicity in the twist may be the reason as to why the twist is rarely visually evident in microscopy images of common CNCs. Despite this, the twisting of the cellulose crystal ultimately causes the formation of chiral nematic liquid crystals in CNC dispersions.

A noteworthy physical distinction in aqueous dispersions of CNFs and CNCs is that CNFs form gels at very low concentrations (<1 wt %), whereas CNCs are fluid dispersions of fairly low viscosity. CNCs do gel, but usually the gelling point is above the critical concentration for liquid crystal formation (ca. 10 wt %). These differences in water binding capacity are a partial reason for the different approaches in applications-related research concerning CNFs and CNCs. CNFs are often applied as scaffold structures in hydrogels, or as entangled networks, whereas CNCs are utilized when, for example, discrete particles are needed or sophisticated chemical modifications are deployed for self-assembly or responsive materials., This distinction in applications is by no means a strict one, but it has set an underlying trend for research over the past 15 years.

Role of Water in Nanocellulose Production

There is no doubt that water plays an important role in the production of nanocellulose, particularly in the hydrolysis reaction utilized to isolate CNCs (discussed in detail in section 2.3.2.2). However, even when not directly involved in chemical reactions of nanocellulose production, the presence of water is pivotal. Figure 4 summarizes the role of water in nanocellulose preparation.

Cellulose Hydrolysis

Hydrolysis is a chemical reaction of a substance with water, leading to the decomposition of both the substance and water. The isolation of CNCs typically occurs through a controlled hydrolysis reaction in which the β-1,4-glycosidic bonds in the disordered regions of the microfibril are cleaved by the addition of a water molecule (Figure 4a). Therefore, all CNC production routes rely on the presence of water as a reagent. Ultimately, as a result of hydrolysis of cellulose, glucose is released in a process called saccharification. However, under ambient conditions, this is a very slow reaction, and it is not applicable for practical purposes. The hydrolysis of cellulose can be expedited via different catalysts such as acids and bases, enzymes, or by using subcritical and supercritical water as a reaction medium. While the hydrolysis in subcritical and near critical conditions of water has been rarely used for the isolation of CNFs,, it has been more actively demonstrated in the production of CNCs. For example, the use of subcritical water (120 °C and 20.3 MPa for 60 min) allows higher diffusion, activity, and ionization of water but leads to relatively low yields of CNCs (around 20%)., Also, in a recent study, supercritical carbon dioxide and enzymes were studied to hydrolyze the disordered regions of the cellulose microfibrils to produce CNCs. As mentioned earlier, the most common method to isolate CNCs is through an acid catalyzed hydrolysis using concentrated aqueous mineral acids such as sulfuric acid, phosphoric acid, and hydrochloric acid to yield charged or uncharged CNCs (such as the case for HCl hydrolyzed CNC). Recently, Pääkkönen et al. reported the production of carboxylated CNCs via HCl gas hydrolysis, followed by a TEMPO-mediated oxidation, leading to lower acid consumption and more effortless process steps toward easier CNC purifications., The use of HCl gas to produce CNCs from cellulose fibers relies on the water naturally present on the cellulose surface: water is able to dissociate the HCl and carry out the acid hydrolysis., In addition, solid acid catalysts (such as carbon catalysts with weakly acidic groups, polymer-based acids, magnetic solid acids, and lignin-based catalysts) have been used.− Bronsted acid active sites on the solid catalysts offer advantages such as selective cellulose hydrolysis, long catalyst lifetime, reusability, reduction of acid pollutants, and reduction of the cost of wastewater treatment. However, the contact between the active sites and cellulose remains a challenge because both reactant and catalyst are present in solid phase. The role of water as the reaction medium is crucial to improve the accessibility of catalyst to cellulose. Additionally, water can act as a catalyst for a autohydrolysis process, as hydronium ions (H3O+) formed on the surface of catalyst further promote cellulose hydrolysis.− Despite the multiple reports on gas or solid based methods to hydrolyze cellulose into nanocellulose, these processes remain to be less common in comparison to liquid acid hydrolysis.

In acid catalyzed hydrolysis, the reaction mechanism involves the activation of the glycosidic oxygen by protonation before water addition, and the rate of hydrolysis is dependent on both the acid concentration (i.e., fraction of water) and the temperature. At very high acid concentrations and temperatures, cellulose undergoes complete degradation into singular sugars. Therefore, for the purposes of implementing acid catalyzed hydrolysis in CNC production, reaction conditions must be strictly controlled. Both the temperature and acid concentration must be sufficiently high to cleave the glycosidic bonds in the disordered regions of the microfibril in a timely manner but low enough to keep the crystalline regions intact (Figure 3b). In the conventional sulfuric acid hydrolysis to produce CNCs, the concentration is generally set to 64–65 wt %, which is fairly close to the value where total hydrolysis/dissolution of crystalline cellulose occurs (72 wt %). Here, the water content is very low because of the formation of oxonium ions, and this is integral for enabling the esterification of sulfate groups which must take place in order to ensure the necessary colloidal stability of CNCs. Furthermore, it is important to note that during the acid hydrolysis of cellulose there exists a competition between the dehydration of cellulose (i.e., cleaving of the glycosidic bonds) and the dissolution of lower DP sugars resulting from the hydrolysis.,−

While the use of enzymes has been reported for the isolation of CNCs, they are typically implemented in the pretreatment of cellulosic substrates prior to high shear mechanical treatments. Hydrolysis of the cellulosic substrates through enzymatic hydrolysis significantly decreases the amount of energy required to mechanically isolate individual cellulose microfibrils from cellulose fibers. In nature, the degradation of cellulose is accelerated by more than 17 orders of magnitude by cellulases, which include a variety of enzymes called glycoside hydrolases (or glycosidases) that catalyze the hydrolysis of the β-1,4-glycosidic bonds of cellulose. Enzymatic hydrolysis involves complex interactions between enzyme, cellulose, and the reaction environment, and although the complete mechanism of action of the above-mentioned enzymes is still unknown it has been shown that enzyme folds and crevices are formed in water into which the substrates fit. Different cellulases will catalyze the hydrolysis at different locations along the cellulose polymer chain, and all of these enzymes act synergistically in order to fully degrade cellulose to glucose for the production of biofuels, for example. In the production of CNFs, however, the enzymatic activity of cellulases is carefully controlled to minimize undesired cellulose degradation. Furthermore, the isolation of CNFs is often aided by the introduction of enzymes such as xylanases, laccases, and lytic polysaccharide monooxygenases, which have an affinity for the glycosidic bonds in other polysaccharides (hemicelluloses in particular).−

Water as a Medium in Nanocellulose Production

Cellulose and cellulosic fibers are insoluble and relatively inert in water under ambient conditions. Nonetheless, the hygroscopic nature of cellulose enables the swelling of cellulose fibers as a result of water sorption, which is key in the production of CNFs. Water-induced swelling of cellulosic fibers “opens” their structure (Figure 4b), increasing their accessibility, and in turn facilitates the penetration of chemical reagents and activity of enzymes (Figure 4c) during the pretreatment stages of CNF production. Additionally, these pretreatment methods often rely heavily on the water present to act as the reaction medium (e.g., in the case of TEMPO-mediated (Figure 4d) or enzymatic oxidation). Pretreatment methods such as swelling or partial dissolution in ionic liquids or deep eutectic solvents (DES) are also heavily dependent on water, further highlighting its importance in the many possible routes available for nanocellulose production.− It is important to note that even in production methods where water does not play an active role in the breakdown of the cellulose structure to the nanoscale (e.g., nanocellulose production through oxidation using an electron beam), water is omnipresent in the purification, workup (e.g., alkaline treatment, sonication, and high-pressure homogenization), and often storage stages of nanocellulose production.−

Nanocellulose–Water Systems: Properties and Dynamics

Before introducing the interactions between water and nanocellulose specifically, it is important to highlight the distinction between the swelling of cellulosic (plant-based) fibers and nanocellulose networks in water. In nature, the geometrical constraints of the cell wall set by their hierarchical structure, especially with rigorous microfibril alignment in the secondary wall, greatly restrict the swelling capacity of fibers. As already stated, swelling in water is highly anisotropic for fibers, as the volume increase occurs solely in the lateral dimension. The isotropic nature of most nanocellulose networks, together with the significant increase in specific surface area (SSA), leads to a much higher water sorption capacity per mass of cellulose. In conjunction with this increase in SSA comes an increase in the accessibility of surface hydroxy groups which can easily interact with water. Furthermore, any charged groups introduced to the surface of the nanocellulose during isolation will also alter its ability to interact with water. Phenomenologically, the nanocellulose–water interaction involves multiple overlapping phenomena such as hydration, condensation, wetting, and diffusion, which are all mediated by various interaction forces including hydrogen bonding, electrostatic interactions, and van der Waals forces. These processes unfold along different length scales, which ultimately gives nanocellulose its extraordinary hygroscopic character.

Accessibility of Cellulose Chains to Water

The accessibility of cellulose chains to water is governed by the availability of hydroxy groups on the surface of a cellulose crystal. While cellulose–cellulose hydrogen bonds often take precedence over cellulose–water hydrogen bonds (hence the insolubility of cellulose in water), there is also an abundance of hydroxy groups on the crystallite surface that have the propensity to hydrogen bond with water. A common method by which to quantify the availability of hydroxy groups in cellulosic materials is to substitute the hydrogen in available hydroxy groups for deuterium through a water/deuterium oxide (H–D) solvent exchange. The availability of hydroxy groups for solvent exchange is dependent on a number of factors: (i) their position in the cellulose chain (i.e., 2-, 3-, or 6-position), (ii) whether they are within the ordered or disordered region of the cellulose microfibril, and (iii) whether they are located on the surface or embedded within the crystallite (microfibril). The hydrogen atoms in the HO(2) and HO(6) hydroxy groups can act as hydrogen-bond donors to water, but the HO(3) behaves as a hydrogen-bond acceptor from water and donor to their intrachain neighbors O(5) (see, Figure 1). The accessibility of these hydroxy groups on the surface of cellulose crystals correlates with the H–D exchange behavior. For a specific hydroxy group to be available for the H–D exchange, it must be able to donate a hydrogen atom via hydrogen bond to a water molecule. For this reason, the HO(3) does not participate in the H–D exchange. Indeed, the HO(2) and HO(6) are more prone to moisture absorption, while the HO(3) has a lower accessibility, given the fact that the intramolecular hydrogen bond with O(5) has a predominant role in stabilizing the cellulose structure. In addition to the molecular position of each hydroxy group, the crystalline structure of cellulose plays a crucial role in the cellulose–water interactions (and therefore −OH group accessibility). On the crystallite itself, water accessibility is also based on the geometrical requirements of the available hydroxy groups of the cellulose that come into contact with water molecules.

The degree of crystallinity of the cellulose substrate plays a role in extreme cases: the accessibility of hydroxy groups in amorphous cellulose (as measured through deuteration using dynamic vapor sorption (DVS)) is estimated to be 63%, whereas the equivalent accessibility for microcrystalline cellulose is 51%, indicating that a higher crystallinity leads to lower −OH group accessibility. Similarly, multiple works in the literature correlate the difference in water uptake capacity of CNFs and CNCs to the difference in their degree of crystallinity and (supposedly) consequent hydroxy group accessibility., As mentioned earlier, CNFs are isolated cellulose microfibrils which exhibit the semicrystalline structure, whereas CNCs represent the crystalline portion of the cellulose microfibril. As such, it has been speculated that the more frequent presence of the disordered region leads to a higher water uptake capacity in CNFs than CNCs., Yet there is no evidence of increased swelling due to an increased number of disordered regions in microfibrils, although (as already mentioned) data published by Nishiyama et al. showed the hydrogen atoms in the hydroxy groups of the disordered domains were in fact susceptible to deuteration. It is also evident that water interacts solely with the surface of CNCs and is unable to penetrate (at least to any significant degree) into the crystal structure,, and deuteration is indicative of the number of available surface hydroxy groups, unless substantial temperature and pressure is applied.

Instead of the disputed role of the crystallinity index, the hydroxy group availability in native cellulosic structures is rather governed by the size of the cellulose crystallite, as shown by Driemeier and Bragatto in their seminal work on microcrystalline cellulose with varying crystallite widths. Also, the amount of residual hemicellulose plays a marked role in general water uptake and must not be confused with hydroxy group accessibility in cellulose per se. Particularly with CNFs, hemicellulose is often intentionally left in the structure because it facilitates the separation of microfibrils from one another. Another factor in accessibility with water is the imperfect packing of aggregated crystallites that may allow a concentration of water molecules in voids created by the phenomenon. Therefore, when examining the differences in hydroxy group availability and subsequent water uptake capacity, it is important to also consider differences in morphology, chemical composition, and flexibility. We will discuss the difference in water uptake capacity of assemblies of different nanocelluloses in section 2.4.1.2.

The accessibility of cellulose to water may also be governed by its polymorphism. Some studies have indicated that nanocelluloses of cellulose II have higher water sorption capacity than those with a cellulose I crystal structure due to the possible changes in the crystallite dimensions and the decrease in overall crystallinity as a result of the mercerization process used to convert cellulose I to cellulose II., Therefore, unlike cellulose I that has small disordered regions that cannot generally be regarded as fully “amorphous”, cellulose II has been speculated to exhibit genuine crystalline–amorphous transition, akin to many synthetic polymers.

Water uptake is also substantially influenced by the number of charged groups in the cellulose matrix because they directly contribute to the osmotic pressure. Intrinsically linked to the osmotic pressure, the induced electrostatic forces direct the water molecules and determine much of the texture of the nanocellulose matrix, as governed by the Derjaguin–Landau–Verwey–Overbeek (DLVO) theory The counterion on the charged group also has a pronounced impact. For example, the sulfate half ester group’s counterion on CNCs directly affects the critical coagulation concentration following the Hofmeister series (N(CH3)4+ < NH4+ < Cs+ < Rb+ < K+ < Na+ < Li+), which also correlates with the interactions they have with water molecules.−

Wettability of Cellulose

The mundane definition of hydrophilic/hydrophobic character of a surface is to have the static water contact angle below or above 90°, respectively. Striving for higher thermodynamic accuracy, alternative takes on the issue have used Gibbs free energy of hydration (ΔGsl): van Oss, for example, proposed that hydrophobic compounds attract each other in water when their ΔGsl > −113 mJ m–2 and repel each other when ΔGsl < −113 mJ m–2. Moreover, factors such as surface roughness and morphology, porosity, and fouling all play an important role in the spreading of a liquid at the air/solid interface.

In addition to, and intrinsically linked to, the hydroxy group availability, native cellulose crystals are amphiphilic (as demonstrated in the cross-sectional schemes of the microfibril in Figure 1).− This amphiphilicity is present at molecular and supramolecular level of cellulose,− and it is governed by the structural and conformational order in addition to the roughness, purity, and porosity of the assembled nanocellulose structures. Cellulose can also undergo conformational changes to accommodate the surrounding medium., The distinction between hydrophilic and hydrophobic faces in the cellulose I crystallite is straightforward (Figure 1), but their behaviors are not. For example, molecular dynamic (MD) simulations have shown that the hydrophilic 110 face, which is the most represented in the external morphology of the native fibers, possesses a water contact angle of 43°, while the other hydrophobic 100 face shows a contact angle of 95°.

As a side note, the noncellulosic materials adsorbed on the surface of cellulose can change the surface characteristics. Dried CNFs have been reported to accumulate a layer of noncellulosic material on the surface, which renders them less reactive than one might expect of a material rich in hydroxy groups. As a conclusion, it is fair to define nanocellulose as a family of cellulosic materials with amphiphilic nature, whereby the free energy of hydration depends on morphological factors on all length scales.

Materials with similar surface energies are inherently compatible, suggesting that understanding the surface energies of both water and nanocelluloses can give us a rough picture of their potential interactions. Surface energy can be divided into a dispersive (i.e., hydrophobic) and a polar (i.e., hydrophilic) component, the former describing the ability of a surface to participate in long-range London type nonpolar interactions and the latter in short-range “polar” interactions. In the case of liquids interacting with surfaces of differing surface energies, one can discuss their interfacial compatibility in terms of wettability (or the ability of water to spread over a surface). A surface can be considered wettable when its θ with a liquid is between 0° and 90° and not wettable at θ above 90°. We will discuss the water sorption capacity (or wettability) of nanocellulose assemblies in sections 2.4.2.4, 4.1.1, and 4.2.2. Simply put, the wettability and the water retention of nanocellulose assemblies is highly dependent on their overall crystallinity, surface chemistry (i.e., charged, uncharged, or chemically modified), and purity of the nanocellulose along with the roughness, morphology, and porosity of its assemblies.

In section 2.4.1.1, we described the ambiguous role of crystallinity in the accessibility of hydroxy groups in cellulosic materials. One can imagine that on the nanoscale the wettability of crystalline cellulose with water is also dependent on its crystal structure and the subsequent degree of amphiphilicity. However, a comparison of the surface energies of nanocelluloses extracted from several plants did not reveal a significant difference (regardless of variability in crystallinity), most likely due to the analogous surface chemistries as a result of the similarity between the biological processes of cellulose production in nature. To provide the reader with an idea of the order of magnitude of the surface energy of cellulose, a few reported values are shown in Table 1.

In general, the total surface energy of cellulose is between 50 and 60 mN m–1 although the contribution of the dispersive and polar components can be significantly different, depending on the type of the cellulose in question.

It is evident that altering the surface chemistry of cellulose will have a significant impact on its interactions with water. The surface energies of nanocelluloses are highly tunable through a multitude of surface modification routes,,,,− which can render the material more hydrophilic or less hydrophilic. These modification pathways will be discussed in detail in section 2.1.

It should also be noted that nanocellulose structures can readily swell upon exposure to water. However, the dynamic changes caused by the wetting and consecutive drying of these structures may significantly alter the perceived surface energies of the nanocellulose surfaces.,,, For example, CNFs and CNCs dried through freeze-drying tend to have a lower surface energy than those dried by air-drying, spray-drying or supercritical-drying, which is linked to their different state of aggregation.

Water Insolubility and the Effect of Water on Cellulose Dissolution

Cellulose is insoluble in water and other conventional solvents, inorganic and organic alike. However, several solvent systems for cellulose include water as a central component. N-Methylmorpholine N-oxide (NMMO)/water, NaOH/water, and urea/NaOH/water are among the most commonly used water-containing cellulose solvents. Unusually rapid dissolution of cellulose has been reported in urea/LiOH/water and urea/NaOH/water, albeit at temperatures below 0 °C (Figure 5). The role of water in cellulose dissolution differs a great deal depending on the solvent. In NMMO, for example, a rather precise water content of 13.7 wt % is necessary to establish the monohydrate form of NMMO, necessary for dissolving cellulose. In many recipes for dissolving cellulose, water plays a role in swelling and improving the accessibility of the chains to the solvent. Chen et al. have studied the kinetics of the dissolution and swelling of different cellulose fibers in the ionic liquid 1-ethyl-3-methylimidazolium acetate ([EMIM][OAc]) and reported that the solvent power was modified from very good (neat ionic liquid) to moderate (with 5 wt % water) and weak (15 wt % water). They showed that while the rate of fiber dissolution in neat ionic liquid depends on fiber accessibility and solvent viscosity, the water-induced decrease in solvent power dominates the general fiber behavior. Furthermore, factors such as cellulose DP, degree of crystallinity, morphology, surface chemistry, degree of substitution, and the surface tension of the solvent all play a pivotal role in the solubility of cellulose. Because dissolution is not a prominent or often-utilized phenomenon with nanocellulose (it obviously destroys the nanoscale morphology), we shall not discuss it further. Several reviews discussing the mechanism of cellulose dissolution in various solvent systems are available in the literature.−

Network Formation and Viscoelastic Behavior

Nanocellulose dispersions form arrested phases (i.e., a state of kinetic arrest), in the case of CNFs even at very low solids contents. Different factors such as nanocellulose aspect ratio and flexibility, surface charge density, counterion of surface charge groups, along with ionic strength of the dispersion, contribute to critical concentration at which this phenomenon occurs.,− The formation of an arrested phase is driven by the decrease of nanocellulose mobility either by increasing the suspension concentration or by reducing the effects of electrostatic or steric repulsion between nanocellulose fibrils/crystals. In either case, once the nanocellulose suspension reaches a critical concentration, it will go through a transition from a dispersed liquid-like state to an arrested solid-like phase. Depending on the dominant interparticle forces, two kinds of ideal arrested phases exist. In a system dominated by electrostatic Coulomb repulsion (more specifically from electrostatic double-layer repulsion due to osmotic pressure), a decrease in the interparticle distance is hindered by so-called caging effects, which leads to the formation of a colloidal glass.,, When van der Waals attractive forces are the dominant forces, the increase in concentration leads to the formation of a gel characterized by a percolated network often with a given fractal dimension.,, In nanocellulose suspensions, both repulsive and attractive forces play a role. For dilute suspensions (i.e., volume fractions below 0.05 wt %), concentrating the nanocellulose suspension will lead to the formation of a mostly reversible colloidal glass with a threshold concentration that is inversely proportional to the aspect ratio of the nanocellulose. On the other hand, increasing the ionic strength of a dilute nanocellulose suspension will result in a screening of repulsive forces between nanocellulose fibrils/crystals and the suspension will transition into an irreversible gel. At higher solids content, the dynamics involving the formation of an arrested phase may be more complicated. For example, the colloidal interactions of carboxylated CNF suspensions with concentrations ranging between 0.5 and 4.9 wt % are dominated by electrostatic Coulomb repulsion in the lower range of concentrations and by van der Waals attraction forces in higher range.

The transition from a suspension to an arrested phase is quite different between CNF and CNC suspensions. Due to their rod-shaped structure and inflexibility, CNCs form a gel at relatively high concentrations. The critical gelation concentration of CNC suspensions is approximately 10 wt %. However, this is of course dependent on their aspect ratio, purity, ionic strength, and surface charge density. At critical concentrations below their gelation concentration, CNCs have a tendency to phase separate into a chiral nematic (anisotropic) phase in which the alignment of CNCs results in birefringence and an isotropic phase where the CNCs remain in suspension and repulsive electrostatic interactions dominate. In the case of CNFs, the formation of an anisotropic phase is hindered by the early onset of an arrested phase promoted by their tendency to form entanglements as a consequence of their higher aspect ratios and their flexibility. Nevertheless, CNFs can form anisotropic nematic phases under some conditions.,

“Types of Water” within Nanocellulose Networks

Water within a nanocellulose network exists either as free water, which fills any voids due to capillary forces, and bound water, which interacts with the cellulose at specific sorption sites. At this stage, it is important to make a clear distinction in terminology: any water that is taken up by a cellulosic matrix is absorbed. However, absorbed water does not necessary interact with the cellulose through molecular interactions. When an interaction between the cellulose and water does occur, water is said to adsorb on the cellulose. Another means by which to distinguish the nature of water within a cellulose matrix, is that bound (or adsorbed) water is water present at moisture contents far below capillary condensation (i.e., the saturation point), while free (or absorbed) water is the water present in the matrix far above capillary condensation (i.e., close to saturation) (Figure 6a). With many routine experimental methods, such as dynamic vapor sorption (DVS) or water retention value (WRV), it is difficult, if not impossible, to distinguish between absorbed and adsorbed water, and hence, the predominant term for quantified water uptake is often “water sorption”.

Interestingly, the properties of water within a nanocellulose network are highly dependent on whether the water is free (absorbed) or bound (adsorbed) (Figure 6b) based on the melting and freezing behavior of water within a nanocellulose network (as measured through differential scanning calorimetry (DSC) and explained in detail in section 4.2.5), water can be categorized as (i) free water, (ii) nonfreezing bound water, or (iii) freezing bound water., The thermal properties of free water are the same as pure water, while bound water shows lower transition temperatures due to its strong interaction with cellulose surfaces (primarily hydroxy groups) mediated by hydrogen bonding and the consequent restructuring of local water environments and nanoconfinement., Bulk water surrounding nanocellulose is distinguishable from free water, as it does not cause observable swelling in the cellulose matrix as in the case of free water.

It is possible to detect whether water bound to cellulose is freezing bound water (or surface bound water) or nonfreezing bound water (or confined bound water) depending on its mobility as measured through 2H NMR and 1H NMR. This classification is particularly interesting (explained in more detail in section 4.2.4), as it allows one to directly connect the properties of water with its distribution inside cellulosic matrices such as fibers and nanocellulose networks. The characteristics of these networks have a great effect on the physicochemical properties of nanocellulose derived materials and on the properties of sorbed water. Another way to distinguish different types of water is thermoporosimetry, also discussed in detail in section 4.2.

CNFs form percolated fractal networks due to the formation of arrested phases upon an increase in concentration during which the 3D network of nanofibers shrink, decreasing the packing space between CNFs and forming agglomerates. Alternatively, phenomena such as coagulation, cross-linking, or ion exchange can be used to promote the formation of CNF networks. At the fiber saturation point, all of the intra-agglomerate (CNF–CNF interface) and interagglomerate (agglomerate–agglomerate interface) pores are fully hydrated. At the interagglomerate level, the surface bound water is located at the surface of the nanofiber belonging to two different agglomerates, while at the intra-agglomerate level, the confined bound water is present at the nanofibers interface belonging to the same agglomerates. Upon increasing hydration, the surface bound water becomes gradually more and more mobile due to the high accessibility between cellulose agglomerates. In contrast, the confined bound water is only marginally influenced by the hydration level due to the lower accessibility within the agglomerates Due to these dynamics, the surface bound water also is sometimes called “movable or mobile bound water”, while the confined bound water as “fixed or immobile bound water”.

Water Sorption Dynamics

The dynamics of water sorption by nanocelluloses are highly dependent on whether the nanocellulose is exposed to water vapor or liquid water as the sorption of liquid water is governed by hydrostatic pressure and capillary forces, which are not present in the sorption of water vapor. Generally speaking, the degree of water vapor sorption by nanocellulose is significantly lower than its liquid counterpart.−

Nanocelluloses can uptake a significant amount of water due to their extremely high surface area to volume ratio and their abundance of accessible hydroxy groups. Furthermore, the swelling of nanocellulose networks exposes even more surface, resulting in a higher number of hydroxy groups available for water sorption. Because they are the primary sites of interaction for water on the nanocellulose surface, rate of sorption, and desorption of water in nanocelluloses has been associated with the accessibility of hydroxy groups. The accessibility is governed by factors such as surface charge content (and charge counterion), degree of aggregation, geometric constraints, porosity, crystallinity, and the thermal history of the nanocellulose (see also section 2.4.1.1).

A number of quartz crystal microbalance with dissipation (QCM-D) and surface plasmon resonance spectroscopy (SPR) studies have been carried out on CNC, and CNF− model films to understand the swelling of nanocellulose networks. The kinetics of CNC film swelling as a function of solvent ionic strength and CNC surface charge was evaluated in an SPR study by Reid et al., Interestingly, in this work, the total water uptake capacity of the CNC films was independent of both CNC surface charge and the ionic strength of the solvent, seemingly due to the restrictions on swelling capacity resulting from the presence of van der Waals forces. However, it was clear that the rate of swelling was greatly impacted by surface charge and ionic strength. Niinivaara et al. gained quantitatively similar results in a combined QCM and ellipsometry study on CNC thin films: apparently a 1 nm layer of water surrounds the CNCs at high (>90%) relative humidity values (Figure 6c). Similarly, other works have also demonstrated that the water sorption capacity of (nano)celluloses generally increases with increasing surface charge content, in addition to changes in charge counterion, ionic strength, and pH.,

Hakalahti et al. studied the water vapor absorption mechanism and dynamics into model carboxylated CNF films. They showed that below 10% relative humidity (RH) water vapor is adsorbed mainly onto the surface of CNFs through specific interaction (e.g., hydrogen bonding), whereas at humidity values between 10% and 75%, multilayers of water molecules were built up inside the CNF network following a Flory–Huggins model. When the RH exceeded 75%, the water vapor condensed in the CNF network via cluster formation, promoting the swelling of the thin film. During sorption, the water volume fraction increased from 0.21 at 75%RH to 0.59 at 97%RH.

The water vapor uptake capacity of CNFs is generally higher than CNCs due to the flexibility of the network, higher hydroxy group accessibility, and residual lignocellulosic components such as hemicellulose. At 95%RH, CNFs have at least 10% more moisture than CNCs. Because of their rigidity, CNCs do not form entangled networks such as CNFs. Comparing celluloses I and II, cellulose II has higher uptake due to the difference in crystallinity, texture, and overall morphology of the samples.

Mass Transport

The mass transport of liquid water in porous cellulosic materials occurs as a result of capillary flow (or wicking), which is often modeled using eq 1 as established independently by both Richard Lucas and Edward W. Washburn, which provides information on how liquids move through porous media and can be used to characterize the surface energies of powdered solids.,,where x is the distance traveled, γl is surface tension of the liquid (i.e., water), r is the radius of the (circular) flow channel, θ is the contact angle (assumed static) between the solid surface and the liquid (i.e., cellulose and water), η is the dynamic viscosity of the liquid (i.e., water), and t is time.

On the contrary, the mass transport of water vapor through porous materials proceeds via diffusion; for dense materials, a solution-diffusion mechanism is usually assumed. The diffusion driven mass transport of water vapor through porous materials is sensitive to changes in temperature and in relative humidity (and thereby partial pressure). As in the case of wetting and sorption, material properties such as thickness, crystallinity, hydrophilicity, along with porosity, and pore size and structure, all influence the rate of mass transport and are all applicable to materials such as nanocelluloses.

As most assembled nanocellulosic structures are porous, the relevant phenomena for water vapor transport through nanocellulose materials are Fickian diffusion, Knudsen diffusion, and surface diffusion. Fickian diffusion refers to classic diffusion governed by local differences in chemical potential, where the interactions between the diffusing molecule and the solid material are insignificant (i.e., when the porosity is high and pore size is large). Knudsen diffusion, on the other hand, occurs when the pore size of the solid material is comparable to or smaller than the mean free path of the diffusing molecule, leading to significant interactions between the vapor and the solid. Surface diffusion, on the other hand, occurs when molecules are mostly adsorbed on a surface, only to jump to the next adsorption site. All of these mechanisms may be found in water vapor mass transport across cellulosic materials and nanocelluloses, depending on their porosity, pore size, and surface energy. While some efforts have been made to model the observed water vapor transport of various cellulosic materials by these mechanisms, most of the literature on the uptake of water vapor by cellulose does not offer a full theoretical explanation to the experimentally observed behavior.,,

Dewatering of Nanocellulose

Recently, Sinquefield et al. published an exhaustive review on the dewatering and drying of nanocellulose. Maintaining the nanoscale properties of nanocelluloses upon dewatering/drying represents a distinct challenge, given the structural changes and irreversible aggregation which occur during the process. The most common dewatering procedures used for nanocelluloses include centrifugation, pressing,, filtration,− shear stress induced dewatering,− and solvent exchange followed by solvent evaporation., More recently, Guccini et al. have used forward osmosis to reproducibly dewater CNFs suspensions into hydrogels with a solid content up to 12 wt %. Using this approach, they were able to retain the viscoelastic properties of the CNFs upon redispersion. After dewatering, a further drying stage is often required to bring nanocellulose to the dried state. The most common technologies used for drying are air and oven drying,,− freeze-drying,− supercritical CO2 drying,,,, and spray drying.,− Each of these drying techniques results in nanocellulose structures with different properties, such as thermal stability, degree of crystallinity, and char residue (upon heating or carbonization). For example, CNF films/aerogels prepared through supercritical drying have a lower stability and degree of crystallinity than those prepared by air drying or spray drying. As such, it is important to note that the drying history of nanocelluloses and nanocellulose-based materials must be carefully taken into consideration, given the influence of the drying method on their physicochemical properties.

Hornification is one of the main phenomena leading to the changes in nanocellulose materials upon drying, presumably by co-crystallization or irreversible binding of hydrophobic sites in the microfibril (see also section 2.2.2). Compared to fibers, hornification is exacerbated to a great deal in a nanocellulose networks because of the immense surface area of CNFs or CNCs. Nanocelluloses can be efficiently dried at temperatures below 100 °C under vacuum or by freeze-drying, but upon exposure to ambient conditions, atmospheric moisture will promptly be resorbed into the material., In fact, in ambient conditions, air-dried nanocelluloses contain between 2 and 5 wt % residual moisture. Hornification usually becomes dominant already at higher water contents, however, leading to a permanent decrease in hydroxy group accessibility. Additionally, nanocelluloses with surface moieties such as carboxyl and aldehyde groups may undergo chemical cross-linking under these conditions, further enhancing the effects of hornification. As a result, the dehydrated nanocelluloses are unable to be returned to their initial state upon rehydration.

The accessibility of the hydroxy groups in both redispersed CNCs and CNFs is reported to be reduced by ca. 84% and 82% upon drying, respectively. The structural collapse of nanocellulose during drying predominantly has negative effects on its redispersibility, chemical modification, and swelling ability. In the process of nanocellulose preparation, hornification of the source material plays a role as well. For example, pulp fibers subjected to hornification prior to TEMPO-mediated oxidation (in the isolation of CNFs) require higher energy and consume more chemicals in comparison to the never-dried pulp. In fibers, different strategies such as beating, addition of bulking agents such as sucrose and glycerol, or derivatization with spacers such as poly(ethylene glycol) (PEG) have been applied to prevent hornification. It is important to note that although the effects of hornification upon drying are usually significant, some sources of nanocellulose, such as Cladophora, show inherently lower extent of hornification., Due to the significant effect of hornification, it is common for nanocelluloses to be stored in their “never-dried” form in order to prevent any additional complications when utilizing these materials. Should nanocelluloses require drying, the effect of hornification (and as such the potential to redisperse the dried material in water) can be limited through the addition of salt or the exchange of counterion on surface charge groups (e.g., replace H+ counterion with Na+), which hinders the formation of new cellulose–cellulose bonding during drying.

Nanocellulose Dispersions

Nanocellulose can be colloidally stable in water but only with a sufficient amount of surface charge, as the inherent attraction between the nanoparticles affects dispersion stability. If nanocellulosic particles do not have sufficient surface charge, a material with dispersion properties comparable to cellulosic powders and macrofibers is created due to aggregation. This is similar to the conventional pulp suspensions and have been discussed in the session of aqueous fiber suspensions in a conference proceeding in 1977. The intermolecular hydrogen bonding between the surface hydroxy groups as well as van der Waals bonding between the hydrophobic sites in nanocellulose play a role in aggregation in many media, such as organic solvents, polymer matrices, and even water. Physical thinning, ultrasonic dispersion, and high-pressure homogenization can weaken these hydrogen bonds and are methods used to facilitate the (re)dispersion of nanocellulose. Introduction of surface charge or long chain molecules to increase either the electrostatic repulsion or steric hindrance between nanocellulose particles have also been used to improve dispersion. In all cases, dispersion of nanocellulose in water requires high energy input (e.g., sonication, microfluidization, high pressure homogenization) to either liberate individual nano-objects during production or redisperse prepared nanocellulose from concentrated/dried forms (Figure 5).

Electrostatic Repulsion

The surface charge density and electrostatic repulsion are important factors influencing the dispersibility of nanocellulose in water, which are affected by the environmental conditions, such as pH, temperature, and salt concentration in aqueous media., Stable nanocellulose dispersions in water can generally be obtained when the absolute value of zeta potential is higher than 30 mV., Sulfate half ester,− sulfonate,, carboxyl,− phosphate half ester,,,− phosphonate, quaternary amine,− and amino functionalities have been used to introduce ionic groups onto the surface and thereby improve the dispersion. The neutral sodium-form of CNCs dried by evaporation, lyophilization, or spray-drying is more easily redispersed in comparison to CNCs in acid form. Monovalent salts in the medium can improve the dispersion through hydrogen bond blocking between hydroxy groups and reducing the aggregation of CNFs and can also potentially help to regenerate hydrogen bonds between water and nanocellulose during the redispersion steps. It is important to bear in mind that the presence of divalent cationic charge in the medium, will result in cross-linking and more aggregation for the nanocelluloses with anionic charge on the surface (discussed more in section 3.3.1).

Water can play a secondary role in desulfation of sulfate half ester groups on the surface of sulfuric acid hydrolyzed CNCs that leads to destabilization and aggregation., Desulfation happens fairly rapidly by acid- or alkaline-catalyzed de-esterification in water. Auto-catalyzed desulfation in acid form CNC suspensions occurs slowly at ambient conditions and fast at higher temperatures and results in loss of surface charge, in addition to aggregation, desulfation has been shown to affect thermal stability, liquid crystal properties, and rheological behavior. Dried solid acid form sulfated CNCs also undergo rapid desulfation in contact with the humidity in air, in which water acts as a medium for de-esterification reaction.

Steric Stability

Neutral polymers can be immobilized on the surface of nanocellulose and expand in the medium to gain configurational entropy. As the grafted polymer layers overlap, steric or entropic repulsion between nanocellulose particles is generated. The length of grafted polymers plays an important role in the stability of the dispersion of nanocellulose in water. The common strategies for polymer induced steric repulsion are grafting PEG chains onto the cellulose surface, silylation of the surface, polymerization from the cellulose surface (e.g., surface-initiated electron transfer atom transfer radical polymerization or SI-ATRP), and adsorption of a polymeric surfactant for nonaqueous dispersions.,− Araki et al. covalently conjugated aminated PEG to carboxylated CNCs and the dispersion of the resulting PEG-grafted CNCs in NaCl solution remained stable. After freeze-drying, these PEG-grafted CNCs could be redispersed in water and chloroform easily. Interestingly, these PEG-grafted CNCs were also used as dispersants for fluorescent probes within cells. Similarly, poly(ethylene oxide) (PEO) grafted CNCs were dispersed stably in water for several months without precipitation., Some plant-based nanocelluloses disperse well in water even after oven drying due to residual pectins on the surface. The molecular weight and content of pectin control its inhibiting effect on the aggregation of CNFs during drying process. Attaching surfactants such as cetyltrimethylammonium bromide (CTAB) onto uncharged (and colloidally unstable) CNC via electrostatic adsorption has been shown to improve their dispersibility in water.

Controlling Aqueous Nanocellulose Dispersion Stability by Surface Modification and Blending with Responsive Polymers

When responsive polymers are grafted onto the surface of nanocelluloses, the dispersion stability in water can be controlled by changing environmental conditions. Thermoresposive polymers such as poly(2-hydroxyethyl methacrylate) (PHEMA) or poly(N-isopropylacrylamide) (PNIPAM) have been grafted onto or from nanocellulose matrices to control the water response of these systems via temperature changes, while both thermoresponsive and polyelectrolyte brushes respond to changes in ionic strength. Yi et al. synthesized the first temperature-sensitive poly[2(dimethylamino)ethyl methacrylate] (PDMAEMA) grafted CNCs by ATRP. In lower temperatures than the critical temperature, the grafted PDMAEMA chains were in extended conformation, leading to a good dispersibility in water. At higher temperatures, water dispersibility decreased. Similar thermoresponsive CNCs grafted with poly(N-isopropylacrylamide) (PNIPAM) were reported by Zoppe et al. Higher ionic strength, graft ratio, and degree of polymerization decreased the dispersibility in water. Azzam et al. synthesized Jeffamine polyetheramine grafted CNCs, which dispersed well in water (and other media) due to the surface carboxyl groups and polymer brushes; furthermore, the dispersion stability could be tuned by ionic strength, pH, and temperature., Other examples of responsive polymer-grafted CNCs prepared by radical polymerization in water (i.e., not “controlled polymerization” reactions) include pH-responsive polyvinylpyridine and dual temperature and pH responsive PDMAEMA; a full review of polymer grafted CNCs, their functionalization routes, and behavior can be found elsewhere. Larsson et al. tuned the interaction between CNF and water by adsorbing charged, heat-responsive block copolymers onto the fibers. They observed the transition of dispersed modified CNFs in water to a macroscopically aggregated state by heating, during which the adsorbed block copolymer transitioned through a critical solution temperature.

Apart from surface modification, blending with different polymers can also be used to create novel forms of nanocellulose dispersions. Bai et al. have reported the formation of water-in-water liquid crystal emulsions of CNCs with permeable colloidal assemblies. They showed CNCs spontaneously self-assemble into a helical arrangement with the coexistence of nonionic, hydrophilic polyethylene glycol (PEG), and dextran. These two polymer solutions are thermodynamically immiscible. Stable water-in-water emulsions are easily prepared by mixing CNC/PEG and CNC/dextran solutions, where micrometric CNC/PEG form the dispersed droplets and CNC/dextran form the continuous phase. Over time, this emulsion breaks into an upper, droplet-lean isotropic phase and a bottom, droplet-rich cholesteric phase. Osmotic pressure gradient between PEG and dextran phases results in target transfer of CNCs across the water/water interface to reassemble into a liquid crystal-in-liquid crystal emulsion with global cholesteric organization. The authors observed that the colloidal particles in the two immiscible phases experience short-range interactions and form long-range assemblies across the interface.

Controlling Aqueous Nanocellulose Dispersion Properties by Drying

Water removal techniques have been applied as an “adjustment tool” in nanocellulose preparation with specific dispersion ability and stability in mind. As discussed earlier, redispersion in water and other solvents or polymeric blends is strongly affected by the drying method. In general, nanocellulose obtained by evaporation from aqueous suspensions is extremely difficult to redisperse, while freeze-dried sulfated CNCs and TOCNFs can be redispersed in water with a correctly chosen counterion.,− CNFs are less commonly dried due to their inherently entangled nature and lower charge, which leads to more difficulty in redispersing them. However, some successful drying processes and additive dispersants have been introduced for this purpose. Hu et al. reported that intrinsic adsorption of hemicellulose imparted a good redispersibility on mechanically defibrillated nanocellulose via good water accessibility of soluble hemicellulose to water comparing to that of cellulose. Foster et al. reported that the concentration of the CNC dispersion being dried influences redispersibility in water, lower concentrations lead to more redispersible dried materials. When redispersing CNCs in water from dried powders, low concentration suspensions are easiest to achieve, but if a high concentration is needed, it is best to prepare a dispersion below 2 wt % with sonication and then gradually add more CNCs with repeated sonication steps. It has also been shown that a combination of surface modification and drying techniques can be used to obtain materials with tailored dispersibility. For example, directly adding capping agents (such as specific counterions, polymers, and surfactants) prevents the agglomeration of CNFs during their dehydration (hornification) leading to CNFs with noteworthy dispersibility and colloidal stability.,

Nanocelluloses as Dispersing Agents

The ability of nanocellulose to partition at solid/liquid, liquid/liquid, and gas/liquid interfaces has opened up new avenues to control dispersions containing nanocellulose. Nanocellulose characteristics such as size, charge, and polymorph affect their surface properties, and their ability to stabilize interfaces and act as dispersants. While nanocelluloses are not strictly “surface active”, their amphiphilicity is governed by the crystalline polymorph and any surface modification. Besides, any colloidal particle has a tendency to enrich at interfaces by default. Pickering emulsions were one of the first applications of these findings with potential in the pharmaceutics/drug delivery, personal care, food, cosmetics, and porous materials, etc.,, Amphiphilic particles like nanocellulose can be wetted by both water and oil and are excellent stabilizers that are essentially irreversibly adsorbed at the oil/water interface and prevent droplet coalescence compared to typical molecular surfactants. Emulsions, and particularly high internal phase emulsions, allow for formulated products with significantly less water overall but the ability to process nanocellulose under favorable and predictable aqueous conditions. CNFs have a higher aspect ratio than CNCs and often have a higher adsorption capacity and wettability by oil, which could result in more stable emulsions. However, their entangled nature often leads them to act more as a rheological modifier in the continuous water phase than as a Pickering stabilizer. Latexes are an extension of emulsion systems because they are made by emulsion or suspension polymerization, they can also be greatly improved by nanocellulose incorporation, where the role of nanocellulose varies from being a monomer–water interface stabilizer, to a water phase additive, or even a polymer particle “seed” with either active or passive participation in the chemical reactions. Importantly, nanocelluloses can be used as dispersants to improve the interfacial compatibility and prevent the agglomeration/aggregation of other noncolloidally stable particles. Amphiphilic nanocellulose is associated with 2D nanomaterials via hydrophobic interactions efficiently, whereas the hydrophilic surfaces help to disperse nanocellulose-bound 2D nanosheet in aqueous media. Surface charges stabilize the nanocellulose-bound 2D nanomaterial dispersions in water through Coulomb repulsion, where nanocellulose–water interaction is vital. Nanocellulose has been intensively used as dispersing agent for 2D nanomaterials such as graphene− and MXenes, through intercalation. In aqueous environment exfoliation occurs via double electrostatic layers build up on 2D nanomaterials that can overcome the van der Waals interactions. Similarly, other nanoparticles, such as metal oxides,,, quantum dots, metal organic frameworks (MOFs), polymer nanofibers, and salt nanoparticles, have also been stabilized by nanocellulose to disperse them in water. Lastly, the unique templating ability of nanocellulose can be used to mediate the nucleation and growth of metal nanoparticles, inhibiting nanoparticle aggregation, improving their dispersion uniformity and stability, and in many cases, enhancing their catalytic or electrochemical function, as reviewed previously.,

Interestingly, Gonzales et al. rationalized that if a surfactant with high HLB (hydrophilic–lipophilic balance) is able to stabilize oil in water emulsions, then the same type of material could hinder the formation of water in oil emulsions. They used nanocellulose as an inhibitor (demulsifier) of water in crude oil emulsion formation, which is a challenge during crude oil extraction and processing.

Pathways to Tune Nanocellulose–Water Interactions

As discussed earlier a few times, cellulose is inherently amphiphilic,− and altering its surface energy is possible through a wide range of surface modification methods. Due to the natural affinity between cellulose and water, it is clear that water plays an important role in the modification of nanocellulosic surfaces. Although most covalent routes are based on organic reactions where water is usually detrimental, several synthetic approaches for nanocellulose modification can accommodate having water as a solvent.,,,− One of the main motivations to surface modify nanocellulose is to improve its compatibility with other materials. For example, the dissociation of charged sulfate half ester groups in water ensures the colloidal stability of CNCs, but if one wants to handle them in nonpolar solvents (which can then be used as further modification medium), they tend to aggregate. Similarly, while as-prepared nanocelluloses are inherently incompatible with many petroleum-based polymers, hydrophobized nanocelluloses may be more easily dispersed throughout a composite matrix. Additionally, the use and functionality of assembled nanocellulose structures may require a specific surface energy (e.g., hydrophobicity in nanocellulose aerogels designed for separating oil from water). In this chapter, we focus on surface modification methods which tune the amphiphilic nature of nanocelluloses, and we further go on to highlight the role of water in these modification procedures.

We re-emphasize that the distinction between hydrophilic/hydrophobic is oversimplified in the literature, particularly when defined by static contact angle measurements. Still, it is a definition that has stuck and is widely recognized and, as such, we feel that adhering to these terms has significance in the scientific community.

When considering surface modification of nanocellulose, it is not only the nature of the substituents being grafted but also the degree of substitution that influences the hydrophilicity/hydrophobicity. Furthermore, contact angle measurements are highly sensitive to surface roughness, which can be altered after surface modification such that interpretation of results is not always straightforward. In this context, Cunha et al. showed that for the esterification of nanocellulose with trifluoroacetic anhydride even a modest degree of substitution of 0.04 had a strong effect on the hydrophilicity of the surface, resulting in a static water contact angle of 126°. This demonstrates how small changes to the cellulosic surface may have large impacts on the wetting characteristics due to both chemistry and topography.

Decreasing Nanocellulose Surface Hydrophilicity

In this section, we focus on surface modification approaches that aim to decrease the hydrophilicity of nanocelluloses and the role of water in these reactions. This often-termed “hydrophobization” of nanocellulose leads to the disruption of the solvation of surface structures by water by capping the available hydroxy groups through the attachment of hydrophobic moieties,− grafted polymers,− or even nanoparticles.− Generally, the reasons to hydrophobize the surface of nanocellulose include increasing the hygromechanical stability (keeping good mechanical properties in the wet state), improving the compatibility with hydrophobic polymers or solvents or reducing the effects of hornification upon drying.,− The palette of the available modification pathways is very diverse, and a full review of these reactions is out of the scope of this paper. The reader is encouraged to follow the details of modification reactions in the previous publications on this topic.,,,,,,,,,,,,,, − However, a short overview of the most important routes to nanocellulose surface hydrophobization is covered here and summarized in Table 2.

Covalent Nanocellulose Hydrophobization

The formation of esters− and carbamates on the surface of nanocellulose usually requires anhydrous environments, which is facilitated by drying techniques or the use of nonaqueous reaction media, such as gas phase esterification.− The esterification of cellulose hydroxy groups with carboxylic acids, anhydrides, and acid derivates is arguably the most versatile tool for surface modification due to the variety of reaction pathways, including simple Fischer esterification, acid chloride or anhydride alcoholysis, and transesterification, which can be conducted in a liquid or gas phase, depending on the moiety to be attached. Polymer grafting through ring-opening polymerization or surface initiation for (controlled or not) radical polymerization on the surface via (trans)esterification have been also widely reported in the literature., Similarly, the grafting of isocyanates onto cellulose surfaces requires an anhydrous environment to avoid side reactions of the reactive electrophiles. The high reaction speed and yield of the addition reaction, the availability of isocyanates, and easy access to polyurethane grafting techniques add to the popularity of this approach. Etherification via thionyl chloride is also performed in nonaqueous environments, substituting the cellulose hydroxy groups with chloride. This activation facilitates subsequent substitutions, as the halogen is a better leaving group compared to hydroxy moieties. Eyley and Thielemans employed a chlorination approach on CNFs, followed by substitution of the chloride group with azide to obtain clickable cellulose moieties.

Some reactions for hydrophobization, such as silanization, can be carried out in both aqueous and anhydrous environments.,− Reactive chlorosilanes undergo hydrolysis in aqueous environments, therefore, they are used to silanize nanocellulose in anhydrous environments. These reagents are chosen for their high reactivity and therefore short reaction times when in contact with cellulose. However, the need for tedious solvent exchange procedures and the release of hydrogen chloride are drawbacks in the synthesis of silylated components by chlorosilanes.− Alternatively, corresponding alkoxysilanes can be used to obtain the same desired compounds. These reagents are not as sensitive to water but are less reactive, and therefore, reaction times are increased., While the deprotonated cellulose hydroxy groups act as nucleophiles in etherification reactions (explained in the next paragraph), auxiliaries can be employed to transform the cellulose component into an electrophile. Historically, this involved the use of thionyl chloride as explained previously. Alternatively, in etherification via employing tosyl chloride reactions, the hydroxy groups can be converted into tosylates, which in turn are better leaving groups than chlorides. While the tosylation of cellulose is usually carried out in a nonaqueous environment such as DMA/LiCl, the reaction can also be conducted in water. Guo et al. used tosylation on nanocellulose to prepare clickable cellulose azides.

Some other cellulose modification reactions are safe to be carried out in water. Etherification of surface hydroxy groups can easily be achieved by reacting cellulose with glycidylethers or chloro-compounds, most prominently chloroacetic acid, in a basic aqueous solution.− Basic media are needed to activate the surface hydroxy groups via deprotonation. The formed alkoxide species are sufficiently nucleophilic to add to epoxide moieties or to substitute halogens. The oxidation of nanocellulosic surfaces in aqueous media to aldehydes and acids (which initially increases the hydrophilicity of the surface and on its own will be discussed in section 3.1.2) followed by further functionalization is an important pathway to preparation of hydrophobized nanocellulose surfaces. As mentioned in the previous section, oxidation is also considered to be a very common step in the isolation of different types of nanocellulose, often ending up in carboxylate moieties on the surface.,− Nanocellulose surfaces containing carbonyl groups (such as in aldehydes and ketones) can be used as substrates for Schiff’s base reactions, including the attachment of amines,, while the carboxylic groups can further be modified through activated peptide coupling.− A variety of coupling agents have been developed over the past decades to facilitate peptide synthesis and can be used for this purpose in aqueous environments. An overview of covalent routes to nanocellulose modification are depicted in Figure 7.

Noncovalent Hydrophobization Routes

In addition to chemical pathways to decrease the hydrophilicity of the surface, physical interactions are other ways to hydrophobize nanocellulose surface in aqueous and nonaqueous systems. Physical surface hydrophobization (essentially adsorption or counterion exchange) can be achieved in a facile and cost-effective process without the need for complex or multiple chemical reactions. These physical routes usually preserve the nanocellulose crystallinity and morphology better, but they are weaker and more likely to be reversible, compared to chemical modification via covalent bonds. Often, nanocellulose surface modifications via physical interactions are based on electrostatic interactions or polymer adsorption.−

The simplest practical way to approach adsorption as a modification system is to use water-soluble polymers. For example, carboxylated CNFs and amphiphilic diblock copolymer poly(methyl methacrylate-b-acrylic acid) form a stable complex. Due to the hydrophobic poly(methyl methacrylate) block, the surface modified CNFs exhibit good dispersibility in different organic solvents including DMF, DMSO, ethanol, and methanol.

In addition to hydrophilic interactions, the charges on the surface of nanocelluloses can be employed to physically modify the surface. For example, the negative surface charge on CNCs prepared by sulfuric acid hydrolysis (i.e., sulfate half esters) and CNFs prepared via TEMPO-mediated oxidation (i.e., carboxyl groups) can interact with polyelectrolytes.,, Hydrophilic CNFs can be hydrophobized through the adsorption of octadecyl amine resulting in their dispersibility in solvents such as toluene, tetrahydrofuran, and isopropyl alcohol. However, this surface modification is unstable and will desorb over time. Esker et al. utilized the adsorption of hydrophobic polyelectrolytes (i.e., cationically derivatized hydrophobized dextran polyelectrolytes) to decrease the surface water on sulfated CNCs and expedite their dewatering kinetics. Using electrostatic interactions, block copolymers based on quaternized poly(2-(dimethylamino)ethyl methacrylate) and polycaprolactone can also be attached to anionic nanocellulose surfaces, resulting in a decrease in the surface energy of the cellulose surface. The benefit of modification pathways such as this is that they can be carried out in an aqueous environment.,− Yahia et al. used poly 1-[4-(bromomethyl)phenyl]-1,2,4-triazole to modify the surface of CNCs through electrostatic adsorption, which significantly altered their electrophoretic mobility and enabled their dispersion in acetone and acetonitrile. They even took the modification a step further by substituting the bromine with bis(trifluoromethane sulfonyl)imide, which resulted in nanocellulose complexes able to disperse in tetrahydrofuran and ethyl acetate.

A simple counterion exchange of the charged groups on nanocellulose surfaces can also be used to tune surface energy in order to decrease self-aggregation and improve compatibility with nonpolar solvents and hydrophobic polymers. In particular, substituting the counterion of CNCs with an imidazolium and phosphonium cation improves CNC compatibility with polymers such as epoxy and polystyrene and decreases their ability to interact with water; phosphonium ion exchanged CNCs absorbed 30% less water than the sulfate CNCs in their sodium form. In the case of CNFs, a mixed system of sodium and tetraethylammonium counterions has been used to control CNF film hydrophilicity. The oxygen and water vapor permeabilities of said films increased with an increase in the molar ratio of bulky tetraethylammonium counterions.

Physical adsorption of surfactants onto nanocellulose is another strategy to reduce the capacity for intermolecular hydrogen bonding. Common surfactants such as cetyltrimethylammonium bromide (CTAB), dimethyldidodecylammonium bromide (DDAB), and dimethyldihexadecylammonium have been demonstrated to stabilize nanocellulose dispersions in THF. Additionally, amphiphilic polymers, which contain both polar and nonpolar moieties, can interact with nanocellulose surface such that their polar end interacts with the nanocellulose and the nonpolar remains in solution. Additionally, nonionic surfactants, such as sorbitan monostearate, have been used to modify CNC surfaces to improve their dispersibility in organic solvents and prevent self-aggregation. The acid phosphate ester of ethoxylated nonylphenol surfactant (Beycostat A B09) was also reported to improve the dispersibility of CNCs in chloroform. Recently, Kontturi et al. presented a nanocellulose surface hydrophobization technique through the adsorption of hydrophobic polymers (e.g., polystyrene and poly(trifluoroethylene)) from aprotic solvents, resulting in nanopapers with water vapor uptake ability yet a strong repellency for liquid water, but this method is restricted to macroscopic substrates such as nanopaper and does not work for individual nanoparticles like CNFs and CNCs.

Carbohydrates and soluble cellulosic materials have also been used to tune the interactions of nanocellulose surfaces with water. Larsson et al., for example, altered the behavior of composite films of both CNFs and CNCs with water through the adsorption of water-soluble hydroxypropylmethylcellulose (HPMC), while numerous works have shown altered CNC–water interactions as a result of insoluble oligosaccharides precipitated onto the surface of nanocellulose.− Adsorption of water-soluble polysaccharides is indeed an often applied approach to alter the surface of (nano)cellulose, but in most cases it does not result in more hydrophobic surfaces. In fact, in many cases the surface becomes more hydrophilic through the attachment of polysaccharides, specifically methylcellulose, hydroxyethylcellulose, guars, carboxymethylcellulose, and hemicelluloses have been demonstrated.

Increasing Nanocellulose Surface Hydrophilicity

In this section, we focus on surface modification pathways to increase the hydrophilicity of nanocelluloses, and we highlight the role of water in these procedures. Despite the hygroscopic nature of cellulose, its amphiphilicity can hinder the use of nanocelluloses in applications where high levels of hydrophilicity are required, such as in the case of superabsorbents, for example. As with surface hydrophobozation methods, both covalent and noncovalent pathways can be implemented. Table 3 is a summary of the most important nanocellulose surface hydrophilization modification routes and the role of water in these procedures.

Covalent Nanocellulose Hydrophilization

The hydrophilicity of nanocelluloses can also be improved by grafting hydrophilic polymers (e.g., acrylate based superabsorbent polymers),,, although grafting hydrophilic polymers is less explored than grafting hydrophobic polymers. Kaldeus et al. reported an all-water-based procedure for “controlled” grafting of hydrophilic polymers from CNFs; polymers and copolymers of PEG, methyl ether methacrylate, and poly(methyl methacrylate) were synthesized by ATRP from the CNF surface in water. This was made possible through an amphiphilic macroinitiator that was electrostatically immobilized on the CNF surface, facilitating both hydrophobic and hydrophilic monomer polymerization in water. Here, the precise mapping of water interactions would be an important fundamental undertaking as the grafted nanocelluloses possess a corona that can hold rather vast amounts of bound water compared to pristine (or charged) CNFs and CNCs that have bound water primarily on their surfaces.

Noncovalent Nanocellulose Hydrophilization Routes

The most popular approach to increase the hydrophilic character of nanocellulose is to impart additional charge onto the surface. Nearly always, nanocellulose bears some degree of surface charge directly after production with a certain degree of tailoribility based on reaction conditions. With TEMPO-oxidation,,, and periodate oxidation, the surface charge can be varied by up to an order of magnitude, whereas sulfuric acid hydrolysis “harshness” can only affect the degree of sulfation within a relatively small window. In addition to mere hydrophilic character, subtle changes in charge caused by varying degrees of TEMPO-oxidation have been applied to control wetting and antifouling properties. However, it is important to bear in mind that surface charge makes the behavior of nanocellulose in water susceptible to ionic strength. The easiest way to suppress electrostatic interactions is to increase the ionic strength of a nanocellulose suspension and this will lead to nanoparticles aggregation and loss of colloidal stability according to the DLVO theory. Furthermore, the counterion on the nanocellulose surface charge group affects the water interactions and leads to different coagulation behavior in water and other solvents. Zhang et al. illustrated the effect of cosolvent choice (i.e., sodium salts of various anions) on the swelling behavior and thus the mechanical properties of polymeric hydrogels. While these principles also apply to cellulose, the overall ionic strength may lead to a screening of the surface charges and in turn to different levels of interaction between water and (aggregated) nanocelluloses.

Role of Water in Controlling Surface Modification Reactions

Unfortunately, the presence of water can be detrimental in some nanocellulose surface modification mechanisms, due to its incompatibility with the required chemical reagent or reaction. In these cases, it is crucially important to remove any residual water prior to initiating the modification of nanocellulose surfaces. An anhydrous chemical environment can be achieved through techniques such as solvent exchange, the subsequent use of molecular sieves, or drying by evaporation and diffusion. However, each of these techniques has its own inherent drawbacks. Drying solvents is tedious and requires working in conditions where contact with air (and ambient moisture) is strictly prevented by working with a vacuum line for example. Molecular sieves, on the other hand, can introduce impurities into the reaction medium, which can also inhibit the surface modification reactions of nanocellulose. There are also other methods for water removal prior to chemical modification, such as adding alkaline materials or exploiting ionic liquids while water is being removed. While solvent exchange is a fast and relatively easy method to remove water from nanocelluloses, residual water often remains in the system afterward. For surface modification techniques requiring anhydrous conditions, one would typically use fully dried nanocellulosic substrates, but it is important to recognize the effect of hornification (irreversible aggregation) on the efficiency of these chemical modifications.,, Indeed, many accounts utilize solvent exchange or extensive drying step to introduce nanocellulose into anhydrous media, perform reactions on the nanocellulose, and report a certain degree of substitution. However, they do not necessarily disclose the morphology of nanocellulose after the reactions. It may be that in some cases large swathes of, for example, CNC particles remain completely unmodified in larger aggregates that have accommodated all the substitutes on their surfaces. All in all, it appears that aqueous medium is the safest place to work on comprehensive modification of nanocellulose in a way that all nanoparticles are evenly modified.

Controlling Dispersion in Modification Reactions by Tuning the Water Content

Solvent-exchange often leaves behind a fraction of residual water in nanocellulose systems, which might be detrimental to some organic reactions, but minute amounts of water may under specific conditions play a positive role, for example, in CNC dispersion in organic media. Viet et al. found that a small amount of water is critical to colloidally stabilize sulfated CNCs in polar aprotic solvents such as DMSO and DMF. Freeze-dried CNCs with residual water contents of 6–8% were able to form stable and well dispersed suspensions. Yet further removal of moisture using molecular sieves resulted in the aggregation of the CNCs. Interestingly, when 0.1% w/v of water was reintroduced into mixture, a stable suspension reformed. The authors concluded that a small amount of water (<0.2% w/v) is indeed necessary for a colloidally stable dispersion. Belgacem et al. investigated the effect of residual water on the particle size of the CNC aggregates by dispersing CNCs in water and subsequently carrying out a solvent exchange with ethanol and acetone. When measured through dynamic light scattering, the apparent size of the solvent exchanged CNCs was ca. 300 nm, whereas dried CNCs redispersed directly into acetone had an apparent size of ca. 635 nm. They concluded that the interactions of residual water with CNCs were not totally lost during solvent exchange, leading to a more stable suspension in acetone. Chang et al. systematically investigated the influence of water on the redispersion of CNCs in DMF. CNCs with a residual moisture content of ca. 4% have the same hydrodynamic radius as the theoretical radius of monodispersed CNCs, indicating that the CNCs were completely dispersed in the DMF.

Controlling Modification Outcomes by Tuning Water Content

When macroscopic nanocellulose substrates, such as films or nanopapers, are subjected to modification, the role of water is ambiguous. The high swelling capacity of CNF networks in water means that under aqueous conditions, the whole network, including its interior, will be modified. The water-immersed modification can also impair the bonding in the network if the fiber–fiber bonds are cleaved and modified. By contrast, when utilizing nonswelling hydrophobic solvents, only the surface of the network will be modified, and the network bonding remains intact. In this realm, Kontturi et al. used aprotic solvents instead of water as medium to adsorb hydrophobic polymers on the surface of nanopapers in the study already quoted in relation to the adsorption-based methods in section 3.1.1.2. Due to the limitations to the ability of these solvents to swell the nanofibers, these nonporous nanopapers were hydrophobized only on their surface. This resulted in CNF nanopapers with tunable hydrophobicity on the surface, while their water vapor absorption capacity was demonstrated to be similar to the pristine, untreated nanopapers. The strong mechanical properties, based partially on the hydrogen bonding between the CNFs have been retained, while the vapor transmission of the surface-hydrophobized nanopapers may be useful in applications such as textiles or building insulations.

Sometimes water is not a good solvent for one of the reagents in a cellulose modification reaction, and in these cases, although water does not interfere with the reaction per se, the concentration of the reagent in water is too low, and this prevents the reaction to proceed to completion. Odabas et al. cationized bleached kraft pulp in systems with different water-miscible organic solvents. Replacing 90% of the water with 2-propanol and particularly with tetrahydrofuran yielded higher degrees of substitution and increased reaction efficiency. The degree of substitution depends on the concentration of the cationization reagent in the reaction medium. Replacing most of water with tetrahydrofuran resulted in a higher concentration while maintaining supramolecular properties such as crystallinity and polymer chain integrity. Although this particular study has been done on pulp fibers, the concept is likely applicable to all cellulosic materials, including different nanocellulose types.

When working with nanocellulose suspensions in water (or other solvents), there is a strong effect of concentration on viscosity and potential flow alignment.− Unless a controlled environment is maintained around the sample, water evaporation can occur during the course of the modification reactions and significantly change the concentrations, viscosity, and alignment due to flow. Water evaporation can (and should) be reduced by implementing a closed or reflux system during surface modification reactions.

Nanocellulose–Water Interactions in Materials Applications

The following subchapters highlight the connection between water interactions and nanocellulose material applications, providing an overview of where water can be a benefit or detriment. Moreover, we discuss different synthetic and technical approaches toward tailoring the water response in nanocellulose-based materials for certain applications. Depending on the production and processing methods, different morphologies and hybrid systems containing nanocellulose can be obtained, e.g., colloids and emulsions, hydrogels, films and membranes, aerogels and foams, and nanofillers, which offer a range of properties useful across various fields (Figure 8).

The overview on nanocellulose applications is not exhaustive. Rather, we aim at exploring how water interactions are influencing the functionality of the materials described by focusing on relevant examples on a certain class of applications where nanocellulose has been used as an integral component. For the readers interested in exhaustive treatises, substantial review articles have been published, and we refer to those reviews with each relevant topic throughout this chapter. Table 4 summarizes the water related applications of nanocellulose in different forms (dispersion, hydrogel, film, aerogel, and powder) and important properties of each form for the mentioned application.

Hydrogels

CNFs, including BC, inherently form weak, physical hydrogels via hydrogelation at low concentrations (0.5–1.5 wt %) owing to their flexibility and ability to entangle.,, In contrast to CNFs and BCs, the rod-like CNCs have a limited ability to entangle. Nevertheless, as described in section 1, CNC aqueous suspensions transition from liquid crystalline to birefringent viscoelastic phases at elevated concentrations., Altogether hydrogels are a widely reviewed,,, class of nanocellulose-based materials. A recent review by Ajdary et al., in particular, gives a comprehensive view on nanocellulose-based hydrogels, inspired by nature toward advanced applications.Figure 9 illustrates the overview of water interactions in hydrogels, their tuning, and their effect on different applications. As explained earlier, the ability of nanocellulosic hydrogels to bind and retain water is a direct result of the nanocellulose surface chemistry, aspect ratio, and flexibility, as well as of the 3D network microscopic and macroscopic structure. Water–network interactions and swelling are therefore related to processes on the molecular (hydration) and supramolecular (wetting, capillarity, and diffusion) level. However, excessive amounts of water can result in structural disintegration over time, especially in the presence of mechanical stress.,− The water ratio impacts the behavior of nanocellulose gels under mechanical stress and makes the prediction of this behavior difficult. Many of the nanocellulose hydrogels are formed physically by ionic interactions or physical cross-linking, which become weaker and eventually might fail with increased water content., Covalent cross-linking is the main strategy to minimize the detrimental effects of excessive water on hydrogel structural integrity (Figure 10a). The cross-linked hydrogels swell in excessive water and might change their shape, but normally these changes are less apparent than non-cross-linked hydrogels and the material usually shows better mechanical properties over time and under stress.− Hydrogels of CNFs prepared by TEMPO-mediated oxidation have a hierarchical porosity in wet state in the meso- and macroporous range depending on their solid content. Subsequently, their mechanical properties and the characteristics of water within the nanofiber network depend on their hierarchical porosity.

Tuning Hydrogel Behavior through Water Interactions

Surface modification/functionalization,, and/or cross-linking,, have been widely used to tune the gelation behavior of nanocellulose and the network properties of their hydrogels. CNCs, for instance, form physically cross-linked nanofibrillar hydrogel networks in the presence of metal salts, with a sol–gel transition appearing at CNC concentrations far below (e.g., with 50 mM Ca2+ at 2 wt % CNC) the range of pristine CNCs. In the case of CNFs, cation cross-linking has been used to tune the mechanical properties of the hydrogels, i.e., via charge screening of the repulsive charges on the negatively charged nanofibril surfaces. Hydrogels made of hydrophobized cellulose have also been reported in an attempt to tune the hydrogel properties. Nigmatullin et al. synthesized CNCs that bind to each other through associative hydrophobic interactions. In this process, the sulfated CNCs were modified with hydrophobic moieties such as octyl groups. These octyl-CNCs form significantly stronger gels at lower concentrations than parent CNCs. Atomic force microscopy (AFM) studies revealed favorable interactions between remnant starch and octyl-CNCs, which is thought to be the source of the dramatic increase in gel strength. They also harnessed these hydrophobic interactions to assemble water-soluble macromolecules and nanoparticles into a transient hybrid network, forming thermosensitive hydrogels with tunable rheological properties.

Matrices and Carriers for Biological and Pharmaceutical Entities

As explained in section 1, water holds its pronounced role of being favorably involved in cellulose functions in nature along the dimensional hierarchy from macroplant down to nanofibers. Water is of paramount importance for the bioactivity in plant cell wall and plant growth. The physiological and biomechanical properties of lignocellulose are strongly influenced by the interaction of water with the biopolymer components within cell wall ultrastructure.− Similar nanocellulose–water interactions, for example, freezing bound water mediated between the biopolymer matrix, and the surrounding water, contribute to the biocompatible functionality in several applications of nanocellulose outside their natural occurrence.,

As a result, nanocellulose has been applied in biomedical fields, such as drug delivery and tissue engineering (Figure 10a,b).,,− In particular, nanocellulose-based hydrogels have attracted enormous interests to be utilized as a biocompatible substrate via different engineering technologies due to structural similarity with collagen., A large category of these systems are the hybrid hydrogels of nanocellulose and hydrophilic natural polymers such as hemicelluloses,− pectins,− lignin,,− chitosan,− alginate,,,− and gelatin.,− Whereas CNCs have been mostly used in hybrid hydrogels (Figure 10b), CNFs find wide-reaching applications as single-component systems, especially in the biomedical realm covering cell cultures, drug release, tissue engineering, and wound healing., Their high water content is an essential prerequisite for biocompatibility, and their nanostructure, porosity, and tunable mechanical properties can offer a biomimetic environment for cell immobilization and cell support., Moreover, network flexibility, porosity, and water content enable diffusivity, i.e., the uptake, transport, and release of low- and high-molecular-weight compounds, as exploited in controlled drug delivery (Figure 10.−

Besides hybrid hydrogels and single-component bulk CNF hydrogels, membranes, films, and microbeads based on swollen CNF networks, that is, somewhat geometrically constrained hydrogels, have been investigated in this context. For example, the effects of nanocellulose charge density and fibril size on the mechanical properties of the films in liquids were investigated. Swelling behavior of the films was studied in deionized water, in complete cell culture medium (DMEM), and in CaCl2 solutions. Cell culture media and CaCl2 solutions reduced the swelling of the films observed in deionized water, most probably due to a bridging effect (physical cross-linking) by the calcium ions. The reduction was proportional to the charge of the nanocellulose. The possibility to tune the softness of a surface by the level of oxidation can potentially be a way to influence cell behavior through mechanical cues. An emerging application of CNF-based hydrogels is support for microalgae with the aim of creating the next generation of solid-state photosynthetic cell factories. The combination of transparency, hydrophilicity and water retention, biocompatibility, good mechanical properties, and appropriate porosity ensures better performance than the alginates traditionally used as substrate., Furthermore, controlling water content and thereby binding of water on nanocellulose enables the manipulation of the diffusion of components within the hydrogel. This permits the regulation of diffusion of the photosynthetic products inside and out of the cell factory matrix.

Anisotropic, Responsive, and Smart Materials

The specific response of nanocellulose to water is the direct functional foundation of a vast area of materials applications including humidity sensors and actuators. Precise tuning of the nanocellulose water-response, chemically or by physical means, enables, e.g., ultrahigh network swelling or water-response gradients in the nanoscale. As an externally effective trigger, water can be harnessed by sorption and desorption with cellulose chains bringing up multiscale movements for sensing.,

Water Responsive Materials

The nanocellulose–water interactions have been used as a tool to tune mechanical properties. Capadona et al. developed responsive CNC-reinforced composites where the formation and disruption of a percolating CNC network was selectively and reversibly modulated via a response to water as a trigger. DMA analysis showed that the observed changes in modulus, elongation at break, and tensile strength are the result of switching off the cellulose–cellulose interactions by water molecules and not a simple result of a plasticizing effect. The authors concluded that the stiffness reduction achieved in the rubbery ethylene oxide–epichlorohydrin 1:1 copolymer nanocomposite is related to the decoupling of the stress-transferring rigid CNC network by water molecules as they competitively make hydrogen bonds. As a result, this switching is fully reversible, and the nanocomposite reverses to its original stiffness upon drying. Annamalai et al. studied the incorporation of cellulose nanocrystals into soft hydrophobic styrene butadiene rubber matrices to create water-responsive mechanically adaptive nanocomposites. In the dry state, all nanocomposites show higher tensile storage moduli than the neat styrene–butadiene rubber (SBR) or the SBR latex. Upon submersion in deionized water, a dramatic reduction of modulus was observed, which was connected to disengagement of the percolating CNC network due to mostly competitive hydrogen bonding of water molecules with the CNCs (solvation effects in the hydrophilic groups play also a role). Zhu et al. reported reversible formation and disruption of a CNC percolation network in an elastomeric thermoplastic polyurethane (PU) matrix that ultimately led to a rapidly switchable shape-memory effect (SME) activated by water. The researchers concluded that a combination of chemomechanical adaptability of the CNC percolation network and the entropic elasticity of the PU facilitates shape fixity for temporary deformation in the dry state and shape recovery in the wet state.

Furthermore, hybridization with other natural or synthetic (macro)molecules (e.g., polymers, peptides) or nanoparticles has been a popular strategy to introduce multifunctionality or stimuli-responsive properties into nanocellulose-based hydrogels. The application prospects of these hybrids or multicomponent hydrogels are broad including, e.g., bioactive tissue scaffolds,,, ophthalmics,, self-healing materials,, high water containing fertilizers, and fingerprint detectors. The hydrogel network structure, in nanometer and micrometer scale, defines wetting characteristics, capillarity, and water diffusion. Moreover, the spatial orientation and distribution of (nanocellulosic) elements decides whether the network swells isotropically or in an anisotropic fashion, the latter paving the way toward swelling gradients and controlled movement. Several techniques exist for precise 3D design of hydrogel network structures, among them, 3D printing as probably the most popular one.

Alignment, Anisotropy, 3D, and 4D Printing

The transformation of digital design to on-demand manufacturing has been one of the predominant trends within the past decade and has established new technologies entering the market. Especially in the biomedical realm, additive manufacturing enables a customized design of, e.g., biomimetic tissues via tailoring the macroscopic hydrogel structure. CNC and CNF hydrogels inherently bear shear-thinning properties, which is a prerequisite for direct ink writing (DIW), the 3D printing technology of choice for hydrogels. Accordingly, the shear during extrusion induces an alignment of the nanoparticles introducing nanoscale anisotropy into the network (Figure 11a,b)., This anisotropy is not only a very relevant attribute from a mechanical, thermal, and cell functional point of view, e.g., guiding cell differentiation in hydrogel-based biotissue mimics,, but also in terms of directing the networks’ water response. Gladman et al. for instance, exploited the alignment during DIW of CNF embedded in a soft acrylamide matrix during DIW for the design of bioinspired shapes with anisotropic swelling characteristics, converting water-response gradients into a controlled mechanical movement. Gradient swelling dynamics of the shapes, thus, introduce a fourth dimension, and the transition of 3D to 4D printing has become an emerging trend in the realm of stimuli-responsive or multifunctional hydrogel systems with prospects, e.g., in soft robotics or biomedical devices (Figure 11d,e). In the case of CNC hydrogel inks, the alignment of the nanocrystals during 3D printing has been observed by a strong birefringence, confirming the anisotropy in the printed scaffolds (Figure 11a,b). Hausmann et al. made an attempt to understand the interplay between the concentration of CNC suspensions, the applied shear stress, and the dynamics of particle alignment using in situ polarization rheology. They showed that the precise adjustment of shear, extensional flow, and printing nozzle geometry can effectively tune the CNC orientation from full alignment to core–shell architectures (Figure 11a).

Freeze-casting is another way toward structural anisotropy (more explanation in section 3.3.3.1) (Figure 11f).,, Chau et al., for instance, prepared CNC-based hydrogels, starting from fabricating aerogels by simultaneous freeze-casting and cross-linking. The morphology of these aerogels, ranging from fibrillar, columnar, or lamellar, was thereby tailored by precisely controlling the composition of a CNC/poly(oligoethylene glycol methacrylate) precursor dispersion and the freeze-casting temperature. De France et al. used a strong magnetic field for the in situ alignment of CNC/poly(oligoethylene glycol methacrylate) nanocomposite hydrogels, which were simultaneously cross-linked via rapidly forming hydrazone bond formation, a promising approach toward injectable, anisotropic hydrogels for in vivo tissue engineering (Figure 10a). Another way to introduce anisotropy into nanocellulose suspensions was proposed by Guccini et al. The authors obtained induced nematic order in CNF suspensions over a wide CNF concentration range (0.5–4.9 wt %) by osmotic dehydration (Figure 11h). Figure 11 summarizes the attempts to prepare anisotropic nanostructures from nanocellulose.

Actuators, Robotics, and Sensors

The controlled movement of hydrogels, realized via aligning the cellulose nanoparticles, as demonstrated by Gladman et al., has an exceptional potential for hydrogel-type actuators, soft robotics, or sensor materials (Figure 10c–e). Nanocellulose-based biomimetic actuators that combine hydrophilicity gradients in the material with exploiting the fast dynamics of hydration have experienced an increasing popularity.− Kuang et al., for instance, showed that CNFs align selectively upon solvent evaporation (Figure 11g). They used this self-assembly behavior to design extremely strong (∼1000 times lifting weight ratio) actuators with reversible shape-morphing properties upon hydration and dehydration. Zhu et al. used CNCs as active coating on poly(vinyl alcohol-co-ethylene) substrates driving humidity-induced actuation. These actuators could bend or twist depending on the CNC alignment direction. In a different example, Wang et al. showed that also asymmetric exposure of CNF thin films to water vapor can lead to controlled movement governed by the humidity difference across the film. Xu and Hsieh transformed the aqueous exfoliated graphene by amphiphilic nanocellulose into moisture-responsive foldable actuators, as discussed in section 2.4.3. The CNF/graphene film was easily obtained by vacuum filtration into nanopapers that exhibited rapid moisture triggered motion attributed to the highly accessible, charged CNF surfaces. Exploiting the responsiveness of nanocelluloses to water, CNCs and CNFs have been further explored as 1D, 2D, and 3D scaffolds for sensor applications,− some of them for humidity sensing. Kafy et al., for instance, designed humidity sensors based on homogeneous CNC/graphene oxide (GO) composite films, in which changes of the surrounding relative humidity stimulated a change of the composite’s relative capacitance. Similarly, Solin et al. used a hybrid film of carbon nanotubes and CNF to detect humidity by a means of altered electrical resistivity due to accumulating water in the conductive film. Another principle toward nanocellulose-based sensors relies on the reversible swelling upon moisture contact and dehydration of chiral nematic CNC films coassembled with poly(ethylene glycol) or treated with N-methylmorpholine-N-oxide solution. This is accompanied by a color change, thus allowing easy detection of humidity changes (Figure 10c)., Also exploiting the sensitivity of CNCs to moisture, Sadasivuni et al. developed a proximity sensor based on a graphene oxide-modified CNC (CNC/GO) sprayed in layers on polymer substrates bearing interdigitated electrodes. This setup offered a controlled proximity sensitivity without physical contact, which was investigated by measuring the current–voltage–resistance of the samples. The key for this application was the sorbed water on the CNC surface serving as an electron donor at low relative humidity, which changed the film resistance. At high relative humidity, the ionization of water to H3O+ ions contributed to the overall conductivity of the material. Additionally, the presence of CNCs in the composite improved the film structure and spatial resolution as an important structural prerequisite for a fast sensor response and signal recovery.

Mechanical Load Bearing Hydrogels

Although nanocellulose hydrogels have water in their structure, the mere measurement of their mechanical properties does not give too much information on water interactions, and these studies will not be covered here.,,,,− In many of these cases, nanocellulose was simply added to an existing hydrogel formulation to tune their water holding capacity (refs (,,,,,, −)).

Turning Mechanical Properties of Hydrogels with Water

Water certainly plays an ambiguous role in the mechanical properties of nanocellulose materials. Structurally, with a trace amount of water, the crystallization of cellulose was increased with ordered molecular arrangement in disordered regions., Similar to other biopolymers, such as chitosan and collagen, the molecular packing of natural cellulose takes a more ordered structure in the presence of water., Consequently, the mechanical strength of cellulose increases in a characteristic amount of water. In a CNF hydrogel, water is not only considered a biocompatible element, but it also acts as a cross-linker for holding the gel integrity,, up to a certain level after which the water is only loosely retained within the CNF network and not contributing to the swell of the nanofiber network. Beyond cellulose–cellulose adhesion, water can be essential for nanocellulose adhesion to other materials for producing a certain cellulose nanocomposite or a reinforced thermoplastic. However, water has also weakening effects on the nanocellulose hydrogels. It may cause the deterioration of mechanical strength over time by weakening cellulose–cellulose adhesion within the gel.,, At lower water contents, moisture can be used for a plasticization effect that enables the bending of wood material without breaking it., The same principle is utilized in the production of mechanical pulps from wood chips or logs.,

Films, Membranes, Textile, and Coatings

From a technical point of view, many films, membranes, textiles, and coatings are categorized as either hydrogels, aerogels, or colloids and could be discussed in sections 2.4.3, 3.3.1, and 3.3.3. Hybrid materials made by combining cellulose fibers and nanocellulose belong to this group as well. In the following section, we focus mainly on permeability and barrier properties of these materials and their application in packaging, filters, textile industry, and energy related and electronic devices with respect to water. As mentioned before, the availability of a large number of hydroxy groups in cellulose causes high water vapor adsorption and therefore increasing water vapor permeability and poor barrier properties. The effect of moisture on the mass transport of water within cellulosic materials is among the most crucial questions when the industrial use of (nano)celluloses is concerned. These effects are of importance in applications such as barrier films, absorbents,, wound care products, biomedical materials, as summarized in Figure 12.

Cellulose Nanopapers

Films of cellulose nanofibers are commonly known as cellulose nanopapers., Because of the high surface area of CNF and the density of the nanopaper network, the mechanical strength of air-dried nanopaper is outstanding, running up to 200 MPa in tensile strength., Contrary to conventional paper, nanopaper can also be transparent due to the nanoscale width of the CNFs. The proposed applications of nanopaper range from advanced packaging solutions to electronic supports.

Perhaps the most well-known effect of water on cellulosic materials is demonstrated when water accumulates on relatively dry networks, such as paper or nanopaper, whereupon an imminent strength loss is encountered., In technical terms, this represents a poor hygromechanical stability of the nanopapers. The mechanical properties of nanopapers depend on mastering structure formation processes and understanding interfibrillar interactions as well as deformation mechanisms of cellulose nanofibrils in bulk. Benitez et al. showed how different dispersion states of cellulose nanofibrils and different relative humidity values influence the mechanical properties of these nanopapers. The materials undergo a humidity-induced transition from a predominantly linear elastic behavior in dry state to films displaying plastic deformation due to disengagement of the hydrogen-bonded network and lower nanofibrillar friction at high humidity. A concurrent loss of stiffness and tensile strength of 1 order of magnitude was observed, while maximum elongation stayed near constant. Multiple yielding phenomena and substantially increased elongation in strongly disengaged networks, swollen in water, show that strain at break in such nanofibril-based materials is coupled to relaxation of structural entities, such as cooperative entanglements and aggregates, which depend on the pathway of material preparation. The results demonstrate the importance of controlling the state of dispersion and aggregation of nanofibrils in water by mediating their interactions and highlight the complexity associated with understanding hierarchically structured nanofibrillar networks under deformation.

Tuning Material Structural Integrity Using Water

Integrity of nanocellulose materials, which is perceived to play a role in mechanical disintegration of nanocellulose materials upon wetting is also strongly affected by water. Swelling is a detriment in many composites where the dimensions and the structure should be preserved, but it can be a benefit in applications such as 4D printing or biodegradable materials, where interaction with water and the change in shape is expected.

When it comes to preparation of flexible CNC chiral nematic films with optical and sensor applications, structural integrity and stability in water is important. Strategies such as cross-linking can limit swelling of the organized chiral nematic films and improve their structural integrity and stability in water and facilitate their use as freestanding template substrate for conducting polymers or metal oxides to form flexible chiral nematic photonic hybrids.

A crucial challenge in characterization of nanocellulose materials is the lack of any standard practice on how to take the swelling into account when reporting mechanical properties at different relative humidity levels or when measuring the mechanical properties of fully hydrated materials, which limits comparisons between different studies. Walther et al. reviewed the current approaches and proposed a potential best practice for measuring and reporting mechanical properties of wet nanocellulose-based materials, highlighting the importance of swelling and the correlation between mechanical properties and volume expansion.

Improving Humid/Wet Mechanical Properties

Tremendous efforts have been taken to minimize the adverse effect of water on mechanical properties. Most of the studies with focus on improving mechanical properties of nanocellulose materials measure the strength, modulus, or ductility to assess the mechanical performance of the material in humid or wet state in comparison to dry state to confirm that the applied modification or blending techniques have improved hygromechanical stability. In this regard, the focus of these studies is mostly on the blending or modification they used to obtain waterproof or water-resistant materials rather than interactions of water and nanocellulose. Addressing these cases one by one is out of the scope of this review (some of them have been mentioned in section 3.1), and we refer the readers to the original publications for details.,− Here we focus on studies that provide deeper analysis of the interaction with water in their method to improve the hydromechanical stability.

Österberg et al. presented a rapid method to prepare robust, solvent-resistant, CNF films that can be further surface-modified for functionality by hot pressing the films. Drying of the films using high pressure and heat resulted in a film with good resistance to solvents. The films could be soaked in both polar and nonpolar solvents (including water) for more than 18 h. They swelled considerably in the solvents. However, their wet strength remained high, and they were easy to handle in the wet state. The enhanced properties are due to a decrease in the film porosity, which restricts the solvent diffusion through the film. In addition to the densification of the film, the hot-pressing affects the hydroxy groups at the surface, further restricting solvent penetration. This system results in structure-controlled hydrogels upon wetting that limits swelling and therefore the loss of mechanical properties by excessive water penetration. Shimizu et al. prepared TOCNF films, dried them, and soaked them in aqueous MgCl2, CaCl2, AlCl3, and FeCl3 solutions to change the counterion and form TOCNFs–COOM films. Dry TOCNF–COOM films showed high Young’s moduli and tensile strength. They found out that TOCNF films with aluminum and iron(III) carboxylates showed good mechanical properties in the wet state. These results are explained in terms of the high water resistance of the films, which is caused by the formation of interfibrillar electrostatic cross-linkages through multivalent metal ions, limiting swelling and consequent loss of structural integrity. Wang et al. pursued the design of ordered hard/soft nanocomposite structures with balanced supramolecular interactions for biomimetic applications. They established a drying procedure that induces a high orientation of CNCs in a matrix of carboxymethylcellulose (CMC) at high level of reinforcements (50 vol %). They showed alignment in thick bulk films and reported synergetic improvement with a simultaneous increase of stiffness, strength, and work of fracture as a function of the degree of alignment. They showed that the decline in the mechanical properties of such waterborne biobased nanocomposites at high relative humidity can be canceled out by using supramolecular modulation of the ionic interactions by exchanging the monovalent Na+ counterion, present in CMC and CNC, with Cu2+ and Fe3+. This leads to a synergetic improvement of the mechanical properties at 90% relative humidity.

Ansari et al. reported on an interface tailoring route to prepare PEG-grafted CNF to address hygromechanical instability. Modified CNF nanopaper shows significantly improved mechanical properties under moist and wet conditions. Fracture surfaces of CNF films soaked in water showed distinct layers and fibrils pulled out in bundles, while modified CNFs showed a dense structure due to polymer grafting, protecting structural integrity and maintaining mechanical properties in water. Hakalahti et al. bonded TEMPO/NaClO2 oxidized CNF with poly(vinyl alcohol) (PVA) covalently to render water stable films. Pure CNF films and CNF–PVA films in the dry state showed similar humidity dependent behavior in the elastic region, while in wet films PVA had a significant effect on the stability and mechanical characteristics of the films. Influence of the amount and the degree of hydrolysis of PVA on the mechanical properties of the films were also investigated.

Duran et al. partially modified CNFs by chemical means to create a shell of derivatized cellulose that surrounds the crystalline core of native cellulose. Through the different modifications, they aimed at creating a toolbox to tune the properties of CNF materials for specific demands. In total, nine different chemical modifications using different aqueous-based procedures were used as chemical pretreatments before CNF production through homogenization. Films produced from the different CNFs were mechanically tested, and it was found that a combination of periodate oxidation and borohydride reduction resulted in a high strain-at-break. The presence of carboxylic acids led to an increase in tensile strength and Young’s modulus, but a decrease in strain-at-break was also observed. The introduction of aldehydes, resulted in brittle films, but also a decrease in the moisture sorption rate, while the modulus even at high relative humidity was maintained.

Zhang et al. suggested an approach for designing a water resistant, assembled nanopaper through controlled and irreversible aqueous complexation of oppositely charged cellulose nanomaterials. They produced cationic cellulose nanocrystals and tempo oxidized anionic cellulose nanofibers and adjusted the features of the nanopaper by altering the cationic CNC/anionic TOCNF ratio. the water resistance and water vapor permeability of obtained NC complexed nanopapers were improved. The full charge neutralization of oppositely charged NCs created a water-stable nanopaper with a wet strength of 11 ± 3 MPa after immersion in water for 24 h.

Some scientists utilized nature inspired designs to waterproof nanocellulose films. For example, inspired by plant epidermis, Heredia-Guerrero et al. sprayed a cutin like coating, aleuritic acid, a polyhydroxylated fatty acid, on CNC films and polymerized the monomers by hot-pressing. Measurement of Young’s modulus and hardness and water uptake and water vapor transmission rate indicated that this design enhances the robustness and waterproof behavior of CNC films.,

Liquid vs Gas Barrier in Nanopapers

As explained in section 2.4.2.4, transportation of gases and liquids in nanocellulose materials proceeds differently, and it is easier to block the flow of liquid water with its high cohesion and surface tension than that of individual water molecules in vapor phase. Water has generally detrimental effects on the barrier properties of nanocellulose. In the context of cellulose nanopapers, the intention is often to produce a barrier film, and the focus of the research field has largely been on how to improve the barrier properties in moist conditions.,,− However, this has been proven to be a difficult task due to the tendency of cellulose to interact with and rearrange itself in the presence of moisture.,,−

Nanopapers exhibit excellent oxygen barrier properties in dry state, and they have been candidates for food packaging for a long time. However, the strong hygroscopic character of the nanofibers limits their use in environments with high relative humidity (Figure 13a,b). Intercalation of water molecules between cellulose chains weakens the interfibrillar bonds between adjacent nanofibers, which leads to a decrease of the films’ barrier properties.,, Therefore, a common approach to use nanocellulose materials for packaging is to modify or blend them to increase the hydrophobicity of the surface of the material.,− Even some studies reported selective gas separation properties of these materials.,−

Strategies to Improve Nanocellulose Barrier Properties

Nanocellulose materials have been modified in different ways to make their barrier properties more resistant to moisture, (mentioned earlier in section 3.1.1). Polyethylenimine (PEI) surface functionalization, silylating, cross-linking with polyamide epichlorohydrin resins, cross-linking with chitosan, and compounding with montmorillonite are among numerous strategies that have been used to improve gas barrier properties at high relative humidity. Rodionova et al. carried out heterogeneous acetylation of microfibrillated cellulose to modify its physical properties, specifically improving barrier properties and at the same time preserving the morphology of cellulose fibrils for application in packaging. Kubo et al. mixed aqueous dispersions of CNF with sodium counterions (CNF-COONa) and CNFs with tetraethylammonium counterions (CNF-COONEt4) with various weight ratios. CNF-COONa/NEt4 films were prepared by casting and drying with different Na/NEt4 molar ratios. The film density, Young’s modulus, tensile strength, hydrophilic properties, and oxygen and water vapor permeability could be tuned by controlling the Na/NEt4 molar ratios in the films by the effect of bulky versus small counterion. However, it is important to note that mere bulk hydrophobization of the films is usually not enough to improve gas barrier properties. Generally, efficient water vapor barriers have not been achieved after bulk hydrophobization treatments that render the nanopapers nonwettable by liquid water. For example, chemical esterification of CNF with the aim of reducing bulk hydrophilicity and producing hydrophobic cellulose nanopaper with reduced moisture sensitivity has resulted in a decrease in barrier performances toward oxygen and water vapor.,, So far, the most efficient ways to block vapor transmission have been reported to include a (continuous) hydrophobic layer on top of the nanopaper,− such as a applying a coating layer of hydrophobic cellulose via hornification or a coating layer of other hydrophobic polymers such as wax via deposition., In the context of food packaging the traditional strategy is to employ cellulosic materials in multilayered or sandwiched systems, which are effective due to isolation of the cellulosic materials from the humid environment and their protection from the effects of moisture.,−

CNFs can also be applied as coatings to other cellulosic materials to improve barrier properties. Yook et al. prepared various types of CNFs coated on linerboard and wood-free paper to evaluate the barrier properties of these papers against air, liquid water, water vapor, oxygen, and grease. The average fibril size and hydrophobicity were strongly related to the barrier properties. CNFs with smaller fibril sizes and hydrophobized CNFs improved the water resistance. Air resistance and oxygen barrier properties and grease resistance were related to the average fibril diameter of CNFs.

Filters, Membranes, Textiles, and Absorbents

In the context of liquid sorption and permeability, the interactions between nanocellulose and water have been used to design materials as filters and membranes. There are numerous literature accounts on the application of nanocellulose materials as membranes. Besides the often-touted biobased “sustainability” aspect of nanocellulose, their more hydrophilic nature in comparison to common synthetic hydrophobic materials used for membranes, improves their resistance against fouling to some extent, not to mention that regenerated cellulose has been used for over a century to produce membranes and filters for different applications, including water treatment.

Nanocellulose may increase the hydrophilicity of hybrid membranes to improve water diffusion, but this may reduce their mechanical properties. For polyethylenimine (PEI)-CNC films, for example, the Young’s modulus at relative humidity values of 30%, 42%, and 64% were found to be 16, 12, and 3.5 GPa, respectively. If the polymer that nanocellulose is mixed or modified with is highly hydrophilic, such as starch-based polymers, the nanocellulose actually decrease water sorption and diffusion. Using inherently hydrophilic polymers prevents the reduction of the mechanical properties but reduces the water flux through the nanocellulose membrane, simultaneously. Therefore, there seems to be a trade-off between the flux and mechanical strength of nanocellulose composite membranes.,,

Network diffusivity, combined with offering sorption sites for pollutants, are key for the use of nanocellulosic absorbent filters in environmental engineering applications, and oil and gas production. Secondary surface modification, cross-linking, or hybridization with other natural or synthetic polymers enables pollutant-specific membrane designs, with enhanced sorption capacities and rates, as well as mechanical and structural integrity, e.g., to withstand water flow for an extended time.,,− The sorption of organic contaminants from water has also been demonstrated with modified nanocellulose matrices. The inherent hydrophilicity of nanocelluloses should be reduced to improve the affinity of the material for hydrophobic compounds. Increasing the hydrophobicity for this purpose has been achieved by inclusion of both organic and inorganic functionalities. Xiong et al., for example, designed flexible and multifunctional CNF membranes, coated with titanate–bismuth oxide for the synergistic treatment of anion/cation-containing oily water. In another study, atomic layer deposition of TiO2 nanoparticles onto the surface of nanocellulose aerogels created a low-energy surface on the fibers to yield a hydrophobic and oleophilic material that can absorb oil and a variety of organic solvents from the surface of water at a capacity of 80–90% vol/vol. Similarly, depositing triethoxyl(octyl)silane or poly(dimethylsiloxane), or freeze-drying methyltrimethoxysilane onto CNF aerogels resulted in even higher sorption capacities.,, Graphene oxide/nanocellulose composites and poly(dopamine)/BC membranes also showed good sorption capacities.,,

A distinctive field of applications of nanocellulose that might require water repellence in some cases is the textile industry. Colloidal dispersions of CNFs are good alternatives to dissolution/regeneration into cellulose II in filament spinning. Cunha et al. investigated the effects of postmodification of wet-spun CNF filaments via chemical vapor deposition of organosilanes with different numbers of methyl substituents. Various surface structures such as continuous and homogeneous coating layers, or three-dimensional and hairy-like layers, reduced the surface energy, which significantly affected the interactions with water. Mechanical testing revealed that the wet strength of the modified filaments were almost 3 times higher than that of the unmodified precursors, while the final product maintained the moisture buffering capacity and breathability.

Energy Storage Devices

Nanocellulose-based mesoporous structures, flexible thin films, fibers, and networks have been often used in photovoltaic devices, energy storage systems, mechanical energy harvesters, binders, separators, structural supports, and catalyst supports, demonstrating the potential of this material in several energy-related fields.,− The presence of surface-adsorbed water opens completely new perspectives for nanocelluloses in electronics.

Aqueous Ion Batteries

Nanocellulose attracted numerous interests in serving as a promising building block for electrolyte wettable and thermally resistant separators as an alternative to synthetic polymers in gel polymer and solid polymer electrolytes in diverse rechargeable battery systems including established Li-ion and Li–S to next generation Na-ion, K-ion, and Zn-ion systems., Nanocellulose is also capable of inducing an increase in viscosity of electrolytes solutions even at minuscule concentrations. High porosity offered by nanocellulose network as electronically insulating physical barrier is desirable in separator design to ensure good electrolyte retention and enhanced ionic conductivity as well as prevent internal short-circuit. Nanocellulose also holds a prevalent role of enabling good affinity for liquid electrolytes ensuring preferential interaction with the salt anion to improve salt solubility and cation transference in the electrolyte. Mittal et al. combined CNFs and CNCs constructed a mesoporous hierarchical structure as gel polymer electrolytes, ensuring a close contact with metallic Na outperforming conventional fossil-based separator in sodium ion batteries. However, the detrimental effect of water on mechanical properties of nanocellulose networks used in energy storage applications, the effect of water on degradation of lithium salts in Li-ion batteries (LIBs) is a concern. Different strategies have been reported to address this issue and unlock the potential that nanocellulose offers in terms of mechanical properties, environmental benignity, and versatility. The manufacturing process of CNFs is essential to improve the performance of CNFs as both an electrode component and a separator. Flexible paper electrodes were also simply obtained using as low as 4 wt % CNFs (prepared by TEMPO-mediated oxidation) as binder. Such low amount minimizes the moisture introduced to the cell and increases the capacity of the electrodes by total weight. A further study by Lu et al. investigates the optimal processing parameters to enhance the cathode in terms of mechanical and electrochemical performance, achieved using high surface charge (ca. 1.5 mmol g–1) and low defibrillation degree. Using a facile paper-making method, Kim et al. assembled CNFs prepared by TEMPO-mediated oxidation into asymmetric mesoporous separators that represented a more environmentally benign approach compared to conventional fossil fuel-derived materials. Furthermore, the performance of CNF based separators were crucially improved by substituting the native Na+ ions of the carboxylate groups and adding 2 wt % of vinylene carbonate to remove Na+ deposition and suppress gas evolution. In addition to solvent exchange to address the issue of Li salt degradation in LIBs, Jabbour et al. and Leijonmarck et al. suggested that prolonged thermal treatment of cellulose papers can also solve this problem., Generally, cellulose, with its intrinsic chemical and physical properties and microstructures, offers a perfect matrix for manufacturing environmentally friendly LIBs. The good compatibility of cellulose with water allows the utilization of aqueous electrolytes instead of hazardous organic solvents, and the safety concern of LIBs can therefore be greatly alleviated. Water can also be used to remove unwanted chemicals in the process of binder preparation. Natural cellulose dissolved in ionic liquids can be used for production of binders. After the preparation of cellulose solution in ionic liquid and mixing graphite and LiFePO4 (LFP) for anode and cathode, respectively, and coating the slurry on metal foils, the electrodes can be immediately immersed in water to extract the ionic liquid. Water is miscible with ionic liquids but does not dissolve cellulose. In this phase-inversion process, the ionic liquid is completely recyclable.

Fuel Cells

Recently, Vilela et al. have reviewed the use of nanocellulose-based materials in polymer electrolyte fuel cells. In such application, the high-water affinity coupled with the mechanical properties of nanocellulose are an excellent combination. Compared to the commercial ionomer Nafion, nanocellulose-based membranes can be fabricated thinner without compromising their gas barrier properties, a factor that can potentially decrease the cell resistance. Bayer et al. incorporated CNF and CNC nanopapers into membrane electrode assemblies replacing the commonly used and expensive ionomer membrane Nafion or nanocellulose/Nafion composites., The researchers showed a superior performance of the nanocellulose membranes in the fuel cells at high operating temperatures up to 80 °C, with a continuous increase of conductivity with the temperature. Moreover, the conductivity of CNF and CNC membranes increased sharply with the relative humidity as water acts as a charge transport medium. A decisive role was also given to the surface charge groups (−COO– for CNF and −OSO3– for CNC) functioning as proton acceptors and donors. CNC-based membranes showed good conductivity and gas barrier properties, attributable to their higher surface charge density and crystallinity. As in the case of LIBs, the physicochemical properties of the nanocellulose are crucial in terms of aspect ratio and surface charge of CNFs in their performance as polymeric electrolytes. The decrease in conductivity between 80 and 70%RH, as described by Bayer et al., can be suppressed by using nanofibers with a high amount of surface water to produce well-defined and homogeneous membranes, in particular with thin nanofibers (ca. 2 nm) and high surface charges (ca. 1.5 mmol/g). In the same study, Guccini et al. achieved a proton conductivity exceeded 1 mS cm–1 at 30 °C between 65 and 95%RH, which is 2 orders of magnitude larger than with previously reported nanocellulose materials., Furthermore, despite being 30% thinner, a lower hydrogen crossover than with conventional Nafion membranes was observed, likely given by the combination of the excellent mechanical properties of CNFs and the homogeneous membrane structure.

Hydrovoltaic Effect

The interaction of nanocellulose with water can generate electricity, a phenomenon which has been denoted as hydrovoltaic effect. In brief, this effect is based on different water activities, including diffusion, evaporation, and flow, which generate water gradients through solids. An electrical pulse results from the concentration gradient of H+ ions. The ability of nanomaterials, including the eagerly advertised carbon nanomaterials, to harvest electric energy from flowing water and moisture, is based on their exceptional sensitivity toward adsorbed species, providing the ideal 1D nanospace for water binding and a rapid transport. In a recent contribution, Li et al., translated the hydrovoltaic effect to naturally derived nanomaterials, including CNFs, for harvesting energy from moist air flow (Figure 13c). They have shown that, analogous to ion channels of cytomembranes, these bionanomaterials can capture moisture from air through hydrated nanochannels due to their inherent hygroscopic properties and surface charges. Accordingly, in a continuous air flow, the dynamic balance between water adsorption and evaporation produced a streaming potential through the aerogel membranes resulting in an open-circuit voltage. Nanocellulosic materials have also been used in solar evaporation systems. A typical interfacial solar evaporator includes a photothermal layer on top, which upon solar irradiation converts light to thermal energy (heat). It also includes a support whose role is to simultaneously provide hydrophilic channels that continuously wick water via capillary forces to the hot layer to generate steam. Nanocellulosic materials have been used as supporting substrates in these systems.

Solar Energy Harvesting Devices

Solar energy-harvesting devices require high surface area and good charge transport properties so that photons can be absorbed and converted into electrical energy. CNF 3D mesoporous structures offer a very large surface area and present good mechanical properties. Therefore, CNFs can be an attractive template/matrix for processing structures used in photoelectrochemical (PEC) electrodes. PEC water splitting is a promising strategy for directly converting solar energy into hydrogen fuels. Rapid charge generation and separation, large surface area, and broadband light absorption are important aspects of PEC development, and nanocellulose based 3D structures can offer a medium for these technologies, due to their water absorption and water retention capacity.− The hydrophilic mesopores within the cellulose film could serve as an ideal host matrix for the embedment of the nanoparticle catalysts with minimized agglomeration. The mesoporous cellulose films can be used as a framework for photosynthetic and photoactive material and to organize the redox couples. The water retention capacity of the mesoporous 3D cellulose nanostructures plays a crucial role in the reactions and processes in these systems because water is the medium for these devices.,

Supercapacitors

An important application of CNC-derived porous carbon materials is supercapacitors that are closely connected to the interactions of nanocellulose and water. In the first step, self-assembly of CNCs in an aqueous environment results in the development of a chiral nematic phase. This structure can be further carbonized to form chiral nematic mesoporous carbon.,, MacLachlan and co-workers synthesized composite films with chiral nematic structures by the evaporation-induced self-assembly of CNC with silica precursors. After pyrolysis and etching of the silica, freestanding films of chiral nematic mesoporous carbon were obtained, which were used in symmetrical capacitor with H2SO4 as the electrolyte. CNCs and CNFs can be integrated together to form porous carbon materials for supercapacitors as well.

Flexible Devices

Nanocellulose can be easily manipulated to make stable physical or chemical bonds with other cellulosic materials such as fibers used in textiles. This characteristic has been used to design flexible electronic devices. Hu et al. has constructed breathable structures with decoupled electrolyte and oxygen gas pathways for Li-oxygen batteries using carbon nanotube-coated nanocellulose cotton textile as a flexible substrate and electrolyte reservoir. Other than Li-oxygen batteries, nanocellulose macrofiber-based textiles have also demonstrated great potential in constructing flexible supercapacitors and lithium-ion batteries., Water is almost always used as the dispersion medium for nanocellulose materials that would be filtered to form positive or negative electrodes in the preparation of flexible electrodes.,− In a typical process to prepare conductive polymer/nanocellulose hybrids by in situ polymerization, the nanocellulose particles are dispersed in a mixture of acid and water to produce a suspension. Oxidant, initiator, and monomers of conductive polymers are then added to the suspension and the polymerization occurs under mild stirring.− Water also plays an important role in full recyclability of the nanocellulose used in the conductive flexible material. In the first report of a flexible, transparent, and metal-free triboelectric nanogenerator that is naturally degradable after 60 min stirring, the aluminum-doped zinc oxide/CNF paper was completely dispersed into the water. The final dispersion was clear and was used to form a CNF gel with the small amount of Zn and Al ions coming from the aluminum-doped zinc oxide coating. This coating can be redispersed in water and further concentrated and filtered to produce CNF film again, which indicates an excellent recyclability. Despite the positive roles of water in these devices, one of the main detrimental effects of water on the energy related applications of nanocellulose is also observed in the case of wearable devices. The washability of these materials exposes them to large amounts of water that can threaten their integrity and function.

Powders, Aerogels, and Foams

Water is usually partially or mostly removed from colloidal dispersions or hydrogels of nanocellulose to produce new diverse products such as powders, aerogels, and foams, to extend the shelf life of the material, to omit the intrusive effect of water on characterization techniques, or simply to facilitate easier and cheaper transportation (Figure 14)., The extremely high surface area present in nanocellulose in comparison to other cellulosic materials can be lost easily during removal of water from the water–nanocellulose systems. Thus, an entire family of novel dewatering techniques have been developed especially for the nanocellulose–water systems to minimize this effect.

Tuning Dried Nanocellulose Morphology by Water Removal Techniques

As mentioned before, CNCs can be freeze-dried, spray dried, supercritically dried, oven-dried, or freeze-spray dried, and the drying techniques are known to have an effect on the properties of the product (refs (,,,,,, −)). However, the difficulty of removing water from nanocellulose suspensions, while retaining the nanoscale properties of the nanocellulose is a substantial challenge. Lavoine et al. have reviewed the methods to prepare nanocellulose-based foams and aerogels, exhaustively (Figure 15a). In a review by Sinquefield et al. on the current state of nanocellulose dewatering and drying methods, the authors present SEM images showing the representative morphology of CNCs and CNFs dried by oven, spray drying, and freeze-drying. Figure 15b illustrates the effect of water removal technique on the morphology of dried nanocelluloses.

For both CNCs and CNFs, oven drying produced the largest agglomerates. Samples of oven-dried CNC and CNF retained some nanoscale surface textures but resulted in a lower surface area than the other drying methods. Spray drying results in aggregates with a wide range of sizes in both CNFs and CNCs. The CNF spray-dried particles were larger than the CNC particles. The nanoscale surface textures of both CNF and CNC spray-dried particles appeared similar. Wang et al. used supercritical drying to preserve the original gel structure and network for CNC aerogel preparation and showed that the produced aerogels have a nanoporous network structure and high specific surface area. The products of freeze-drying are usually networked multiscalar structures., Freeze-dried CNFs maintain at least partially the nanoscale features with reduced fibril agglomeration relative to oven-dried samples.

The morphology of freeze-dried CNCs can be templated by ice formation during the freezing process which can be adjusted by freezing rate, initial dispersion concentration, and including additives. On the other hand, aerogel preparation with uniform pore size is a formidable challenge (Figure 16a,b). Han et al. studied the self-assembling behavior of both CNFs and CNCs during freeze-drying. Within a certain range of concentration, the fibrils self-aligned into a lamellar-structure foam composed of aligned membrane layers. The authors described the mechanism of these assemblies, again, as a result of ice crystal growth. When the stable nanocellulose suspension was frozen, ice crystals gradually grew in the same preferred direction and created a lamellar structure oriented in the direction of the freezing front. Nanocellulose was expelled and separated by ice crystals and formed a morphology templated by ice crystals (Figure 18a). Huang et al. reported that when the solid content in the original suspension of CNF varied between 4 and 10 wt %, the morphology of the aerogel transformed from the membranous to fibrillar network, increasing its specific surface area and redispersibility, while further dehydration was detrimental. They attributed this phenomenon mainly to the entanglement of cellulose fibrils in the cellulose network, which suppressed the growth of ice crystal during the process. The interaction between intra/intermolecular hydrogen bonds was also responsible for the variation of the cellulose morphologies. The ice templating effect during freeze-drying was also reported by Deville, and the mechanism of ice templating and nanocellulose behavior during freezing was studied in detail, although their study did not include the drying step. Lewis et al. used cyclic physical confinement of CNCs between growing ice crystal domains to promote aggregation of CNCs. Freeze thawing (FT) cycling was employed to form larger aggregates of CNCs without changing the surface chemistry or ionic strength of the suspensions. They showed that the rheology of CNC suspensions can be tuned by FT cycling for suspensions with 4% or more concentration. The complex modulus of 4 wt % CNC suspensions after each FT cycle shows a significant increase, reaching a plateau finally. SEM images of the freeze-dried CNC aerogel formed by this method demonstrated the formation of an interconnected, porous cellulosic sheet network.

In the case of BC aerogels, Gromovykh et al. investigated the effect of culturing conditions on the structure and anisotropy of the produced bacterial cellulose aerogels and found out that ice crystal templating is not the only mechanism for formation of layered morphology of BC aerogels. They suggested apart from the dewatering techniques, geometry, source of carbon and nitrogen, and oxygen availability of the aqueous culture influence the anisotropy and structure of the produced bacterial cellulose network and subsequently result in different morphologies in the formed aerogels.

Some efforts have been taken to decrease the detrimental effects of water crystal growth on dispersion stability, and subsequently, the structural uniformity of the aerogel. For example, freeze-drying from water dispersions can result in significant CNF aggregation. If the aggregation is not desired, especially for dispersibility or surface area reasons, solvent exchange to tert-butanol prior to freeze-drying can be helpful.,, Saito et al. converted CNF aqueous suspensions into hydrogels, which were afterward solvent exchanged to tert-butanol and freeze-dried in order to obtain aerogels with less aggregations.

Peng et al. investigated the effect of drying method on thermal stability and crystallinity of the dried products. Supercritical-drying produced CNFs with the least thermal stability and the lowest crystallinity index. Air-drying or spray-drying produced CNFs which were more thermally stable compared to freeze-dried CNFs. The different drying methods resulted in various char weight percentages at 600 °C for the dried CNFs or CNCs. The dried CNFs are pure cellulose I, while the dried CNCs consist of cellulose I and II.,

Effect of Water Content on the Results of Characterization Methods

As mentioned briefly in section 3.3.2.1, a very important challenge in the field of nanocellulose characterization is the difference in the analytic data based on the difference in water content. It is important to compare the qualities of different nanocelluloses reported in different studies, only with the same dewatering/drying history. Nanocellulose materials hold residual moisture contents of approximately 2–5 wt % in their powder form, which can greatly increase the difficulty of analyzing results for many characterization techniques, such as specific surface area measurements and some processing conditions like melt compounding, which imposes serious issues in their applications. By annealing at 100 °C in vacuum, most moisture can be removed but nanocellulose readsorbs water immediately upon coming into contact with the atmosphere., In practice, characterization techniques such as DVS of celluloses in general, but especially of nanocelluloses, are greatly influenced by the treatment and drying history of the material, e.g., whether air-dried from water or from another solvent, by freeze-drying, or by supercritical drying. The structural changes affect the moisture uptake and its retention in the material, and therefore special care should be devoted to the method of sample preparation to obtain relevant information on its water uptake properties.

Dewatering for Preservation

As mentioned in section 2.2.2, drying of the cellulose source material before nanocellulose isolation procedure, results in hornification and can result in CNFs or CNCs, with different characteristics than the ones produced from never-dried cellulose sources. More critically, drying the already produced CNFs and CNCs irreversibly alters their characteristics mainly due to pronounced hornification, as stated on several occasions in this review. However, keeping large amounts of water in the nanocellulose samples causes many problems such as transportation difficulties, storage problems, and vulnerability toward fouling. Dewatering methods (not fully drying) are a compromise to minimize the complexities of having large quantities of water in the system without completely drying the samples. Nanocellulose is typically stored and transported as a gel with a nominal solid content of up to 5 wt % to avoid interfibril hornification, which means a large amount of water should remain in the gel. There are strategies to reduce the volume of nanocellulose gels for preservation and transport. For example, Reverse dialysis in poly(ethylene glycol) (PEG) has been shown to be a safe dewatering method via osmotic dehydration, without causing irreversible aggregation and sample heterogeneity. Santmarti et al. used low molecular weight PEG as a replacement for the water phase in nanocellulose aqueous gels. These gels had solid contents of up to 70% without interfibril hornification. Despite such reports, the majority of research laboratories and industries report preservation of nanocellulose in water. Some studies have focused on accelerating the dewatering process by changing the pH and ionic strength of the dispersion. According to the suggestions for best practices in storing nanocellulose materials, all nanocellulose in wet state should be stored in the refrigerator or small amounts of sodium azide or toluene should be added to the suspensions. Dried powders should be stored under low temperature and humidity conditions. However, if the nanocellulose materials are intended to be used in toxicity testing or biomedical applications the use of antimicrobial agents is prohibited, and dewatering, refrigeration, or a combination of both are the only secure ways to store the materials.

Reinforcing Nanofillers in Composites

One of the major potential industrial applications of nanocellulose particles, CNFs and CNCs, is their use as reinforcing fillers for nanocomposites due to the inherently high mechanical strength of crystalline cellulose. One of the critical parameters for polymer composites, which governs the properties of the material, is the compatibility of the interfaces between constituting components. The interface is particularly important for nanoscale components because of their immense surface area (refs (,,,,,,,,,,,,,,,,, −)). In this section, we are not delving into the vastly researched topic of how to disperse nanocellulose fillers as efficiently as possible within the continuous matrix in polymer composites. Rather, we investigate the interactions of water and nanocellulose reinforcing fillers, which have been used in polymer nanocomposites and describe the effect of these interactions on the applications (Figure 17). For the full review on strategies on how to solve the issues in nanocellulose applications in polymer nanocomposites, the readers are referred to numerous available reviews.,,,−

Water Sensitivity in Nanocellulose Composites/Blends

There are many potential applications where adding an easily dispersible reinforcing nanomaterial to polymer matrices results in nanocomposites, with the advantages such as improved mechanical properties. These nanocomposites can be manufactured in 1D (fibers), 2D (films, nanopapers, fabrics), and 3D (aerogels, foams, and hydrogels) forms tailored toward different applications (Figure 18). Most polymers used in nanocomposites are more hydrophobic than CNFs or CNCs and, in consequence, there are usually compatibility issues between the components. Besides the compatibility problems, the main drawback in application of nanocellulose in polymeric matrices is their sensitivity to water, which has a profound effect on dispersion, wetting, interfacial adhesion, matrix crystallization, water uptake, and hydrothermal stability (see sections 3.1.1 and 3.1.2). Nanocellulose surfaces are rich in hydroxy groups, which absorb significant amount of water under moist conditions. Surface water molecules weaken the cellulose–cellulose interactions, act as plasticizers, and reduce the network stiffness and strength. Apart from compatibility issues water could be also detrimental to the processing and product performance in some techniques such as melt compounding for nanocomposites. Addition of CNFs or CNCs to nanocomposites may also affect the glass transition temperature (Tg) of the material. This effect, although not reported for all nanocellulose nanocomposites, is shown especially in the case of moisture-sensitive systems. Plasticization effects of water, whose concentration can be increased by the presence of nanocellulose, and the strong interaction between water and the matrix can be the main reasons for this effect. Change in Tg has a potentially important effect on some applications of these nanocomposites that require thermal stability, and nevertheless, it is an issue that must be taken into account. Therefore, a large number of studies aim at improving the outcome of nanocellulose applications in nonaqueous polymeric systems and the key to these approaches is usually surface modification (Figure 19a) and cross-linking (Figure 19b).

Reducing Water Sensitivity of Nanocellulose Composites/Blends

Several attempts have been taken to modify CNCs and CNFs in composites physically or chemically to address water sensitivity. Models have been developed to investigate the effect of modifications on water–matrix interaction to predict the final materials performance of a nanocomposite structure. Lyubimova et al. performed MD simulations of neutral and negatively charged sulfated CNC in water and employed a statistical mechanical molecular theory of solvation to evaluate the solvation structure and thermodynamics of the relaxed CNC in ambient aqueous NaCl solution. This model predicts molecular recognition interactions in solution and can be used to improve the compatibilization of CNC with matrix polymers to enhance the CNC loading levels in composites. The method was shown to be able to accurately predict the degree and type of CNC surface modifications necessary to achieve a good dispersion in polymer solutions while preserving the desired crystallinity and mechanical properties. Chemical and physical surface modification, counterion change, and emulsification are among approaches that have been used to improve the qualities of nanocellulose–polymer composites. Wei et al. used computational approaches to obtain understanding of water adsorption and interfacial mechanics of modified CNC surfaces to address the issues regarding the response to moisture. They found both experimentally and theoretically that methyl(triphenyl) phosphonium (MePh3P+)-exchanged CNCs have lower water uptake than Na-CNCs due to the disruption caused by the bulky ionic structure of MePh3P+. The adsorbed water accumulates near the cations and is oriented by electrostatic interactions as well as water–water hydrogen bonding. Traction–separation behavior of these interfaces is highly dependent on the surface chemistry. MePh3P+ cations serve to change the interface in a way that it exhibits hydrophobic behavior, such as formation of capillary bridges and preservation of mechanical properties upon wetting. The researchers showed that chemical surface modification is a viable option for changing the adsorption and traction–separation behavior of CNC as an important first step toward the design of moisture-tolerant CNC–polymer nanocomposites. Carrillo et al. proposed double emulsion systems for the compatibilization of aqueous dispersions of CNFs with a nonpolar polymer matrix (Figure 19c). Nonionic surfactants were used in CNF aqueous dispersions equilibrated with an organic phase. This method of CNF integration within hydrophobic polymers removed the need for drying or solvent-exchanging of the CNF aqueous dispersion prior to processing, proving double emulsion systems as a novel, efficient, and scalable platform for CNF coprocessing with nonpolar systems in nanocomposite preparations.

Hydrophilic Nanocellulose Composites

Due to the hydrophilic character of nanocellulose, the simplest polymer systems that incorporate nanocellulose are water-based systems. In these systems, water plays a positive role. Nanocellulose dispersions can be simply mixed with aqueous polymer solutions or dispersions (both natural and synthetic polymers). Although these systems suffer from limited applications and are only appropriate for water-soluble or dispersible polymers such as latexes, they can be very useful in the scope of colloids, emulsions, hydrogels, films, membranes, 3D printable, and responsive materials, as discussed in section 3.3.1, 3.3.2, and 3.3.3 (refs (,,,,,,,,,, −)). For example, cross-linked CNF/poly(acrylic acid) (PAA) composites have been prepared in order to improve the material properties in humid environments., Nanocellulose/PVA composites have similarly been popular. In fact, Lee et al. managed to prepare a fiber composite that bears one of the highest reported tensile strength values of all nanocellulose-based fiber composites, ca. 900 MPa (Figure 19d). But such materials with all-hydrophilic components are usually susceptible to moisture and water, which possesses an intrinsic constraint for their usage.

Computational Methods to Uncover Water–Nanocellulose Interactions

MD simulation is an appropriate tool for performing atomistic computer simulations of moleculear interactions within material itself, with other molecules, and with solvents under given thermodynamic conditions. Both water and cellulose have been studied by MD simulations. For both of these materials, some parallels appear in simulation studies and experimental results. Simulations allow the creation of hypothetical measurements and the predicted results for these measurements. These simulated test results are then compared with real experimental results, and the results of other simulated measurements with different assumptions and conditions, to both understand the real structure of the material, and the origin of the experimental signal.

The first atomistic MD simulations of cellulose–water interface were performed already in the late 1990s by Andreas Heiner and Olle Teleman, who found that the interactions with water gave rise to structural disorder in the first cellulose layer, with respect to the crystal lattice parameters., Since then, the importance of using computational modeling for the understanding of cellulose and cellulose–water interactions has grown rapidly. Specifically, developments in molecular modeling methods such as MD and quantum mechanical density functional theory (DFT) have been instrumental for this advancement and has recently been reviewed by Bergenstråhle-Wohlert and Brady, Zhang et al., and by Buehler and co-workers.

While MD is based on classical physics and treats atoms as point particles that are interacting pairwise through empirical potentials, DFT takes the electronic configuration into account and is therefore considered very close to an ab initio method. This has consequences for its practical use. While DFT is more precise, it is only efficient in systems consisting of a few molecules, whereas MD currently can treat systems of millions of atoms and reach millisecond simulation times. In addition, there has been considerable effort in developing coarse-grained potentials for cellulose simulations, in which atomistic details are sacrificed for the benefit of significantly extending available time- and length-scales., Therefore, in these models, the details such as hydrogen bonding and water molecular orientation are averaged out, and they are less suitable for specific investigations of cellulose–water interaction on the molecular scale.

There exist several empirical force fields for atomistic MD that are specifically designed to treat carbohydrates in aqueous solution. Among the most popular are CHARMM (Chemistry at Harvard Macromolecular Mechanics),, GLYCAM (developed and maintained by Complex Carbohydrate Research Center at the University of Georgia in Athens GA), GROMOS (GROningen MOlecular Simulation computer program package), and OPLS-AA (Optimized Potentials for Liquid Simulations-All Atom) force field (developed and maintained at Purdue and Yale universities), which are all frequently used for simulation studies of cellulose. The potentials are developed in close connection with a water model, which thus can be considered part of the force field. The GROMOS potentials uses the SPC (simple point-charge) water model, while CHARMM, GLYCAM, and OPLS-AA are developed with the TIP3P (a 3-site rigid) water model. In spite of the relative simplicity of these models, they have proven to be accurate enough for average properties related to hydrated cellulose systems. In fact, one study which used a more complex water model that included electronic polarizability reported only minor differences compared to static models. For a detailed comparison between the performances of different water models, the reader is referred to the literature.

Cellulose Is Insoluble in Water

From a fundamental perspective the nature of cellulose is ambiguous. Owing to its large number of hydroxyl functionalities, it is considered a hydrophilic molecule. On the other hand, it is completely insoluble in water at ambient conditions (Figure 5). It has been suggested that this phenomenon is due to the many intermolecular hydrogen bonds of the aggregated structure. This view was contested by Lindman and co-workers,, who argued that cellulose is an amphiphilic molecule and that aggregation is a consequence of hydrophobic assembly. Indeed, early MD simulations had shown that the contribution from hydrogen bonding to the dissolution free energy is an order of magnitude smaller than from dispersion interactions and the hydrophobic effect., The latter was later explicitly shown to originate in a large entropic penalty of the water in the first hydration shell. The entropic cost was however significantly reduced at elevated temperature and pressure and as a consequence cellulose was soluble in simulations of water at supercritical conditions. The entropic cost associated with water can also be mitigated by addition of cosolvents such as urea,, which is exploited for enhancing cellulose dissolution in cold alkali (Figure 5).

Cellulose Twist in Water

The fiber/fibril twist of cellulose is an intriguing and significant observation of morphological changes in model cellulose crystals solvated with explicit water molecules with bulk water properties,,,− although from an experimental perspective the mechanisms behind its occurrence, and even its existence, are still a debated subject.,− To a certain extent, the twist is speculated to cause the inability of individual microfibrils to coalesce into merged fibrils over long distances. Until now, MD studies have simulated microfibrils with either a rectangular, diamond, or hexagonal cross-section made up of up to 100 cellulose chains and of length between 10 and 50 nm, and a right-handed twist of a few degrees per nanometer of length has been found. Furthermore, the twist has been found to scale inversely with the cross-sectional area yet be independent of fibril length.,, The molecular origins of the twist were suggested to be the result of a combination of intra- or intermolecular hydrogen bonding, electrostatic interactions, van der Waals forces, and the chirality of cellulose chains. Isolated glucan chains in water deviate from the strict 2-fold symmetry assumed in the crystal structure of cellulose rendering them a slight right-handed twist. This is a common feature of all β-1–4 linked oligosaccharides and has been shown to be caused mainly by steric effects with negligeable contribution from intramolecular hydrogen bonding., It is likely that this single-chain twist propagates up within the structural hierarchy giving twisted microfibrils. This conclusion is reinforced by a study where the microfibril twist is shown to be insensitive to intrachain hydrogen bonding. Some other studies have also suggested that hydrogen bonding may not influence the twist at all., The microfibril twist in turn progresses to the next hierarchical level of the fibril bundle. However, the twist results in an increase in conformational disorder from the microfibril core toward the surface in the presence of both water and vacuum, causing a longitudinal variation in the bundle structures that prevents cocrystallization and opens up routes for the diffusion of water molecules into said bundles (Figure 20a,b). The amount of interfibrillar water was found to be roughly half of that of extrafibrillar surface water in MD simulations of microfibril bundles, which correlates well with the experimental analysis of bleached hardwood pulp.

The role of water or solvation for the mechanisms behind fibril twisting is not clear. It has been shown, however, that the physical presence of water significantly mitigates the extent of twisting due to the ability of water to form hydrogen bonds with the crystal surface. On the other hand, Conley et al. found that water only has a limited effect on the twist unless it disrupts the hydrogen bonds across the glycosidic bonds. Further, adding an excess of water beyond the first solvation shell does not change the degree of twisting, but this is dependent on the water model used; when using TIP5P water resulted in a noticeable reduction of the twist compared to the TIP3P model, for example.

Effect of Hydration on Cellulose Dynamics

The structure of cellulose at the surface is significantly different from the crystalline bulk structure, as is evidenced by the distribution of the hydroxy groups and torsional angels., These angles are strongly affected due to changes in the hydrogen bonding potential in the presence of water at the cellulose surface. Moreover, the dynamics of surface polymers is distinctly different from those inside the crystal. MD simulations of cross-polarization and magic angle spinning (CP/MAS) solid-state 13C nuclear magnetic resonance (NMR) longitudinal relaxation enabled quantitative interpretation of experimental NMR data (explained in detail in section 4.2.2). The experimental data along with the simulations demonstrated a direct correlation between dynamic and structural heterogeneity at atomic resolution, enabling the understanding of structure–function relationships in controlled hydration conditions. It was found that the doublet at resonance ca. 84 ppm for C4 atoms was due to the nonequivalence of accessible surfaces located on top of different crystallographic planes. Within hydrated cellulose fibril aggregates, localized cellulose macromolecular dynamics have been deconvoluted into contributions from distinct molecular sources within the aggregated CNFs: (i) the hydroxy groups in the core of CNFs, (ii) the less accessible and accessible surface regions, and (iii) within structurally different surface groups. Upon hydration, this leads to an increased disorder in the hydroxy group conformation at the cellulose surface. As found in MD simulations, and confirmed with neutron reflectivity experiments, cellulose hydrated to 10% w/w with water is more rigid than dry cellulose as a result of one water molecule forming two or more hydrogen bonds with cellulose to bridge cellulose chains.

Water Structure and Dynamics at Cellulose Surfaces and within Fibril Aggregates

The solvation of cellulose is also of importance in understanding the reactivity of cellulose as it relates to its interfacial properties. Understanding the role of water at cellulosic surfaces and within fibril aggregates will aid the discovery of the underlying process not only for deconstructing cellulose but also for designing functional, chemically modified cellulosic materials for targeted applications.

The solvation structure is determined by asymmetry of crystallographic cellulose surfaces due to the topographical and chemical heterogeneity of each surface. As a result of the heterogeneity resulting form of C–H and O–H rich regions, respectively, the local water density in different hydration layer differs considerably, as illustrated in (Figure 20c,d). Around the O–H rich regions, a high water density leads to a dense first solvation shell, which has been hypothesized to slow down the diffusion of other molecules toward the cellulose surface., Due to the lack of affinity toward the C–H rich regions, water molecules form strong hydrogen bonds with each other, causing small-scale hydrophobic effects. Along the longitudinal direction of microfibrils, water molecules near the C–H rich surface, i.e., the (2̅00) and (100) planes of the cellulose Iβ crystal, and the (1̅1̅0) and (110) planes of the cellulose Iα crystal, have a higher compressibility than those in other solvation shells (Figure 20b). Miyamoto et al. focused their simulation specifically on the orientational structuring of water molecules over the (100) crystal plane of cellulose Iβ. In terms of orientation, they showed that water molecules can approach hydrophilic troughs between cellulose chains and form hydrogen bonds to hydroxy groups to form interchain hydrogen bonding. The hydrophobic strips of cellulose crystals are sufficiently narrower in comparison to the fibril size.

In general, the behavior of the bound water to cellulose surface and fibrils is thermodynamic-driven. With confirmations from quasi-elastic neutron scattering (QENS) studies on deuterated bacteria cellulose on a picosecond scale, O’Neill applied MD simulations to elucidate two unambiguous populations of water (explained in detail in section 4.2.7). As explained in subchapter section 2.4.2.2, “nonfreezing bound” water gradually becomes mobile with increasing temperature in the vicinity of cellulose surface. The second population is “confined water”, which can be attributed to water accumulation in the narrow spaces between microfibrils. Langan et al. found that fibril aggregation during thermochemical pretreatment with increased temperature up to 160 °C would cause core water expelling among the fibrils. An induced increase of fibril crystalline domain indicating fibril coalescence was also experimentally observed by Kuribayashi et al. However, water steadily stays between fibrils when the applied temperature is maintained below 76 °C and Chen et al. showed that this population of water is in thermodynamic equilibrium as opposed to being kinetically trapped. This means that interfibrillar water lowers the free energy of the bundle and thus acts as an adhesive. On the other hand, interfibrillar water lowers the friction between fibrils facilitating shear deformation, contributing to the ductility of cellulose materials. Surface charge was also shown to interfere with cellulose–water interactions. Paajanen et al. presented an informative understanding of the water interactions between fibrils of TOCNF regarding its rheological, aggregation, and disintegration properties using MD simulations.

Wetting and Water Sorption

Cellulose Iβ crystals with the existence of both hydrophilic surface (e.g., (010), (110), and (11̅0) surface with exposed −OH) and hydrophobic surface (e.g., (100) plane with buried −OH and exclusively −CH moieties) show a featured hygroscopic property. The ab initio studies of interactions between (100) plane and single water molecule were carried out using dispersion corrected DFT method. It was concluded that water adsorption on the Iβ (100) plane is depending on the adsorption size on the plane (Figure 20e,f). Hydrogen bonds could be formed with more accessible CH moieties protruding out of the plane than oxygen atoms of the equatorial hydroxys. Wetting of two cellulose surfaces, (010) and (100), was carried out by MD simulations of contact angle using the native Iβ model. In the simulation, a nanodroplet of around 3 nm TIP1P/2005 water was placed near the surfaces. The calculated contact angle in the simulation was around 16° for the (010) plane and around 23° for (100) plane (Figure 20i,j), exhibiting hydrophilic behavior. Similarly, Nawrocki et al. found a contact angle of 25° for TIP3P water with cellulose (100) plane, predicted in their MD simulations using CHARMM force field. In a comprehensive study using the CHARMM force field Trentin et al. studied the spreading of water nanodroplets on the different crystallographic planes in several cellulose polymorphs. It was found that all surfaces were hydrophilic (even those commonly termed “hydrophobic”) with static contact angles ranging from <5° (complete wetting) up to 48°. Interestingly, the highest contact angle was found for the “hydrophilic” (001) surface of cellulose Ia. The differences in wetting were correlated with the conformation and accessibility of surface hydroxymethyl groups. Karna et al. conducted contact angle simulations between water and cellulose surface at the presence of an external electric field. The application of an electric field with varied direction and magnitude would tune the wettability of cellulose surface, which could be beneficial to the dewatering process of nanocellulose related products. Albeit the wetting behavior is rather similar for both (010) and (100) planes, the solvent molecular organization interacting with each plane is substantially different. It is observed that water penetrating in the interstices between cellulose molecules in the (010) plane forms hydrogen bonds with the exposed surface −OH groups due to high surface roughness. However, on top of the (100) plane, water is inclined to form water structure at the interface along with a characteristic gap on top of the apolar ring (Figure 20g,h). Water molecules also prefer to occupy the specific positions, particularly between the glycosidic oxygen atom and the adjacent O-2 and O-3 hydroxy groups.

A phenomenon related to wetting is the formation of capillary bridges. Ogawa et al. used MD to study capillary effects during drying of model CNF. As water was gradually removed a meniscus formed, exerting a capillary force large enough to plastically deform the fibrils. At the end of the simulated drying, the two fibrils had partially fused, although some water still remained trapped within the aggregate.

Simulation of the Interactions of Functionalized Cellulose with the Environment

In general, MD simulation studies can be an appropriate tool to understand the role of water in functionalized nanocellulose surface and composite in terms of tailoring interfacial behaviors and tuning compatibilities in composite materials on both bulk and molecular level. As discussed in section 3.3.4, the presence of water at nanocellulose surface detrimentally weakens the interaction between hydrophilic cellulose and hydrophobic polymer matrices, which becomes a problem in cellulose nanocomposite materials. A cellulose Iβ (11̅0) surface was grafted with caprolactone of different degrees of substitution by Bergenstråhle et al. The hydroxy groups in the native cellulose surfaces interact with other medium such as caprolactone not limited by present water. Surfaces with modified O6H6 and a DS of at least 50% interacted with the surrounding medium mainly through the grafted monomer unit instead of hydroxy groups. However, the adhesion between grafted surfaces and surrounding polymer medium was still prohibited by the presence of water. Increasing the degree of polymerization of the grafts was suggested to diminish the effect of surface water. Simulations of the interactions between functionalized cellulose surfaces and surrounding medium leading to increased understanding of the self-assembly of nanocellulose would help the development of novel materials. Bouchard et al. studied the interaction and adsorption of water and electrolyte on the cellulose nanocrystal pristine surface and its modified surfaces, i.e., carboxylic and sulfate groups, by DFT quantum chemical calculations. The cellulose Iβ (11̅0) surfaces were more repulsive toward each other, possessing a slightly more negative electrostatic potential map than (110) surfaces. The negative surface functionalities impart a greater CNC surface hydrophilicity, while hydrogen-bonding network within cellulose was restructured in the presence of positive electrolyte ions. Recently, Chen et al. investigated the influence of topochemical modification of cellulose surface on its interaction with water and among the modified nanocellulose particles. It was concluded that acetylation in the C6 position led to hydrophobization of cellulose fibrils and the decrease of the work of adhesion between the acetylated model surface and water. Most interestingly, the acetylation was found to greatly increase the dispersibility of nanocellulose.

Experimental Methods to Uncover Nanocellulose–Water Interactions

This section introduces the key analytical techniques that are currently used to investigate cellulose–water interactions and gives a few selected examples of published works from each that specifically measure the effect of water on nanocellulose-based materials. The overview of analytical methods is not exhaustive and is limited to the key analytical techniques that are currently used to investigate cellulose–water interactions. For each of the discussed techniques, we provide selected examples of works that specifically measure the effect of water on nanocellulose-based materials.

The wide variety of analytical techniques and protocols developed to probe nanocellulose–water interactions reflects the complexity of these interactions and the need to examine them from different perspectives. In paper making processes, well-established technical process-orientated standard methods such as freeness value (Schopper Riegler (°SR) test), water retention value, and other online paper web moisture measurements reflect cellulose–water interaction including runnability and processability in a macroscale level. However, most of these techniques are not directly applicable for studies of nanocellulose materials, unless further development takes place. This section introduces the key analytical techniques that are currently used to investigate cellulose–water interactions and gives a few examples of published works from each that specifically measure the effects of water on nanocellulose-based materials. These techniques and their analytical focus are summarized in Figure 21a,b to guide the reader to the appropriate analytical technique for their research needs.

Microscopic Methods

Microscopy, including electron microscopy (EM) and optical microscopy can be used as an indirect analytical tool to shed light on water related phenomena in nanocelluloses, mostly with respect to drying and, in some cases, also to swelling processes.

Electron Microscopy (EM)

Conventional scanning electron microscopy (SEM) and transmission electron microscopy (TEM) have been used to observe the morphology of CNCs and CNFs, to determine their dimensions,,,, and to study the impact of different treatments and drying conditions on nanocellulose structures.,,,,, While an excellent tool to study nanocellulose, EM measurements are carried out in vacuum, and so sample drying (e.g., ambient drying, freeze-drying, heated drying) has an important and sometimes irreversible effect on the morphology of the structures, demanding careful image interpretation. Moreover, SEM imaging often involves sputtering of the samples with thin conductive layers which can distort sample features, particularly at the nanoscale. In contrast to conventional SEM, environmental SEM (ESEM) does not require as high a vacuum, thus enabling measurements to be carried out with some residual moisture and/or relative humidity. However, controlling the imaging conditions is difficult, and the limited resolution of the microscope may explain the restraint in using this technique to explore nanocellulose–water interactions. Nevertheless, a few examples highlighting the analytical value of SEM and ESEM are briefly described below.

Natarajan et al. used SEM to quantitatively investigate the morphology and chiral nematic structure of sulfated CNC films, whereby the CNCs were neutralized with different cations and dried under controlled conditions. SEM images revealed that faster evaporation rates caused a disruption in the chiral nematic liquid crystal ordering of the film due to vitrification. The images were also used to quantify the nominal pitch (i.e., the helical modulation length) distribution from fractured film cross-sections using a novel image processing method (Figure 22a,b). The calculated pitch distributions were in good agreement with UV–vis–NIR total reflectance spectra. While Gaussian fitting the pitch distribution from SEM helped to obtain peak positions and peak widths, the measured pitch and standard deviation values showed an identical dependence on the evaporation rate of water. For example, greater sample uniformity upon slow evaporation gave a much smaller pitch (i.e., a tighter chiral nematic twist) and smaller standard deviation. Moreover, the SEM was sensitive to the multidomain structures of the fast-dried films. In addition to pitch variations related to different water evaporation rates, a gradient in pitch was observed in going from the top to the bottom of each film down the cross-section, which was larger for films and dried more quickly. Finally, the SEM images showed that the shape of moisture inclusions and water confinement in the CNC films varied with the different counterions investigated.

Lewis et al. used SEM to investigate the morphology of freeze-dried hydrogels formed by cyclic freeze–thawing of CNC suspensions and confirmed the formation of an interconnected, porous cellulosic sheet network. Ansari et al. used fractography studies in SEM images of nanopapers from phenyl glycidyl ether oligomer-grafted CNFs to relate property differences to structural changes. Moreover, differences in swelling could be observed from the SEM micrographs. Rapid dewatering of nanocellulose suspensions was also a key point in the study of Österberg et al., who used hot pressing to prepare robust, solvent-resistant, CNF films. SEM revealed a significantly increased film density after extensive pressing (2 h). In contrast to SEM studies of dried nanocellulose structures, ESEM enabled Gelin et al. to obtain information about the nanostructure of BC with respect to water content at different relative humidity values. ESEM images taken at 77% relative humidity showed that the inner side of the BC gel tubes contained between 10 and 40% water.

Even though TEM has been widely used to investigate the size and shape of nanocelluloses either frozen (cryo-TEM) or dried from water and other solvents, the technique has not been directly used to investigate nanocellulose–water interactions. This is likely due to sample preparation and imaging limitations despite the nanometer spatial resolution. Nevertheless, TEM has been used to corroborate the results obtained from other methods. Gelin et al. coupled the information from freeze-fractured samples imaged by TEM with the magnitude of diffusion coefficients extracted from dielectric spectroscopy, supporting the theory that free (or bulk-like) water present in BC gels is confined as “lakes” rather than forming a continuous phase throughout the gel structure.

Atomic Force Microscopy (AFM)

AFM, a scanning probe microscopy technique, is another visualization tool to investigate nanocellulose. Its versatility is based on the different possible measurement modes and experimental setups including imaging modes (e.g., contact mode or alternating current/tapping mode), and surface force measurement modes (e.g., to determine precontact attractive/repulsive/steric, adhesive, and frictional forces, as well as mechanical properties), e.g., AFM measurements can be done in ambient conditions, under controlled temperature/humidity, or samples can be fully submerged in liquid all while ensuring nanoscale and piconewton resolution. For example, Reid et al., studied the swelling behavior of CNC thin films in the presence of water, by imagining the height profiles of scratches made into the film before and after exposure to water (Figure 22c,d). Ahola et al. used colloidal probe AFM to measure forces between a cellulose sphere, glued to a tipless cantilever, and a CNF surface., They studied the effect of nanofibril charge density, ionic strength, and pH on the swelling and surface interactions of CNF model films; AFM and QCM-D were used in conjunction to infer that both steric and electrostatic forces were present in water and that steric forces dominated between cellulose surfaces under low pH and high ionic strength conditions.,

Optical Microscopy

The limited resolution of optical (or light) microscopy compared to other techniques has restricted its application as a visualization tool for nanomaterial characterization. Nevertheless, there are examples of indirectly using optical microscopy to investigate nanocellulose–water interactions. For example, Shrestha et al. used a contrast enhanced microscopy digital image correlation technique to characterize the dimensional changes induced during hygroscopic swelling of self-assembled and shear-oriented CNC films (Figure 22e,f). The authors applied the distinct microstructure and birefringence of CNC films to explore the in-plane hygroscopic swelling by correlating cross-polarized microscopy images at relative humidity levels ranging from 0 to 97%. The in-plane coefficient of hygroscopic swelling of the CNC films was thereby determined by optically tracking humidity-driven strain fields in a contact-free manner.

Surface Energy and Mass Transport Methods

As discussed earlier, surface energy together with the surface roughness, determines the wettability of a surface by a liquid. Among the most common ways to characterize the surface energy of cellulosic materials are inverse gas chromatography (IGC), thin-layer wicking (TLW), and different types of contact angle measurements, which will be outlined in the following section. Moreover, as elucidated in sections 2.4.1.2 and 2.4.2.4, surface energy and wettability are intimately linked with mass transfer, the phenomenon of a net movement of species from one location to another. Here, we will only consider methods to characterize the mass transfer of water in cellulosic materials and make a distinction between the transfer of liquid water and water vapor. The mass transfer of liquid water can be characterized using TLW experiments using the Lucas-Washburn eq (eq 1), introduced in section 2.4.2.4. Moreover, the water mass transfer across, for example, cellulose nanopapers can be measured gravimetrically by different flow tests (gravitational or pressurized) or even by diffusion cells equipped with tritium oxide labeling and radioactivity monitoring. In the case of water vapor transfer over cellulosic films, the vast majority of literature report either the water vapor transmission rate (WVTR) or its close variant water vapor permeability (WVP) using a gravimetric method described in the following.

Contact Angle

Among the most common ways to analyze the contact angle is sessile drop goniometry, where a high-speed camera captures a video of a surface wetted by a droplet of liquid. In the simplest setup, this is done on a horizontal surface (Figure 23a), although other possibilities also exist.− The captured images are then analyzed by computer by numerically fitting a function to the images,, yielding an estimate for the contact angle at each moment of time. The time-dependency of the contact angle varies a lot: for example, a water droplet will wet a rough, high surface energy solid almost instantly, whereas hydrophobic surfaces will resist wetting by the droplet and the droplet will retain its shape until it slowly evaporates. It is therefore common to record not just initial (or static) contact angle but also to observe how stable the droplet is over time. One of the limitations of static contact angle measurements is that they are not always reproducible, but one way to overcome this is to record advancing and receding contact angles, which tend to be more reliable.

A dynamic extension of the static sessile drop technique allows the detection of advancing and receding contact angles by increasing and decreasing the volume of the deposited droplet (Figure 23b). The difference between these angles is referred to as contact angle hysteresis, which provides an indication of surface roughness, possible surface contaminations, etc., In the case of cellulosic materials, contact angle hysteresis can also infer tendency of the material to absorb moisture. The more pronounced the hysteresis, the more firmly the droplet is attached to the surface and the more wettable the surface is by the liquid.,

To determine surface energies by contact angle measurements, multiple probe liquids of varying polarities are used, including ethylene glycol, formamide, toluene, glycerol, and diiodomethane., Surface energies can then be determined using the Fowkes method, where the surface energy is divided into the dispersive and the polar component, combined by a geometric mean approach.

As contact angle measurements are sensitive to surface roughness, they are at their most accurate on smooth and rigid surfaces. Nanocellulosic surfaces are not considered smooth or rigid, and as such this limitation should be kept in mind even though contact angle analysis, especially by the static sessile drop technique, is commonplace within the cellulosic materials research literature. Spin-coating and multilayer Langmuir–Blodgett/Schaefer deposition of nanocellulose films can be used to obtain smoother films than those from solvent casting, but the degree of aggregation of nanocellulose in liquid prior to film preparation can also affect surface roughness and porosity; AFM is a good method to quantify these film properties. Owing to its operational simplicity, contact angle analysis has most often been used in a semiquantitative fashion, where the wettability by a static droplet of liquid water on a series of samples is compared.,, At the very least, significant differences in wettability can be detected by this simple approach, allowing for a quick check of, for example, the success of a surface hydrophobization treatment.

The multiple probe liquid approach has been applied to calculate the surface energies of cellulose nanopapers, CNC thin films, ultrathin films of amorphous cellulose, etc. Moreover, through hysteresis analysis, cellulosic surfaces have been shown to be sensitive to moisture uptake; some water molecules inevitably remain on the surface upon retraction of the droplet, further enhancing their wettability by water. It should also be noted that cellulose readily swells and curls under water during contact angle measurements, and these dynamic changes caused by wetting and drying may significantly alter the perceived surface energies of cellulosic surfaces.,,, These effects complicate the interpretation of contact angle values, so an alternative strategy employing the Washburn technique may be considered.

Washburn Technique and Thin-Layer Wicking

Closely connected with contact angle analysis, the Washburn technique (or the capillary rise technique) is based on the spontaneous flow of a probe liquid through a column filled with the porous material to be analyzed. It enables the simultaneous determination of the pore radius, contact angle, and surface energies of porous samples. The uptake of the probe liquid can be detected either gravimetrically or by observing the change in the height of the liquid layer. Very similar in operational principle, TLW is an example of dynamic wetting that is based on liquid penetration into a porous solid., All of these techniques rely on a phenomenon called wicking, i.e., the spontaneous spreading of a liquid into a porous material caused by the pressure difference resulting from the spherical meniscus of the wetting liquid. To determine the surface energy components of a solid by TLW, a multiple liquid approach is used, much in the same way as in the contact angle measurements. At least three probe liquids of known dispersive and polar components are required, and their contact angle, vapor adsorption isotherm, or the penetration rate should be measured. Operating under a set of assumptions, a modified form of the Lucas–Washburn equation relates the rate of penetration to the surface energy components:where x is the distance traveled in time t, η is the liquid viscosity, R is the effective capillary radius, and ΔG is the Gibbs energy change accompanying liquid penetration into the solid. ΔG may then be converted to the surface energy by different means, depending on the type of the liquid–solid system in question.

TLW has been applied to measure the surface energy of microcrystalline cellulose (MCC) and cotton fabrics, but its role in the cellulose materials science has remained much more peripheral than the omnipresent contact angle measurements. The same applies to other wicking-based techniques, including capillary intrusion that has also been utilized to measure the surface energy of MCC. As we noted in the context of contact angle analysis, the adsorption of water vapor on nanocellulose surfaces has an influence on the wicking behavior of water. This is a relevant concern for an extremely hygroscopic material like cellulose that is in practice covered by a layer of adsorbed water molecules at all times.

Inverse Gas Chromatography (IGC)

In contrast to contact angle and wicking-based experiments that are sensitive to sample roughness and porosity, IGC can be used to characterize the surface energies of particles. The basic principle of IGC is similar to gas chromatography (GC) in the sense that there is a gaseous substance passing through a column of a stationary phase. In IGC, the sample to be investigated acts as the stationary phase, whereas in traditional GC, the sample would be carried by an eluent gas.

IGC analysis can be run at different relative humidity and temperature and can yield information on, for example, the specific surface area, degree of crystallinity, solubility, and thermodynamic interaction parameters, glass transition temperatures, and the dispersive and polar components of surface energy., IGC surface energy analysis is run at infinite-dilution conditions utilizing a number of different probe molecules, usually a series of alkanes (e.g., hexane, heptane, octane, etc.) in combination with polar probes (e.g., dichloromethane, acetone, acetonitrile, and ethyl acetate)., The retention times and surface coverages are then recorded and used to calculate the dispersive component, polar component, and total surface energies. This requires the assumption that all probe liquid retention is due to adsorption solely to the sample, and that the interactions between the probe molecules are negligible.,

For cellulose and nanomaterials made thereof, IGC has been used to assess the surface energies of wood-based and cotton fibers,,, MCC,, CNFs,,, and CNCs, nanostructured cellulose II particles, and even amorphous cellulose, although the reliability of the analysis of amorphous samples may be affected by probe diffusion into the material.

In the context of cellulose–water interactions, the possibility to determine the surface energy components at different relative humidity values offers insights into the rearrangements that take place when cellulose is subjected to moisture (Figure 23c,d). Differences in cellulose reactivity have been reported, depending on the utilized drying method, and it is likely that the measured surface energies are also sensitive to such effects, as evidenced by XPS and contact angle measurements.

Gas Permeability Studies

Several standardized tests exist for the permeability of various gases through a number of polymeric materials. Here, we will only consider water vapor permeability measurements of cellulosic films, although the permeability of other gases through cellulose nanopapers also increases at relative humidity values of approximately 70–80%., The simplest way to assess the water vapor permeability of cellulose nanopapers is gravimetrically, by the so-called wet cup method, although corrections have been proposed to the method., In the common wet cup setup, a sealable cup is filled with a constant volume of distilled water, covered tightly by the tested material, and placed on the top of a balance that records weight loss as a function of evaporation time.,, Relative humidity inside the cup is assumed to be 100%, and the relative humidity outside the cup can be controlled by the use of saturated salt solutions, for example., An analogous but reversed setup (i.e., the dry cup method) also exists, where a desiccant material is used on one side of the material (Figure 23e,f).

This diffusion-driven process is sensitive to changes in temperature and relative humidity (and thereby partial pressure) on both sides of the nanopaper, and meaningful comparisons of mass transfer rates can only be made when these factors are kept constant. Obviously, properties of the nanopaper such as thickness, crystallinity, porosity, and pore size as well as pore structure, and hydrophilicity, also influence mass transfer rate, and it is usually necessary to characterize these properties in combination with the measured WVTR values to truly understand the material behavior. WVTR can be calculated from the steady-state region of the mass loss:where Δm is the change in sample mass, A is the evaporation area, and t is time.

Obviously, the underlying phenomena in WVTR are related to mass transport as elaborated in section 2.4.2.4. As the foremost application potential of cellulose nanopapers is as barrier films, the focus research in the field has largely been on improving their barrier properties in humid conditions,,,, rather than maintaining efficient mass transfer across the nanopaper. As the transport of gases and liquids proceed differently, and it is easier to block the flow of liquid water with its high cohesion and surface tension than that of individual water molecules.

Liquid Permeability Studies

In the nanocellulose literature, liquid water mass transfer values are often omitted from the experimental setup, even if different iterations of contact angles and WVTRs are frequently reported. The ease of dewatering during cellulose nanopaper preparation has received far more attention,,, than the permeability of liquid water through pre-existing cellulose nanopapers, although some accounts do exist (Figure 23g,h).,

For relatively water-permeable nanocellulose films, different flow tests have been applied which rely on either atmospheric pressure or an added pressure gradient for mass transfer,, and the permeated water is recorded as either volume or mass. Despite their tendency to swell and lose their gas barrier function in water, cellulose nanopapers can efficiently slow down the transport of liquid water. To characterize the mass transfer that is too slow to be meaningfully determined by gravimetric or volumetric methods (due to evaporation), an alternative strategy of employing tritium oxide labeling may be considered., In such a setup, a dual chamber is divided by the tested film and filled with deionized water simultaneously on both sides to avoid any pressure differences. Then, a small quantity of tritiated water (tritium oxide) is added on the donor side of the chamber, and the radioactivity of water on the acceptor side is monitored at regular time intervals (the measurement is carried out under constant stirring)., This technique is more cumbersome than gravimetric flow tests and requires special facilities suitable for working with radioisotopes.

Gravimetric Methods

Several gravimetric methods exist for the analysis of water retention and water uptake capacity of pulp and paper materials,,− and many of them have been applied to the analysis of nanocelluloses as well. In this section, we will move from more crude techniques such as water retention value (WRV) and Cobb tests to those of higher sensitivity such as DVS and QCM-D.

Water Retention Value and Cobb Test

The WRV and the Cobb test provide slightly different perspectives on the water retention and water uptake capacity of cellulosic materials. As the swelling ability of cellulosic materials depends on the pH and ionic strength of the solvent, and the charge group and counterion of the nanocellulose, these should be kept constant when running these types of analyses in order to yield comparable data., WRV can be used for the quantification of the liquid water that remains in a saturated cellulose sample after a controlled centrifugation cycle (i.e., a capillary swelling test) (Figure 24a,b), whereas in a Cobb test, a preconditioned cellulose sample is wet with a constant volume of water for a given time, followed by a rapid removal of any excess water.

The quantity of retained (WRV) or absorbed (Cobb test) water is then determined through gravimetric analysis. For WRV, the quantity of retained water is expressed as g of water per g of cellulose and calculated by eq 4:where m1 is the mass of the centrifuged wet test pad and m2 is the mass of the test pad after oven drying.

The Cobb test result, or absorptiveness, is expressed as g of water per m2 cellulose, and calculated by eq 5:where mw is the mass of the wet sample, mC is the mass of the conditioned sample, and the multiplication factor 100 is used for the standard specimen area of 100 cm2.

Both WRV and the Cobb test have been applied with slight modifications for the analysis of microfibrillated cellulose and CNFs,,− whereas WRV has been used to characterize BC. However, the characterization of CNCs using these means it is not advisible due to the risk of film disintegration and/or material loss during the experiments.

Dynamic Vapor Sorption Analysis (DVS)

DVS has been widely applied to study the adsorption–desorption behavior of gases on solids. In relation to cellulose–water interactions, it has been utilized extensively to study wood, various plant fibers, MCC, CNFs, and CNCs. In its most simple application, DVS can be used to quantify how much a given mass of material “takes up” water vapor at a given relative humidity and temperature (i.e., its equilibrium moisture content) (Figure 24c,d). The measuring device is essentially a high-precision mass balance that measures the weight of the sample at different relative humidity values (or partial pressures of gases other than water vapor) and temperatures. DVS can also be used to study the kinetics of the water uptake. The rate of adsorption and desorption of water from nanocellulose structures has been associated with the accessibility of cellulose hydroxy groups, another parameter frequently researched using DVS, often in conjunction with deuterium exchange., Moreover, cellulose hydroxy accessibility has been found to correlate well with the equilibrium moisture content of the material.,

When the relative humidity is increased and decreased gradually, a sigmoidal adsorption–desorption isotherm is obtained, the shape of which provides indirect information on material properties such as pore size, cumulation mechanism of the vapor (i.e., monolayer or multilayer formation), and capillary condensation.,, It should also be noted that the adsorption and desorption isotherms are different; this phenomenon is referred to as hysteresis, reminiscent of the difference between the advancing and receding contact angles. Part of the reason may lie in that the mechanisms of adsorption and desorption are different (sorption on an initially dry surface as opposed to evaporation from a capillary meniscus). Another proposed explanation is that the adsorption and desorption take place from different material states (a dry/collapsed vs a swollen one)., The sorption hysteresis of freeze-dried CNFs has been reported to be larger than that of CNCs, which is interpreted to be the result of the higher portion of disordered cellulose in CNFs. DVS data has been compared with that extracted from techniques such as WRV and thermoporometry, during both the initial building of a hydrated layer and after all of the material pores have been filled with water (i.e., saturation). DVS and thermoporometry data from macroscopic cellulose fibers by Driemeier et al. suggested that both the hysteresis behavior and wet porosity are the result of the suprafibrillar organization of cellulosic material and that there may be an “ink bottle” type of effect that would further explain the difficulty of water removal upon desorption.

The topic of sample preparation is crucial, especially when applied to nanocellulose. Usually, DVS experiments are carried out for predried samples that are wetted during the measurement, although it is in principle possible to dry the sample in situ while monitoring the weight loss of the sample. As discussed in sections 2.4.2.5, 3.1.1, and 3.2.1, all cellulosic materials undergo structural collapse upon drying, and this is especially true for CNFs that change from a swollen hydrogel state to a rigid film-like material. This structural collapse has an influence on the swelling ability and accessibility of nanocelluloses, as is evident from experiments attempting to redisperse dried CNFs− or modify them chemically., In practice, DVS analysis of celluloses (and especially of nanocelluloses), is influenced by the treatment and drying history of the material (e.g., air-dried from water or another solvent, freeze-dried, or supercritical drying). The structural changes affect the moisture sorption and retention in the material, and therefore special care should be devoted to the method of sample preparation to obtain relevant information on its water uptake properties. The main limitation of DVS is that it only provides quantitative assessment of the vapor uptake of a material, with no information about the structural changes that take place during the process such as swelling or changes in viscoelastic properties as is the case with QCM-D.

Quartz Crystal Microbalance with Dissipation Monitoring (QCM-D)

QCM-D is a microgravimetry technique which simultaneously measures changes in the resonance frequency and energy dissipation of an oscillating piezoelectric quartz crystal sensor as a result of changes in the mass of the crystal. Experiments can be carried out in both liquid and vapor environments, yielding quantitative information on the adsorption of, for example dissolved polymers or water vapor, respectively. QCM-D is a highly sensitive microbalance that detects extremely small changes (<1 ng/cm2) in mass of the sensor as a change in the oscillation frequency (Δf). For uniform and rigid layers, the change in mass of the sensor (Δm) is proportional to Δf, according to the Sauerbrey equation:where C is the sensitivity constant of the device (typically C ≈ 0.177 mg m2 Hz–1), and n is the measurement harmonic number (n = 1, 3, 5,...). The simultaneous monitoring of energy dissipation when the sensor stops oscillating provides a measure of the viscoelastic properties of the film. The dissipation of energy is defined through eq 7:where Elost is the dissipated energy during one cycle of oscillation and Estored is the total energy stored in the oscillator.

QCM-D therefore provides quantifiable information on the mass of adsorbed molecules onto an ultrathin model film and also yields information on the changes in the physical properties of the film as a result of adsorption. Indeed, a number of studies have been carried out on model films of regenerated cellulose,, CNCs,, and CNFs,, to better understand the swelling of these materials (Figure 24e,f). It is important to note that the method of film deposition onto the quartz sensors greatly influences film morphology and thereby also its water uptake capacity. For cellulose solutions, the main techniques of ultrathin film preparation on QCM sensors are spin-coating, and Langmuir–Schaeffer deposition,, the former being much faster but yielding films that are not in thermodynamic equilibrium, whereas Langmuir–Schaeffer films, are deposited slowly (one monolayer at a time), allowing for the organization of the cellulose into stable films. Spin-coating has been widely used for the preparation of CNF and CNC surfaces but accounts on their adsorption and electrophoretic deposition exist too. QCM-D has been used in multiple studies to determine the water adsorption capacity of the cellulose following a solvent-exchange protocol, whereby H2O is exchanged for D2O (originally on regenerated cellulose). Delepierre et al. used the same technique to measure the bound water in CNC films and reported that a decrease in remnant surface oligosaccharides of different grades of CNCs corresponded to an increase in the water binding capacity. Niinivaara et al. surface modified CNCs with oligosaccharides and used the same technique to show that oligosaccharide coated CNCs demonstrated slightly lower water adsorption capacities,

Nuclear Magnetic Resonance Spectroscopy (NMR)

13C solid-state NMR has long been recognized as viable tool to determine the degree of crystallinity of celluloses by taking advantage of variations in chemical shifts and 13C spin–lattice relaxation time constants in ordered and disordered molecular regions. Consequently, the amorphous and crystalline signals of the C4 and C6 carbon appear at a different chemical shift, and their ratio can be used to calculate degree of crystallinity with sufficient accuracy., Besides providing information on the molecular order of cellulose, different 1D and 2D solid-state NMR spectroscopy techniques are also used to characterize specific cellulose–water interactions. For instance, signals of surface crystalline domains observed through 13C CP/MAS NMR provide qualitative insights into the (irreversible) structural changes upon drying, as a consequence of cellulose microfibril aggregation (i.e., hornification)., As with many of the analytical techniques discussed, sample preparation is of particular importance here to ensure minimal changes to the cellulose crystallinity due to, for example, previous drying, milling, or chemical treatments., For example, Newman et al. were able to demonstrate changes within the surface crystalline domains of softwood kraft pulp simply due to wetting and drying cycles.

Both 1H and 2H (after a hydrogen–deuterium exchange) solid-state NMR experiments can be used to probe water interaction dynamics with nanocelluloses and gain an understanding of the state of the water present (i.e., free or bound water). 1H MAS NMR has also been used to investigate water mobility as a function of the moisture content. Vittadini et al. showed that with decreasing relative humidity (<12%), the 1H spectra of cellulose show a sharp Lorentzian signal typically observed for the free water component, and a wide Gaussian contribution, which dominated the spectrum at low relative humidity and was attributed to the rigid protons (i.e., low mobility) of the cellulose backbone and bound water.

High-resolution 2H NMR has significant advantages over 1H NMR for identifying different water populations in a cellulose sample as it is (i) selective toward accessible hydroxy groups and (ii) based on the quadrupolar coupling of intramolecular and single-spin properties, thus favoring intramolecular interactions., Combined, these features enable the identification and quantification of distinct water populations. Less mobile molecules (i.e., those with a slow 2H-exchange) give broad, Pake patterned 2H NMR spectra, while narrow Lorentzian peaks are typically observed for highly mobile molecules (i.e., those with a rapid 2H-exchange) (Figure 25a).,,2H single-pulse experiments are known to result in broad spectral components, making the interpretation of immobile domains at low water contents speculative. On the other hand, 2H static quadrupolar echo (QE) NMR provides a high-resolution information by refocusing the large quadrupolar broadening, which enables the observation of slow molecular dynamics. However, the experiment is restricted by a low signal-to-noise ratio (SNR), which complicates the identification and quantification of the different water populations.

Furthermore, 2H MAS NMR has been used to confirm the existence of an immobile and a mobile adsorbed water phase in hydrated cellulose, and to quantify the fraction of each population. Through magic angle spinning, orientation averaging can be used to remove chemical shift anisotropy and produce spectra resembling that of liquid water with an improved SNR. Such experiments rely mainly on the interpretation of spinning sidebands (SSBs) (i.e., the contribution of immobile water and cellulose 2HO) (Figure 25b), which become visible if the sample is spun at a rate less than the magnitude of the anisotropic interaction. The ratio of integrals and line width of the SSBs compared to the central peak (i.e., mobile water) at different relative humidity, thus providing direct quantitative information on the different adsorbed water phases after subtracting the contribution of cellulose deuteroxys. Furthermore, it provides information on the different locations of immobile and mobile adsorbed water on/within the microfibril aggregates. Moreover, 2H MAS NMR can provide information on the state of the cellulose hydroxy groups and site specific 1H–2H exchange.

In addition to 1D NMR experiments, 2D heteronuclear 1H–13C wide-line separation (WISE) NMR can provide information on water localization and organization in cellulose and cellulose–polymer blends. This technique is based on the correlation between a high-resolution 13C spectrum with a wide line 1H spectrum, where the proton line width refers to the polymer chain dynamics. Moreover, the insertion of a spin diffusion time enables direct observation of dipolar couplings between mobile water and cellulose protons, where the spin diffusion coefficient is related to the distance between cellulose and water.

Another approach to characterize cellulose–water interactions is through the acquisition of spin–lattice (i.e., longitudinal, T1) and spin–spin (i.e., transverse, T2) relaxation times using NMR relaxometry.,, The relaxation behavior of nuclei after excitation is a fingerprint in molecular dynamics that can provide information on, e.g., water adsorption. Terenzi et al. used 2H transverse and 13C longitudinal NMR relaxation measurements to assess the hydration of CNF/xyloglucan nanocomposites. The length and width of T2 as measured by 2H NMR provided information on the orientational molecular mobility of water molecules present in the nanocomposites, in addition to water molecule distribution and characteristic length scales, respectively. They demonstrated that a short T2 can be attributed to slow water mobility and, thus, strong polysaccharide–water interactions. On the other hand, T1, as measured by 13C CP/MAS, was used to quantify the difference in molecular mobility between ordered and disordered (including surface) regions in CNF as a function of relative humidity. Chen et al. compared molecular dynamic simulations and experimental relaxation data to quantify nanoscale structure–function relationships of CNFs in a highly hydrated and aggregated state. This approach enabled the deconvolution of experimental 13C NMR T1 distributions into contributions from both accessible and inaccessible regions of the aggregated CNFs and to distinguish between local C–H dynamics at different carbon sites (i.e., C1, C4, and C6) (Figure 25c). In addition to 13C and 2H, 17O relaxation data has also been used to study cellulose–water interactions. Similar to NMR relaxometry, low-field time domain (LF-TD) NMR can also be used to study the dynamic properties of polymer chains from the relaxation of 1H spins. Felby et al., for instance, used FT-TD NMR to study cellulose–water interactions during enzymatic hydrolysis.

Fourier Transform Infrared Spectroscopy (FTIR)

FTIR spectroscopy is commonly used to elucidate cellulose–water interactions. Particularly, it is sensitive toward differences in OH conformation and the hydrogen bonds of different cellulose polymorphs, even though the exact assignment of the strongly overlapping bands of cellulose hydroxy groups, and the different water populations is a matter of debate. For example, when observing cellulose–water interactions, strongly bound water is associated with the 3200 cm–1 band (−OH stretching range) in the cellulose spectrum, whereas the 3600 cm–1 band is associated with loosely bound water that bridges via another water molecule to cellulose. Moreover, the main spectral regions affected by water adsorption are between 3700 and 3000 cm–1 (mainly −OH stretch), 1740–1618 cm–1 (−OH bending), and 1190–1139 cm–1 (C–O–C asymmetric stretch of the glycosidic linkage)., Thereby, the signal at ca. 1640 cm–1 is very often loosely used as a reference for adsorbed water.−

Different IR instrumentation setups offer various possibilities to characterize cellulose–water interactions. Micro-FTIR is equipped with a light microscope, which allowed for the combined analysis of changes in sample morphology and in situ spectral analysis during water sorption. Polarized IR, on the other hand, relies on the polarization dependence of specific IR absorptions of oriented molecules and can be used to unravel the origins of the −OH signals found in the vibrational spectra of crystalline cellulose. Hofstetter et al. used dynamic FTIR, which couples dynamic mechanical analysis with step-scan FTIR and has better spectral resolution compared to static FTIR, due to the mechanical extension to investigate the interactions between cellulose and moisture. Moreover, the authors conducted a controlled 1H2O–2H2O (H2O–D2O) exchange, which provided direct evidence on the accessibility of the different cellulose domains, (Figure 25d).,,

Dielectric Spectroscopy (DS)

DS is a powerful tool to examine molecular motions of polymeric systems in an extended time span (0.1 ns to 100 s) by probing the dielectric properties of the material. Hence, the central prerequisite of this method is the existence of mobile molecular units with a permanent dipole moment or the presence of free mobile charges creating space charges at interfaces., In the case of cellulose, for example, only the dipolar sites (Figure 25e) in its specific orientation are of interest. The application of DS in cellulose research dates back over a century, and its principles, parametrizations, and experimental aspects are presented in an excellent way by Einfeldt et al.

In brief, DS measures the response of the dielectric properties of a material in an alternating electric field with a frequency range typically between 10–6 and 1012 Hz (i.e., broadband dielectric spectroscopy (BDS)) The latter is of particular relevance for cellulose, and in fact cellulose has often been characterized in the low-frequency range, i.e., by dielectric relaxation spectroscopy (DRS), in which the dielectric response is largely dominated by structural effects. Consequently, sample preparation for DRS analysis is highly important, and the dielectric response is highly sensitive to water content.

The response of the sample’s electric dipole moment (i.e., electric polarizability) is directly measured as complex impedance (Z*), giving the real (ε′, dielectric store coefficient) and the imaginary (ε″, dielectric loss coefficient) part of the complex permittivity (ε*(f, T))., Both parameters, ε′ and ε″, are central for the interpretation of cellulose–water systems and are typically recorded and interpreted as a function of the field frequency (f) and/or the temperature (T)., Isothermal measurements at varied frequencies are thereby favored because of their possible quantitative interpretation. Moreover, if the sample has a noticeable conductivity (e.g., wet samples), conductivity spectra (i.e., σ*(f, T)) are necessarily discussed.

As explained by Einfeldt et al., the macroscopic dipolar moment (Μ) considers all molecular groups with a permanent dipole moment, which in the case of cellulose is three types of dipolar and movable sites: (i) the pyranose ring (orientational motions around the glycosidic linkage), (ii) the C2/C3 side groups (rotational mobility around the C–O linkage), and (iii) the C6 side group (mobility around the C5–C6 linkage and the C6–O linkage). Water bound to cellulose hydroxy groups increases the dipolar moment of the side groups affecting the main polymer chain mobility and produces an additional relaxation process. Moreover, the polymeric relaxation, expressed by Μ and ε*, is affected by cross-correlation functions of different dipolar moments within the same chain and between neighboring chains, as a consequence of the complex hydrogen bonding network.

Parts e and f of Figure 25 show the different secondary relaxation processes for wet cellulose in the form of a dielectric loss (ε″) spectrum, in which β and βwet relaxations are the most relevant processes. They are observed below the glass transition temperature and in the low frequency range. β relaxations have been related to local motions of the main chain at low temperatures, whereas βwet relaxations are observed in wet samples in the room temperature range and are attributed to orientational motions of cellulose and water in a mixed phase., The latter disappears completely in dry samples and must be distinguished from σ relaxations which are observed for well-dried polysaccharides in the high temperature range. The relaxation strength of βwet relaxations decreases with lower water contents, accompanied by a shift of βwet to lower frequencies, which has been related to the effect of water on the activation energy of local polymer reorientational motions.,

The presence of water in a cellulose sample increases the electric conductivity, which superimposes the dielectric processes of the loss spectrum. This has been associated with the ionization of water, leading to an increase in the number of OH– and H+ ions. Thus, the dielectric loss spectrum must be corrected by a simultaneous measurement of the conductivity (σ0)., As consequence of the drastic effect of water on the electric conductivity of cellulose, the investigation of cellulose–water interactions and mixed-phase dielectric processes using DRS is limited to low water contents (max 12–15 wt %). Seemingly, low water contents (<6 wt %) do not affect the high frequency ε′ of cellulose, which is related to bound water that does not contribute to the dielectric response.

Sum Frequency Generation Vibration Spectroscopy (SFG-VS)

SFG-VS is a versatile method for in situ study of molecular arrangement at surfaces and interfaces. SFG is a second-order nonlinear optical process where a tunable pulse infrared (IR) laser beam is mixed by spatial and temporal overlap with a fixed wavelength visible (VIS) laser beam to generate a sum frequency output beam. Because SFG at the phase-matching condition require noncentrosymmetry, it is highly sensitive and specific to surfaces and interfaces as long as the bulk phase is amorphous or centrosymmetric., Crystalline cellulose bulk has a noncentrosymmetrical environment, which makes it difficult for SFG to confidently distinguish the OH groups of the surface vs bulk. However, regenerated cellulose models (amorphous cellulose),, would be a promising substrate for circumventing this problem with cellulose–water interface studies using SFG.

Spectroscopic Ellipsometry (SE)

SE is an optical technique which can be utilized to measure the thickness of thin films based on changes in the polarization of light as it is reflected through the film. A beam of single wavelength or spectroscopic light is passed through a polarizer, which is then reflected off the surface of a thin film. Traveling through the film, the light undergoes a change in its elliptic polarization dependent on the thickness (and porosity) of the film. The magnitude of the change in polarization can directly be used to model thin film properties such as thickness, refractive index, and extinction coefficient. For cellulosic materials, the classic Cauchy model is typically applicable to nonabsorbing transparent films, and as such is commonly used to model cellulose thin films. SE is a well-established and nonintrusive technique with very high precision and accuracy reaching a resolution in the order of 1 Å for optically uniform and transparent films. However, it is worth mentioning, that ellipsometry data is most meaningful when used in conjunction with complementary characterization techniques such as AFM, QCM-D, or surface plasmon resonance (SPR).

In terms of nanocellulose–water interactions, SE can be used to monitor changes in the film upon water vapor sorption in situ at the nanoscale (Figure 25g–i). Furthermore, because swelling upon water sorption in nanocellulose thin films is restricted only in the lateral dimension, SE can also be used to carry out volumetric analysis. For example, Niinivaara et al. unveiled that upon hydration with water vapor, each CNC in a spin-coated film become enveloped in a 1 nm thick layer of adsorbed water (or three monolayers of water molecules), resulting in a two nanometer increase in film thickness for every layer of CNCs within the film as measured by SE. Hakalahti et al. used SE (and QCM-D) for determination of thickness fractions of water in the TOCNF thin films in different relative humidity values. Thickness fractions of water in the TOCNF thin film were calculated by dividing the thickness increase due to water vapor sorption at a given point along the % relative humidity spectrum by the total thickness of the TOCNF thin film at the same % relative humidity point under the assumption that all changes in thickness or optical thickness occurred due to water vapor uptake. Hence, this method describes the added thickness due to sorption of water, but it does not differentiate between actual thickness of the water molecules and thickness changes in the film due to structural changes like swelling or reconfiguration of individual fibrils or hemicellulose.

Surface Plasmon Resonance Spectroscopy

SPR is a surface sensitive optical technique used to measure the adsorption/desorption of molecules or swelling of a thin film deposited onto a surface plasmon active metal substrate. P-polarized light is focused on the surface of the substrate resulting in the generation of a plasmonic wave at the substrate–film interface, the refractive index of which dictates the angle at which the light is coupled into the sensor to excite the plasmons. When a molecule binds (or adsorbs) to the surface of the substrate, or the film swells, the refractive index in the space where the plasmonic wave propagates is changed, as is the surface plasmon resonance angle., Multiparameter surface plasmon resonance spectroscopy (MP-SPR) acquires spectra which are dependent on the angle of the incident light in various media (i.e., gas or liquid) at different wavelengths (i.e., 670 and 785 nm) during a single experiment. From the data, one can deconvolute film thickness and effective refractive index based on optical modeling (using the Fresnel equations). Typically, the refractive index of nanocellulose is reported to range from 1.51 to 1.62.,,

To examine the swelling dynamics of CNC thin films, Reid et al. utilized SPR to monitor changes in film thickness as a function of CNC surface chemistry and charge density in various solvents and aqueous environments with different ionic strengths (Figure 25j–l). The authors found that while the total water uptake capacity of each film was similar due to the restrictions imposed be van der Waals forces between particles, the rate of swelling was highly dependent on CNC surface charge and solvent ionic strength. SPR has also been frequently used in the studies that include surface modification of nanocellulose films to tailor the interactions between nanocellulose and water. However, in these studies, SPR is mostly used to show the adsorption of the polymer on the surface. For example, Ahola et al. and Eronen et al. used SPR to surveil the adsorption profile of multiple synthetic and natural polymers on CNF films for the purpose of changing water binding capacity of the material.

Differential Scanning Calorimetry (DSC)

DSC is a thermoanalytical technique that measures the energy transferred to or from a sample undergoing a chemical or physical change as a function of temperature. The heat flow profiles attained through a DSC measurement (i.e., DSC curves) can be interpreted to provide detailed information on the enthalpies of transition of a material. When utilized on wet samples at low temperatures, DSC can yield direct information on the pore size distribution of the sample with a method called thermoporosimetry where the Gibbs–Thomson relation yields the relationship between melting point depression and capillary pore diameter. In practice, the sample is frozen, and an increasing temperature ramp detects the melting water in pores of varying size. In terms of cellulose–water interactions, DSC has been intensively investigated for its ability to quantitatively evaluate the different water populations in celluloses, i.e., the contents of free and bound water (section 2.4.2.2).,

The DSC curves of free water within cellulosic materials have similar profiles to that of pure water, indicating similar transition temperatures and enthalpies. Bound water, on the other hand, shows a lower transition temperature than that of pure water due to the restriction caused by the hydroxy groups of cellulose. The enthalpy of melting of freezing bound water adsorbed to cellulose can be quantified by integrating the area under the endothermic DSC curve (Figure 26a–f). In the case of celluloses, two exothermic peaks of crystallization of adsorbed water are observable during the cooling step: (i) a sharp peak at ca. 255 K for bound water (peak I) and (ii) a broad peak between 230 and 250 K (peak II), indicating free water and freezing bound water in cellulose (Figure 26i). The melting enthalpy can be plotted against the total water content in the cellulose sample (g water/g dry cellulose sample). Theoretically, the points should fall on a straight line with a slope equal to the heat of fusion of bulk water (ΔHf = 79.7 g cal–1) and an x-intercept showing the nonfreezing water content (ΔH = 0).

DSC can yield indirect information on the crystallinity and fiber structure of cellulosic materials,, as well as the accessibility of the cellulose hydroxy groups (Figure 26g,h)., As such, DSC can also help to garner an understanding on the effects of nanocellulose hornification as a result of removal of water. For instance, Ding et al. implemented DSC to demonstrate a collapse in the mesoporous structure of nanocellulose fibers and a subsequent loss in hydroxy group accessibility of redispersed nanocellulose upon the removal of water. Furthermore, DSC can also be used to attain information on the pore size distribution of a material such as a wet cellulose nanopaper. Thermoporosimetry is typically carried out after isothermal heating where temperature is kept constant until the enthalpy of melting has stabilized. This technique assumes that water contained within pores is subjected to elevated pressures and has a higher melting temperature than free water. Hence, the different isothermal melting points obtained during the measurements provide information about the number of pores and their respective size, as reported by Rojo et al. However, a clear limitation of DSC-based thermoporosimetry are nanocavities smaller than several Å, which cause the formation of nonfreezing water and might hinder an accurate size measurement.

Rheology

The rheological behavior of aqueous nanocellulose suspensions has been studied to determine the effects such as size or morphology, surface chemistry, and aspect ratio, which have been discussed in multiple comprehensive reviews.,,,,, Furthermore, the flow behavior of aqueous nanocellulose suspensions has been studied in dilute, semidilute, and concentrated regimes, all providing information related to nanocellulose–water interactions. Simply put, the dilute regime typically provides information on the aspect ratio of nanocelluloses and their particle–particle interactions, while the semidilute and concentrated regimes shed light on the viscoelastic properties and structure of suspensions as a function of the shear rate. Additionally, rheological measurements can provide in situ information on the dewatering of nanocellulose suspensions (Figure 27a,b). Dimic-Misic et al. studied the relationship between shear stress-induced dewatering of CNFs and microfibrillated (MFC)-containing furnishes and their rheological behavior., Dynamic dewatering as a function of shear was studied under vacuum in an immobilization cell combined with a rheometer. Dewatering led to an increase in the elastic modulus and viscosity of the suspension as a function of the increase in solids content. The shear-thinning behavior of the cellulosic materials was thereby found to be the central feature influencing shear-induced dewatering and was related to the creation of dewatering channels. Moreover, the work showed the surface charges of both MFC and CNFs affect both rheological and dewatering properties, which was attributed to fibrillar swelling and nonremovable surface-bound water.

Dynamic Mechanical Analysis (DMA)

DMA is a characterization technique used to measure the viscoelastic properties of a material under an oscillating load as a function of oscillation frequency and temperature. While DMA has mostly been used to investigate the effect of water on the performance of (mostly) nanocellulose nanocomposite materials, it can also provide insights into the reversible water-response different types of materials.,

Utilizing DMA, Hakalahti et al. compared the mechanical properties of TOCNF/poly(vinyl alcohol) (PVA) films in both the dry and wet state to demonstrate that PVA significantly improved the wet stability of the films (Figure 27c,d). In a different study, Capadona et al. also used DMA to understand the reversible water response of sea cucumber-like CNC reinforced polymer composites (Figure 27e–g). DMA analysis showed that upon contact changes in composite modulus, elongation at break, and tensile strength were the result of “switching off” the CNC–CNC interactions through water adsorption. Conversely, in the dry state, strong hydrogen bonding between the CNCs maximized the stress transfer and improved the modulus of the nanocomposite. Zhu et al. used DMA to understand the mechanisms behind the shape-memory and the water sensitivity of a CNC/TPUs (thermoplastic polyurethane) nanocomposite. They also evaluated the reversibility of the change in modulus by repeated drying–wetting cycles.

Small-Angle Scattering (SAS)

Small-angle X-ray scattering (SAXS) and small-angle neutron scattering (SANS) are able to provide information on the structure and morphology of nanocellulose on a multiscale length,,− although data interpretation can be complex. One of the major benefits of small-angle scattering techniques is that changes in sample properties can be measured in real time when exposed to an external force. For example, the alignment of CNCs in aqueous suspension in a relatively weak (0–1.2 T) and strong (up to 6.8 T) magnetic field has been monitored in situ using SAXS and SANS, respectively. Furthermore, Håkansson et al. utilized SAXS to detect nanocellulose hydrodynamic alignment in filaments produced using a flow focusing device. This approach gave very detailed information on the dynamics and parameters affecting the aligned assembly of CNF and CNC using such a set up., Lastly, the self-assembly of sulfated CNCs upon drying and rewetting was measured in situ by Liu et al. using time-resolved SAXS (Figure 28a–c). They were able to quantitatively follow the nanoscale assembly of CNCs and the reswelling of the dry structure upon hydration as a function of the counterion of the sulfate half ester charge group (hydrogen or lithium).

Using SAXS, Guccini et al. assessed the influence of atmospheric moisture content on the structure of carboxylated CNF membrane as a function of surface charge and counterion. Strips of the membranes were introduced to a humidity-controlled cell, while the scattering pattern was recorded. The team was able to track the formation of pores and water channels within the nanofiber network in a range of 55–95% relative humidity and concluded that the amount of water absorbed and the swelling increases with the surface charge density of the CNF and decreases with the substitution of sodium with hydrogen ions. Others have also used small-angle scattering to understand the liquid crystalline properties of CNC suspensions as a functions of solids content, total surface charge, and ionic strength,,, while fewer reports are available regarding the nematic ordering of CNF suspensions using SAS.,

Using grazing incident SANS (GISANS), Brett et al. studied the morphological features of ultrasmooth carboxylated CNF thin films as a function of relative humidity. They observed that the size of the three-dimensional CNF aggregates were not affected by an increase in humidity, but their average distance increased as more water is absorbed and condensed into the films. Compared to microscopic techniques such as TEM and SEM, GISANS (and GISAXS) have versatile sample environments do not require some degree of electrical conductivity and are able to scan a bigger area with high resolution and fast acquisition rates both parallel and perpendicular to the sample surface. Valencia et al. monitored the effect of water flow during a filtration process across a porous membrane of carboxylated CNFs. Using SAXS, they were able to monitor changes in the porosity of the membranes during filtration and assess the antifouling performance of the membrane. An interesting feature specific to SANS is the possibility to contrast-match (or make components “invisible” to the neutron beam) individual components of a multicomponent system by varying the H2O/D2O ratio, which allows one to study individual characteristics and structural features. O’Neil et al. used this technique in SANS to selectively highlight the effect of hydration on BC surface and to compare the nanostructure and bulk morphology of dry and hydrated BC (Figure 28d–f).

Inelastic Scattering (IS)

The dynamics of water in nanocellulose can be directly probed as a function of temperature using inelastic scattering methods as quasielastic neutron scattering (QENS) and inelastic neutron scattering (INS). The information accessible through these techniques are characteristics of a length scale ranging from Ångstroms to a few tens of nanometers level, and the phenomena probed are within the time scales from a fraction of picoseconds to microseconds. The results given by INS are resolved according to the change of the kinetic energy of the sample interacting with the neutron beam.

The applications of these techniques on nanocellulose–water systems may not have reached their full potential as there are less reports available compared to other techniques. Nonetheless, Müller et al. investigate the dynamics of water within cellulose using INS, concluding the water accessible sites correspond to the disordered cellulose chains mostly located on the surface of CNFs (Figure 28h). The peculiarity of QENS is to quantitatively determine the dynamical relaxation processes of water to distinguish between localized rotational and long-range translational motions. This characteristic has been used to determine how the hydration level affect the water dynamics within cellulose and its mechanical properties. As mentioned in section 4.1, O’Neil et al. detected two populations of water within crystalline BC depending on their relaxation dynamics as a function of temperature, one consisted of surface bound water and the other of confined bound water (Figure 28g). Guccini et al. were able to detect two types of motions for the water inside a TOCNF network by QENS: one with fast, localized movement of water molecules and the other with slower, diffusive motion. The slower motion was independent of the surface charge of the TOCNFs.

Future Trends in Nanocellulose–Water Interactions

As implied by the very title of this contribution, the role of water in nanocellulosic materials is considered ambiguous. While many regard water as a problematic component in, e.g., nanopaper or composite structures, it is in fact a necessity in hydrogel-based structures. Much of the potential of water in, for instance, smart materials and energy-related applications entailing nanocellulose has not materialized, and it is the task of the coming years to push the research further in this respect. Perhaps the biggest quest is to merge fundamental knowledge of nanocellulose structures and cellulose–water interactions with design and buildup of new functional materials from nanocellulose. Properties like injectability, responsive behavior, thermal and electrical conductivity, and just chemical modification of cellulose to reach a certain property are strongly linked to water interactions.

Overall, the dominant trend in future is to adhere to the principles of green chemistry more avidly, not just in research but within the whole society, and water-based systems are in a central role in those principles. Because of the vast amount of knowledge that has been gathered over the years on cellulose–water interactions, we know that water is compatible with cellulose and the behavior of cellulose–water systems can be largely, if not fully, predicted. Therefore, processing cellulose in water will need to be the goal even in those cases when ultimately hydrophobic bioproducts are the end goal. These premises will dictate the future development of truly sustainable production and usage of cellulose-based materials. Figure 29 summarizes the future outlook in the field of nanocellulose–water interactions.

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    Li T.; Chen C.; Brozena A. H.; Zhu J.; Xu L.; Driemeier C.; Dai J.; Rojas O. J.; Isogai A.; Wågberg L.; Hu L. Developing Fibrillated Cellulose as a Sustainable Technological Material. Nature 2021, 590, 47–56..

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    Yilmaz N.; Kodama Y.; Numata K. Revealing the Architecture of the Cell Wall in Living Plant Cells by Bioimaging and Enzymatic Degradation. Biomacromolecules 2020, 21, 95–103..

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    Scallan A.; Tigerström A. Swelling and Elasticity of the Cell Walls of Pulp Fibres. J. Pulp Pap. Sci. 1992, 18, J188–J193.

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    Maloney T. C.; Paulapuro H.; Stenius P. Hydration and Swelling of Pulp Fibers Measured with Differential Scanning Calorimetry. Nordic Pulp Pap. Res. J. 1998, 13, 31–36..

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    Nechyporchuk O.; Belgacem M. N.; Bras J. Production of Cellulose Nanofibrils: A Review of Recent Advances. Ind. Crops Prod. 2016, 93, 2–25..

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    Aarne N.; Kontturi E.; Laine J. Influence of Adsorbed Polyelectrolytes on Pore Size Distribution of a Water-Swollen Biomaterial. Soft Matter 2012, 8, 4740–4749..

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    Daicho K.; Kobayashi K.; Fujisawa S.; Saito T. Recovery of the Irreversible Crystallinity of Nanocellulose by Crystallite Fusion: A Strategy for Achieving Efficient Energy Transfers in Sustainable Biopolymer Skeletons. Angew. Chem., Int. Ed. 2021, 60, 24630–24636..

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    Newman R. H. Carbon-13 NMR Evidence for Cocrystallization of Cellulose as a Mechanism for Hornification of Bleached Kraft Pulp. Cellulose 2004, 11, 45–52..

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    Solala I.; Driemeier C.; Mautner A.; Penttilä P. A.; Seitsonen J.; Leppänen M.; Mihhels K.; Kontturi E. Directed Assembly of Cellulose Nanocrystals in Its Native Solid State Template of a Natural Fiber. Macromol. Rapid Commun. 2021, 42, 2100092.

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    Pääkkönen T.; Spiliopoulos P.; Nonappa; Kontturi K. S.; Penttilä P.; Viljanen M.; Svedström K.; Kontturi E. Sustainable High Yield Route to Cellulose Nanocrystals from Bacterial Cellulose. ACS Sustainable Chem. Eng. 2019, 7, 14384–14388..

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    Suchy M.; Virtanen J.; Kontturi E.; Vuorinen T. Impact of Drying on Wood Ultrastructure Observed by Deuterium Exchange and Photoacoustic Ft-Ir Spectroscopy. Biomacromolecules 2010, 11, 515–520..

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    Suchy M.; Kontturi E.; Vuorinen T. Impact of Drying on Wood Ultrastructure: Similarities in Cell Wall Alteration between Native Wood and Isolated Wood-Based Fibers. Biomacromolecules 2010, 11, 2161–2168..

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    Htun M.; de Ruvo A. Relation between drying stresses and internal stresses and the mechanical properties of paper. In Fiber–Water Interactions in Papermaking, Transactions of the VIth Fundamental Research Symposium, Oxford, 1977; Fundamental Research Committee: Manchester, UK, 2018; pp 477–487.

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    de Yong J.; Higgins H. G.; Irvine G. M. Moisture response of thermomechanical and other fibres. In Fiber–Water Interactions in Papermaking, Transactions of the VIth Fundamental Research Symposium, Oxford, 1977; Fundamental Research Committee: Manchester, UK, 2018; pp 589–606.

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    Huang S.; Makarem M.; Kiemle S. N.; Zheng Y.; He X.; Ye D.; Gomez E. W.; Gomez E. D.; Cosgrove D. J.; Kim S. H. Dehydration-Induced Physical Strains of Cellulose Microfibrils in Plant Cell Walls. Carbohydr. Polym. 2018, 197, 337–348..

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    Jarvis M. C. Structure of Native Cellulose Microfibrils, the Starting Point for Nanocellulose Manufacture. Philosophical Trans. R. Soc. A 2018, 376, 20170045.

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    Steele D. F.; Moreton R. C.; Staniforth J. N.; Young P. M.; Tobyn M. J.; Edge S. Surface Energy of Microcrystalline Cellulose Determined by Capillary Intrusion and Inverse Gas Chromatography. AAPS J. 2008, 10, 494–503..

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    Paajanen A.; Zitting A.; Rautkari L.; Ketoja J. A.; Penttilä P. A. Nanoscale Mechanism of Moisture-Induced Swelling in Wood Microfibril Bundles. Nano Lett. 2022, 22, 5143–5150..

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    Zhang S.; Zhang F.; Jin L.; Liu B.; Mao Y.; Liu Y.; Huang J. Preparation of Spherical Nanocellulose from Waste Paper by Aqueous Naoh/Thiourea. Cellulose 2019, 26, 5177–5185..

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    Satyamurthy P.; Vigneshwaran N. A Novel Process for Synthesis of Spherical Nanocellulose by Controlled Hydrolysis of Microcrystalline Cellulose Using Anaerobic Microbial Consortium. Enzyme Microb. Technol. 2013, 52, 20–25..

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    Abitbol T.; Rivkin A.; Cao Y.; Nevo Y.; Abraham E.; Ben-Shalom T.; Lapidot S.; Shoseyov O. Nanocellulose, a Tiny Fiber with Huge Applications. Curr. Opin. Biotechnol. 2016, 39, 76–88..

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    Schütz C.; Agthe M.; Fall A. B.; Gordeyeva K.; Guccini V.; Salajkova M.; Plivelic T. S.; Lagerwall J. P.; Salazar-Alvarez G.; Bergström L. Rod Packing in Chiral Nematic Cellulose Nanocrystal Dispersions Studied by Small-Angle X-Ray Scattering and Laser Diffraction. Langmuir 2015, 31, 6507–6513..

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    Guccini V.; Yu S.; Agthe M.; Gordeyeva K.; Trushkina Y.; Fall A.; Schütz C.; Salazar-Alvarez G. Inducing Nematic Ordering of Cellulose Nanofibers Using Osmotic Dehydration. Nanoscale 2018, 10, 23157–23163..

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    Dufresne A.; Cavaillé J. Y.; Vignon M. R. Mechanical Behavior of Sheets Prepared from Sugar Beet Cellulose Microfibrils. J. Appl. Polym. Sci. 1997, 64, 1185–1194..

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    Habibi Y.; Goffin A.-L.; Schiltz N.; Duquesne E.; Dubois P.; Dufresne A. Bionanocomposites Based on Poly (Ε-Caprolactone)-Grafted Cellulose Nanocrystals by Ring-Opening Polymerization. J. Mater. Chem. 2008, 18, 5002–5010..

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  124. 124.

    Barud H. S.; Barrios C.; Regiani T.; Marques R. F.; Verelst M.; Dexpert-Ghys J.; Messaddeq Y.; Ribeiro S. J. Self-Supported Silver Nanoparticles Containing Bacterial Cellulose Membranes. Materials Science and Engineering: C 2008, 28, 515–518..

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    Saito T.; Isogai A. Tempo-Mediated Oxidation of Native Cellulose. The Effect of Oxidation Conditions on Chemical and Crystal Structures of the Water-Insoluble Fractions. Biomacromolecules 2004, 5, 1983–1989..

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    Henriksson M.; Berglund L. A.; Isaksson P.; Lindstrom T.; Nishino T. Cellulose Nanopaper Structures of High Toughness. Biomacromolecules 2008, 9, 1579–1585..

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    Hoeng F.; Denneulin A.; Bras J. Use of Nanocellulose in Printed Electronics: A Review. Nanoscale 2016, 8, 13131–13154..

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    Isogai A.; Bergström L. Preparation of Cellulose Nanofibers Using Green and Sustainable Chemistry. Curr. Opin. Green Sustainable Chem. 2018, 12, 15–21..

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    Schütz C.; Bruckner J. R.; Honorato-Rios C.; Tosheva Z.; Anyfantakis M.; Lagerwall J. P. From Equilibrium Liquid Crystal Formation and Kinetic Arrest to Photonic Bandgap Films Using Suspensions of Cellulose Nanocrystals. Crystals 2020, 10, 199.

    Not in our library10.3390/cryst10030199

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    Fleming K.; Gray D. G.; Matthews S. Cellulose Crystallites. Chem.–Eur. J. 2001, 7, 1831–1836..

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  132. 132.

    Dong X. M.; Revol J.-F.; Gray D. G. Effect of Microcrystallite Preparation Conditions on the Formation of Colloid Crystals of Cellulose. Cellulose 1998, 5, 19–32..

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    Lorenz M.; Sattler S.; Reza M.; Bismarck A.; Kontturi E. Cellulose Nanocrystals by Acid Vapour: Towards More Effortless Isolation of Cellulose Nanocrystals. Faraday Discuss. 2017, 202, 315–330..

    Not in our library10.1039/c7fd00053g

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    Dong X. M.; Gray D. G. Effect of Counterions on Ordered Phase Formation in Suspensions of Charged Rodlike Cellulose Crystallites. Langmuir 1997, 13, 2404–2409..

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    Niu F.; Li M.; Huang Q.; Zhang X.; Pan W.; Yang J.; Li J. The Characteristic and Dispersion Stability of Nanocellulose Produced by Mixed Acid Hydrolysis and Ultrasonic Assistance. Carbohydr. Polym. 2017, 165, 197–204..

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  136. 136.

    Roman M.; Winter W. T. Effect of Sulfate Groups from Sulfuric Acid Hydrolysis on the Thermal Degradation Behavior of Bacterial Cellulose. Biomacromolecules 2004, 5, 1671–1677..

    Not in our library10.1021/bm034519+

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    Luo J.; Semenikhin N.; Chang H.; Moon R. J.; Kumar S. Post-Sulfonation of Cellulose Nanofibrils with a One-Step Reaction to Improve Dispersibility. Carbohydr. Polym. 2018, 181, 247–255..

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    Kontturi E. Preparation of Cellulose Nanocrystals: Background, Conventions and New Developments; Lee K.-Y., Ed., CRC Press: Boca Raton, FL, 2018; pp 27–44.

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    Camarero Espinosa S.; Kuhnt T.; Foster E. J.; Weder C. Isolation of Thermally Stable Cellulose Nanocrystals by Phosphoric Acid Hydrolysis. Biomacromolecules 2013, 14, 1223–1230..

    Not in our library10.1021/bm400219u

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    Vanderfleet O. M.; Osorio D. A.; Cranston E. D. Optimization of Cellulose Nanocrystal Length and Surface Charge Density through Phosphoric Acid Hydrolysis. Philosophical Trans. R. Soc. A 2018, 376, 20170041.

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    Chen L.; Zhu J. Y.; Baez C.; Kitin P.; Elder T. Highly Thermal-Stable and Functional Cellulose Nanocrystals and Nanofibrils Produced Using Fully Recyclable Organic Acids. Green Chem. 2016, 18, 3835–3843..

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    Peyre J.; Pääkkönen T.; Reza M.; Kontturi E. Simultaneous Preparation of Cellulose Nanocrystals and Micron-Sized Porous Colloidal Particles of Cellulose by Tempo-Mediated Oxidation. Green Chem. 2015, 17, 808–811..

    Not in our library10.1039/c4gc02001d

  143. 143.

    Vanderfleet O. M.; Cranston E. D. Production Routes to Tailor the Performance of Cellulose Nanocrystals. Nature Rev. Mater. 2021, 6, 124–144..

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    Trache D.; Hussin M. H.; Haafiz M. K. M.; Thakur V. K. Recent Progress in Cellulose Nanocrystals: Sources and Production. Nanoscale 2017, 9, 1763–1786..

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    Revol J.-F.; Bradford H.; Giasson J.; Marchessault R.; Gray D. Helicoidal Self-Ordering of Cellulose Microfibrils in Aqueous Suspension. Int. J. Biol. Macromol. 1992, 14, 170–172..

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    Lagerwall J. P.; Schütz C.; Salajkova M.; Noh J.; Hyun Park J.; Scalia G.; Bergström L. Cellulose Nanocrystal-Based Materials: From Liquid Crystal Self-Assembly and Glass Formation to Multifunctional Thin Films. NPG Asia Mater. 2014, 6, e80–e80..

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    Kelly J. A.; Giese M.; Shopsowitz K. E.; Hamad W. Y.; MacLachlan M. J. The Development of Chiral Nematic Mesoporous Materials. Acc. Chem. Res. 2014, 47, 1088–1096..

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    Jacucci G.; Schertel L.; Zhang Y.; Yang H.; Vignolini S. Light Management with Natural Materials: From Whiteness to Transparency. Adv. Mater. 2021, 33, 2001215.

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    Jozala A. F.; de Lencastre-Novaes L. C.; Lopes A. M.; de Carvalho Santos-Ebinuma V.; Mazzola P. G.; Pessoa-Jr A.; Grotto D.; Gerenutti M.; Chaud M. V. Bacterial Nanocellulose Production and Application: A 10-Year Overview. Appl. Microbiol. Biotechnol. 2016, 100, 2063–2072..

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  150. 150.

    Yamamoto H.; Horn F. In Situ Crystallization of Bacterial Cellulose I. Influences of Polymeric Additives, Stirring and Temperature on the Formation Celluloses Iα and Iβ as Revealed by Cross Polarization/Magic Angle Spinning (CP/MAS) 13 C NMR Spectroscopy. Cellulose 1994, 1, 57–66..

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    Picheth G. F.; Pirich C. L.; Sierakowski M. R.; Woehl M. A.; Sakakibara C. N.; de Souza C. F.; Martin A. A.; da Silva R.; de Freitas R. A. Bacterial Cellulose in Biomedical Applications: A Review. Int. J. Biol. Macromol. 2017, 104, 97–106..

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  153. 153.

    Ogawa Y. Electron Microdiffraction Reveals the Nanoscale Twist Geometry of Cellulose Nanocrystals. Nanoscale 2019, 11, 21767–21774..

    Not in our library10.1039/c9nr06044h

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    Conley K.; Godbout L.; Whitehead M. T.; van de Ven T. G. Origin of the Twist of Cellulosic Materials. Carbohydr. Polym. 2016, 135, 285–299..

    Not in our library10.1016/j.carbpol.2015.08.029

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    Matthews J. F.; Skopec C. E.; Mason P. E.; Zuccato P.; Torget R. W.; Sugiyama J.; Himmel M. E.; Brady J. W. Computer Simulation Studies of Microcrystalline Cellulose Iβ. Carbohydr. Res. 2006, 341, 138–152..

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  156. 156.

    Paavilainen S.; Róg T.; Vattulainen I. Analysis of Twisting of Cellulose Nanofibrils in Atomistic Molecular Dynamics Simulations. J. Phys. Chem. B 2011, 115, 3747–3755..

    Not in our library10.1021/jp111459b

  157. 157.

    Gray D. G.; Mu X. Twist–Bend Stage in the Relaxation of Sheared Chiral Nematic Suspensions of Cellulose Nanocrystals. ACS Omega 2016, 1, 212–219..

    Not in our library10.1021/acsomega.6b00100

  158. 158.

    Xie H.; Du H.; Yang X.; Si C. Recent Strategies in Preparation of Cellulose Nanocrystals and Cellulose Nanofibrils Derived from Raw Cellulose Materials. Int. J. Polym. Sci. 2018, 2018, 1.

    Not in our library10.1155/2018/7923068

  159. 159.

    Obodovskiy I. Radiation: Fundamentals, Applications, Risks, and Safety; Elsevier: Amsterdam, 2019.

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  160. 160.

    Fleming K. L.; Pfaendtner J. Characterizing the Catalyzed Hydrolysis of β-1, 4 Glycosidic Bonds Using Density Functional Theory. J. Phys. Chem. A 2013, 117, 14200–14208..

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  161. 161.

    Buffiere J.; Balogh-Michels Z.; Borrega M.; Geiger T.; Zimmermann T.; Sixta H. The Chemical-Free Production of Nanocelluloses from Microcrystalline Cellulose and Their Use as Pickering Emulsion Stabilizer. Carbohydr. Polym. 2017, 178, 48–56..

    Not in our library10.1016/j.carbpol.2017.09.028

  162. 162.

    Olanrewaju K. B. Reaction Kinetics of Cellulose Hydrolysis in Subcritical and Supercritical Water. Ph.D. Thesis. University of Iowa, 2012.

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  163. 163.

    Novo L. P.; Bras J.; García A.; Belgacem N.; Curvelo A. A. Subcritical Water: A Method for Green Production of Cellulose Nanocrystals. ACS Sustainable Chem. Eng. 2015, 3, 2839–2846..

    Not in our library10.1021/acssuschemeng.5b00762

  164. 164.

    Novo L. P.; Bras J.; García A.; Belgacem N.; da Silva Curvelo A. A. A Study of the Production of Cellulose Nanocrystals through Subcritical Water Hydrolysis. Ind. Crops Prod. 2016, 93, 88–95..

    Not in our library10.1016/j.indcrop.2016.01.012

  165. 165.

    Li L.; Zhuang J.; Zou H.; Pang J.; Yu S. Partition Usage of Cellulose by Coupling Approach of Supercritical Carbon Dioxide and Cellulase to Reducing Sugar and Nanocellulose. Carbohydr. Polym. 2020, 229, 115533.

    Not in our library10.1016/j.carbpol.2019.115533

  166. 166.

    Chen P.; Shrotri A.; Fukuoka A. Unraveling the Hydrolysis of Β-1, 4-Glycosidic Bonds in Cello-Oligosaccharides over Carbon Catalysts. Catal. Sci. Technol. 2020, 10, 4593–4601..

    Not in our library10.1039/d0cy00783h

  167. 167.

    To A. T.; Chung P. W.; Katz A. Weak-Acid Sites Catalyze the Hydrolysis of Crystalline Cellulose to Glucose in Water: Importance of Post-Synthetic Functionalization of the Carbon Surface. Angew. Chem., Int. Ed. 2015, 54, 11050–11053..

    Not in our library10.1002/anie.201504865

  168. 168.

    Huang Y.-B.; Fu Y. Hydrolysis of Cellulose to Glucose by Solid Acid Catalysts. Green Chem. 2013, 15, 1095–1111..

    Not in our library10.1039/c3gc40136g

  169. 169.

    Suganuma S.; Nakajima K.; Kitano M.; Yamaguchi D.; Kato H.; Hayashi S.; Hara M. Hydrolysis of Cellulose by Amorphous Carbon Bearing SO3H, COOH, and OH Groups. J. Am. Chem. Soc. 2008, 130, 12787–12793..

    Not in our library10.1021/ja803983h

  170. 170.

    Hu S.; Jiang F.; Hsieh Y.-L. 1d Lignin-Based Solid Acid Catalysts for Cellulose Hydrolysis to Glucose and Nanocellulose. ACS Sustainable Chem. Eng. 2015, 3, 2566–2574..

    Not in our library10.1021/acssuschemeng.5b00780

  171. 171.

    Zeng M.; Pan X. Insights into Solid Acid Catalysts for Efficient Cellulose Hydrolysis to Glucose: Progress, Challenges, and Future Opportunities. Catal. Rev. 2022, 64, 445–490..

    Not in our library10.1080/01614940.2020.1819936

  172. 172.

    Lin Y.-C.; Huber G. W. The Critical Role of Heterogeneous Catalysis in Lignocellulosic Biomass Conversion. Energy Environ. Sci. 2009, 2, 68–80..

    Not in our library10.1039/b814955k

  173. 173.

    Lanzafame P.; Temi D.; Perathoner S.; Spadaro A.; Centi G. Direct Conversion of Cellulose to Glucose and Valuable Intermediates in Mild Reaction Conditions over Solid Acid Catalysts. Catal. Today 2012, 179, 178–184..

    Not in our library10.1016/j.cattod.2011.07.018

  174. 174.

    Dutta S. Catalytic Materials That Improve Selectivity of Biomass Conversions. RSC Adv. 2012, 2, 12575–12593..

    Not in our library10.1039/c2ra20922e

  175. 175.

    Fan L.-t.; Gharpuray M. M.; Lee Y.-H. Cellulose Hydrolysis; Springer Science & Business Media, 2012.

    Not in our library

  176. 176.

    Chen H. Lignocellulose Biorefinery Engineering: Principles and Applications; Woodhead Publishing: Sawston, Cambridge, UK, 2015.

    Not in our library

  177. 177.

    Cabiac A.; Guillon E.; Chambon F.; Pinel C.; Rataboul F.; Essayem N. Cellulose Reactivity and Glycosidic Bond Cleavage in Aqueous Phase by Catalytic and Non Catalytic Transformations. Appl. Catal., A 2011, 402, 1–10..

    Not in our library10.1016/j.apcata.2011.05.029

  178. 178.

    Björnerbäck F.; Hedin N. Microporous Humins Prepared from Sugars and Bio-Based Polymers in Concentrated Sulfuric Acid. ACS Sustainable Chem. Eng. 2019, 7, 1018–1027..

    Not in our library10.1021/acssuschemeng.8b04658

  179. 179.

    Isahak W. N. R. W.; Hisham M. W. M.; Yarmo M. A. Highly Porous Carbon Materials from Biomass by Chemical and Carbonization Method: A Comparison Study. J. Chem. 2013, 2013, 620346.

    Not in our library10.1155/2013/620346

  180. 180.

    Avci A.; Saha B. C.; Kennedy G. J.; Cotta M. A. High Temperature Dilute Phosphoric Acid Pretreatment of Corn Stover for Furfural and Ethanol Production. Ind. Crops Prod. 2013, 50, 478–484..

    Not in our library10.1016/j.indcrop.2013.07.055

  181. 181.

    Yarbrough J. M.; Zhang R.; Mittal A.; Vander Wall T.; Bomble Y. J.; Decker S. R.; Himmel M. E.; Ciesielski P. N. Multifunctional Cellulolytic Enzymes Outperform Processive Fungal Cellulases for Coproduction of Nanocellulose and Biofuels. ACS Nano 2017, 11, 3101–3109..

    Not in our library10.1021/acsnano.7b00086

  182. 182.

    Vermaas J. V.; Kont R.; Beckham G. T.; Crowley M. F.; Gudmundsson M.; Sandgren M.; Ståhlberg J.; Väljamäe P.; Knott B. C. The Dissociation Mechanism of Processive Cellulases. Proc. Natl. Acad. Sci. U.S.A. 2019, 116, 23061–23067..

    Not in our library10.1073/pnas.1913398116

  183. 183.

    Ye Z.; Berson R. E. Kinetic Modeling of Cellulose Hydrolysis with First Order Inactivation of Adsorbed Cellulase. Bioresour. Technol. 2011, 102, 11194–11199..

    Not in our library10.1016/j.biortech.2011.09.044

  184. 184.

    Rezaei K.; Jenab E.; Temelli F. Effects of Water on Enzyme Performance with an Emphasis on the Reactions in Supercritical Fluids. Crit. Rev. Biotechnol. 2007, 27, 183–195..

    Not in our library10.1080/07388550701775901

  185. 185.

    Cavaco-Paulo A. Mechanism of Cellulase Action in Textile Processes. Carbohydr. Polym. 1998, 37, 273–277..

    Not in our library10.1016/s0144-8617(98)00070-8

  186. 186.

    Zhang K.; Zhang Y.; Yan D.; Zhang C.; Nie S. Enzyme-Assisted Mechanical Production of Cellulose Nanofibrils: Thermal Stability. Cellulose 2018, 25, 5049–5061..

    Not in our library10.1007/s10570-018-1928-7

  187. 187.

    Nie S.; Zhang K.; Lin X.; Zhang C.; Yan D.; Liang H.; Wang S. Enzymatic Pretreatment for the Improvement of Dispersion and Film Properties of Cellulose Nanofibrils. Carbohydr. Polym. 2018, 181, 1136–1142..

    Not in our library10.1016/j.carbpol.2017.11.020

  188. 188.

    Nie S.; Zhang C.; Zhang Q.; Zhang K.; Zhang Y.; Tao P.; Wang S. Enzymatic and Cold Alkaline Pretreatments of Sugarcane Bagasse Pulp to Produce Cellulose Nanofibrils Using a Mechanical Method. Ind. Crops Prod. 2018, 124, 435–441..

    Not in our library10.1016/j.indcrop.2018.08.033

  189. 189.

    Perzon A.; Jørgensen B.; Ulvskov P. Sustainable Production of Cellulose Nanofiber Gels and Paper from Sugar Beet Waste Using Enzymatic Pre-Treatment. Carbohydr. Polym. 2020, 230, 115581.

    Not in our library10.1016/j.carbpol.2019.115581

  190. 190.

    Bian H.; Chen L.; Dong M.; Fu Y.; Wang R.; Zhou X.; Wang X.; Xu J.; Dai H. Cleaner Production of Lignocellulosic Nanofibrils: Potential of Mixed Enzymatic Treatment. J. Cleaner Prod. 2020, 270, 122506.

    Not in our library10.1016/j.jclepro.2020.122506

  191. 191.

    Song K.; Ji Y.; Wang L.; Wei Y.; Yu Z. A Green and Environmental Benign Method to Extract Cellulose Nanocrystal by Ball Mill Assisted Solid Acid Hydrolysis. J. Cleaner Prod. 2018, 196, 1169–1175..

    Not in our library10.1016/j.jclepro.2018.06.128

  192. 192.
  193. 193.

    Fu X.; Ji H.; Wang B.; Zhu W.; Pang Z.; Dong C. Preparation of Thermally Stable and Surface-Functionalized Cellulose Nanocrystals by a Fully Recyclable Organic Acid and Ionic Liquid Mediated Technique under Mild Conditions. Cellulose 2020, 27, 1289–1299..

    Not in our library10.1007/s10570-019-02875-2

  194. 194.

    Wang H.; Li J.; Zeng X.; Tang X.; Sun Y.; Lei T.; Lin L. Extraction of Cellulose Nanocrystals Using a Recyclable Deep Eutectic Solvent. Cellulose 2020, 27, 1301–1314..

    Not in our library10.1007/s10570-019-02867-2

  195. 195.

    Matsuki S.; Kayano H.; Takada J.; Kono H.; Fujisawa S.; Saito T.; Isogai A. Nanocellulose Production Via One-Pot Formation of C2 and C3 Carboxylate Groups Using Highly Concentrated Naclo Aqueous Solution. ACS Sustainable Chem. Eng. 2020, 8, 17800–17806..

    Not in our library10.1021/acssuschemeng.0c06515

  196. 196.

    Lee M.; Heo M. H.; Lee H.; Lee H.-H.; Jeong H.; Kim Y.-W.; Shin J. Facile and Eco-Friendly Extraction of Cellulose Nanocrystals Via Electron Beam Irradiation Followed by High-Pressure Homogenization. Green Chem. 2018, 20, 2596–2610..

    Not in our library10.1039/c8gc00577j

  197. 197.

    Kim H. G.; Lee U. S.; Kwac L. K.; Lee S. O.; Kim Y.-S.; Shin H. K. Electron Beam Irradiation Isolates Cellulose Nanofiber from Korea “Tall Goldenrod” Invasive Alien Plant Pulp. Nanomaterials 2019, 9, 1358.

    Not in our library10.3390/nano9101358

  198. 198.

    Dee S. J.; Bell A. T. A Study of the Acid-Catalyzed Hydrolysis of Cellulose Dissolved in Ionic Liquids and the Factors Influencing the Dehydration of Glucose and the Formation of Humins. ChemSusChem 2011, 4, 1166–1173..

    Not in our library10.1002/cssc.201000426

  199. 199.

    Penttilä P. A.; Paajanen A.; Ketoja J. A. Combining Scattering Analysis and Atomistic Simulation of Wood-Water Interactions. Carbohydr. Polym. 2021, 251, 117064.

    Not in our library10.1016/j.carbpol.2020.117064

  200. 200.

    Sanjaya R. E.; Putri K. D. A.; Kurniati A.; Rohman A.; Puspaningsih N. N. T. In Silico Characterization of the Gh5-Cellulase Family from Uncultured Microorganisms: Physicochemical and Structural Studies. J. Genet. Eng. Biotechnol. 2021, 19, 143.

    Not in our library10.1186/s43141-021-00236-w

  201. 201.

    Bettotti P.; Scarpa M. Nanocellulose and Its Interface: On the Road to the Design of Emerging Materials. Adv. Mater. Interfaces 2022, 9, 2101593.

    Not in our library10.1002/admi.202101593

  202. 202.

    Reishofer D.; Spirk S. Deuterium and Cellulose: A Comprehensive Review. In Cellulose Chemistry and Properties: Fibers, Nanocelluloses and Advanced Materials; Rojas O. J., Ed.; Springer International, 2016; pp 93–114.

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  203. 203.

    Lindh E. L.; Bergenstråhle-Wohlert M.; Terenzi C.; Salmén L.; Furó I. Non-Exchanging Hydroxyl Groups on the Surface of Cellulose Fibrils: The Role of Interaction with Water. Carbohydr. Res. 2016, 434, 136–142..

    Not in our library10.1016/j.carres.2016.09.006

  204. 204.

    Hofstetter K.; Hinterstoisser B.; Salmén L. Moisture Uptake in Native Cellulose–the Roles of Different Hydrogen Bonds: A Dynamic FT-IR Study Using Deuterium Exchange. Cellulose 2006, 13, 131–145..

    Not in our library10.1007/s10570-006-9055-2

  205. 205.

    Väisänen S.; Pönni R.; Hämäläinen A.; Vuorinen T. Quantification of Accessible Hydroxyl Groups in Cellulosic Pulps by Dynamic Vapor Sorption with Deuterium Exchange. Cellulose 2018, 25, 6923–6934..

    Not in our library10.1007/s10570-018-2064-0

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    Lindh E. L.; Salmén L. Surface Accessibility of Cellulose Fibrils Studied by Hydrogen–Deuterium Exchange with Water. Cellulose 2017, 24, 21–33..

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    Salmén L.; Bergström E. Cellulose Structural Arrangement in Relation to Spectral Changes in Tensile Loading Ftir. Cellulose 2009, 16, 975–982..

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    Ibbett R.; Wortmann F.; Varga K.; Schuster K. C. A Morphological Interpretation of Water Chemical Exchange and Mobility in Cellulose Materials Derived from Proton NMR T 2 Relaxation. Cellulose 2014, 21, 139–152..

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    Tammelin T.; Abburi R.; Gestranius M.; Laine C.; Setälä H.; Österberg M. Correlation between Cellulose Thin Film Supramolecular Structures and Interactions with Water. Soft Matter 2015, 11, 4273–4282..

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    Zabler S.; Paris O.; Burgert I.; Fratzl P. Moisture Changes in the Plant Cell Wall Force Cellulose Crystallites to Deform. J. Struct. Biol. 2010, 171, 133–141..

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    Müller M.; Czihak C.; Schober H.; Nishiyama Y.; Vogl G. All Disordered Regions of Native Cellulose Show Common Low-Frequency Dynamics. Macromolecules 2000, 33, 1834–1840..

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    Nishiyama Y.; Isogai A.; Okano T.; Müller M.; Chanzy H. Intracrystalline Deuteration of Native Cellulose. Macromolecules 1999, 32, 2078–2081..

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    Driemeier C.; Bragatto J. Crystallite Width Determines Monolayer Hydration across a Wide Spectrum of Celluloses Isolated from Plants. J. Phys. Chem. B 2013, 117, 415–421..

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    Stana-Kleinschek K.; Strnad S.; Ribitsch V. Surface Characterization and Adsorption Abilities of Cellulose Fibers. Polym. Eng. Sci. 1999, 39, 1412–1424..

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    Paajanen A.; Sonavane Y.; Ignasiak D.; Ketoja J. A.; Maloney T.; Paavilainen S. Atomistic Molecular Dynamics Simulations on the Interaction of TEMPO-Oxidized Cellulose Nanofibrils in Water. Cellulose 2016, 23, 3449–3462..

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    Cao T.; Elimelech M. Colloidal Stability of Cellulose Nanocrystals in Aqueous Solutions Containing Monovalent, Divalent, and Trivalent Inorganic Salts. J. Colloid Interface Sci. 2021, 584, 456–463..

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    Parsons D. F.; Ninham B. W. Surface Charge Reversal and Hydration Forces Explained by Ionic Dispersion Forces and Surface Hydration. Colloids Surf., A 2011, 383, 2–9..

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    Marcus Y. Effect of Ions on the Structure of Water: Structure Making and Breaking. Chem. Rev. 2009, 109, 1346–1370..

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    Kalashnikova I.; Bizot H.; Cathala B.; Capron I. Modulation of Cellulose Nanocrystals Amphiphilic Properties to Stabilize Oil/Water Interface. Biomacromolecules 2012, 13, 267–275..

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    Biermann O.; Hädicke E.; Koltzenburg S.; Müller-Plathe F. Hydrophilicity and Lipophilicity of Cellulose Crystal Surfaces. Angew. Chem., Int. Ed. 2001, 40, 3822–3825..

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    Heiner A. P.; Teleman O. Interface between Monoclinic Crystalline Cellulose and Water: Breakdown of the Odd/Even Duplicity. Langmuir 1997, 13, 511–518..

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    Alqus R.; Eichhorn S. J.; Bryce R. A. Molecular Dynamics of Cellulose Amphiphilicity at the Graphene–Water Interface. Biomacromolecules 2015, 16, 1771–1783..

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    Johansson L.-S.; Tammelin T.; Campbell J. M.; Setälä H.; Österberg M. Experimental Evidence on Medium Driven Cellulose Surface Adaptation Demonstrated Using Nanofibrillated Cellulose. Soft Matter 2011, 7, 10917–10924..

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    Cordeiro N.; Mendonça C.; Pothan L. A.; Varma A. Monitoring Surface Properties Evolution of Thermochemically Modified Cellulose Nanofibres from Banana Pseudo-Stem. Carbohydr. Polym. 2012, 88, 125–131..

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    Deepa B.; Abraham E.; Cordeiro N.; Mozetic M.; Mathew A. P.; Oksman K.; Faria M.; Thomas S.; Pothan L. A. Utilization of Various Lignocellulosic Biomass for the Production of Nanocellulose: A Comparative Study. Cellulose 2015, 22, 1075–1090..

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    Belgacem M. N.; Czeremuszkin G.; Sapieha S.; Gandini A. Surface by XPS Characterization and Inverse Gas of Cellulose Fibres Chromatography. Cellulose 1995, 2, 145–157..

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    Ly B.; Belgacem M.N.; Bras J.; Brochier Salon M.C. Grafting of Cellulose by Fluorine-Bearing Silane Coupling Agents. Mater. Sci. Eng., C 2010, 30, 343–347..

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    Beaumont M.; Kondor A.; Plappert S.; Mitterer C.; Opietnik M.; Potthast A.; Rosenau T. Surface Properties and Porosity of Highly Porous, Nanostructured Cellulose II Particles. Cellulose 2017, 24, 435–440..

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    Faria M.; Vilela C.; Silvestre A. J.; Deepa B.; Resnik M.; Freire C. S.; Cordeiro N. Physicochemical Surface Properties of Bacterial Cellulose/Polymethacrylate Nanocomposites: An Approach by Inverse Gas Chromatography. Carbohydr. Polym. 2019, 206, 86–93..

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    Kontturi E.; Suchy M.; Penttilä P.; Jean B.; Pirkkalainen K.; Torkkeli M.; Serimaa R. Amorphous Characteristics of an Ultrathin Cellulose Film. Biomacromolecules 2011, 12, 770–777..

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    Phanthong P.; Reubroycharoen P.; Hao X.; Xu G.; Abudula A.; Guan G. Nanocellulose: Extraction and Application. Carbon Resour. Convers. 2018, 1, 32–43..

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    Chu Y.; Sun Y.; Wu W.; Xiao H. Dispersion Properties of Nanocellulose: A Review. Carbohydr. Polym. 2020, 250, 116892.

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    Isogai A. Emerging Nanocellulose Technologies: Recent Developments. Adv. Mater. 2021, 33, 2000630.

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    Dhali K.; Ghasemlou M.; Daver F.; Cass P.; Adhikari B. A Review of Nanocellulose as a New Material Towards Environmental Sustainability. Sci. Total Environ. 2021, 775, 145871.

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    Thomas P.; Duolikun T.; Rumjit N. P.; Moosavi S.; Lai C. W.; Bin Johan M. R.; Fen L. B. Comprehensive Review on Nanocellulose: Recent Developments, Challenges and Future Prospects. J. Mech. Behav. Biomed. Mater. 2020, 110, 103884.

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    Solala I.; Bordes R.; Larsson A. Water Vapor Mass Transport across Nanofibrillated Cellulose Films: Effect of Surface Hydrophobization. Cellulose 2018, 25, 347–356..

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    Chibowski E.; Gonzalez-Caballero F. Theory and Practice of Thin-Layer Wicking. Langmuir 1993, 9, 330–340..

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    Peng Y.; Gardner D. J.; Han Y.; Cai Z.; Tshabalala M. A. Influence of Drying Method on the Surface Energy of Cellulose Nanofibrils Determined by Inverse Gas Chromatography. J. Colloid Interface Sci. 2013, 405, 85–95..

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    Cai J.; Zhang L. Rapid Dissolution of Cellulose in LiOH/Urea and NaOH/Urea Aqueous Solutions. Macromol. Biosci. 2005, 5, 539–548..

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    Chen F.; Sawada D.; Hummel M.; Sixta H.; Budtova T. Swelling and Dissolution Kinetics of Natural and Man-Made Cellulose Fibers in Solvent Power Tuned Ionic Liquid. Cellulose 2020, 27, 7399–7415..

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    Medronho B.; Lindman B. Competing Forces During Cellulose Dissolution: From Solvents to Mechanisms. Curr. Opin. Colloid Interface Sci. 2014, 19, 32–40..

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    Heinze T.; Koschella A. Solvents Applied in the Field of Cellulose Chemistry: A Mini Review. Polímeros 2005, 15, 84–90..

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    Fink H.-P.; Weigel P.; Purz H.; Ganster J. Structure Formation of Regenerated Cellulose Materials from Nmmo-Solutions. Prog. Polym. Sci. 2001, 26, 1473–1524..

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    Liebert T. Cellulose Solvents–Remarkable History, Bright Future. ACS Symp. Ser. 2010, 1033, 3–54..

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    Zhu S.; Wu Y.; Chen Q.; Yu Z.; Wang C.; Jin S.; Ding Y.; Wu G. Dissolution of Cellulose with Ionic Liquids and Its Application: A Mini-Review. Green Chem. 2006, 8, 325–327..

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    Peterson A. A.; Vogel F.; Lachance R. P.; Fröling M.; Antal M. J. Jr; Tester J. W. Thermochemical Biofuel Production in Hydrothermal Media: A Review of Sub-and Supercritical Water Technologies. Energy Environ. Sci. 2008, 1, 32–65..

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    Liu Y.; Stoeckel D.; Gordeyeva K.; Agthe M.; Schutz C.; Fall A. B.; Bergström L. Nanoscale Assembly of Cellulose Nanocrystals During Drying and Redispersion. ACS Macro Lett. 2018, 7, 172–177..

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    Nordenström M.; Fall A.; Nyström G.; Wågberg L. Formation of Colloidal Nanocellulose Glasses and Gels. Langmuir 2017, 33, 9772–9780..

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    Maestri C.; Abrami M.; Hazan S.; Chistè E.; Golan Y.; Rohrer J.; Bernkop-Schnürch A.; Grassi M.; Scarpa M.; Bettotti P. Role of Sonication Pre-Treatment and Cation Valence in the Sol-Gel Transition of Nano-Cellulose Suspensions. Sci. Rep. 2017, 7, 11129.

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    Tanaka H.; Meunier J.; Bonn D. Nonergodic States of Charged Colloidal Suspensions: Repulsive and Attractive Glasses and Gels. Phys. Rev. E 2004, 69, 031404.

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    Zaccarelli E. Colloidal Gels: Equilibrium and Non-Equilibrium Routes. J. Phys.: Condens. Matter 2007, 19, 323101.

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    Zhao M.; Ansari F.; Takeuchi M.; Shimizu M.; Saito T.; Berglund L. A.; Isogai A. Nematic Structuring of Transparent and Multifunctional Nanocellulose Papers. Nanoscale Horiz. 2018, 3, 28–34..

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    Lindh E. L.; Terenzi C.; Salmén L.; Furó I. Water in Cellulose: Evidence and Identification of Immobile and Mobile Adsorbed Phases by 2H MAS NMR. Phys. Chem. Chem. Phys. 2017, 19, 4360–4369..

    Not in our library10.1039/c6cp08219j

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    Niinivaara E.; Faustini M.; Tammelin T.; Kontturi E. Water Vapor Uptake of Ultrathin Films of Biologically Derived Nanocrystals: Quantitative Assessment with Quartz Crystal Microbalance and Spectroscopic Ellipsometry. Langmuir 2015, 31, 12170–12176..

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    Nakamura K.; Hatakeyama T.; Hatakeyama H. Studies on Bound Water of Cellulose by Differential Scanning Calorimetry. Text. Res. J. 1981, 51, 607–613..

    Not in our library10.1177/004051758105100909

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    O’Neill H.; Pingali S. V.; Petridis L.; He J.; Mamontov E.; Hong L.; Urban V.; Evans B.; Langan P.; Smith J. C.; Davison B. H. Dynamics of Water Bound to Crystalline Cellulose. Sci. Rep. 2017, 7, 11840.

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    Langan P.; Petridis L.; O’Neill H. M.; Pingali S. V.; Foston M.; Nishiyama Y.; Schulz R.; Lindner B.; Hanson B. L.; Harton S.; et al. Common Processes Drive the Thermochemical Pretreatment of Lignocellulosic Biomass. Green Chem. 2014, 16, 63–68..

    Not in our library10.1039/c3gc41962b

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    Luukkonen P.; Maloney T.; Rantanen J.; Paulapuro H.; Yliruusi J. Microcrystalline Cellulose-Water Interaction—a Novel Approach Using Thermoporosimetry. Pharm. Res. 2001, 18, 1562–1569..

    Not in our library10.1023/a:1013030414555

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    Kittle J. D.; Du X.; Jiang F.; Qian C.; Heinze T.; Roman M.; Esker A. R. Equilibrium Water Contents of Cellulose Films Determined Via Solvent Exchange and Quartz Crystal Microbalance with Dissipation Monitoring. Biomacromolecules 2011, 12, 2881–2887..

    Not in our library10.1021/bm200352q

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    Aulin C.; Ahola S.; Josefsson P.; Nishino T.; Hirose Y.; Österberg M.; Wågberg L. Nanoscale Cellulose Films with Different Crystallinities and Mesostructures— Their Surface Properties and Interaction with Water. Langmuir 2009, 25, 7675–7685..

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    Niinivaara E.; Faustini M.; Tammelin T.; Kontturi E. Mimicking the Humidity Response of the Plant Cell Wall by Using Two-Dimensional Systems: The Critical Role of Amorphous and Crystalline Polysaccharides. Langmuir 2016, 32, 2032–2040..

    Not in our library10.1021/acs.langmuir.5b04264

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    Pirich C. L.; de Freitas R. A.; Torresi R. M.; Picheth G. F.; Sierakowski M. R. Piezoelectric Immunochip Coated with Thin Films of Bacterial Cellulose Nanocrystals for Dengue Detection. Biosens. Bioelectron. 2017, 92, 47–53..

    Not in our library10.1016/j.bios.2017.01.068

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    Wilson B. P.; Yliniemi K.; Gestranius M.; Hakalahti M.; Putkonen M.; Lundström M.; Karppinen M.; Tammelin T.; Kontturi E. Structural Distinction Due to Deposition Method in Ultrathin Films of Cellulose Nanofibres. Cellulose 2018, 25, 1715–1724..

    Not in our library10.1007/s10570-018-1665-y

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    Kontturi K. S.; Kontturi E.; Laine J. Specific Water Uptake of Thin Films from Nanofibrillar Cellulose. J. Mater. Chem. A 2013, 1, 13655–13663..

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    Hakalahti M.; Faustini M.; Boissière C. d.; Kontturi E.; Tammelin T. Interfacial Mechanisms of Water Vapor Sorption into Cellulose Nanofibril Films as Revealed by Quantitative Models. Biomacromolecules 2017, 18, 2951–2958..

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    Reid M. S.; Kedzior S. A.; Villalobos M.; Cranston E. D. Effect of Ionic Strength and Surface Charge Density on the Kinetics of Cellulose Nanocrystal Thin Film Swelling. Langmuir 2017, 33, 7403–7411..

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    Reid M. S.; Villalobos M.; Cranston E. D. Cellulose Nanocrystal Interactions Probed by Thin Film Swelling to Predict Dispersibility. Nanoscale 2016, 8, 12247–12257..

    Not in our library10.1039/c6nr01737a

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    Ponni R.; Kontturi E.; Vuorinen T. Accessibility of Cellulose: Structural Changes and Their Reversibility in Aqueous Media. Carbohydr. Polym. 2013, 93, 424–429..

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    Lucas R. Ueber Das Zeitgesetz Des Kapillaren Aufstiegs Von Flüssigkeiten. Kolloid-Z. 1918, 23, 15–22..

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    Washburn E. W. The Dynamics of Capillary Flow. Phys. Rev. 1921, 17, 273.

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    Chibowski E.; Holysz L. Use of the Washburn Equation for Surface Free Energy Determination. Langmuir 1992, 8, 710–716..

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    Costanzo P.; Giese R.; van Oss C. The Determination of Surface Tension Parameters of Powders by Thin Layer Wicking. In Advances in Measurement and Control of Colloidal Processes; Williams R. A., de Jaeger N. C., Eds., Elsevier: Amsterdam, 1991; pp 223–232.

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    Bedane A. H.; Eić M.; Farmahini-Farahani M.; Xiao H. Theoretical Modeling of Water Vapor Transport in Cellulose-Based Materials. Cellulose 2016, 23, 1537–1552..

    Not in our library10.1007/s10570-016-0917-y

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    Bedane A. H.; Xiao H.; Eić M. Water Vapor Adsorption Equilibria and Mass Transport in Unmodified and Modified Cellulose Fiber-Based Materials. Adsorption 2014, 20, 863–874..

    Not in our library10.1007/s10450-014-9628-6

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    Bertuzzi M. A.; Castro Vidaurre E. F.; Armada M.; Gottifredi J. Water Vapor Permeability of Edible Starch Based Films. J. Food Eng. 2007, 80, 972–978..

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    Gårdebjer S.; Larsson M.; Gebäck T.; Skepö M.; Larsson A. An Overview of the Transport of Liquid Molecules through Structured Polymer Films, Barriers and Composites–Experiments Correlated to Structure-Based Simulations. Adv. Colloid Interface Sci. 2018, 256, 48–64..

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    Shogren R. Water Vapor Permeability of Biodegradable Polymers. J. Environ. Polym. Degrad. 1997, 5, 91–95..

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    Andersson H.; Hjärtstam J.; Stading M.; von Corswant C.; Larsson A. Effects of Molecular Weight on Permeability and Microstructure of Mixed Ethyl-Hydroxypropyl-Cellulose Films. Eur. J. Pharm. Sci. 2013, 48, 240–248..

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    Philibert J. One and a Half Century of Diffusion: Fick, Einstein, before and beyond. Diffusion Fundamentals 2006, 6, 1.

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    Solala I.; Bordes R.; Larsson A. Water Vapor Mass Transport across Nanofibrillated Cellulose Films: Effect of Surface Hydrophobization. Cellulose 2018, 25, 347–356..

    Not in our library10.1007/s10570-017-1608-z

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    Bedane A. H.; Eić M.; Farmahini-Farahani M.; Xiao H. Water Vapor Transport Properties of Regenerated Cellulose and Nanofibrillated Cellulose Films. J. Membr. Sci. 2015, 493, 46–57..

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    Sinquefield S.; Ciesielski P. N.; Li K.; Gardner D. J.; Ozcan S. Nanocellulose Dewatering and Drying: Current State and Future Perspectives. ACS Sustainable Chem. Eng. 2020, 8, 9601.

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    Amini E. N.; Tajvidi M.; Bousfield D. W.; Gardner D. J.; Shaler S. M. Dewatering Behavior of a Wood-Cellulose Nanofibril Particulate System. Sci. Rep. 2019, 9, 14584.

    Not in our library10.1038/s41598-019-51177-x

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    Rantanen J.; Maloney T. C. Consolidation and Dewatering of a Microfibrillated Cellulose Fiber Composite Paper in Wet Pressing. Eur. Polym. J. 2015, 68, 585–591..

    Not in our library10.1016/j.eurpolymj.2015.03.045

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    Clayton S.; Scholes O. N.; Hoadley A. F. A.; Wheeler R. A.; McIntosh M. J.; Huynh D. Q. Dewatering of Biomaterials by Mechanical Thermal Expression. Drying Technol. 2006, 24, 819–834..

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    Sethi J.; Oksman K.; Illikainen M.; Sirviö J. A. Sonication-Assisted Surface Modification Method to Expedite the Water Removal from Cellulose Nanofibers for Use in Nanopapers and Paper Making. Carbohydr. Polym. 2018, 197, 92–99..

    Not in our library10.1016/j.carbpol.2018.05.072

  304. 304.

    Wetterling J.; Jonsson S.; Mattsson T.; Theliander H. The Influence of Ionic Strength on the Electroassisted Filtration of Microcrystalline Cellulose. Ind. Eng. Chem. Res. 2017, 56, 12789–12798..

    Not in our library10.1021/acs.iecr.7b03575

  305. 305.

    Wetterling J.; Sahlin K.; Mattsson T.; Westman G.; Theliander H. Electroosmotic Dewatering of Cellulose Nanocrystals. Cellulose 2018, 25, 2321–2329..

    Not in our library10.1007/s10570-018-1733-3

  306. 306.

    Sim K.; Lee J.; Lee H.; Youn H. J. Flocculation Behavior of Cellulose Nanofibrils under Different Salt Conditions and Its Impact on Network Strength and Dewatering Ability. Cellulose 2015, 22, 3689–3700..

    Not in our library10.1007/s10570-015-0784-y

  307. 307.

    Dimic-Misic K.; Puisto A.; Paltakari J.; Alava M.; Maloney T. The Influence of Shear on the Dewatering of High Consistency Nanofibrillated Cellulose Furnishes. Cellulose 2013, 20, 1853–1864..

    Not in our library10.1007/s10570-013-9964-9

  308. 308.

    Dimic-Misic K.; Maloney T.; Liu G.; Gane P. Micro Nanofibrillated Cellulose (MNFC) Gel Dewatering Induced at Ultralow-Shear in Presence of Added Colloidally-Unstable Particles. Cellulose 2017, 24, 1463–1481..

    Not in our library10.1007/s10570-016-1181-x

  309. 309.

    Dimic-Misic K.; Maloney T.; Gane P. Effect of Fibril Length, Aspect Ratio and Surface Charge on Ultralow Shear-Induced Structuring in Micro and Nanofibrillated Cellulose Aqueous Suspensions. Cellulose 2018, 25, 117–136..

    Not in our library10.1007/s10570-017-1584-3

  310. 310.

    Dimic-Misic K.; Puisto A.; Gane P.; Nieminen K.; Alava M.; Paltakari J.; Maloney T. The Role of MFC/NFC Swelling in the Rheological Behavior and Dewatering of High Consistency Furnishes. Cellulose 2013, 20, 2847–2861..

    Not in our library10.1007/s10570-013-0076-3

  311. 311.

    Liu G.; Maloney T.; Dimic-Misic K.; Gane P. Acid Dissociation of Surface Bound Water on Cellulose Nanofibrils in Aqueous Micro Nanofibrillated Cellulose (MNFC) Gel Revealed by Adsorption of Calcium Carbonate Nanoparticles under the Application of Ultralow Shear. Cellulose 2017, 24, 3155–3178..

    Not in our library10.1007/s10570-017-1371-1

  312. 312.

    Laaksonen T.; Helminen J. K.; Lemetti L.; Långbacka J.; Rico del Cerro D.; Hummel M.; Filpponen I.; Rantamäki A. H.; Kakko T.; Kemell M. L.; et al. WTF-Nano: One-Pot Dewatering and Water-Free Topochemical Modification of Nanocellulose in Ionic Liquids or Γ-Valerolactone. ChemSusChem 2017, 10, 4879–4890..

    Not in our library10.1002/cssc.201701344

  313. 313.

    Li K.; Choudhary H.; Rogers R. D. Ionic Liquids for Sustainable Processes: Liquid Metal Catalysis. Curr. Opin. Green Sustainable Chem. 2018, 11, 15–21..

    Not in our library10.1016/j.cogsc.2018.02.011

  314. 314.

    Guccini V.; Phiri J.; Trifol J.; Rissanen V.; Mousavi S. M.; Vapaavuori J.; Tammelin T.; Maloney T.; Kontturi E. Tuning the Porosity, Water Interaction, and Redispersion of Nanocellulose Hydrogels by Osmotic Dehydration. ACS Appl. Polym. Mater. 2022, 4, 24–28..

    Not in our library10.1021/acsapm.1c01430

  315. 315.

    Peng Y.; Gardner D. J.; Han Y. Drying Cellulose Nanofibrils: In Search of a Suitable Method. Cellulose 2012, 19, 91–102..

    Not in our library10.1007/s10570-011-9630-z

  316. 316.

    Baez C.; Considine J.; Rowlands R. Influence of Drying Restraint on Physical and Mechanical Properties of Nanofibrillated Cellulose Films. Cellulose 2014, 21, 347–356..

    Not in our library10.1007/s10570-013-0159-1

  317. 317.

    Li K.; Skolrood L. N.; Aytug T.; Tekinalp H.; Ozcan S. Strong and Tough Cellulose Nanofibrils Composite Films: Mechanism of Synergetic Effect of Hydrogen Bonds and Ionic Interactions. ACS Sustainable Chem. Eng. 2019, 7, 14341–14346..

    Not in our library10.1021/acssuschemeng.9b03442

  318. 318.

    Lovikka V. A.; Khanjani P.; Väisänen S.; Vuorinen T.; Maloney T. C. Porosity of Wood Pulp Fibers in the Wet and Highly Open Dry State. Microporous Mesoporous Mater. 2016, 234, 326–335..

    Not in our library10.1016/j.micromeso.2016.07.032

  319. 319.

    Aulin C.; Netrval J.; Wågberg L.; Lindström T. Aerogels from Nanofibrillated Cellulose with Tunable Oleophobicity. Soft Matter 2010, 6, 3298–3305..

    Not in our library10.1039/c001939a

  320. 320.

    Lavoine N.; Bergström L. Nanocellulose-Based Foams and Aerogels: Processing, Properties, and Applications. J. Mater. Chem. A 2017, 5, 16105–16117..

    Not in our library10.1039/c7ta02807e

  321. 321.

    Han J.; Zhou C.; Wu Y.; Liu F.; Wu Q. Self-Assembling Behavior of Cellulose Nanoparticles During Freeze-Drying: Effect of Suspension Concentration, Particle Size, Crystal Structure, and Surface Charge. Biomacromolecules 2013, 14, 1529–1540..

    Not in our library10.1021/bm4001734

  322. 322.

    Deville S. Freeze-Casting of Porous Biomaterials: Structure, Properties and Opportunities. Materials 2010, 3, 1913–1927..

    Not in our library10.3390/ma3031913

  323. 323.

    Voronova M. I.; Zakharov A. G.; Kuznetsov O. Y.; Surov O. V. The Effect of Drying Technique of Nanocellulose Dispersions on Properties of Dried Materials. Mater. Lett. 2012, 68, 164–167..

    Not in our library10.1016/j.matlet.2011.09.115

  324. 324.

    Ishwarya S. P.; Anandharamakrishnan C.; Stapley A. G. Spray-Freeze-Drying: A Novel Process for the Drying of Foods and Bioproducts. Trends Food Sci. Technol. 2015, 41, 161–181..

    Not in our library10.1016/j.tifs.2014.10.008

  325. 325.

    Yu Z.; Johnston K. P.; Williams R. O. III Spray Freezing into Liquid Versus Spray-Freeze Drying: Influence of Atomization on Protein Aggregation and Biological Activity. Eur. J. Pharm. Sci. 2006, 27, 9–18..

    Not in our library10.1016/j.ejps.2005.08.010

  326. 326.

    Zimmermann M. V.; Borsoi C.; Lavoratti A.; Zanini M.; Zattera A. J.; Santana R. M. Drying Techniques Applied to Cellulose Nanofibers. J. Reinf. Plast. Compos. 2016, 35, 628–643..

    Not in our library10.1177/0731684415626286

  327. 327.

    Peng Y.; Gardner D. J.; Han Y.; Kiziltas A.; Cai Z.; Tshabalala M. A. Influence of Drying Method on the Material Properties of Nanocellulose I: Thermostability and Crystallinity. Cellulose 2013, 20, 2379–2392..

    Not in our library10.1007/s10570-013-0019-z

  328. 328.

    Peng Y.; Han Y.; Gardner D. J. Spray-Drying Cellulose Nanofibrils: Effect of Drying Process Parameters on Particle Morphology and Size Distribution. Wood Fiber Sci. 2012, 44, 448–461.

    Not in our library

  329. 329.

    Aguiar-Ricardo A. Building Dry Powder Formulations Using Supercritical Co2 Spray Drying. Curr. Opin. Green Sustainable Chem. 2017, 5, 12–16..

    Not in our library10.1016/j.cogsc.2017.03.005

  330. 330.

    Assaf A.; Haas R.; Purves C. A New Interpretation of the Cellulose-Water Adsorption Isotherm and Data Concerning the Effect of Swelling and Drying on the Colloidal Surface of Cellulose1, 2. J. Am. Chem. Soc. 1944, 66, 66–73..

    Not in our library10.1021/ja01229a020

  331. 331.

    Shrestha S.; Diaz J. A.; Ghanbari S.; Youngblood J. P. Hygroscopic Swelling Determination of Cellulose Nanocrystal (Cnc) Films by Polarized Light Microscopy Digital Image Correlation. Biomacromolecules 2017, 18, 1482–1490..

    Not in our library10.1021/acs.biomac.7b00026

  332. 332.

    Ding Q.; Zeng J.; Wang B.; Tang D.; Chen K.; Gao W. Effect of Nanocellulose Fiber Hornification on Water Fraction Characteristics and Hydroxyl Accessibility During Dehydration. Carbohydr. Polym. 2019, 207, 44–51..

    Not in our library10.1016/j.carbpol.2018.11.075

  333. 333.

    Dufresne A. Nanocellulose: From Nature to High Performance Tailored Materials; Walter de Gruyter: Berlin, 2017.

    Not in our library

  334. 334.

    Kekäläinen K.; Liimatainen H.; Illikainen M.; Maloney T. C.; Niinimäki J. The Role of Hornification in the Disintegration Behaviour of Tempo-Oxidized Bleached Hardwood Fibres in a High-Shear Homogenizer. Cellulose 2014, 21, 1163–1174..

    Not in our library10.1007/s10570-014-0210-x

  335. 335.

    Fernandes Diniz J.; Gil M.; Castro J. Hornification—Its Origin and Interpretation in Wood Pulps. Wood Sci. Technol. 2004, 37, 489–494..

    Not in our library10.1007/s00226-003-0216-2

  336. 336.

    Zhou S.; Nyholm L.; Strømme M.; Wang Z. Cladophora Cellulose: Unique Biopolymer Nanofibrils for Emerging Energy, Environmental, and Life Science Applications. Acc. Chem. Res. 2019, 52, 2232–2243..

    Not in our library10.1021/acs.accounts.9b00215

  337. 337.

    Missoum K.; Bras J.; Belgacem M. N. Water Redispersible Dried Nanofibrillated Cellulose by Adding Sodium Chloride. Biomacromolecules 2012, 13, 4118–4125..

    Not in our library10.1021/bm301378n

  338. 338.

    Qi W.; Xu H.-N.; Zhang L. The Aggregation Behavior of Cellulose Micro/Nanoparticles in Aqueous Media. RSC Adv. 2015, 5, 8770–8777..

    Not in our library10.1039/c4ra08844a

  339. 339.

    Ben Abd Hamid S.; Zain S. K.; Das R.; Centi G. Synergic Effect of Tungstophosphoric Acid and Sonication for Rapid Synthesis of Crystalline Nanocellulose. Carbohydr. Polym. 2016, 138, 349–355..

    Not in our library10.1016/j.carbpol.2015.10.023

  340. 340.

    Suopajärvi T.; Liimatainen H.; Karjalainen M.; Upola H.; Niinimäki J. Lead Adsorption with Sulfonated Wheat Pulp Nanocelluloses. J. Water Process Eng. 2015, 5, 136–142..

    Not in our library10.1016/j.jwpe.2014.06.003

  341. 341.

    Zoppe J. O.; Johansson L.-S.; Seppälä J. Manipulation of Cellulose Nanocrystal Surface Sulfate Groups toward Biomimetic Nanostructures in Aqueous Media. Carbohydr. Polym. 2015, 126, 23–31..

    Not in our library10.1016/j.carbpol.2015.03.005

  342. 342.

    Saito T.; Kimura S.; Nishiyama Y.; Isogai A. Cellulose Nanofibers Prepared by Tempo-Mediated Oxidation of Native Cellulose. Biomacromolecules 2007, 8, 2485–2491..

    Not in our library10.1021/bm0703970

  343. 343.

    Liimatainen H.; Visanko M.; Sirviö J. A.; Hormi O. E.; Niinimaki J. Enhancement of the Nanofibrillation of Wood Cellulose through Sequential Periodate–Chlorite Oxidation. Biomacromolecules 2012, 13, 1592–1597..

    Not in our library10.1021/bm300319m

  344. 344.

    Spinella S.; Maiorana A.; Qian Q.; Dawson N. J.; Hepworth V.; McCallum S. A.; Ganesh M.; Singer K. D.; Gross R. A. Concurrent Cellulose Hydrolysis and Esterification to Prepare a Surface-Modified Cellulose Nanocrystal Decorated with Carboxylic Acid Moieties. ACS Sustainable Chem. Eng. 2016, 4, 1538–1550..

    Not in our library10.1021/acssuschemeng.5b01489

  345. 345.

    Abou-Zeid R. E.; Dacrory S.; Ali K. A.; Kamel S. Novel Method of Preparation of Tricarboxylic Cellulose Nanofiber for Efficient Removal of Heavy Metal Ions from Aqueous Solution. Int. J. Biol. Macromol. 2018, 119, 207–214..

    Not in our library10.1016/j.ijbiomac.2018.07.127

  346. 346.

    Yu H.-Y.; Zhang D.-Z.; Lu F.-F.; Yao J. New Approach for Single-Step Extraction of Carboxylated Cellulose Nanocrystals for Their Use as Adsorbents and Flocculants. ACS Sustainable Chem. Eng. 2016, 4, 2632–2643..

    Not in our library10.1021/acssuschemeng.6b00126

  347. 347.

    Kokol V.; Božič M.; Vogrinčič R.; Mathew A. P. Characterisation and Properties of Homo-and Heterogenously Phosphorylated Nanocellulose. Carbohydr. Polym. 2015, 125, 301–313..

    Not in our library10.1016/j.carbpol.2015.02.056

  348. 348.

    Ghanadpour M.; Carosio F.; Larsson P. T.; Wågberg L. Phosphorylated Cellulose Nanofibrils: A Renewable Nanomaterial for the Preparation of Intrinsically Flame-Retardant Materials. Biomacromolecules 2015, 16, 3399–3410..

    Not in our library10.1021/acs.biomac.5b01117

  349. 349.

    Liu K.; Nasrallah J.; Chen L.; Huang L.; Ni Y. Preparation of CNC-Dispersed Fe3O4 Nanoparticles and Their Application in Conductive Paper. Carbohydr. Polym. 2015, 126, 175–178..

    Not in our library10.1016/j.carbpol.2015.03.009

  350. 350.

    Sirviö J. A.; Hasa T.; Ahola J.; Liimatainen H.; Niinimäki J.; Hormi O. Phosphonated Nanocelluloses from Sequential Oxidative–Reductive Treatment—Physicochemical Characteristics and Thermal Properties. Carbohydr. Polym. 2015, 133, 524–532..

    Not in our library10.1016/j.carbpol.2015.06.090

  351. 351.

    Selkälä T.; Suopajärvi T.; Sirviö J. A.; Luukkonen T.; Kinnunen P.; Kling K. I.; Wagner J. B.; Liimatainen H. Efficient Entrapment and Separation of Anionic Pollutants from Aqueous Solutions by Sequential Combination of Cellulose Nanofibrils and Halloysite Nanotubes. Chem. Eng. J. 2019, 374, 1013–1024..

    Not in our library10.1016/j.cej.2019.06.008

  352. 352.

    Li P.; Sirviö J. A.; Asante B.; Liimatainen H. Recyclable Deep Eutectic Solvent for the Production of Cationic Nanocelluloses. Carbohydr. Polym. 2018, 199, 219–227..

    Not in our library10.1016/j.carbpol.2018.07.024

  353. 353.

    Zaman M.; Xiao H.; Chibante F.; Ni Y. Synthesis and Characterization of Cationically Modified Nanocrystalline Cellulose. Carbohydr. Polym. 2012, 89, 163–170..

    Not in our library10.1016/j.carbpol.2012.02.066

  354. 354.

    Rosilo H.; McKee J. R.; Kontturi E.; Koho T.; Hytönen V. P.; Ikkala O.; Kostiainen M. A. Cationic Polymer Brush-Modified Cellulose Nanocrystals for High-Affinity Virus Binding. Nanoscale 2014, 6, 11871–11881..

    Not in our library10.1039/c4nr03584d

  355. 355.

    Jin L.; Li W.; Xu Q.; Sun Q. Amino-Functionalized Nanocrystalline Cellulose as an Adsorbent for Anionic Dyes. Cellulose 2015, 22, 2443–2456..

    Not in our library10.1007/s10570-015-0649-4

  356. 356.

    Liu L.; Borghei M.; Wang Z.; Xu J.; Fan Y.; Rojas O. J. Salt-Induced Colloidal Destabilization, Separation, Drying, and Redispersion in Aqueous Phase of Cationic and Anionic Nanochitins. J. Agric. Food. Chem. 2018, 66, 9189–9198..

    Not in our library10.1021/acs.jafc.8b02062

  357. 357.

    Beck S.; Bouchard J. Auto-Catalyzed Acidic Desulfation of Cellulose Nanocrystals. Nordic Pulp Pap. Res. J. 2014, 29, 6–14..

    Not in our library10.3183/npprj-2014-29-01-p006-014

  358. 358.

    Jiang F.; Esker A. R.; Roman M. Acid-Catalyzed and Solvolytic Desulfation of H2SO4-Hydrolyzed Cellulose Nanocrystals. Langmuir 2010, 26, 17919–17925..

    Not in our library10.1021/la1028405

  359. 359.

    Azzam F.; Heux L.; Putaux J.-L.; Jean B. Preparation by Grafting onto, Characterization, and Properties of Thermally Responsive Polymer-Decorated Cellulose Nanocrystals. Biomacromolecules 2010, 11, 3652–3659..

    Not in our library10.1021/bm101106c

  360. 360.

    Harrisson S.; Drisko G. L.; Malmstrom E.; Hult A.; Wooley K. L. Hybrid Rigid/Soft and Biologic/Synthetic Materials: Polymers Grafted onto Cellulose Microcrystals. Biomacromolecules 2011, 12, 1214–1223..

    Not in our library10.1021/bm101506j

  361. 361.

    Cheng D.; Wen Y.; Wang L.; An X.; Zhu X.; Ni Y. Adsorption of Polyethylene Glycol (PEG) onto Cellulose Nano-Crystals to Improve Its Dispersity. Carbohydr. Polym. 2015, 123, 157–163..

    Not in our library10.1016/j.carbpol.2015.01.035

  362. 362.

    Araki J.; Wada M.; Kuga S. Steric Stabilization of a Cellulose Microcrystal Suspension by Poly (Ethylene Glycol) Grafting. Langmuir 2001, 17, 21–27..

    Not in our library10.1021/la001070m

  363. 363.

    Chu Y.; Song R.; Zhang L.; Dai H.; Wu W. Water-Dispersible, Biocompatible and Fluorescent Poly (Ethylene Glycol)-Grafted Cellulose Nanocrystals. Int. J. Biol. Macromol. 2020, 153, 46–54..

    Not in our library10.1016/j.ijbiomac.2020.02.286

  364. 364.

    Kloser E.; Gray D. G. Surface Grafting of Cellulose Nanocrystals with Poly (Ethylene Oxide) in Aqueous Media. Langmuir 2010, 26, 13450–13456..

    Not in our library10.1021/la101795s

  365. 365.

    Impoolsup T.; Chiewchan N.; Devahastin S. On the Use of Microwave Pretreatment to Assist Zero-Waste Chemical-Free Production Process of Nanofibrillated Cellulose from Lime Residue. Carbohydr. Polym. 2020, 230, 115630.

    Not in our library10.1016/j.carbpol.2019.115630

  366. 366.

    Shang Z.; An X.; Seta F. T.; Ma M.; Shen M.; Dai L.; Liu H.; Ni Y. Improving Dispersion Stability of Hydrochloric Acid Hydrolyzed Cellulose Nano-Crystals. Carbohydr. Polym. 2019, 222, 115037.

    Not in our library10.1016/j.carbpol.2019.115037

  367. 367.

    Shi K.; Sha D.; Xu J.-D.; Yang X.; Wang B.-L.; Pan Y.-X.; Ji X.-L. Hofmeister Effect on Thermo-Responsive Poly (N-Isopropylacrylamide) Hydrogels Grafted on Macroporous Poly (Vinyl Alcohol) Formaldehyde Sponges. Chin. J. Polym. Sci. 2020, 38, 257–267..

    Not in our library10.1007/s10118-019-2320-2

  368. 368.

    Delcroix M.; Demoustier-Champagne S.; Dupont-Gillain C. C. Quartz Crystal Microbalance Study of Ionic Strength and Ph-Dependent Polymer Conformation and Protein Adsorption/Desorption on Paa, Peo, and Mixed Peo/Paa Brushes. Langmuir 2014, 30, 268–277..

    Not in our library10.1021/la403891k

  369. 369.

    Yi J.; Xu Q.; Zhang X.; Zhang H. Temperature-Induced Chiral Nematic Phase Changes of Suspensions of Poly (N, N-Dimethylaminoethyl Methacrylate)-Grafted Cellulose Nanocrystals. Cellulose 2009, 16, 989–997..

    Not in our library10.1007/s10570-009-9350-9

  370. 370.

    Zoppe J. O.; Osterberg M.; Venditti R. A.; Laine J.; Rojas O. J. Surface Interaction Forces of Cellulose Nanocrystals Grafted with Thermoresponsive Polymer Brushes. Biomacromolecules 2011, 12, 2788–2796..

    Not in our library10.1021/bm200551p

  371. 371.

    Azzam F.; Siqueira E.; Fort S. b.; Hassaini R.; Pignon F. d. r.; Travelet C.; Putaux J.-L.; Jean B. Tunable Aggregation and Gelation of Thermoresponsive Suspensions of Polymer-Grafted Cellulose Nanocrystals. Biomacromolecules 2016, 17, 2112–2119..

    Not in our library10.1021/acs.biomac.6b00344

  372. 372.

    Kan K. H.; Li J.; Wijesekera K.; Cranston E. D. Polymer-Grafted Cellulose Nanocrystals as Ph-Responsive Reversible Flocculants. Biomacromolecules 2013, 14, 3130–3139..

    Not in our library10.1021/bm400752k

  373. 373.

    Tang J.; Lee M. F. X.; Zhang W.; Zhao B.; Berry R. M.; Tam K. C. Dual Responsive Pickering Emulsion Stabilized by Poly [2-(Dimethylamino) Ethyl Methacrylate] Grafted Cellulose Nanocrystals. Biomacromolecules 2014, 15, 3052–3060..

    Not in our library10.1021/bm500663w

  374. 374.

    Kedzior S. A.; Zoppe J. O.; Berry R. M.; Cranston E. D. Recent Advances and an Industrial Perspective of Cellulose Nanocrystal Functionalization through Polymer Grafting. Curr. Opin. Solid State Mater. Sci. 2019, 23, 74–91..

    Not in our library10.1016/j.cossms.2018.11.005

  375. 375.

    Larsson E.; Sanchez C. C.; Porsch C.; Karabulut E.; Wågberg L.; Carlmark A. Thermo-Responsive Nanofibrillated Cellulose by Polyelectrolyte Adsorption. Eur. Polym. J. 2013, 49, 2689–2696..

    Not in our library10.1016/j.eurpolymj.2013.05.023

  376. 376.

    Bai L.; Huan S.; Zhao B.; Zhu Y.; Esquena J.; Chen F.; Gao G.; Zussman E.; Chu G.; Rojas O. J. All-Aqueous Liquid Crystal Nanocellulose Emulsions with Permeable Interfacial Assembly. ACS Nano 2020, 14, 13380–13390..

    Not in our library10.1021/acsnano.0c05251

  377. 377.

    Beck S.; Bouchard J.; Berry R. Dispersibility in Water of Dried Nanocrystalline Cellulose. Biomacromolecules 2012, 13, 1486–1494..

    Not in our library10.1021/bm300191k

  378. 378.

    Khoshkava V.; Kamal M. Effect of Surface Energy on Dispersion and Mechanical Properties of Polymer/Nanocrystalline Cellulose Nanocomposites. Biomacromolecules 2013, 14, 3155–3163..

    Not in our library10.1021/bm400784j

  379. 379.

    Khalil H. P. S.; Davoudpour Y.; Islam M. N.; Mustapha A.; Sudesh K.; Dungani R.; Jawaid M. Production and Modification of Nanofibrillated Cellulose Using Various Mechanical Processes: A Review. Carbohydr. Polym. 2014, 99, 649–665..

    Not in our library10.1016/j.carbpol.2013.08.069

  380. 380.

    Hu L.; Xu W.; Gustafsson J.; Koppolu R.; Wang Q.; Rosqvist E.; Sundberg A.; Peltonen J.; Willför S.; Toivakka M.; Xu C. Water-Soluble Polysaccharides Promoting Production of Redispersible Nanocellulose. Carbohydr. Polym. 2022, 297, 119976.

    Not in our library10.1016/j.carbpol.2022.119976

  381. 381.

    Kwak H. W.; You J.; Lee M. E.; Jin H.-J. Prevention of Cellulose Nanofibril Agglomeration During Dehydration and Enhancement of Redispersibility by Hydrophilic Gelatin. Cellulose 2019, 26, 4357–4369..

    Not in our library10.1007/s10570-019-02387-z

  382. 382.

    Velasquez-Cock J.; Ganan P.; Gomez H. C.; Posada P.; Castro C.; Dufresne A.; Zuluaga R. Improved Redispersibility of Cellulose Nanofibrils in Water Using Maltodextrin as a Green, Easily Removable and Non-Toxic Additive. Food Hydrocolloids 2018, 79, 30–39..

    Not in our library10.1016/j.foodhyd.2017.12.024

  383. 383.

    Bertsch P.; Fischer P. Adsorption and Interfacial Structure of Nanocelluloses at Fluid Interfaces. Adv. Colloid Interface Sci. 2020, 276, 102089.

    Not in our library10.1016/j.cis.2019.102089

  384. 384.

    Kedzior S. A.; Gabriel V. A.; Dubé M. A.; Cranston E. D. Nanocellulose in Emulsions and Heterogeneous Water-Based Polymer Systems: A Review. Adv. Mater. 2021, 33, 2002404.

    Not in our library10.1002/adma.202002404

  385. 385.

    Li X.; Li J.; Gong J.; Kuang Y.; Mo L.; Song T. Cellulose Nanocrystals (CNCs) with Different Crystalline Allomorph for Oil in Water Pickering Emulsions. Carbohydr. Polym. 2018, 183, 303–310..

    Not in our library10.1016/j.carbpol.2017.12.085

  386. 386.

    Nigmatullin R.; Johns M. A.; Muñoz-García J. C.; Gabrielli V.; Schmitt J.; Angulo J.; Khimyak Y. Z.; Scott J. L.; Edler K. J.; Eichhorn S. J. Hydrophobization of Cellulose Nanocrystals for Aqueous Colloidal Suspensions and Gels. Biomacromolecules 2020, 21, 1812–1823..

    Not in our library10.1021/acs.biomac.9b01721

  387. 387.

    Binks B. P. Particles as Surfactants—Similarities and Differences. Curr. Opin. Colloid Interface Sci. 2002, 7, 21–41..

    Not in our library10.1016/s1359-0294(02)00008-0

  388. 388.

    Kalashnikova I.; Bizot H.; Cathala B.; Capron I. New Pickering Emulsions Stabilized by Bacterial Cellulose Nanocrystals. Langmuir 2011, 27, 7471–7479..

    Not in our library10.1021/la200971f

  389. 389.

    Bai L.; Huan S.; Xiang W.; Rojas O. J. Pickering Emulsions by Combining Cellulose Nanofibrils and Nanocrystals: Phase Behavior and Depletion Stabilization. Green Chem. 2018, 20, 1571–1582..

    Not in our library10.1039/c8gc00134k

  390. 390.

    Capron I.; Rojas O. J.; Bordes R. Behavior of Nanocelluloses at Interfaces. Curr. Opin. Colloid Interface Sci. 2017, 29, 83–95..

    Not in our library10.1016/j.cocis.2017.04.001

  391. 391.

    Goi Y.; Fujisawa S.; Saito T.; Yamane K.; Kuroda K.; Isogai A. Dual Functions of Tempo-Oxidized Cellulose Nanofibers in Oil-in-Water Emulsions: A Pickering Emulsifier and a Unique Dispersion Stabilizer. Langmuir 2019, 35, 10920–10926..

    Not in our library10.1021/acs.langmuir.9b01977

  392. 392.

    Malho J.-M.; Laaksonen P. i.; Walther A.; Ikkala O.; Linder M. B. Facile Method for Stiff, Tough, and Strong Nanocomposites by Direct Exfoliation of Multilayered Graphene into Native Nanocellulose Matrix. Biomacromolecules 2012, 13, 1093–1099..

    Not in our library10.1021/bm2018189

  393. 393.

    Xu X.; Hsieh Y.-L. Aqueous Exfoliated Graphene by Amphiphilic Nanocellulose and Its Application in Moisture-Responsive Foldable Actuators. Nanoscale 2019, 11, 11719–11729..

    Not in our library10.1039/c9nr01602c

  394. 394.

    Lund S.; Björnvik E.; Wang Q.; Wang X.; Vajravel S.; Wey L. T.; Allahverdiyeva Y.; Kauppila J.; Smått J.-H.; Peltonen J.; et al. Shear Exfoliated Few-Layer Graphene and Cellulose Nanocrystal Composite as Biocompatible Anode with Efficient Charge Transfer. Carbon Trends 2022, 9, 100210.

    Not in our library10.1016/j.cartre.2022.100210

  395. 395.

    Xu J.; Peng T.; Qin X.; Zhang Q.; Liu T.; Dai W.; Chen B.; Yu H.; Shi S. Recent Advances in 2d Mxenes: Preparation, Intercalation and Applications in Flexible Devices. J. Mater. Chem. A 2021, 9, 14147–14171..

    Not in our library10.1039/d1ta03070a

  396. 396.

    Li Y.; Zhu H.; Shen F.; Wan J.; Lacey S.; Fang Z.; Dai H.; Hu L. Nanocellulose as Green Dispersant for Two-Dimensional Energy Materials. Nano Energy 2015, 13, 346–354..

    Not in our library10.1016/j.nanoen.2015.02.015

  397. 397.

    Low L. E.; Tey B. T.; Ong B. H.; Chan E. S.; Tang S. Y. Dispersion Stability, Magnetivity and Wettability of Cellulose Nanocrystal (Cnc)-Dispersed Superparamagnetic Fe 3 O 4 Nanoparticles: Impact of Cnc Concentration. RSC Adv. 2016, 6, 113132–113138..

    Not in our library10.1039/c6ra16109j

  398. 398.

    Yang X.; Shi K.; Zhitomirsky I.; Cranston E. D. Cellulose Nanocrystal Aerogels as Universal 3D Lightweight Substrates for Supercapacitor Materials. Adv. Mater. 2015, 27, 6104–6109..

    Not in our library10.1002/adma.201502284

  399. 399.

    Tang A.; Liu Y.; Wang Q.; Chen R.; Liu W.; Fang Z.; Wang L. A New Photoelectric Ink Based on Nanocellulose/Cds Quantum Dots for Screen-Printing. Carbohydr. Polym. 2016, 148, 29–35..

    Not in our library10.1016/j.carbpol.2016.04.034

  400. 400.

    Zhu H.; Yang X.; Cranston E. D.; Zhu S. Flexible and Porous Nanocellulose Aerogels with High Loadings of Metal–Organic-Framework Particles for Separations Applications. Adv. Mater. 2016, 28, 7652–7657..

    Not in our library10.1002/adma.201601351

  401. 401.

    Xie W.-Q.; Yu K.-X.; Gong Y.-X. Preparation of Fluorescent and Antibacterial Nanocomposite Films Based on Cellulose Nanocrystals/ZnS Quantum Dots/Polyvinyl Alcohol. Cellulose 2019, 26, 2363–2373..

    Not in our library10.1007/s10570-019-02245-y

  402. 402.

    Ye Y.; Kong T.; Yu X.; Wu Y.; Zhang K.; Wang X. Enhanced Nonenzymatic Hydrogen Peroxide Sensing with Reduced Graphene Oxide/Ferroferric Oxide Nanocomposites. Talanta 2012, 89, 417–421..

    Not in our library10.1016/j.talanta.2011.12.054

  403. 403.

    Kaushik M.; Moores A. Nanocelluloses as Versatile Supports for Metal Nanoparticles and Their Applications in Catalysis. Green Chem. 2016, 18, 622–637..

    Not in our library10.1039/c5gc02500a

  404. 404.

    Chu Y.; Sun Y.; Wu W.; Xiao H. Dispersion Properties of Nanocellulose: A Review. Carbohydr. Polym. 2020, 250, 116892.

    Not in our library10.1016/j.carbpol.2020.116892

  405. 405.

    González M. M.; Blanco-Tirado C.; Combariza M. Y. Nanocellulose as an Inhibitor of Water-in-Crude Oil Emulsion Formation. Fuel 2020, 264, 116830.

    Not in our library10.1016/j.fuel.2019.116830

  406. 406.

    Lin N.; Dufresne A. Nanocellulose in Biomedicine: Current Status and Future Prospect. Eur. Polym. J. 2014, 59, 302–325..

    Not in our library10.1016/j.eurpolymj.2014.07.025

  407. 407.

    Littunen K.; Hippi U.; Johansson L.-S.; Österberg M.; Tammelin T.; Laine J.; Seppälä J. Free Radical Graft Copolymerization of Nanofibrillated Cellulose with Acrylic Monomers. Carbohydr. Polym. 2011, 84, 1039–1047..

    Not in our library10.1016/j.carbpol.2010.12.064

  408. 408.

    Rol F.; Belgacem M. N.; Gandini A.; Bras J. Recent Advances in Surface-Modified Cellulose Nanofibrils. Prog. Polym. Sci. 2019, 88, 241–264..

    Not in our library10.1016/j.progpolymsci.2018.09.002

  409. 409.

    Sato A.; Kabusaki D.; Okumura H.; Nakatani T.; Nakatsubo F.; Yano H. Surface Modification of Cellulose Nanofibers with Alkenyl Succinic Anhydride for High-Density Polyethylene Reinforcement. Composites, Part A 2016, 83, 72–79..

    Not in our library10.1016/j.compositesa.2015.11.009

  410. 410.

    Yano H.; Omura H.; Honma Y.; Okumura H.; Sano H.; Nakatsubo F. Designing Cellulose Nanofiber Surface for High Density Polyethylene Reinforcement. Cellulose 2018, 25, 3351–3362..

    Not in our library10.1007/s10570-018-1787-2

  411. 411.

    Isogai A.; Hänninen T.; Fujisawa S.; Saito T. Catalytic Oxidation of Cellulose with Nitroxyl Radicals under Aqueous Conditions. Prog. Polym. Sci. 2018, 86, 122–148..

    Not in our library10.1016/j.progpolymsci.2018.07.007

  412. 412.

    Kalia S.; Boufi S.; Celli A.; Kango S. Nanofibrillated Cellulose: Surface Modification and Potential Applications. Colloid Polym. Sci. 2014, 292, 5–31..

    Not in our library10.1007/s00396-013-3112-9

  413. 413.
  414. 414.

    Khalil H.; Davoudpour Y.; Aprilia N. S.; Mustapha A.; Hossain S.; Islam N.; Dungani R. Nanocellulose-Based Polymer Nanocomposite: Isolation, Characterization and Applications. In Nanocellulose Polymer Nanocomposites; Thakur V. K., Ed., Scrivener: Beverly MA, 2014; pp 273–309.

    Not in our library

  415. 415.

    Eyley S.; Thielemans W. Surface Modification of Cellulose Nanocrystals. Nanoscale 2014, 6, 7764–7779..

    Not in our library10.1039/c4nr01756k

  416. 416.

    Wohlhauser S.; Delepierre G.; Labet M.; Morandi G. l.; Thielemans W.; Weder C.; Zoppe J. O. Grafting Polymers from Cellulose Nanocrystals: Synthesis, Properties, and Applications. Macromolecules 2018, 51, 6157–6189..

    Not in our library10.1021/acs.macromol.8b00733

  417. 417.

    Guigo N.; Mazeau K.; Putaux J.-L.; Heux L. Surface Modification of Cellulose Microfibrils by Periodate Oxidation and Subsequent Reductive Amination with Benzylamine: A Topochemical Study. Cellulose 2014, 21, 4119–4133..

    Not in our library10.1007/s10570-014-0459-0

  418. 418.

    Azzam F.; Galliot M.; Putaux J.-L.; Heux L.; Jean B. Surface Peeling of Cellulose Nanocrystals Resulting from Periodate Oxidation and Reductive Amination with Water-Soluble Polymers. Cellulose 2015, 22, 3701–3714..

    Not in our library10.1007/s10570-015-0785-x

  419. 419.

    Sirviö J. A.; Visanko M.; Laitinen O.; Ämmälä A.; Liimatainen H. Amino-Modified Cellulose Nanocrystals with Adjustable Hydrophobicity from Combined Regioselective Oxidation and Reductive Amination. Carbohydr. Polym. 2016, 136, 581–587..

    Not in our library10.1016/j.carbpol.2015.09.089

  420. 420.

    Shao C.; Wang M.; Meng L.; Chang H.; Wang B.; Xu F.; Yang J.; Wan P. Mussel-Inspired Cellulose Nanocomposite Tough Hydrogels with Synergistic Self-Healing, Adhesive, and Strain-Sensitive Properties. Chem. Mater. 2018, 30, 3110–3121..

    Not in our library10.1021/acs.chemmater.8b01172

  421. 421.

    Shao C.; Meng L.; Wang M.; Cui C.; Wang B.; Han C.-R.; Xu F.; Yang J. Mimicking Dynamic Adhesiveness and Strain-Stiffening Behavior of Biological Tissues in Tough and Self-Healable Cellulose Nanocomposite Hydrogels. ACS Appl. Mater. Interfaces 2019, 11, 5885–5895..

    Not in our library10.1021/acsami.8b21588

  422. 422.

    Lin F.; Wang Z.; Shen Y.; Tang L.; Zhang P.; Wang Y.; Chen Y.; Huang B.; Lu B. Natural Skin-Inspired Versatile Cellulose Biomimetic Hydrogels. J. Mater. Chem. A 2019, 7, 26442–26455..

    Not in our library10.1039/c9ta10502f

  423. 423.

    Cunha A. G.; Freire C. S.; Silvestre A. J.; Neto C. P.; Gandini A. Reversible Hydrophobization and Lipophobization of Cellulose Fibers Via Trifluoroacetylation. J. Colloid Interface Sci. 2006, 301, 333–336..

    Not in our library10.1016/j.jcis.2006.04.078

  424. 424.

    Johnson R. K.; Zink-Sharp A.; Glasser W. G. Preparation and Characterization of Hydrophobic Derivatives of Tempo-Oxidized Nanocelluloses. Cellulose 2011, 18, 1599–1609..

    Not in our library10.1007/s10570-011-9579-y

  425. 425.

    Lin W.; Hu X.; You X.; Sun Y.; Wen Y.; Yang W.; Zhang X.; Li Y.; Chen H. Hydrophobic Modification of Nanocellulose Via a Two-Step Silanation Method. Polymers 2018, 10, 1035.

    Not in our library10.3390/polym10091035

  426. 426.

    Rafieian F.; Hosseini M.; Jonoobi M.; Yu Q. Development of Hydrophobic Nanocellulose-Based Aerogel Via Chemical Vapor Deposition for Oil Separation for Water Treatment. Cellulose 2018, 25, 4695–4710..

    Not in our library10.1007/s10570-018-1867-3

  427. 427.

    Tang C.; Chen Y.; Luo J.; Low M. Y.; Shi Z.; Tang J.; Zhang Z.; Peng B.; Tam K. C. Pickering Emulsions Stabilized by Hydrophobically Modified Nanocellulose Containing Various Structural Characteristics. Cellulose 2019, 26, 7753–7767..

    Not in our library10.1007/s10570-019-02648-x

  428. 428.

    Morits M.; McKee J. R.; Majoinen J.; Malho J.-M.; Houbenov N.; Seitsonen J.; Laine J.; Gröschel A. H.; Ikkala O. Polymer Brushes on Cellulose Nanofibers: Modification, Si-Atrp, and Unexpected Degradation Processes. ACS Sustainable Chem. Eng. 2017, 5, 7642–7650..

    Not in our library10.1021/acssuschemeng.7b00972

  429. 429.

    Soeta H.; Fujisawa S.; Saito T.; Isogai A. Controlling Miscibility of the Interphase in Polymer-Grafted Nanocellulose/Cellulose Triacetate Nanocomposites. ACS Omega 2020, 5, 23755–23761..

    Not in our library10.1021/acsomega.0c02772

  430. 430.
  431. 431.

    Sreenivasan R.; Suma Mahesh S.; Sumi V. Synthesis and Application of Polymer-Grafted Nanocellulose/Graphene Oxide Nano Composite for the Selective Recovery of Radionuclides from Aqueous Media. Sep. Sci. Technol. 2019, 54, 1453–1468..

    Not in our library10.1080/01496395.2018.1534868

  432. 432.

    Azzam F.; Frka-Petesic B.; Semeraro E. F.; Cousin F.; Jean B. Small-Angle Neutron Scattering Reveals the Structural Details of Thermosensitive Polymer-Grafted Cellulose Nanocrystal Suspensions. Langmuir 2020, 36, 8511–8519..

    Not in our library10.1021/acs.langmuir.0c01103

  433. 433.

    Wohlhauser S.; Kuhnt T.; Meesorn W.; Montero de Espinosa L.; Zoppe J. O.; Weder C. One-Component Nanocomposites Based on Polymer-Grafted Cellulose Nanocrystals. Macromolecules 2020, 53, 821–834..

    Not in our library10.1021/acs.macromol.9b01612

  434. 434.

    Bagheri S.; Julkapli N. M. Grafted Nanocellulose as an Advanced Smart Biopolymer. In Biopolymer Grafting; Thakur V. K., Ed., Elsevier: Amsterdam, 2018; pp 521–549.

    Not in our library

  435. 435.

    Xu Q.; Yi J.; Zhang X.; Zhang H. A Novel Amphotropic Polymer Based on Cellulose Nanocrystals Grafted with Azo Polymers. Eur. Polym. J. 2008, 44, 2830–2837..

    Not in our library10.1016/j.eurpolymj.2008.06.010

  436. 436.

    Zoppe J. O.; Xu X.; Känel C.; Orsolini P.; Siqueira G.; Tingaut P.; Zimmermann T.; Klok H.-A. Effect of Surface Charge on Surface-Initiated Atom Transfer Radical Polymerization from Cellulose Nanocrystals in Aqueous Media. Biomacromolecules 2016, 17, 1404–1413..

    Not in our library10.1021/acs.biomac.6b00011

  437. 437.

    Junka K.; Guo J.; Filpponen I.; Laine J.; Rojas O. J. Modification of Cellulose Nanofibrils with Luminescent Carbon Dots. Biomacromolecules 2014, 15, 876–881..

    Not in our library10.1021/bm4017176

  438. 438.

    Wu B.; Zhu G.; Dufresne A.; Lin N. Fluorescent Aerogels Based on Chemical Crosslinking between Nanocellulose and Carbon Dots for Optical Sensor. ACS Appl. Mater. Interfaces 2019, 11, 16048–16058..

    Not in our library10.1021/acsami.9b02754

  439. 439.

    Quraishi S.; Plappert S. F.; Grießer T.; Gindl-Altmutter W.; Liebner F. W. Chemical Versus Physical Grafting of Photoluminescent Amino-Functional Carbon Dots onto Transparent Nematic Nanocellulose Gels and Aerogels. Cellulose 2019, 26, 7781–7796..

    Not in our library10.1007/s10570-019-02619-2

  440. 440.

    Xue B.; Yang Y.; Tang R.; Sun Y.; Sun S.; Cao X.; Li P.; Zhang Z.; Li X. One-Step Hydrothermal Synthesis of a Flexible Nanopaper-Based Fe 3+ Sensor Using Carbon Quantum Dot Grafted Cellulose Nanofibrils. Cellulose 2020, 27, 729–742..

    Not in our library10.1007/s10570-019-02846-7

  441. 441.

    Li P.; Zeng J.; Wang B.; Cheng Z.; Xu J.; Gao W.; Chen K. Waterborne Fluorescent Dual Anti-Counterfeiting Ink Based on Yb/Er-Carbon Quantum Dots Grafted with Dialdehyde Nano-Fibrillated Cellulose. Carbohydr. Polym. 2020, 247, 116721.

    Not in our library10.1016/j.carbpol.2020.116721

  442. 442.

    Zhang Z.; Chang H.; Xue B.; Zhang S.; Li X.; Wong W.-K.; Li K.; Zhu X. Near-Infrared and Visible Dual Emissive Transparent Nanopaper Based on Yb (Iii)–Carbon Quantum Dots Grafted Oxidized Nanofibrillated Cellulose for Anti-Counterfeiting Applications. Cellulose 2018, 25, 377–389..

    Not in our library10.1007/s10570-017-1594-1

  443. 443.

    Zhang Q.; Zhang L.; Wu W.; Xiao H. Methods and Applications of Nanocellulose Loaded with Inorganic Nanomaterials: A Review. Carbohydr. Polym. 2020, 229, 115454.

    Not in our library10.1016/j.carbpol.2019.115454

  444. 444.

    Ansari F.; Lindh E. L.; Furo I.; Johansson M. K.; Berglund L. A. Interface Tailoring through Covalent Hydroxyl-Epoxy Bonds Improves Hygromechanical Stability in Nanocellulose Materials. Compos. Sci. Technol. 2016, 134, 175–183..

    Not in our library10.1016/j.compscitech.2016.08.002

  445. 445.

    López Durán V.; Hellwig J.; Larsson P. T.; Wågberg L.; Larsson P. A. Effect of Chemical Functionality on the Mechanical and Barrier Performance of Nanocellulose Films. ACS Appl. Nano Mater. 2018, 1, 1959–1967..

    Not in our library10.1021/acsanm.8b00452

  446. 446.

    Boujemaoui A.; Ansari F.; Berglund L. A. Nanostructural Effects in High Cellulose Content Thermoplastic Nanocomposites with a Covalently Grafted Cellulose–Poly (Methyl Methacrylate) Interface. Biomacromolecules 2019, 20, 598–607..

    Not in our library10.1021/acs.biomac.8b00701

  447. 447.

    Islam M. T.; Alam M. M.; Zoccola M. Review on Modification of Nanocellulose for Application in Composites. Int. J. Innov. Res. Sci. Eng. Technol. 2013, 2, 5444–5451.

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  448. 448.

    Daud J. B.; Lee K.-Y. Surface Modification of Nanocellulose. In Handbook of Nanocellulose and Cellulose Nanocomposites; Kargarzadeh H., Ahmad I., Thomas S., Dufresne A., Eds., Wiley-VCH: Berlin, 2017, Vol. 1, pp 101–122.

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  449. 449.

    Wang J.; Liu X.; Jin T.; He H.; Liu L. Preparation of Nanocellulose and Its Potential in Reinforced Composites: A Review. Journal of Biomaterials Science, Polymer Edition 2019, 30, 919–946..

    Not in our library10.1080/09205063.2019.1612726

  450. 450.

    Mautner A. Nanocellulose Water Treatment Membranes and Filters: A Review. Polym. Int. 2020, 69, 741–751..

    Not in our library10.1002/pi.5993

  451. 451.
  452. 452.

    Ng H.-M.; Sin L. T.; Bee S.-T.; Tee T.-T.; Rahmat A. Review of Nanocellulose Polymer Composite Characteristics and Challenges. Polym.-Plast. Technol. Eng. 2017, 56, 687–731..

    Not in our library10.1080/03602559.2016.1233277

  453. 453.

    Hubbe M. A.; Ferrer A.; Tyagi P.; Yin Y.; Salas C.; Pal L.; Rojas O. J. Nanocellulose in Thin Films, Coatings, and Plies for Packaging Applications: A Review. BioResources 2016, 12, 2143–2233..

    Not in our library10.15376/biores.12.1.hubbe

  454. 454.

    Hao W.; Wang M.; Zhou F.; Luo H.; Xie X.; Luo F.; Cha R. A Review on Nanocellulose as a Lightweight Filler of Polyolefin Composites. Carbohydr. Polym. 2020, 243, 116466.

    Not in our library10.1016/j.carbpol.2020.116466

  455. 455.

    Ferreira F. V.; Pinheiro I. F.; de Souza S. F.; Mei L. H.; Lona L. M. Polymer Composites Reinforced with Natural Fibers and Nanocellulose in the Automotive Industry: A Short Review. J. Comp. Sci. 2019, 3, 51.

    Not in our library10.3390/jcs3020051

  456. 456.

    Tang J.; Sisler J.; Grishkewich N.; Tam K. C. Functionalization of Cellulose Nanocrystals for Advanced Applications. J. Colloid Interface Sci. 2017, 494, 397–409..

    Not in our library10.1016/j.jcis.2017.01.077

  457. 457.

    Tortorella S.; Vetri Buratti V.; Maturi M.; Sambri L.; Comes Franchini M.; Locatelli E. Surface-Modified Nanocellulose for Application in Biomedical Engineering and Nanomedicine: A Review. Int. J. Nanomed. 2020, 15, 9909.

    Not in our library10.2147/ijn.s266103

  458. 458.

    Chin K. M.; Sung Ting S.; Ong H. L.; Omar M. Surface Functionalized Nanocellulose as a Veritable Inclusionary Material in Contemporary Bioinspired Applications: A Review. J. Appl. Polym. Sci. 2018, 135, 46065.

    Not in our library10.1002/app.46065

  459. 459.

    Trache D.; Tarchoun A. F.; Derradji M.; Mehelli O.; Hussin M. H.; Bessa W. Cellulose Fibers and Nanocrystals: Preparation, Characterization and Surface Modification. In Functionalized Nanomaterials I: Fabrication; Kumar V., Guleria P., Dasgupta N., Ranjan S., Eds.; CRC Press: Boca Raton, FL, 2020; pp 171–190.

    Not in our library

  460. 460.

    Neves R. M.; Ornaghi H. L. Jr; Zattera A. J.; Amico S. C. Recent Studies on Modified Cellulose/Nanocellulose Epoxy Composites: A Systematic Review. Carbohydr. Polym. 2021, 255, 117366.

    Not in our library10.1016/j.carbpol.2020.117366

  461. 461.

    Li Q.; McGinnis S.; Sydnor C.; Wong A.; Renneckar S. Nanocellulose Life Cycle Assessment. ACS Sustainable Chem. Eng. 2013, 1, 919–928..

    Not in our library10.1021/sc4000225

  462. 462.

    Pachuau L. S. A Mini Review on Plant-Based Nanocellulose: Production, Sources, Modifications and Its Potential in Drug Delivery Applications. Mini-Rev. Med. Chem. 2015, 15, 543–552..

    Not in our library10.2174/1389557515666150415150327

  463. 463.

    Kumar R.; Rai B.; Gahlyan S.; Kumar G. A Comprehensive Review on Production, Surface Modification and Characterization of Nanocellulose Derived from Biomass and Its Commercial Applications. eXPRESS Polym. Lett. 2021, 15, 104–120..

    Not in our library10.3144/expresspolymlett.2021.11

  464. 464.

    Dufresne A. Nanocellulose: A New Ageless Bionanomaterial. Mater. Today 2013, 16, 220–227..

    Not in our library10.1016/j.mattod.2013.06.004

  465. 465.

    Börjesson M.; Westman G. Crystalline Nanocellulose—Preparation, Modification, and Properties. In Cellulose-Fundamental Aspects and Current Trends; Poletto M., Ornaghi H. L. Jr., Eds., InTechOpen: London, 2015; pp 159–191.

    Not in our library

  466. 466.

    Salajková M. Nanocelluloses—Surface Modification and Use in Functional Materials. Ph.D Thesis. KTH Royal Institute of Technology, 2012.

    Not in our library

  467. 467.

    Panchal P.; Ogunsona E.; Mekonnen T. Trends in Advanced Functional Material Applications of Nanocellulose. Processes 2019, 7, 10.

    Not in our library10.3390/pr7010010

  468. 468.

    Dufresne A. Nanocellulose Processing Properties and Potential Applications. Curr. For. Rep. 2019, 5, 76–89..

    Not in our library10.1007/s40725-019-00088-1

  469. 469.

    Li F.; Mascheroni E.; Piergiovanni L. The Potential of Nanocellulose in the Packaging Field: A Review. Packag. Technol. Sci. 2015, 28, 475–508..

    Not in our library10.1002/pts.2121

  470. 470.

    Mondal S. Review on Nanocellulose Polymer Nanocomposites.. Polym.-Plast. Technol. Eng. 2018, 57, 1377–1391..

    Not in our library10.1080/03602559.2017.1381253

  471. 471.

    Rebouillat S.; Pla F. State of the Art Manufacturing and Engineering of Nanocellulose: A Review of Available Data and Industrial Applications. J. Biomater. Bionanotechnol. 2013, 94, 165–188..

    Not in our library10.4236/jbnb.2013.42022

  472. 472.

    Gan P.; Sam S.; Abdullah M. F. b.; Omar M. F. Thermal Properties of Nanocellulose-Reinforced Composites: A Review. J. Appl. Polym. Sci. 2020, 137, 48544.

    Not in our library10.1002/app.48544

  473. 473.

    Zoppe J. O.; Larsson P. A.; Cusola O. Surface Modification of Nanocellulosics and Functionalities. In Lignocellulosics; Filpponen I., Peresin M. S., Nypelö T., Eds.; Elsevier: Amsterdam, 2020; pp 17–63.

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  474. 474.

    Chakrabarty A.; Teramoto Y. Recent Advances in Nanocellulose Composites with Polymers: A Guide for Choosing Partners and How to Incorporate Them. Polymers 2018, 10, 517.

    Not in our library10.3390/polym10050517

  475. 475.

    Halib N.; Perrone F.; Cemazar M.; Dapas B.; Farra R.; Abrami M.; Chiarappa G.; Forte G.; Zanconati F.; Pozzato G.; et al. Potential Applications of Nanocellulose-Containing Materials in the Biomedical Field. Materials 2017, 10, 977.

    Not in our library10.3390/ma10080977

  476. 476.

    Katiyar V.; Dhar P. Cellulose Nanocrystals: An Emerging Nanocellulose for Numerous Chemical Processes; Walter de Gruyter: Berlin, 2020.

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    Kargarzadeh H.; Mariano M.; Huang J.; Lin N.; Ahmad I.; Dufresne A.; Thomas S. Recent Developments on Nanocellulose Reinforced Polymer Nanocomposites: A Review. Polymer 2017, 132, 368–393..

    Not in our library10.1016/j.polymer.2017.09.043

  478. 478.

    Peresin M. S.; Kammiovirta K.; Heikkinen H.; Johansson L.-S.; Vartiainen J.; Setälä H.; Österberg M.; Tammelin T. Understanding the Mechanisms of Oxygen Diffusion through Surface Functionalized Nanocellulose Films. Carbohydr. Polym. 2017, 174, 309–317..

    Not in our library10.1016/j.carbpol.2017.06.066

  479. 479.

    Gardner D. J.; Oporto G. S.; Mills R.; Samir M. A. S. A. Adhesion and Surface Issues in Cellulose and Nanocellulose. J. Adhes. Sci. Technol. 2008, 22, 545–567..

    Not in our library10.1163/156856108x295509

  480. 480.

    Afrin S.; Karim Z. Isolation and Surface Modification of Nanocellulose: Necessity of Enzymes over Chemicals. ChemBioEng. Rev. 2017, 4, 289–303..

    Not in our library10.1002/cben.201600001

  481. 481.

    Lu Y.; Tekinalp H. L.; Eberle C. C.; Peter W.; Naskar A. K.; Ozcan S. Nanocellulose in Polymer Composites and Biomedical Applications. TAPPI J. 2014, 13, 47–54..

    Not in our library10.32964/tj13.6.47

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    Chen P.; Lo Re G.; Berglund L. A.; Wohlert J. Surface Modification Effects on Nanocellulose–Molecular Dynamics Simulations Using Umbrella Sampling and Computational Alchemy. J. Mater. Chem. A 2020, 8, 23617–23627..

    Not in our library10.1039/d0ta09105g

  483. 483.

    Zhu G.; Lin N. Surface Chemistry of Nanocellulose. In Nanocellulose: from Fundamentals to Advanced Materials; Huang J., Dufresne A., Lin N., Eds.; Wiley-VCH: Weinheim, Germany, 2019; pp 115–153.

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  484. 484.

    Rana A. K.; Frollini E.; Thakur V. K. Cellulose Nanocrystals: Pretreatments, Preparation Strategies, and Surface Functionalization. Int. J. Biol. Macromol. 2021, 182, 1554–1581..

    Not in our library10.1016/j.ijbiomac.2021.05.119

  485. 485.

    Ghasemlou M.; Daver F.; Ivanova E. P.; Habibi Y.; Adhikari B. Surface Modifications of Nanocellulose: From Synthesis to High-Performance Nanocomposites. Prog. Polym. Sci. 2021, 119, 101418.

    Not in our library10.1016/j.progpolymsci.2021.101418

  486. 486.
  487. 487.

    Lee K. -Y.; Blaker J.; Bismarck A.; Improving the Properties of Nanocellulose/Polylactide Composites by Esterification of Nanocellulose. Can It Be Done? In ICCM International Conferences on Composite Materials, 27–31 July, 2009, Edinburgh, UK, 2009.

    Not in our library

  488. 488.

    Agustin M. B.; Nakatsubo F.; Yano H. Improving the Thermal Stability of Wood-Based Cellulose by Esterification. Carbohydr. Polym. 2018, 192, 28–36..

    Not in our library10.1016/j.carbpol.2018.02.071

  489. 489.

    Cellante L.; Costa R.; Monaco I.; Cenacchi G.; Locatelli E. One-Step Esterification of Nanocellulose in a Bro̷nsted Acid Ionic Liquid for Delivery to Glioblastoma Cancer Cells. New J. Chem. 2018, 42, 5237–5242..

    Not in our library10.1039/c7nj04633b

  490. 490.

    Wang Y.; Wang X.; Xie Y.; Zhang K. Functional Nanomaterials through Esterification of Cellulose: A Review of Chemistry and Application. Cellulose 2018, 25, 3703–3731..

    Not in our library10.1007/s10570-018-1830-3

  491. 491.

    Fumagalli M.; Sanchez F.; Boisseau S. M.; Heux L. Gas-Phase Esterification of Cellulose Nanocrystal Aerogels for Colloidal Dispersion in Apolar Solvents. Soft Matter 2013, 9, 11309–11317..

    Not in our library10.1039/c3sm52062e

  492. 492.

    Fumagalli M.; Ouhab D.; Boisseau S. M.; Heux L. Versatile Gas-Phase Reactions for Surface to Bulk Esterification of Cellulose Microfibrils Aerogels. Biomacromolecules 2013, 14, 3246–3255..

    Not in our library10.1021/bm400864z

  493. 493.

    Fumagalli M.; Sanchez F.; Molina-Boisseau S.; Heux L. Surface-Restricted Modification of Nanocellulose Aerogels in Gas-Phase Esterification by Di-Functional Fatty Acid Reagents. Cellulose 2015, 22, 1451–1457..

    Not in our library10.1007/s10570-015-0585-3

  494. 494.

    Abushammala H.; Mao J. A Review of the Surface Modification of Cellulose and Nanocellulose Using Aliphatic and Aromatic Mono-and Di-Isocyanates. Molecules 2019, 24, 2782.

    Not in our library10.3390/molecules24152782

  495. 495.

    Hasani M.; Cranston E. D.; Westman G.; Gray D. G. Cationic Surface Functionalization of Cellulose Nanocrystals. Soft Matter 2008, 4, 2238–2244..

    Not in our library10.1039/b806789a

  496. 496.

    Bonollo S.; Lanari D.; Vaccaro L. Ring-Opening of Epoxides in Water. Eur. J. Org. Chem. 2011, 2011, 2587–2598..

    Not in our library10.1002/ejoc.201001693

  497. 497.

    Heinze T.; Liebert T.; Klüfers P.; Meister F. Carboxymethylation of Cellulose in Unconventional Media. Cellulose 1999, 6, 153–165..

    Not in our library10.1023/a:1009271427760

  498. 498.

    Ho T.; Zimmermann T.; Hauert R.; Caseri W. Preparation and Characterization of Cationic Nanofibrillated Cellulose from Etherification and High-Shear Disintegration Processes. Cellulose 2011, 18, 1391–1406..

    Not in our library10.1007/s10570-011-9591-2

  499. 499.

    Price C. C.; Carmelite D. D. Reactions of Epoxides in Dimethyl Sulfoxide Catalyzed by Potassium T-Butoxide. J. Am. Chem. Soc. 1966, 88, 4039–4044..

    Not in our library10.1021/ja00969a026

  500. 500.
  501. 501.

    Eyley S.; Thielemans W. Imidazolium Grafted Cellulose Nanocrystals for Ion Exchange Applications. Chem. Commun. 2011, 47, 4177–4179..

    Not in our library10.1039/c0cc05359g

  502. 502.

    BOEHM R. L. Chlorination of Cellulose with Thionyl Chloride in a Pyridine Medium. J. Org. Chem. 1958, 23, 1716–1720..

    Not in our library10.1021/jo01105a038

  503. 503.

    Dash R.; Elder T.; Ragauskas A. J. Grafting of Model Primary Amine Compounds to Cellulose Nanowhiskers through Periodate Oxidation. Cellulose 2012, 19, 2069–2079..

    Not in our library10.1007/s10570-012-9769-2

  504. 504.

    Orelma H.; Vuoriluoto M.; Johansson L.-S.; Campbell J. M.; Filpponen I.; Biesalski M.; Rojas O. J. Preparation of Photoreactive Nanocellulosic Materials Via Benzophenone Grafting. RSC Adv. 2016, 6, 85100–85106..

    Not in our library10.1039/c6ra15015b

  505. 505.

    Sadeghifar H.; Filpponen I.; Clarke S. P.; Brougham D. F.; Argyropoulos D. S. Production of Cellulose Nanocrystals Using Hydrobromic Acid and Click Reactions on Their Surface. J. Mater. Sci. 2011, 46, 7344–7355..

    Not in our library10.1007/s10853-011-5696-0

  506. 506.

    Barazzouk S.; Daneault C. Amino Acid and Peptide Immobilization on Oxidized Nanocellulose: Spectroscopic Characterization. Nanomaterials 2012, 2, 187–205..

    Not in our library10.3390/nano2020187

  507. 507.

    Albericio F.; El-Faham A. Choosing the Right Coupling Reagent for Peptides: A Twenty-Five-Year Journey. Org. Process Res. Dev. 2018, 22, 760–772..

    Not in our library10.1021/acs.oprd.8b00159

  508. 508.

    Billman J. H.; Diesing A. C. Reduction of Schiff Bases with Sodium Borohydride. J. Org. Chem. 1957, 22, 1068–1070..

    Not in our library10.1021/jo01360a019

  509. 509.

    Andresen M.; Johansson L.-S.; Tanem B. S.; Stenius P. Properties and Characterization of Hydrophobized Microfibrillated Cellulose. Cellulose 2006, 13, 665–677..

    Not in our library10.1007/s10570-006-9072-1

  510. 510.

    Goussé C.; Chanzy H.; Excoffier G.; Soubeyrand L.; Fleury E. Stable Suspensions of Partially Silylated Cellulose Whiskers Dispersed in Organic Solvents. Polymer 2002, 43, 2645–2651..

    Not in our library10.1016/s0032-3861(02)00051-4

  511. 511.

    Gousse C.; Chanzy H.; Cerrada M.; Fleury E. Surface Silylation of Cellulose Microfibrils: Preparation and Rheological Properties. Polymer 2004, 45, 1569–1575..

    Not in our library10.1016/j.polymer.2003.12.028

  512. 512.

    Zhang Z.; Sèbe G.; Rentsch D.; Zimmermann T.; Tingaut P. Ultralightweight and Flexible Silylated Nanocellulose Sponges for the Selective Removal of Oil from Water. Chem. Mater. 2014, 26, 2659–2668..

    Not in our library10.1021/cm5004164

  513. 513.

    Beaumont M.; Bacher M.; Opietnik M.; Gindl-Altmutter W.; Potthast A.; Rosenau T. A General Aqueous Silanization Protocol to Introduce Vinyl, Mercapto or Azido Functionalities onto Cellulose Fibers and Nanocelluloses. Molecules 2018, 23, 1427.

    Not in our library10.3390/molecules23061427

  514. 514.

    Kaldéus T.; Telaretti Leggieri M. R.; Cobo Sanchez C.; Malmström E. All-Aqueous Si-Arget Atrp from Cellulose Nanofibrils Using Hydrophilic and Hydrophobic Monomers. Biomacromolecules 2019, 20, 1937–1943..

    Not in our library10.1021/acs.biomac.9b00153

  515. 515.

    Majoinen J.; Walther A.; McKee J. R.; Kontturi E.; Aseyev V.; Malho J. M.; Ruokolainen J.; Ikkala O. Polyelectrolyte Brushes Grafted from Cellulose Nanocrystals Using Cu-Mediated Surface-Initiated Controlled Radical Polymerization. Biomacromolecules 2011, 12, 2997–3006..

    Not in our library10.1021/bm200613y

  516. 516.

    Dong H.; Napadensky E.; Orlicki J. A.; Snyder J. F.; Chantawansri T. L.; Kapllani A. Cellulose Nanofibrils and Diblock Copolymer Complex: Micelle Formation and Enhanced Dispersibility. ACS Sustainable Chem. Eng. 2017, 5, 1264–1271..

    Not in our library10.1021/acssuschemeng.6b00811

  517. 517.

    Gimåker M.; Wågberg L. Adsorption of Polyallylamine to Lignocellulosic Fibres: Effect of Adsorption Conditions on Localisation of Adsorbed Polyelectrolyte and Mechanical Properties of Resulting Paper Sheets. Cellulose 2009, 16, 87–101..

    Not in our library10.1007/s10570-008-9240-6

  518. 518.

    Kittle J. D.; Wondraczek H.; Wang C.; Jiang F.; Roman M.; Heinze T.; Esker A. R. Enhanced Dewatering of Polyelectrolyte Nanocomposites by Hydrophobic Polyelectrolytes. Langmuir 2012, 28, 11086–11094..

    Not in our library10.1021/la3016996

  519. 519.

    Utsel S.; Bruce C.; Pettersson T. r.; Fogelström L.; Carlmark A.; Malmström E.; Wågberg L. Physical Tuning of Cellulose-Polymer Interactions Utilizing Cationic Block Copolymers Based on PCL and Quaternized PDMAEMA. ACS Appl. Mater. Interfaces 2012, 4, 6796–6807..

    Not in our library10.1021/am301981r

  520. 520.

    Utsel S.; Carlmark A.; Pettersson T.; Bergström M.; Malmström E. E.; Wågberg L. Synthesis, Adsorption and Adhesive Properties of a Cationic Amphiphilic Block Copolymer for Use as Compatibilizer in Composites. Eur. Polym. J. 2012, 48, 1195–1204..

    Not in our library10.1016/j.eurpolymj.2012.05.004

  521. 521.

    Vuoriluoto M.; Orelma H.; Johansson L.-S.; Zhu B.; Poutanen M.; Walther A.; Laine J.; Rojas O. J. Effect of Molecular Architecture of Pdmaema–Poegma Random and Block Copolymers on Their Adsorption on Regenerated and Anionic Nanocelluloses and Evidence of Interfacial Water Expulsion. J. Phys. Chem. B 2015, 119, 15275–15286..

    Not in our library10.1021/acs.jpcb.5b07628

  522. 522.

    Ly M.; Mekonnen T. H. Cationic Surfactant Modified Cellulose Nanocrystals for Corrosion Protective Nanocomposite Surface Coatings. J. Ind. Eng. Chem. 2020, 83, 409–420..

    Not in our library10.1016/j.jiec.2019.12.014

  523. 523.

    Villalobos R.; Hernández-Muñoz P.; Chiralt A. Effect of Surfactants on Water Sorption and Barrier Properties of Hydroxypropyl Methylcellulose Films. Food Hydrocolloids 2006, 20, 502–509..

    Not in our library10.1016/j.foodhyd.2005.04.006

  524. 524.

    Kontturi K. S.; Biegaj K.; Mautner A.; Woodward R. T.; Wilson B. P.; Johansson L.-S.; Lee K.-Y.; Heng J. Y.; Bismarck A.; Kontturi E. Noncovalent Surface Modification of Cellulose Nanopapers by Adsorption of Polymers from Aprotic Solvents. Langmuir 2017, 33, 5707–5712..

    Not in our library10.1021/acs.langmuir.7b01236

  525. 525.

    Larsson M.; Johnsson A.; Gårdebjer S.; Bordes R.; Larsson A. Swelling and Mass Transport Properties of Nanocellulose-HPMC Composite Films. Mater. Des. 2017, 122, 414–421..

    Not in our library10.1016/j.matdes.2017.03.011

  526. 526.

    Bouchard J.; Méthot M.; Fraschini C.; Beck S. Effect of Oligosaccharide Deposition on the Surface of Cellulose Nanocrystals as a Function of Acid Hydrolysis Temperature. Cellulose 2016, 23, 3555–3567..

    Not in our library10.1007/s10570-016-1036-5

  527. 527.

    Beck S.; Bouchard J.; Berry R. Controlling the Reflection Wavelength of Iridescent Solid Films of Nanocrystalline Cellulose. Biomacromolecules 2011, 12, 167–172..

    Not in our library10.1021/bm1010905

  528. 528.

    Niinivaara E.; Vanderfleet O. M.; Kontturi E.; Cranston E. D. Tuning the Physicochemical Properties of Cellulose Nanocrystals through an In Situ Oligosaccharide Surface Modification Method. Biomacromolecules 2021, 22, 3284–3296..

    Not in our library10.1021/acs.biomac.1c00384

  529. 529.

    Kubo R.; Saito T.; Isogai A. Dual Counterion Systems of Carboxylated Nanocellulose Films with Tunable Mechanical, Hydrophilic, and Gas-Barrier Properties. Biomacromolecules 2019, 20, 1691–1698..

    Not in our library10.1021/acs.biomac.9b00057

  530. 530.

    Kim J.; Montero G.; Habibi Y.; Hinestroza J. P.; Genzer J.; Argyropoulos D. S.; Rojas O. J. Dispersion of Cellulose Crystallites by Nonionic Surfactants in a Hydrophobic Polymer Matrix. Polym. Eng. Sci. 2009, 49, 2054–2061..

    Not in our library10.1002/pen.21417

  531. 531.

    Fortunati E.; Mattioli S.; Armentano I.; Kenny J. M. Spin Coated Cellulose Nanocrystal/Silver Nanoparticle Films. Carbohydr. Polym. 2014, 113, 394–402..

    Not in our library10.1016/j.carbpol.2014.07.010

  532. 532.

    Salajková M.; Berglund L. A.; Zhou Q. Hydrophobic Cellulose Nanocrystals Modified with Quaternary Ammonium Salts. J. Mater. Chem. 2012, 22, 19798–19805..

    Not in our library10.1039/c2jm34355j

  533. 533.

    Abitbol T.; Marway H.; Cranston E. D. Surface Modification of Cellulose Nanocrystals with Cetyltrimethylammonium Bromide. Nordic Pulp Pap. Res. J. 2014, 29, 46–57..

    Not in our library10.3183/npprj-2014-29-01-p046-057

  534. 534.

    Fox D. M.; Rodriguez R. S.; Devilbiss M. N.; Woodcock J.; Davis C. S.; Sinko R.; Keten S.; Gilman J. W. Simultaneously Tailoring Surface Energies and Thermal Stabilities of Cellulose Nanocrystals Using Ion Exchange: Effects on Polymer Composite Properties for Transportation, Infrastructure, and Renewable Energy Applications. ACS Appl. Mater. Interfaces 2016, 8, 27270–27281..

    Not in our library10.1021/acsami.6b06083

  535. 535.

    Wang X.; Xu S.; Tan Y.; Du J.; Wang J. Synthesis and Characterization of a Porous and Hydrophobic Cellulose-Based Composite for Efficient and Fast Oil–Water Separation. Carbohydr. Polym. 2016, 140, 188–194..

    Not in our library10.1016/j.carbpol.2015.12.028

  536. 536.

    Lazzari L. K.; Zampieri V. B.; Zanini M.; Zattera A. J.; Baldasso C. Sorption Capacity of Hydrophobic Cellulose Cryogels Silanized by Two Different Methods. Cellulose 2017, 24, 3421–3431..

    Not in our library10.1007/s10570-017-1349-z

  537. 537.

    Sousa Pereira A. L.; Andrade Feitosa J. P.; Saraiva Morais J. P.; de Freitas Rosa M. Bacterial Cellulose Aerogels: Influence of Oxidation and Silanization on Mechanical and Absorption Properties. Carbohydr. Polym. 2020, 250, 116927.

    Not in our library10.1016/j.carbpol.2020.116927

  538. 538.

    Robles E.; Urruzola I.; Labidi J.; Serrano L. Surface-Modified Nano-Cellulose as Reinforcement in Poly (Lactic Acid) to Conform New Composites. Ind. Crops Prod. 2015, 71, 44–53..

    Not in our library10.1016/j.indcrop.2015.03.075

  539. 539.

    Zanini M.; Lavoratti A.; Lazzari L. K.; Galiotto D.; Pagnocelli M.; Baldasso C.; Zattera A. J. Producing Aerogels from Silanized Cellulose Nanofiber Suspension. Cellulose 2017, 24, 769–779..

    Not in our library10.1007/s10570-016-1142-4

  540. 540.

    Frank B. P.; Durkin D. P.; Caudill E. R.; Zhu L.; White D. H.; Curry M. L.; Pedersen J. A.; Fairbrother D. H. Impact of Silanization on the Structure, Dispersion Properties, and Biodegradability of Nanocellulose as a Nanocomposite Filler. ACS Appl. Nano Mater. 2018, 1, 7025–7038..

    Not in our library10.1021/acsanm.8b01819

  541. 541.

    Jin K.; Tang Y.; Zhu X.; Zhou Y. Polylactic Acid Based Biocomposite Films Reinforced with Silanized Nanocrystalline Cellulose. Int. J. Biol. Macromol. 2020, 162, 1109–1117..

    Not in our library10.1016/j.ijbiomac.2020.06.201

  542. 542.

    Gericke M.; Schaller J.; Liebert T.; Fardim P.; Meister F.; Heinze T. Studies on the Tosylation of Cellulose in Mixtures of Ionic Liquids and a Co-Solvent. Carbohydr. Polym. 2012, 89, 526–536..

    Not in our library10.1016/j.carbpol.2012.03.040

  543. 543.

    Elchinger P.-H.; Faugeras P.-A.; Zerrouki C.; Montplaisir D.; Brouillette F.; Zerrouki R. Tosylcellulose Synthesis in Aqueous Medium. Green Chem. 2012, 14, 3126–3131..

    Not in our library10.1039/c2gc35592b

  544. 544.

    Guo J.; Filpponen I.; Su P.; Laine J.; Rojas O. J. Attachment of Gold Nanoparticles on Cellulose Nanofibrils Via Click Reactions and Electrostatic Interactions. Cellulose 2016, 23, 3065–3075..

    Not in our library10.1007/s10570-016-1042-7

  545. 545.

    Salminen R.; Reza M.; Pääkkönen T.; Peyre J.; Kontturi E. Tempo-Mediated Oxidation of Microcrystalline Cellulose: Limiting Factors for Cellulose Nanocrystal Yield. Cellulose 2017, 24, 1657–1667..

    Not in our library10.1007/s10570-017-1228-7

  546. 546.

    Isogai A.; Zhou Y. Diverse Nanocelluloses Prepared from Tempo-Oxidized Wood Cellulose Fibers: Nanonetworks, Nanofibers, and Nanocrystals. Curr. Opin. Solid State Mater. Sci. 2019, 23, 101–106..

    Not in our library10.1016/j.cossms.2019.01.001

  547. 547.

    Iwamoto S.; Kai W.; Isogai T.; Saito T.; Isogai A.; Iwata T. Comparison Study of Tempo-Analogous Compounds on Oxidation Efficiency of Wood Cellulose for Preparation of Cellulose Nanofibrils. Polym. Degrad. Stab. 2010, 95, 1394–1398..

    Not in our library10.1016/j.polymdegradstab.2010.01.017

  548. 548.

    Beaumont M.; König J.; Opietnik M.; Potthast A.; Rosenau T. Drying of a Cellulose Ii Gel: Effect of Physical Modification and Redispersibility in Water. Cellulose 2017, 24, 1199–1209..

    Not in our library10.1007/s10570-016-1166-9

  549. 549.

    Xia T.; Huang Y.; Lan P.; Lan L.; Lin N. Physical Modification of Cellulose Nanocrystals with a Synthesized Triblock Copolymer and Rheological Thickening in Silicone Oil/Grease. Biomacromolecules 2019, 20, 4457–4465..

    Not in our library10.1021/acs.biomac.9b01186

  550. 550.

    Zhu G.; Chen Z.; Wu B.; Lin N. Dual-Enhancement Effect of Electrostatic Adsorption and Chemical Crosslinking for Nanocellulose-Based Aerogels. Ind. Crops Prod. 2019, 139, 111580.

    Not in our library10.1016/j.indcrop.2019.111580

  551. 551.

    Ma X.; Wang Y.; Shen Y.; Huang J.; Dufresne A. Current Status of Nanocellulose-Based Nanocomposites. In Nanocellulose: From Fundamentals to Advanced Materials; Huang J., Dufresne A., Ning L., Eds., Wiley-VCH: Weinheim, Germany, 2019; pp 155–200.

    Not in our library

  552. 552.

    Tardy B. L.; Yokota S.; Ago M.; Xiang W.; Kondo T.; Bordes R.; Rojas O. J. Nanocellulose–Surfactant Interactions. Curr. Opin. Colloid Interface Sci. 2017, 29, 57–67..

    Not in our library10.1016/j.cocis.2017.02.004

  553. 553.

    Souza A.; Santos D.; Ferreira R.; Pinto V.; Rosa D. Innovative Process for Obtaining Modified Nanocellulose from Soybean Straw. Int. J. Biol. Macromol. 2020, 165, 1803–1812..

    Not in our library10.1016/j.ijbiomac.2020.10.036

  554. 554.

    Santmarti A.; Tammelin T.; Lee K.- Y. Prevention of Interfibril Hornification by Replacing Water in Nanocellulose Gel with Low Molecular Weight Liquid Poly (Ethylene Glycol). Carbohydr. Polym. 2020, 250, 116870.

    Not in our library10.1016/j.carbpol.2020.116870

  555. 555.

    Reid M. S.; Villalobos M.; Cranston E. D. The Role of Hydrogen Bonding in Non-Ionic Polymer Adsorption to Cellulose Nanocrystals and Silica Colloids. Curr. Opin. Colloid Interface Sci. 2017, 29, 76–82..

    Not in our library10.1016/j.cocis.2017.03.005

  556. 556.

    Yahia M.; Mei S.; Mathew A. P.; Yuan J. Linear Main-Chain 1, 2, 4-Triazolium Poly (Ionic Liquid) S: Single-Step Synthesis and Stabilization of Cellulose Nanocrystals. ACS Macro Lett. 2019, 8, 1372–1377..

    Not in our library10.1021/acsmacrolett.9b00542

  557. 557.

    Michalek L.; Mundsinger K.; Barner-Kowollik C.; Barner L. The Long and the Short of Polymer Grafting. Polym. Chem. 2019, 10, 54–59..

    Not in our library10.1039/c8py01470a

  558. 558.

    Zhang M.; Wiener C. G.; Sepulveda-Medina P. I.; Douglas J. F.; Vogt B. D. Influence of Sodium Salts on the Swelling and Rheology of Hydrophobically Cross-Linked Hydrogels Determined by QCM-D. Langmuir 2019, 35, 16612–16623..

    Not in our library10.1021/acs.langmuir.9b03063

  559. 559.

    Djafari Petroudy S. R.; Ranjbar J.; Rasooly Garmaroody E. Eco-Friendly Superabsorbent Polymers Based on Carboxymethyl Cellulose Strengthened by Tempo-Mediated Oxidation Wheat Straw Cellulose Nanofiber. Carbohydr. Polym. 2018, 197, 565–575..

    Not in our library10.1016/j.carbpol.2018.06.008

  560. 560.

    Isogai A.; Saito T.; Fukuzumi H. TEMPO-Oxidized Cellulose Nanofibers. Nanoscale 2011, 3, 71–85..

    Not in our library10.1039/c0nr00583e

  561. 561.

    Hamad W. Y.; Hu T. Q. Structure–Process–Yield Interrelations in Nanocrystalline Cellulose Extraction. Can. J. Chem. Eng. 2010, 88, 392–402..

    Not in our library10.1002/cjce.20298

  562. 562.

    Yang M.; Hadi P.; Yin X.; Yu J.; Huang X.; Ma H.; Walker H.; Hsiao B. S. Antifouling Nanocellulose Membranes: How Subtle Adjustment of Surface Charge Lead to Self-Cleaning Property. J. Membr. Sci. 2021, 618, 118739.

    Not in our library10.1016/j.memsci.2020.118739

  563. 563.

    Cherhal F.; Cousin F.; Capron I. Influence of Charge Density and Ionic Strength on the Aggregation Process of Cellulose Nanocrystals in Aqueous Suspension, as Revealed by Small-Angle Neutron Scattering. Langmuir 2015, 31, 5596–5602..

    Not in our library10.1021/acs.langmuir.5b00851

  564. 564.

    Niinivaara E.; Cranston E. D. Bottom-up Assembly of Nanocellulose Structures. Carbohydr. Polym. 2020, 247, 116664.

    Not in our library10.1016/j.carbpol.2020.116664

  565. 565.

    Barajas-Ledesma R. M.; Patti A. F.; Wong V. N.; Raghuwanshi V. S.; Garnier G. Engineering Nanocellulose Superabsorbent Structure by Controlling the Drying Rate. Colloids Surf., A 2020, 600, 124943.

    Not in our library10.1016/j.colsurfa.2020.124943

  566. 566.

    Viet D.; Beck-Candanedo S.; Gray D. G. Dispersion of Cellulose Nanocrystals in Polar Organic Solvents. Cellulose 2007, 14, 109–113..

    Not in our library10.1007/s10570-006-9093-9

  567. 567.

    Le Gars M.; Roger P.; Belgacem N.; Bras J. Role of Solvent Exchange in Dispersion of Cellulose Nanocrystals and Their Esterification Using Fatty Acids as Solvents. Cellulose 2020, 27, 4319–4336..

    Not in our library10.1007/s10570-020-03101-0

  568. 568.

    Chang H.; Luo J.; Bakhtiary Davijani A. A.; Chien A.-T.; Wang P.-H.; Liu H. C.; Kumar S. Individually Dispersed Wood-Based Cellulose Nanocrystals. ACS Appl. Mater. Interfaces 2016, 8, 5768–5771..

    Not in our library10.1021/acsami.6b00094

  569. 569.

    Odabas N.; Amer H.; Bacher M.; Henniges U.; Potthast A.; Rosenau T. Properties of Cellulosic Material after Cationization in Different Solvents. ACS Sustainable Chem. Eng. 2016, 4, 2295–2301..

    Not in our library10.1021/acssuschemeng.5b01752

  570. 570.

    Bercea M.; Navard P. Shear Dynamics of Aqueous Suspensions of Cellulose Whiskers. Macromolecules 2000, 33, 6011–6016..

    Not in our library10.1021/ma000417p

  571. 571.

    Ureña-Benavides E. E.; Ao G.; Davis V. A.; Kitchens C. L. Rheology and Phase Behavior of Lyotropic Cellulose Nanocrystal Suspensions. Macromolecules 2011, 44, 8990–8998..

    Not in our library10.1021/ma201649f

  572. 572.

    Shafiei-Sabet S.; Hamad W. Y.; Hatzikiriakos S. G. Rheology of Nanocrystalline Cellulose Aqueous Suspensions. Langmuir 2012, 28, 17124–17133..

    Not in our library10.1021/la303380v

  573. 573.

    Agoda-Tandjawa G.; Durand S.; Berot S.; Blassel C.; Gaillard C.; Garnier C.; Doublier J.-L. Rheological Characterization of Microfibrillated Cellulose Suspensions after Freezing. Carbohydr. Polym. 2010, 80, 677–686..

    Not in our library10.1016/j.carbpol.2009.11.045

  574. 574.

    Dumanli A. G.; Kamita G.; Landman J.; van der Kooij H.; Glover B. J.; Baumberg J. J.; Steiner U.; Vignolini S. Controlled, Bio-Inspired Self-Assembly of Cellulose-Based Chiral Reflectors. Adv. Opt. Mater. 2014, 2, 646–650..

    Not in our library10.1002/adom.201400112

  575. 575.

    Markstedt K.; Mantas A.; Tournier I.; Martínez Ávila H. c.; Hagg D.; Gatenholm P. 3d Bioprinting Human Chondrocytes with Nanocellulose–Alginate Bioink for Cartilage Tissue Engineering Applications. Biomacromolecules 2015, 16, 1489–1496..

    Not in our library10.1021/acs.biomac.5b00188

  576. 576.

    Saremi R.; Borodinov N.; Laradji A. M.; Sharma S.; Luzinov I.; Minko S. Adhesion and Stability of Nanocellulose Coatings on Flat Polymer Films and Textiles. Molecules 2020, 25, 3238.

    Not in our library10.3390/molecules25143238

  577. 577.

    Vilela C.; Silvestre A. J. D.; Figueiredo F. M. L.; Freire C. S. R. Nanocellulose-Based Materials as Components of Polymer Electrolyte Fuel Cells. J. Mater. Chem. A 2019, 7, 20045–20074..

    Not in our library10.1039/c9ta07466j

  578. 578.

    Liu D. Y.; Sui G.; Bhattacharyya D. Synthesis and Characterisation of Nanocellulose-Based Polyaniline Conducting Films. Compos. Sci. Technol. 2014, 99, 31–36..

    Not in our library10.1016/j.compscitech.2014.05.001

  579. 579.

    Ludwicka K.; Kolodziejczyk M.; Gendaszewska-Darmach E.; Chrzanowski M.; Jedrzejczak-Krzepkowska M.; Rytczak P.; Bielecki S. Stable Composite of Bacterial Nanocellulose and Perforated Polypropylene Mesh for Biomedical Applications. J. Biomed. Mater. Res. Part B: Appl. Biomater. 2019, 107, 978–987..

    Not in our library10.1002/jbm.b.34191

  580. 580.

    Hubbe M. A.; Tayeb P.; Joyce M.; Tyagi P.; Kehoe M.; Dimic-Misic K.; Pal L. Rheology of Nanocellulose-Rich Aqueous Suspensions: A Review. BioResources 2017, 12, 9556–9661..

    Not in our library10.15376/biores.12.4.hubbe

  581. 581.

    Gatenholm P.; Klemm D. Bacterial Nanocellulose as a Renewable Material for Biomedical Applications. MRS Bull. 2010, 35, 208–213..

    Not in our library10.1557/mrs2010.653

  582. 582.

    Gray D. G. Order and Gelation of Cellulose Nanocrystal Suspensions: An Overview of Some Issues. Philos. Trans. R. Soc. A 2018, 376, 20170038.

    Not in our library10.1098/rsta.2017.0038

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    Nascimento D. M.; Nunes Y. L.; Figueirêdo M. C.; de Azeredo H. M.; Aouada F. A.; Feitosa J. P.; Rosa M. F.; Dufresne A. Nanocellulose Nanocomposite Hydrogels: Technological and Environmental Issues. Green Chem. 2018, 20, 2428–2448..

    Not in our library10.1039/c8gc00205c

  584. 584.

    Curvello R.; Raghuwanshi V. S.; Garnier G. Engineering Nanocellulose Hydrogels for Biomedical Applications. Adv. Colloid Interface Sci. 2019, 267, 47–61..

    Not in our library10.1016/j.cis.2019.03.002

  585. 585.

    Yang J.; Xu F.; Han C.-R. Metal Ion Mediated Cellulose Nanofibrils Transient Network in Covalently Cross-Linked Hydrogels: Mechanistic Insight into Morphology and Dynamics. Biomacromolecules 2017, 18, 1019–1028..

    Not in our library10.1021/acs.biomac.6b01915

  586. 586.

    Lasseuguette E.; Roux D.; Nishiyama Y. Rheological Properties of Microfibrillar Suspension of Tempo-Oxidized Pulp. Cellulose 2008, 15, 425–433..

    Not in our library10.1007/s10570-007-9184-2

  587. 587.

    Li Y.; Li X.; Chen C.; Zhao D.; Su Z.; Ma G.; Yu R. A Rapid, Non-Invasive and Non-Destructive Method for Studying Swelling Behavior and Microstructure Variations of Hydrogels. Carbohydr. Polym. 2016, 151, 1251–1260..

    Not in our library10.1016/j.carbpol.2016.06.054

  588. 588.

    Wu Q.; Meng Y.; Wang S.; Li Y.; Fu S.; Ma L.; Harper D. Rheological Behavior of Cellulose Nanocrystal Suspension: Influence of Concentration and Aspect Ratio. J. Appl. Polym. Sci. 2014, 131, 40525.

    Not in our library10.1002/app.40525

  589. 589.

    Jhon M. S.; Andrade J. D. Water and Hydrogels. J. Biomed. Mater. Res. 1973, 7, 509–522..

    Not in our library10.1002/jbm.820070604

  590. 590.

    Pasqui D.; De Cagna M.; Barbucci R. Polysaccharide-Based Hydrogels: The Key Role of Water in Affecting Mechanical Properties. Polymers 2012, 4, 1517–1534..

    Not in our library10.3390/polym4031517

  591. 591.

    Bonilla M. R.; Lopez-Sanchez P.; Gidley M.; Stokes J. Micromechanical Model of Biphasic Biomaterials with Internal Adhesion: Application to Nanocellulose Hydrogel Composites. Acta Biomater. 2016, 29, 149–160..

    Not in our library10.1016/j.actbio.2015.10.032

  592. 592.

    Dong H.; Snyder J. F.; Williams K. S.; Andzelm J. W. Cation-Induced Hydrogels of Cellulose Nanofibrils with Tunable Moduli. Biomacromolecules 2013, 14, 3338–3345..

    Not in our library10.1021/bm400993f

  593. 593.

    Zander N. E.; Dong H.; Steele J.; Grant J. T. Metal Cation Cross-Linked Nanocellulose Hydrogels as Tissue Engineering Substrates. ACS Appl. Mater. Interfaces 2014, 6, 18502–18510..

    Not in our library10.1021/am506007z

  594. 594.

    Xu C.; Zhang Molino B.; Wang X.; Cheng F.; Xu W.; Molino P.; Bacher M.; Su D.; Rosenau T.; Willför S.; Wallace G. 3d Printing of Nanocellulose Hydrogel Scaffolds with Tunable Mechanical Strength Towards Wound Healing Application. J. Mater. Chem. B 2018, 6, 7066–7075..

    Not in our library10.1039/c8tb01757c

  595. 595.

    Liang L.; Bhagia S.; Li M.; Huang C.; Ragauskas A. J. Cross-Linked Nanocellulosic Materials and Their Applications. ChemSusChem 2020, 13, 78.

    Not in our library10.1002/cssc.201901676

  596. 596.

    Al-Sabah A.; Burnell S. E.; Simoes I. N.; Jessop Z.; Badiei N.; Blain E.; Whitaker I. S. Structural and Mechanical Characterization of Crosslinked and Sterilised Nanocellulose-Based Hydrogels for Cartilage Tissue Engineering. Carbohydr. Polym. 2019, 212, 242–251..

    Not in our library10.1016/j.carbpol.2019.02.057

  597. 597.

    Phogat K.; Bandyopadhyay-Ghosh S. Nanocellulose Mediated Injectable Bio-Nanocomposite Hydrogel Scaffold-Microstructure and Rheological Properties. Cellulose 2018, 25, 5821–5830..

    Not in our library10.1007/s10570-018-2001-2

  598. 598.

    Shahzamani M.; Taheri S.; Roghanizad A.; Naseri N.; Dinari M. Preparation and Characterization of Hydrogel Nanocomposite Based on Nanocellulose and Acrylic Acid in the Presence of Urea. Int. J. Biol. Macromol. 2020, 147, 187–193..

    Not in our library10.1016/j.ijbiomac.2020.01.038

  599. 599.

    Nair S. S.; Zhu J.; Deng Y.; Ragauskas A. J. Hydrogels Prepared from Cross-Linked Nanofibrillated Cellulose. ACS Sustainable Chem. Eng. 2014, 2, 772–780..

    Not in our library10.1021/sc400445t

  600. 600.

    Way A. E.; Hsu L.; Shanmuganathan K.; Weder C.; Rowan S. J. Ph-Responsive Cellulose Nanocrystal Gels and Nanocomposites. ACS Macro Lett. 2012, 1, 1001–1006..

    Not in our library10.1021/mz3003006

  601. 601.

    Hu Z.; Cranston E. D.; Ng R.; Pelton R. Tuning Cellulose Nanocrystal Gelation with Polysaccharides and Surfactants. Langmuir 2014, 30, 2684–2692..

    Not in our library10.1021/la404977t

  602. 602.

    Mendoza L.; Gunawardhana T.; Batchelor W.; Garnier G. Nanocellulose for Gel Electrophoresis. J. Colloid Interface Sci. 2019, 540, 148–154..

    Not in our library10.1016/j.jcis.2019.01.017

  603. 603.

    Basu A.; Lindh J.; Ålander E.; Strømme M.; Ferraz N. On the Use of Ion-Crosslinked Nanocellulose Hydrogels for Wound Healing Solutions: Physicochemical Properties and Application-Oriented Biocompatibility Studies. Carbohydr. Polym. 2017, 174, 299–308..

    Not in our library10.1016/j.carbpol.2017.06.073

  604. 604.

    Chau M.; Sriskandha S. E.; Pichugin D.; Thérien-Aubin H. l.; Nykypanchuk D.; Chauve G. g.; Méthot M.; Bouchard J.; Gang O.; Kumacheva E. Ion-Mediated Gelation of Aqueous Suspensions of Cellulose Nanocrystals. Biomacromolecules 2015, 16, 2455–2462..

    Not in our library10.1021/acs.biomac.5b00701

  605. 605.

    Nigmatullin R.; Harniman R.; Gabrielli V.; Muñoz-García J. C.; Khimyak Y. Z.; Angulo J. s.; Eichhorn S. J. Mechanically Robust Gels Formed from Hydrophobized Cellulose Nanocrystals. ACS Appl. Mater. Interfaces 2018, 10, 19318–19322..

    Not in our library10.1021/acsami.8b05067

  606. 606.

    Nigmatullin R.; Gabrielli V.; Muñoz-García J. C.; Lewandowska A. E.; Harniman R.; Khimyak Y. Z.; Angulo J.; Eichhorn S. J. Thermosensitive Supramolecular and Colloidal Hydrogels Via Self-Assembly Modulated by Hydrophobized Cellulose Nanocrystals. Cellulose 2019, 26, 529–542..

    Not in our library10.1007/s10570-018-02225-8

  607. 607.

    De France K. J.; Yager K. G.; Chan K. J.; Corbett B.; Cranston E. D.; Hoare T. Injectable Anisotropic Nanocomposite Hydrogels Direct in Situ Growth and Alignment of Myotubes. Nano Lett. 2017, 17, 6487–6495..

    Not in our library10.1021/acs.nanolett.7b03600

  608. 608.

    Supramaniam J.; Adnan R.; Mohd Kaus N. H.; Bushra R. Magnetic Nanocellulose Alginate Hydrogel Beads as Potential Drug Delivery System. Int. J. Biol. Macromol. 2018, 118, 640–648..

    Not in our library10.1016/j.ijbiomac.2018.06.043

  609. 609.

    Yao K.; Meng Q.; Bulone V.; Zhou Q. Flexible and Responsive Chiral Nematic Cellulose Nanocrystal/Poly (Ethylene Glycol) Composite Films with Uniform and Tunable Structural Color. Adv. Mater. 2017, 29, 1701323.

    Not in our library10.1002/adma.201701323

  610. 610.

    Olsson A.-M.; Salmén L. The Association of Water to Cellulose and Hemicellulose in Paper Examined by Ftir Spectroscopy. Carbohydr. Res. 2004, 339, 813–818..

    Not in our library10.1016/j.carres.2004.01.005

  611. 611.

    Salmén L.; Olsson A.-M. Interaction between Hemicelluloses, Lignin and Cellulose: Structure-Property Relationships. J. Pulp Pap. Sci. 1998, 24, 99–103.

    Not in our library

  612. 612.

    Berry S. L.; Roderick M. L. Plant–Water Relations and the Fibre Saturation Point. New Phytol. 2005, 168, 25–37..

    Not in our library10.1111/j.1469-8137.2005.01528.x

  613. 613.

    Engelund E. T.; Thygesen L. G.; Svensson S.; Hill C. A. A Critical Discussion of the Physics of Wood–Water Interactions. Wood Sci. Technol. 2013, 47, 141–161..

    Not in our library10.1007/s00226-012-0514-7

  614. 614.

    Hatakeyama T.; Tanaka M.; Hatakeyama H. Studies on Bound Water Restrained by Poly (2-Methacryloyloxyethyl Phosphorylcholine): Comparison with Polysaccharide–Water Systems. Acta Biomater. 2010, 6, 2077–2082..

    Not in our library10.1016/j.actbio.2009.12.018

  615. 615.

    Hatakeyama T.; Tanaka M.; Hatakeyama H. Thermal Properties of Freezing Bound Water Restrained by Polysaccharides. J. Biomater. Sci., Polym. Ed. 2010, 21, 1865–1875..

    Not in our library10.1163/092050610x486946

  616. 616.

    Jorfi M.; Foster E. J. Recent Advances in Nanocellulose for Biomedical Applications. J. Appl. Polym. Sci. 2015, 132, 41719.

    Not in our library10.1002/app.41719

  617. 617.

    Liu W.; Du H.; Zhang M.; Liu K.; Liu H.; Xie H.; Zhang X.; Si C. Bacterial Cellulose Based Composite Scaffolds for Biomedical Applications: A Review. ACS Sustainable Chem. Eng. 2020, 8, 7536.

    Not in our library10.1021/acssuschemeng.0c00125

  618. 618.

    Nishiguchi A.; Taguchi T. A Thixotropic, Cell-Infiltrative Nanocellulose Hydrogel That Promotes in Vivo Tissue Remodeling. ACS Biomater. Sci. Eng. 2020, 6, 946–958..

    Not in our library10.1021/acsbiomaterials.9b01549

  619. 619.

    Monfared M.; Mawad D.; Rnjak-Kovacina J.; Stenzel M. H. 3D Bioprinting of Dual-Crosslinked Nanocellulose Hydrogels for Tissue Engineering Applications. J. Mater. Chem. B 2021, 9, 6163–6175..

    Not in our library10.1039/d1tb00624j

  620. 620.

    Balalakshmi C.; Jeyachandran S. Advances of Nanocellulose in Biomedical Applications. In Handbook of Nanocelluloses: Classification, Properties, Fabrication, and Emerging Applications; Barhoum A., Ed.; Springer: New York, 2022; pp 1–31.

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  621. 621.

    Chinga-Carrasco G. Potential and Limitations of Nanocelluloses as Components in Biocomposite Inks for Three-Dimensional Bioprinting and for Biomedical Devices. Biomacromolecules 2018, 19, 701–711..

    Not in our library10.1021/acs.biomac.8b00053

  622. 622.

    Xu W.; Wang X.; Sandler N.; Willför S.; Xu C. Three-Dimensional Printing of Wood-Derived Biopolymers: A Review Focused on Biomedical Applications. ACS Sustainable Chem. Eng. 2018, 6, 5663–5680..

    Not in our library10.1021/acssuschemeng.7b03924

  623. 623.

    Liu J.; Chinga-Carrasco G.; Cheng F.; Xu W.; Willför S.; Syverud K.; Xu C. Hemicellulose-Reinforced Nanocellulose Hydrogels for Wound Healing Application. Cellulose 2016, 23, 3129–3143..

    Not in our library10.1007/s10570-016-1038-3

  624. 624.

    Luo J.; Huang K.; Zhou X.; Xu Y. Hybrid Films Based on Holistic Celery Nanocellulose and Lignin/Hemicellulose with Enhanced Mechanical Properties and Dye Removal. Int. J. Biol. Macromol. 2020, 147, 699–705..

    Not in our library10.1016/j.ijbiomac.2020.01.102

  625. 625.

    Kovalenko A. Predictive Multiscale Modeling of Nanocellulose Based Materials and Systems. In 2nd International Conference on Structural Nano Composites (NANOSTRUC 2014) 20–21 May 2014, Madrid, Spain; IOP Conference Series: Materials Science and Engineering, IOP, 2014; Vol. 64.

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  626. 626.

    Arola S.; Ansari M.; Oksanen A.; Retulainen E.; Hatzikiriakos S. G.; Brumer H. The Sol–Gel Transition of Ultra-Low Solid Content Tempo-Cellulose Nanofibril/Mixed-Linkage Β-Glucan Bionanocomposite Gels. Soft Matter 2018, 14, 9393–9401..

    Not in our library10.1039/c8sm01878b

  627. 627.

    Pääkkönen T.; Dimic-Misic K.; Orelma H.; Pönni R.; Vuorinen T.; Maloney T. Effect of Xylan in Hardwood Pulp on the Reaction Rate of Tempo-Mediated Oxidation and the Rheology of the Final Nanofibrillated Cellulose Gel. Cellulose 2016, 23, 277–293..

    Not in our library10.1007/s10570-015-0824-7

  628. 628.

    Talantikite M.; Beury N. g.; Moreau C. l.; Cathala B. Arabinoxylan/Cellulose Nanocrystal Hydrogels with Tunable Mechanical Properties. Langmuir 2019, 35, 13427–13434..

    Not in our library10.1021/acs.langmuir.9b02080

  629. 629.

    Dimic-Misic K.; Gane P.; Budtova T.; Pradille C.; Sixta H.; Ville L.; Maloney T. Influence of Xylan on Nanocellulose (Nfc) Suspension Rheology and Aerogel Morphology. In 6th International Symposium on Industrial Engineering, 24-25 September 2015, Belgrade, 2015.

    Not in our library

  630. 630.

    Talantikite M.; Stimpson T. C.; Gourlay A.; Le-Gall S.; Moreau C.; Cranston E. D.; Moran-Mirabal J. M.; Cathala B. Bioinspired Thermoresponsive Xyloglucan–Cellulose Nanocrystal Hydrogels. Biomacromolecules 2021, 22, 743.

    Not in our library10.1021/acs.biomac.0c01521

  631. 631.

    Talantikite M.; Gourlay A.; Le Gall S. L.; Cathala B. Influence of Xyloglucan Molar Mass on Rheological Properties of Cellulose Nanocrystal/Xyloglucan Hydrogels. J. Renewable Mater. 2019, 7, 1381–1390..

    Not in our library10.32604/jrm.2019.07838

  632. 632.

    Xu W.; Zhang X.; Yang P.; Långvik O.; Wang X.; Zhang Y.; Cheng F.; Österberg M.; Willför S.; Xu C. Surface Engineered Biomimetic Inks Based on Uv Cross-Linkable Wood Biopolymers for 3d Printing. ACS Appl. Mater. Interfaces 2019, 11, 12389–12400..

    Not in our library10.1021/acsami.9b03442

  633. 633.

    Cernencu A. I.; Lungu A.; Stancu I.-C.; Serafim A.; Heggset E.; Syverud K.; Iovu H. Bioinspired 3d Printable Pectin-Nanocellulose Ink Formulations. Carbohydr. Polym. 2019, 220, 12–21..

    Not in our library10.1016/j.carbpol.2019.05.026

  634. 634.

    Khorasani A. C.; Shojaosadati S. A. Starch-and Carboxymethylcellulose-Coated Bacterial Nanocellulose-Pectin Bionanocomposite as Novel Protective Prebiotic Matrices. Food Hydrocolloids 2017, 63, 273–285..

    Not in our library10.1016/j.foodhyd.2016.09.002

  635. 635.

    Paulraj T.; Riazanova A.; Svagan A. Bioinspired Capsules Based on Nanocellulose, Xyloglucan and Pectin–the Influence of Capsule Wall Composition on Permeability Properties. Acta Biomater. 2018, 69, 196–205..

    Not in our library10.1016/j.actbio.2018.01.003

  636. 636.

    Meneguin A. B.; Stringhetti Ferreira Cury B.; Dos Santos A. M.; Franco D. F.; Barud H. S.; da Silva Filho E. C. Resistant Starch/Pectin Free-Standing Films Reinforced with Nanocellulose Intended for Colonic Methotrexate Release. Carbohydr. Polym. 2017, 157, 1013–1023..

    Not in our library10.1016/j.carbpol.2016.10.062

  637. 637.

    Wang L.; Ago M.; Borghei M.; Ishaq A.; Papageorgiou A. C.; Lundahl M.; Rojas O. J. Conductive Carbon Microfibers Derived from Wet-Spun Lignin/Nanocellulose Hydrogels. ACS Sustainable Chem. Eng. 2019, 7, 6013–6022..

    Not in our library10.1021/acssuschemeng.8b06081

  638. 638.

    Zhao H.-k.; Wei X.-y.; Xie Y.-m.; Feng Q.-h. Preparation of Nanocellulose and Lignin-Carbohydrate Complex Composite Biological Carriers and Culture of Heart Coronary Artery Endothelial Cells. Int. J. Biol. Macromol. 2019, 137, 1161–1168..

    Not in our library10.1016/j.ijbiomac.2019.07.062

  639. 639.

    Lê H. Q.; Dimic-Misic K.; Johansson L.-S.; Maloney T.; Sixta H. Effect of Lignin on the Morphology and Rheological Properties of Nanofibrillated Cellulose Produced from Γ-Valerolactone/Water Fractionation Process. Cellulose 2018, 25, 179–194..

    Not in our library10.1007/s10570-017-1602-5

  640. 640.

    Zmejkoski D.; Spasojević D.; Orlovska I.; Kozyrovska N.; Soković M.; Glamočlija J.; Dmitrović S.; Matović B.; Tasić N.; Maksimović V.; et al. Bacterial Cellulose-Lignin Composite Hydrogel as a Promising Agent in Chronic Wound Healing. Int. J. Biol. Macromol. 2018, 118, 494–503..

    Not in our library10.1016/j.ijbiomac.2018.06.067

  641. 641.

    Sampath U. T. M.; Ching Y. C.; Chuah C. H.; Singh R.; Lin P.-C. Preparation and Characterization of Nanocellulose Reinforced Semi-Interpenetrating Polymer Network of Chitosan Hydrogel. Cellulose 2017, 24, 2215–2228..

    Not in our library10.1007/s10570-017-1251-8

  642. 642.

    Udeni Gunathilake T. M. S.; Ching Y. C.; Chuah C. H. Enhancement of Curcumin Bioavailability Using Nanocellulose Reinforced Chitosan Hydrogel. Polymers 2017, 9, 64.

    Not in our library10.3390/polym9020064

  643. 643.

    Udeni Gunathilake T. M. S.; Ching Y. C.; Chuah C. H.; Illias H. A.; Ching K. Y.; Singh R.; Nai-Shang L. Influence of a Nonionic Surfactant on Curcumin Delivery of Nanocellulose Reinforced Chitosan Hydrogel. Int. J. Biol. Macromol. 2018, 118, 1055–1064..

    Not in our library10.1016/j.ijbiomac.2018.06.147

  644. 644.

    H P S A. K.; Saurabh C. K.; A S A.; Fazita M. N.; Syakir M.; Davoudpour Y.; Rafatullah M.; Abdullah C.; Haafiz M. K. M.; Dungani R. A Review on Chitosan-Cellulose Blends and Nanocellulose Reinforced Chitosan Biocomposites: Properties and Their Applications. Carbohydr. Polym. 2016, 150, 216–226..

    Not in our library10.1016/j.carbpol.2016.05.028

  645. 645.

    Hänninen A.; Sarlin E.; Lyyra I.; Salpavaara T.; Kellomäki M.; Tuukkanen S. Nanocellulose and Chitosan Based Films as Low Cost, Green Piezoelectric Materials. Carbohydr. Polym. 2018, 202, 418–424..

    Not in our library10.1016/j.carbpol.2018.09.001

  646. 646.

    Khan A.; Wang B.; Ni Y. Chitosan-Nanocellulose Composites for Regenerative Medicine Applications. Curr. Med. Chem. 2020, 27, 4584–4592..

    Not in our library10.2174/0929867327666200127152834

  647. 647.

    Sharma V.; Shahnaz T.; Subbiah S.; Narayanasamy S. New Insights into the Remediation of Water Pollutants Using Nanobentonite Incorporated Nanocellulose Chitosan Based Aerogel. J. Polym. Environ. 2020, 28, 2008–2019..

    Not in our library10.1007/s10924-020-01740-9

  648. 648.

    Yin K.; Divakar P.; Wegst U. G. Plant-Derived Nanocellulose as Structural and Mechanical Reinforcement of Freeze-Cast Chitosan Scaffolds for Biomedical Applications. Biomacromolecules 2019, 20, 3733–3745..

    Not in our library10.1021/acs.biomac.9b00784

  649. 649.

    Zhang P.; Chen L.; Zhang Q.; Hong F. F. Using in Situ Dynamic Cultures to Rapidly Biofabricate Fabric-Reinforced Composites of Chitosan/Bacterial Nanocellulose for Antibacterial Wound Dressings. Front. Microbiol. 2016, 7, 260.

    Not in our library10.3389/fmicb.2016.00260

  650. 650.

    Maturavongsadit P.; Narayanan L. K.; Chansoria P.; Shirwaiker R.; Benhabbour S. R. Cell-Laden Nanocellulose/Chitosan-Based Bioinks for 3d Bioprinting and Enhanced Osteogenic Cell Differentiation. ACS Appl. Bio Mater. 2021, 4, 2342.

    Not in our library10.1021/acsabm.0c01108

  651. 651.

    Xu X.; Ouyang X.-k.; Yang L.-Y. Adsorption of Pb (Ii) from Aqueous Solutions Using Crosslinked Carboxylated Chitosan/Carboxylated Nanocellulose Hydrogel Beads. J. Mol. Liq. 2021, 322, 114523.

    Not in our library10.1016/j.molliq.2020.114523

  652. 652.

    Xu Q.; Ji Y.; Sun Q.; Fu Y.; Xu Y.; Jin L. Fabrication of Cellulose Nanocrystal/Chitosan Hydrogel for Controlled Drug Release. Nanomaterials 2019, 9, 253.

    Not in our library10.3390/nano9020253

  653. 653.

    Shahnaz T.; Sharma V.; Subbiah S.; Narayanasamy S. Multivariate Optimisation of Cr (Vi), Co (Iii) and Cu (Ii) Adsorption onto Nanobentonite Incorporated Nanocellulose/Chitosan Aerogel Using Response Surface Methodology. J. Water Process Eng. 2020, 36, 101283.

    Not in our library10.1016/j.jwpe.2020.101283

  654. 654.

    Park M.; Lee D.; Hyun J. Nanocellulose-Alginate Hydrogel for Cell Encapsulation. Carbohydr. Polym. 2015, 116, 223–228..

    Not in our library10.1016/j.carbpol.2014.07.059

  655. 655.

    Leppiniemi J.; Lahtinen P.; Paajanen A.; Mahlberg R.; Metsä-Kortelainen S.; Pinomaa T.; Pajari H.; Vikholm-Lundin I.; Pursula P.; Hytönen V. P. 3D-Printable Bioactivated Nanocellulose–Alginate Hydrogels. ACS Appl. Mater. Interfaces 2017, 9, 21959–21970..

    Not in our library10.1021/acsami.7b02756

  656. 656.

    Wang B.; Ran M.; Fang G.; Wu T.; Tian Q.; Zheng L.; Romero-Zerón L.; Ni Y. Palladium Nano-Catalyst Supported on Cationic Nanocellulose–Alginate Hydrogel for Effective Catalytic Reactions. Cellulose 2020, 27, 6995–7008..

    Not in our library10.1007/s10570-020-03127-4

  657. 657.
  658. 658.
  659. 659.

    Müller M.; Öztürk E.; Arlov Ø.; Gatenholm P.; Zenobi-Wong M. Alginate Sulfate–Nanocellulose Bioinks for Cartilage Bioprinting Applications. Ann. Biomed. Eng. 2017, 45, 210–223..

    Not in our library10.1007/s10439-016-1704-5

  660. 660.

    Jessop Z. M.; Al-Sabah A.; Gao N.; Kyle S.; Thomas B.; Badiei N.; Hawkins K.; Whitaker I. S. Printability of Pulp Derived Crystal, Fibril and Blend Nanocellulose-Alginate Bioinks for Extrusion 3D Bioprinting. Biofabrication 2019, 11, 045006.

    Not in our library10.1088/1758-5090/ab0631

  661. 661.

    Ojansivu M.; Rashad A.; Ahlinder A.; Massera J.; Mishra A.; Syverud K.; Finne-Wistrand A.; Miettinen S.; Mustafa K. Wood-Based Nanocellulose and Bioactive Glass Modified Gelatin–Alginate Bioinks for 3D Bioprinting of Bone Cells. Biofabrication 2019, 11, 035010.

    Not in our library10.1088/1758-5090/ab0692

  662. 662.

    Wei J.; Wang B.; Li Z.; Wu Z.; Zhang M.; Sheng N.; Liang Q.; Wang H.; Chen S. A 3D-Printable Tempo-Oxidized Bacterial Cellulose/Alginate Hydrogel with Enhanced Stability Via Nanoclay Incorporation. Carbohydr. Polym. 2020, 238, 116207.

    Not in our library10.1016/j.carbpol.2020.116207

  663. 663.

    Heggset E. B.; Strand B. L.; Sundby K. W.; Simon S.; Chinga-Carrasco G.; Syverud K. Viscoelastic Properties of Nanocellulose Based Inks for 3D Printing and Mechanical Properties of Cnf/Alginate Biocomposite Gels. Cellulose 2019, 26, 581–595..

    Not in our library10.1007/s10570-018-2142-3

  664. 664.

    Wang Y.; Liang Z.; Su Z.; Zhang K.; Ren J.; Sun R.; Wang X. All-Biomass Fluorescent Hydrogels Based on Biomass Carbon Dots and Alginate/Nanocellulose for Biosensing. ACS Appl. Bio Mater. 2018, 1, 1398–1407..

    Not in our library10.1021/acsabm.8b00348

  665. 665.

    Poonguzhali R.; Basha S. K.; Kumari V. S. Synthesis of Alginate/Nanocellulose Bionanocomposite for in Vitro Delivery of Ampicillin. Polym. Bull. 2018, 75, 4165–4173..

    Not in our library10.1007/s00289-017-2253-2

  666. 666.

    Espinosa E.; Filgueira D.; Rodríguez A.; Chinga-Carrasco G. Nanocellulose-Based Inks—Effect of Alginate Content on the Water Absorption of 3D Printed Constructs. Bioengineering 2019, 6, 65.

    Not in our library10.3390/bioengineering6030065

  667. 667.

    Li J.; Wang Y.; Zhang L.; Xu Z.; Dai H.; Wu W. Nanocellulose/Gelatin Composite Cryogels for Controlled Drug Release. ACS Sustainable Chem. Eng. 2019, 7, 6381–6389..

    Not in our library10.1021/acssuschemeng.9b00161

  668. 668.

    Erdagi S. I.; Ngwabebhoh F. A.; Yildiz U. Genipin Crosslinked Gelatin-Diosgenin-Nanocellulose Hydrogels for Potential Wound Dressing and Healing Applications. Int. J. Biol. Macromol. 2020, 149, 651–663..

    Not in our library10.1016/j.ijbiomac.2020.01.279

  669. 669.

    Xu W.; Molino B. Z.; Cheng F.; Molino P. J.; Yue Z.; Su D.; Wang X.; Willför S.; Xu C.; Wallace G. G. On Low-Concentration Inks Formulated by Nanocellulose Assisted with Gelatin Methacrylate (Gelma) for 3D Printing toward Wound Healing Application. ACS Appl. Mater. Interfaces 2019, 11, 8838–8848..

    Not in our library10.1021/acsami.8b21268

  670. 670.

    Xu X.; Zhou J.; Jiang Y.; Zhang Q.; Shi H.; Liu D. 3D Printing Process of Oxidized Nanocellulose and Gelatin Scaffold. J. Biomater. Sci., Polym. Ed. 2018, 29, 1498–1513..

    Not in our library10.1080/09205063.2018.1472450

  671. 671.

    Taokaew S.; Seetabhawang S.; Siripong P.; Phisalaphong M. Biosynthesis and Characterization of Nanocellulose-Gelatin Films. Materials 2013, 6, 782–794..

    Not in our library10.3390/ma6030782

  672. 672.

    Kwak H. W.; Lee H.; Park S.; Lee M. E.; Jin H.-J. Chemical and Physical Reinforcement of Hydrophilic Gelatin Film with Di-Aldehyde Nanocellulose. Int. J. Biol. Macromol. 2020, 146, 332–342..

    Not in our library10.1016/j.ijbiomac.2019.12.254

  673. 673.

    Carlström I. E.; Rashad A.; Campodoni E.; Sandri M.; Syverud K.; Bolstad A. I.; Mustafa K. Cross-Linked Gelatin-Nanocellulose Scaffolds for Bone Tissue Engineering. Mater. Lett. 2020, 264, 127326.

    Not in our library10.1016/j.matlet.2020.127326

  674. 674.

    Luo H.; Cha R.; Li J.; Hao W.; Zhang Y.; Zhou F. Advances in Tissue Engineering of Nanocellulose-Based Scaffolds: A Review. Carbohydr. Polym. 2019, 224, 115144.

    Not in our library10.1016/j.carbpol.2019.115144

  675. 675.

    Athukoralalage S. S.; Balu R.; Dutta N. K.; Roy Choudhury N. 3D Bioprinted Nanocellulose-Based Hydrogels for Tissue Engineering Applications: A Brief Review. Polymers 2019, 11, 898.

    Not in our library10.3390/polym11050898

  676. 676.

    Müller A.; Ni Z.; Hessler N.; Wesarg F.; Müller F. A.; Kralisch D.; Fischer D. The Biopolymer Bacterial Nanocellulose as Drug Delivery System: Investigation of Drug Loading and Release Using the Model Protein Albumin. J. Pharm. Sci. 2013, 102, 579–592..

    Not in our library10.1002/jps.23385

  677. 677.

    Moritz S.; Wiegand C.; Wesarg F.; Hessler N.; Müller F. A.; Kralisch D.; Hipler U.-C.; Fischer D. Active Wound Dressings Based on Bacterial Nanocellulose as Drug Delivery System for Octenidine. Int. J. Pharm. 2014, 471, 45–55..

    Not in our library10.1016/j.ijpharm.2014.04.062

  678. 678.

    Bhandari J.; Mishra H.; Mishra P. K.; Wimmer R.; Ahmad F. J.; Talegaonkar S. Cellulose Nanofiber Aerogel as a Promising Biomaterial for Customized Oral Drug Delivery. Int. J. Nanomed. 2017, 12, 2021.

    Not in our library10.2147/ijn.s124318

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    Lunardi V. B.; Soetaredjo F. E.; Putro J. N.; Santoso S. P.; Yuliana M.; Sunarso J.; Ju Y.-H.; Ismadji S. Nanocelluloses: Sources, Pretreatment, Isolations, Modification, and Its Application as the Drug Carriers. Polymers 2021, 13, 2052.

    Not in our library10.3390/polym13132052

  680. 680.

    Liu S.; Qamar S. A.; Qamar M.; Basharat K.; Bilal M. Engineered Nanocellulose-Based Hydrogels for Smart Drug Delivery Applications. Int. J. Biol. Macromol. 2021, 181, 275–290..

    Not in our library10.1016/j.ijbiomac.2021.03.147

  681. 681.

    Plackett D.; Letchford K.; Jackson J.; Burt H. A Review of Nanocellulose as a Novel Vehicle for Drug Delivery. Nordic Pulp Pap. Res. J. 2014, 29, 105–118..

    Not in our library10.3183/npprj-2014-29-01-p105-118

  682. 682.

    Kummala R.; Xu W.; Xu C.; Toivakka M. Stiffness and Swelling Characteristics of Nanocellulose Films in Cell Culture Media. Cellulose 2018, 25, 4969–4978..

    Not in our library10.1007/s10570-018-1940-y

  683. 683.

    Jämsä M.; Kosourov S.; Rissanen V.; Hakalahti M.; Pere J.; Ketoja J. A.; Tammelin T.; Allahverdiyeva Y. Versatile Templates from Cellulose Nanofibrils for Photosynthetic Microbial Biofuel Production. J. Mater. Chem. A 2018, 6, 5825–5835..

    Not in our library10.1039/c7ta11164a

  684. 684.

    Rissanen V.; Vajravel S.; Kosourov S.; Arola S.; Kontturi E.; Allahverdiyeva Y.; Tammelin T. Nanocellulose-Based Mechanically Stable Immobilization Matrix for Enhanced Ethylene Production: A Framework for Photosynthetic Solid-State Cell Factories. Green Chem. 2021, 23, 3715–3724..

    Not in our library10.1039/d1gc00502b

  685. 685.

    Montero de Espinosa L.; Meesorn W.; Moatsou D.; Weder C. Bioinspired Polymer Systems with Stimuli-Responsive Mechanical Properties. Chem. Rev. 2017, 117, 12851–12892..

    Not in our library10.1021/acs.chemrev.7b00168

  686. 686.

    Nandi S.; Aggarwal H.; Wahiduzzaman M.; Belmabkhout Y.; Maurin G.; Eddaoudi M.; Devautour-Vinot S. Revisiting the Water Sorption Isotherm of Mof Using Electrical Measurements. Chem. Commun. 2019, 55, 13251–13254..

    Not in our library10.1039/c9cc06012j

  687. 687.

    Capadona J. R.; Shanmuganathan K.; Tyler D. J.; Rowan S. J.; Weder C. Stimuli-Responsive Polymer Nanocomposites Inspired by the Sea Cucumber Dermis. Science 2008, 319, 1370–1374..

    Not in our library10.1126/science.1153307

  688. 688.

    Annamalai P. K.; Dagnon K. L.; Monemian S.; Foster E. J.; Rowan S. J.; Weder C. Water Responsive Mechanically Adaptive Nanocomposites Based on Styrene–Butadiene Rubber and Cellulose Nanocrystals Processing Matters. ACS Appl. Mater. Interfaces 2014, 6, 967–976..

    Not in our library10.1021/am404382x

  689. 689.

    Zhu Y.; Hu J.; Luo H.; Young R. J.; Deng L.; Zhang S.; Fan Y.; Ye G. Rapidly Switchable Water-Sensitive Shape-Memory Cellulose/Elastomer Nano-Composites. Soft Matter 2012, 8, 2509–2517..

    Not in our library10.1039/c2sm07035a

  690. 690.

    Hu S.; Zhi Y.; Shan S.; Ni Y. Research Progress of Smart Response Composite Hydrogels Based on Nanocellulose. Carbohydr. Polym. 2022, 275, 118741.

    Not in our library10.1016/j.carbpol.2021.118741

  691. 691.

    Tummala G. K.; Rojas R.; Mihranyan A. Poly (Vinyl Alcohol) Hydrogels Reinforced with Nanocellulose for Ophthalmic Applications: General Characteristics and Optical Properties. J. Phys. Chem. B 2016, 120, 13094–13101..

    Not in our library10.1021/acs.jpcb.6b10650

  692. 692.

    Tummala G. K.; Joffre T.; Lopes V. R.; Liszka A.; Buznyk O.; Ferraz N.; Persson C.; Griffith M.; Mihranyan A. Hyperelastic Nanocellulose-Reinforced Hydrogel of High Water Content for Ophthalmic Applications. ACS Biomater. Sci. Eng. 2016, 2, 2072–2079..

    Not in our library10.1021/acsbiomaterials.6b00484

  693. 693.

    McKee J. R.; Appel E. A.; Seitsonen J.; Kontturi E.; Scherman O. A.; Ikkala O. Healable, Stable and Stiff Hydrogels: Combining Conflicting Properties Using Dynamic and Selective Three-Component Recognition with Reinforcing Cellulose Nanorods. Adv. Funct. Mater. 2014, 24, 2706–2713..

    Not in our library10.1002/adfm.201303699

  694. 694.

    Shao C.; Wang M.; Chang H.; Xu F.; Yang J. A Self-Healing Cellulose Nanocrystal-Poly (Ethylene Glycol) Nanocomposite Hydrogel Via Diels–Alder Click Reaction. ACS Sustainable Chem. Eng. 2017, 5, 6167–6174..

    Not in our library10.1021/acssuschemeng.7b01060

  695. 695.

    Wang Y.; Shaghaleh H.; Hamoud Y. A.; Zhang S.; Li P.; Xu X.; Liu H. Synthesis of a Ph-Responsive Nano-Cellulose/Sodium Alginate/Mofs Hydrogel and Its Application in the Regulation of Water and N-Fertilizer. Int. J. Biol. Macromol. 2021, 187, 262–271..

    Not in our library10.1016/j.ijbiomac.2021.07.154

  696. 696.

    Hai J.; Li T.; Su J.; Liu W.; Ju Y.; Wang B.; Hou Y. Reversible Response of Luminescent Terbium (Iii)–Nanocellulose Hydrogels to Anions for Latent Fingerprint Detection and Encryption. Angew. Chem., Int. Ed. 2018, 57, 6786–6790..

    Not in our library10.1002/anie.201800119

  697. 697.

    Joseph B.; James J.; Grohens Y.; Kalarikkal N.; Thomas S. Material Aspects During Additive Manufacturing of Nano-Cellulose Composites. In Structure and Properties of Additive Manufactured Polymer Components; Friedrich K., Walter R., Soutis C., Advani S. G., Fiedler B., Eds.; Elsevier: Amsterdam, 2020; pp 409–428.

    Not in our library

  698. 698.

    Sultan S.; Siqueira G.; Zimmermann T.; Mathew A. P. 3D Printing of Nano-Cellulosic Biomaterials for Medical Applications. Curr. Opin. Biomed. Eng. 2017, 2, 29–34..

    Not in our library10.1016/j.cobme.2017.06.002

  699. 699.

    Siqueira G.; Kokkinis D.; Libanori R.; Hausmann M. K.; Gladman A. S.; Neels A.; Tingaut P.; Zimmermann T.; Lewis J. A.; Studart A. R. Cellulose Nanocrystal Inks for 3D Printing of Textured Cellular Architectures. Adv. Funct. Mater. 2017, 27, 1604619.

    Not in our library10.1002/adfm.201604619

  700. 700.
  701. 701.

    Gladman A. S.; Matsumoto E. A.; Nuzzo R. G.; Mahadevan L.; Lewis J. A. Biomimetic 4D Printing. Nat. Mater. 2016, 15, 413–418..

    Not in our library10.1038/nmat4544

  702. 702.
  703. 703.

    Sultan S.; Mathew A. P. 3D Printed Scaffolds with Gradient Porosity Based on a Cellulose Nanocrystal Hydrogel. Nanoscale 2018, 10, 4421–4431..

    Not in our library10.1039/c7nr08966j

  704. 704.

    Hausmann M. K.; Ruhs P. A.; Siqueira G.; Läuger J. r.; Libanori R.; Zimmermann T.; Studart A. R. Dynamics of Cellulose Nanocrystal Alignment During 3D Printing. ACS Nano 2018, 12, 6926–6937..

    Not in our library10.1021/acsnano.8b02366

  705. 705.

    Fourmann O.; Hausmann M. K.; Neels A.; Schubert M.; Nyström G.; Zimmermann T.; Siqueira G. 3D Printing of Shape-Morphing and Antibacterial Anisotropic Nanocellulose Hydrogels. Carbohydr. Polym. 2021, 259, 117716.

    Not in our library10.1016/j.carbpol.2021.117716

  706. 706.

    Chau M.; De France K. J.; Kopera B.; Machado V. R.; Rosenfeldt S.; Reyes L.; Chan K. J.; Förster S.; Cranston E. D.; Hoare T.; Kumacheva E. Composite Hydrogels with Tunable Anisotropic Morphologies and Mechanical Properties. Chem. Mater. 2016, 28, 3406–3415..

    Not in our library10.1021/acs.chemmater.6b00792

  707. 707.

    Kuang Y.; Chen C.; Cheng J.; Pastel G.; Li T.; Song J.; Jiang F.; Li Y.; Zhang Y.; Jang S.-H.; et al. Selectively Aligned Cellulose Nanofibers Towards High-Performance Soft Actuators. Extreme Mech. Lett. 2019, 29, 100463.

    Not in our library10.1016/j.eml.2019.100463

  708. 708.

    Köhnke T.; Elder T.; Theliander H.; Ragauskas A. J. Ice Templated and Cross-Linked Xylan/Nanocrystalline Cellulose Hydrogels. Carbohydr. Polym. 2014, 100, 24–30..

    Not in our library10.1016/j.carbpol.2013.03.060

  709. 709.

    Dash R.; Li Y.; Ragauskas A. J. Cellulose Nanowhisker Foams by Freeze Casting. Carbohydr. Polym. 2012, 88, 789–792..

    Not in our library10.1016/j.carbpol.2011.12.035

  710. 710.

    Bettotti P.; Maestri C. A.; Guider R.; Mancini I.; Nativ-Roth E.; Golan Y.; Scarpa M. Dynamics of Hydration of Nanocellulose Films. Adv. Mater. Interfaces 2016, 3, 1500415.

    Not in our library10.1002/admi.201500415

  711. 711.

    Kim J.; Kim J. W.; Kim H. C.; Zhai L.; Ko H.-U.; Muthoka R. M. Review of Soft Actuator Materials. Int. J. Precis. Eng. Manuf. 2019, 20, 2221.

    Not in our library10.1007/s12541-019-00255-1

  712. 712.

    Zhu Q.; Liu S.; Sun J.; Liu J.; Kirubaharan C. J.; Chen H.; Xu W.; Wang Q. Stimuli-Responsive Cellulose Nanomaterials for Smart Applications. Carbohydr. Polym. 2020, 235, 115933.

    Not in our library10.1016/j.carbpol.2020.115933

  713. 713.

    Ansari J. R.; Hegazy S. M.; Houkan M. T.; Kannan K.; Aly A.; Sadasivuni K. K. Nanocellulose-Based Materials/Composites for Sensors. In Nanocellulose Based Composites for Electronics; Thomas S., Pottathara Y. B., Eds.; Elsevier: Amsterdam, 2021; pp 185–214.

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    Zhu Q.; Jin Y.; Wang W.; Sun G.; Wang D. Bioinspired Smart Moisture Actuators Based on Nanoscale Cellulose Materials and Porous, Hydrophilic EVOH Nanofibrous Membranes. ACS Appl. Mater. Interfaces 2019, 11, 1440–1448..

    Not in our library10.1021/acsami.8b17538

  715. 715.

    Wang M.; Tian X.; Ras R. H.; Ikkala O. Sensitive Humidity-Driven Reversible and Bidirectional Bending of Nanocellulose Thin Films as Bio-Inspired Actuation. Adv. Mater. Interfaces 2015, 2, 1500080.

    Not in our library10.1002/admi.201500080

  716. 716.

    Golmohammadi H.; Morales-Narvaez E.; Naghdi T.; Merkoci A. Nanocellulose in Sensing and Biosensing. Chem. Mater. 2017, 29, 5426–5446..

    Not in our library10.1021/acs.chemmater.7b01170

  717. 717.

    Nguyen L. H.; Naficy S.; Chandrawati R.; Dehghani F. Nanocellulose for Sensing Applications. Adv. Mater. Interfaces 2019, 6, 1900424.

    Not in our library10.1002/admi.201900424

  718. 718.

    Dai L.; Wang Y.; Zou X.; Chen Z.; Liu H.; Ni Y. Ultrasensitive Physical, Bio, and Chemical Sensors Derived from 1-, 2-, and 3-D Nanocellulosic Materials. Small 2020, 16, 1906567.

    Not in our library10.1002/smll.201906567

  719. 719.

    Kafy A.; Akther A.; Shishir M. I.; Kim H. C.; Yun Y.; Kim J. Cellulose Nanocrystal/Graphene Oxide Composite Film as Humidity Sensor. Sens. Actuators, A 2016, 247, 221–226..

    Not in our library10.1016/j.sna.2016.05.045

  720. 720.

    Solin K.; Borghei M.; Sel O.; Orelma H.; Johansson L.-S.; Perrot H.; Rojas O. J. Electrically Conductive Thin Films Based on Nanofibrillated Cellulose: Interactions with Water and Applications in Humidity Sensing. ACS Appl. Mater. Interfaces 2020, 12, 36437–36448..

    Not in our library10.1021/acsami.0c09997

  721. 721.

    Zhang Y.; Tian Z.; Fu Y.; Wang Z.; Qin M.; Yuan Z. Responsive and Patterned Cellulose Nanocrystal Films Modified by N-Methylmorpholine-N-Oxide. Carbohydr. Polym. 2020, 228, 115387.

    Not in our library10.1016/j.carbpol.2019.115387

  722. 722.

    Sadasivuni K. K.; Kafy A.; Zhai L.; Ko H. U.; Mun S.; Kim J. Transparent and Flexible Cellulose Nanocrystal/Reduced Graphene Oxide Film for Proximity Sensing. Small 2015, 11, 994–1002..

    Not in our library10.1002/smll.201402109

  723. 723.

    Buyanov A.; Gofman I.; Revel’skaya L.; Khripunov A.; Tkachenko A. Anisotropic Swelling and Mechanical Behavior of Composite Bacterial Cellulose–Poly (Acrylamide or Acrylamide–Sodium Acrylate) Hydrogels. J. Mech. Behav. Biomed. Mater. 2010, 3, 102–111..

    Not in our library10.1016/j.jmbbm.2009.06.001

  724. 724.

    Millon L.; Wan W. The Polyvinyl Alcohol–Bacterial Cellulose System as a New Nanocomposite for Biomedical Applications. J. Biomed. Mater. Res. Part B: Appl. Biomater. 2006, 79B, 245–253..

    Not in our library10.1002/jbm.b.30535

  725. 725.

    Pääkkö M.; Vapaavuori J.; Silvennoinen R.; Kosonen H.; Ankerfors M.; Lindström T.; Berglund L. A.; Ikkala O. Long and Entangled Native Cellulose I Nanofibers Allow Flexible Aerogels and Hierarchically Porous Templates for Functionalities. Soft Matter 2008, 4, 2492–2499..

    Not in our library10.1039/b810371b

  726. 726.

    Xu H.; Liu Y.; Xie Y.; Zhu E.; Shi Z.; Yang Q.; Xiong C. Doubly Cross-Linked Nanocellulose Hydrogels with Excellent Mechanical Properties. Cellulose 2019, 26, 8645–8654..

    Not in our library10.1007/s10570-019-02689-2

  727. 727.

    McKee J. R.; Hietala S.; Seitsonen J.; Laine J.; Kontturi E.; Ikkala O. Thermoresponsive Nanocellulose Hydrogels with Tunable Mechanical Properties. ACS Macro Lett. 2014, 3, 266–270..

    Not in our library10.1021/mz400596g

  728. 728.

    Frensemeier M.; Koplin C.; Jaeger R.; Kramer F.; Klemm D. Mechanical Properties of Bacterially Synthesized Nanocellulose Hydrogels. Macromol. Symp. 2010, 294, 38–44..

    Not in our library10.1002/masy.200900030

  729. 729.

    Yue Y.; Wang X.; Han J.; Yu L.; Chen J.; Wu Q.; Jiang J. Effects of Nanocellulose on Sodium Alginate/Polyacrylamide Hydrogel: Mechanical Properties and Adsorption-Desorption Capacities. Carbohydr. Polym. 2019, 206, 289–301..

    Not in our library10.1016/j.carbpol.2018.10.105

  730. 730.

    Xu H.; Xie Y.; Zhu E.; Liu Y.; Shi Z.; Xiong C.; Yang Q. Supertough and Ultrasensitive Flexible Electronic Skin Based on Nanocellulose/Sulfonated Carbon Nanotube Hydrogel Films. J. Mater. Chem. A 2020, 8, 6311–6318..

    Not in our library10.1039/d0ta00158a

  731. 731.

    Huang S.; Zhao Z.; Feng C.; Mayes E.; Yang J. Nanocellulose Reinforced P(Aam-Co-Aac) Hydrogels with Improved Mechanical Properties and Biocompatibility. Composites, Part A 2018, 112, 395–404..

    Not in our library10.1016/j.compositesa.2018.06.028

  732. 732.

    Dorishetty P.; Balu R.; Athukoralalage S. S.; Greaves T. L.; Mata J.; De Campo L.; Saha N.; Zannettino A. C.; Dutta N. K.; Choudhury N. R. Tunable Biomimetic Hydrogels from Silk Fibroin and Nanocellulose. ACS Sustainable Chem. Eng. 2020, 8, 2375–2389..

    Not in our library10.1021/acssuschemeng.9b05317

  733. 733.

    Chen Y.; Xu W.; Liu W.; Zeng G. Responsiveness, Swelling, and Mechanical Properties of Pnipa Nanocomposite Hydrogels Reinforced by Nanocellulose. J. Mater. Res. 2015, 30, 1797.

    Not in our library10.1557/jmr.2015.94

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    Tummala G. K.; Joffre T.; Rojas R.; Persson C.; Mihranyan A. Strain-Induced Stiffening of Nanocellulose-Reinforced Poly (Vinyl Alcohol) Hydrogels Mimicking Collagenous Soft Tissues. Soft Matter 2017, 13, 3936–3945..

    Not in our library10.1039/c7sm00677b

  735. 735.

    Tummala G. K.; Bachi I.; Mihranyan A. Role of Solvent on Structure, Viscoelasticity, and Mechanical Compressibility in Nanocellulose-Reinforced Poly (Vinyl Alcohol) Hydrogels. J. Appl. Polym. Sci. 2019, 136, 47044.

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    Nakamura K.; Hatakeyama T.; Hatakeyama H. Effect of Bound Water on Tensile Properties of Native Cellulose. Text. Res. J. 1983, 53, 682–688..

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    Hatakeyama T.; Ikeda Y.; Hatakeyama H. Structural Change of the Amorphous Region of Cellulose in the Presence of Water. In Wood and Cellulosics: Industrial Utilisation, Biotechnology, Structure and Properties; Kennedy J. F., Phillips G. O., Williams P. A., Eds.; Ellis Horwood: Chichester, UK, 1987; pp 23–30.

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    Sampath U. G.; Ching Y. C.; Chuah C. H.; Sabariah J. J.; Lin P.-C. Fabrication of Porous Materials from Natural/Synthetic Biopolymers and Their Composites. Materials 2016, 9, 991.

    Not in our library10.3390/ma9120991

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    Hatakeyama H.; Hatakeyama T. Interaction between Water and Hydrophilic Polymers. Thermochim. Acta 1998, 308, 3–22..

    Not in our library10.1016/s0040-6031(97)00325-0

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    Kuljich S.; Cáceres C. B.; Hernández R. E. Steam-Bending Properties of Seven Poplar Hybrid Clones. Int. J. Mater. Form. 2015, 8, 67–72..

    Not in our library10.1007/s12289-013-1148-5

  742. 742.

    Kutnar A.; Kamke F. A. Compression of Wood under Saturated Steam, Superheated Steam, and Transient Conditions at 150 C, 160 C, and 170 C. Wood Sci. Technol. 2012, 46, 73–88..

    Not in our library10.1007/s00226-010-0380-0

  743. 743.

    Salmén L. Viscoelastic Properties Ofin Situ Lignin under Water-Saturated Conditions. J. Mater. Sci. 1984, 19, 3090–3096..

    Not in our library10.1007/bf01026988

  744. 744.

    Thickens J. H. Grinding of Steamed and Boiled Spruce. Excerpts from Forest Service Bulletin 127 (1913) and U.S. Dept. Agri. Bull. 343 (1916); United States Department of Agriculture, Forest Service, Forest Products Laboratory: Madison, WI, 1916; Vol. 127, pp 1–8.

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  745. 745.

    Aulin C.; Gällstedt M.; Lindström T. Oxygen and Oil Barrier Properties of Microfibrillated Cellulose Films and Coatings. Cellulose 2010, 17, 559–574..

    Not in our library10.1007/s10570-009-9393-y

  746. 746.

    Kettunen M.; Silvennoinen R. J.; Houbenov N.; Nykänen A.; Ruokolainen J.; Sainio J.; Pore V.; Kemell M.; Ankerfors M.; Lindström T.; et al. Photoswitchable Superabsorbency Based on Nanocellulose Aerogels. Adv. Funct. Mater. 2011, 21, 510–517..

    Not in our library10.1002/adfm.201001431

  747. 747.

    Barajas-Ledesma R. M.; Wong V. N.; Little K.; Patti A. F.; Garnier G. Carboxylated Nanocellulose Superabsorbent: Biodegradation and Soil Water Retention Properties. J. Appl. Polym. Sci. 2022, 139, 51495.

    Not in our library10.1002/app.51495

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    Sulaeva I.; Henniges U.; Rosenau T.; Potthast A. Bacterial Cellulose as a Material for Wound Treatment: Properties and Modifications. A Review. Biotechnol. Adv. 2015, 33, 1547–1571..

    Not in our library10.1016/j.biotechadv.2015.07.009

  749. 749.

    Benítez A. J.; Walther A. Cellulose Nanofibril Nanopapers and Bioinspired Nanocomposites: A Review to Understand the Mechanical Property Space. J. Mater. Chem. A 2017, 5, 16003–16024..

    Not in our library10.1039/c7ta02006f

  750. 750.

    Barhoum A.; Samyn P.; Öhlund T.; Dufresne A. Review of Recent Research on Flexible Multifunctional Nanopapers. Nanoscale 2017, 9, 15181–15205..

    Not in our library10.1039/c7nr04656a

  751. 751.

    Kontturi K. S.; Lee K.-Y.; Jones M. P.; Sampson W. W.; Bismarck A.; Kontturi E. Influence of Biological Origin on the Tensile Properties of Cellulose Nanopapers. Cellulose 2021, 28, 6619–6628..

    Not in our library10.1007/s10570-021-03935-2

  752. 752.

    Galland S.; Berthold F.; Prakobna K.; Berglund L. A. Holocellulose Nanofibers of High Molar Mass and Small Diameter for High-Strength Nanopaper. Biomacromolecules 2015, 16, 2427–2435..

    Not in our library10.1021/acs.biomac.5b00678

  753. 753.

    Fukuzumi H.; Saito T.; Iwata T.; Kumamoto Y.; Isogai A. Transparent and High Gas Barrier Films of Cellulose Nanofibers Prepared by TEMPO-Mediated Oxidation. Biomacromolecules 2009, 10, 162–165..

    Not in our library10.1021/bm801065u

  754. 754.

    Kress O.; Silverstein P. Some Observations on the Influence of Humidity on the Physical Constants of Paper. Ind. Eng. Chem. 1917, 9, 277–282..

    Not in our library10.1021/ie50087a017

  755. 755.

    Sehaqui H.; Zimmermann T.; Tingaut P. Hydrophobic Cellulose Nanopaper through a Mild Esterification Procedure. Cellulose 2014, 21, 367–382..

    Not in our library10.1007/s10570-013-0110-5

  756. 756.

    Benítez A. J.; Torres-Rendon J.; Poutanen M.; Walther A. Humidity and Multiscale Structure Govern Mechanical Properties and Deformation Modes in Films of Native Cellulose Nanofibrils. Biomacromolecules 2013, 14, 4497–4506..

    Not in our library10.1021/bm401451m

  757. 757.

    Hanif Z.; Choi D.; Tariq M. Z.; La M.; Park S. J. Water-Stable Flexible Nanocellulose Chiral Nematic Films through Acid Vapor Cross-Linked Glutaraldehyde for Chiral Nematic Templating. ACS Macro Lett. 2020, 9, 146–151..

    Not in our library10.1021/acsmacrolett.9b00826

  758. 758.

    Walther A.; Lossada F.; Benselfelt T.; Kriechbaum K.; Berglund L.; Ikkala O.; Saito T.; Wagberg L.; Bergström L. Best Practice for Reporting Wet Mechanical Properties of Nanocellulose-Based Materials. Biomacromolecules 2020, 21, 2536–2540..

    Not in our library10.1021/acs.biomac.0c00330

  759. 759.

    Hakalahti M.; Salminen A.; Seppälä J.; Tammelin T.; Hänninen T. Effect of Interfibrillar Pva Bridging on Water Stability and Mechanical Properties of TEMPO/NaClO2 Oxidized Cellulosic Nanofibril Films. Carbohydr. Polym. 2015, 126, 78–82..

    Not in our library10.1016/j.carbpol.2015.03.007

  760. 760.

    Österberg M.; Vartiainen J.; Lucenius J.; Hippi U.; Seppälä J.; Serimaa R.; Laine J. A Fast Method to Produce Strong Nfc Films as a Platform for Barrier and Functional Materials. ACS Appl. Mater. Interfaces 2013, 5, 4640–4647..

    Not in our library10.1021/am401046x

  761. 761.

    Farooq M.; Zou T.; Riviere G.; Sipponen M. H.; Österberg M. Strong, Ductile, and Waterproof Cellulose Nanofibril Composite Films with Colloidal Lignin Particles. Biomacromolecules 2019, 20, 693–704..

    Not in our library10.1021/acs.biomac.8b01364

  762. 762.

    Shimizu M.; Saito T.; Isogai A. Water-Resistant and High Oxygen-Barrier Nanocellulose Films with Interfibrillar Cross-Linkages Formed through Multivalent Metal Ions. J. Membr. Sci. 2016, 500, 1–7..

    Not in our library10.1016/j.memsci.2015.11.002

  763. 763.

    Wang B.; Torres-Rendon J. G.; Yu J.; Zhang Y.; Walther A. Aligned Bioinspired Cellulose Nanocrystal-Based Nanocomposites with Synergetic Mechanical Properties and Improved Hygromechanical Performance. ACS Appl. Mater. Interfaces 2015, 7, 4595–4607..

    Not in our library10.1021/am507726t

  764. 764.

    Zhang K.; Ismail M. Y.; Liimatainen H. Water-Resistant Nanopaper with Tunable Water Barrier and Mechanical Properties from Assembled Complexes of Oppositely Charged Cellulosic Nanomaterials. Food Hydrocolloids 2021, 120, 106983.

    Not in our library10.1016/j.foodhyd.2021.106983

  765. 765.

    Heredia-Guerrero J. A.; Williams C. A.; Guidetti G.; Cataldi P.; Ceseracciu L.; Debellis D.; Athanassiou A.; Guzman-Puyol S.; Hamad W. Y.; Vignolini S. Plant-Inspired Polyaleuritate–Nanocellulose Composite Photonic Films. ACS Appl. Polym. Mater. 2020, 2, 1528–1534..

    Not in our library10.1021/acsapm.9b01205

  766. 766.

    Tedeschi G.; Guzman-Puyol S.; Ceseracciu L.; Benitez J. J.; Cataldi P.; Bissett M.; Heredia A.; Athanassiou A.; Heredia-Guerrero J. A. Sustainable, High-Barrier Polyaleuritate/Nanocellulose Biocomposites. ACS Sustainable Chem. Eng. 2020, 8, 10682–10690..

    Not in our library10.1021/acssuschemeng.0c00909

  767. 767.

    Lavoine N.; Desloges I.; Dufresne A.; Bras J. Microfibrillated Cellulose - Its Barrier Properties and Applications in Cellulosic Materials: A Review. Carbohydr. Polym. 2012, 90, 735–764..

    Not in our library10.1016/j.carbpol.2012.05.026

  768. 768.

    Rodionova G.; Lenes M.; Eriksen Ø.; Gregersen Ø. Surface Chemical Modification of Microfibrillated Cellulose: Improvement of Barrier Properties for Packaging Applications. Cellulose 2011, 18, 127–134..

    Not in our library10.1007/s10570-010-9474-y

  769. 769.

    Nair S. S.; Zhu J.; Deng Y.; Ragauskas A. J. High Performance Green Barriers Based on Nanocellulose. Sustain. Chem. Process. 2014, 2, 23.

    Not in our library10.1186/s40508-014-0023-0

  770. 770.

    Tyagi P.; Lucia L. A.; Hubbe M. A.; Pal L. Nanocellulose-Based Multilayer Barrier Coatings for Gas, Oil, and Grease Resistance. Carbohydr. Polym. 2019, 206, 281–288..

    Not in our library10.1016/j.carbpol.2018.10.114

  771. 771.

    Herrera M. A.; Mathew A. P.; Oksman K. Barrier and Mechanical Properties of Plasticized and Cross-Linked Nanocellulose Coatings for Paper Packaging Applications. Cellulose 2017, 24, 3969–3980..

    Not in our library10.1007/s10570-017-1405-8

  772. 772.

    Agarwal U. P.; Ralph S. A.; Baez C.; Reiner R. S.; Verrill S. P. Effect of Sample Moisture Content on Xrd-Estimated Cellulose Crystallinity Index and Crystallite Size. Cellulose 2017, 24, 1971–1984..

    Not in our library10.1007/s10570-017-1259-0

  773. 773.

    Pircher N.; Carbajal L.; Schimper C.; Bacher M.; Rennhofer H.; Nedelec J.-M.; Lichtenegger H. C.; Rosenau T.; Liebner F. Impact of Selected Solvent Systems on the Pore and Solid Structure of Cellulose Aerogels. Cellulose 2016, 23, 1949–1966..

    Not in our library10.1007/s10570-016-0896-z

  774. 774.

    Ferrer A.; Pal L.; Hubbe M. Nanocellulose in Packaging: Advances in Barrier Layer Technologies. Ind. Crops Prod. 2017, 95, 574–582..

    Not in our library10.1016/j.indcrop.2016.11.012

  775. 775.

    Hazrol M. D.; Ilyas R. A.; Sapuan M. S.; Ishak M. R.; Zainudin E. S.; Mahamud A.; Mohd Roslim M. H. Water Barrier Properties of Biodegradable Films Reinforced with Nanocellulose for Food Packaging Application: A Review. In 6th Postgraduate Seminar on Natural Fiber Reinforced Polymer Composites (NFRP 2018), Malaysia, 2018.

    Not in our library

  776. 776.

    Herrera M. A.; Sirviö J. A.; Mathew A. P.; Oksman K. Environmental Friendly and Sustainable Gas Barrier on Porous Materials: Nanocellulose Coatings Prepared Using Spin-and Dip-Coating. Mater. Des. 2016, 93, 19–25..

    Not in our library10.1016/j.matdes.2015.12.127

  777. 777.

    Wu Y.; Liang Y.; Mei C.; Cai L.; Nadda A.; Le Q. V.; Peng Y.; Lam S. S.; Sonne C.; Xia C. Advanced Nanocellulose-Based Gas Barrier Materials: Present Status and Prospects. Chemosphere 2022, 286, 131891.

    Not in our library10.1016/j.chemosphere.2021.131891

  778. 778.

    Bideau B.; Loranger E.; Daneault C. Nanocellulose-Polypyrrole-Coated Paperboard for Food Packaging Application. Prog. Org. Coat. 2018, 123, 128–133..

    Not in our library10.1016/j.porgcoat.2018.07.003

  779. 779.

    Liu A.; Walther A.; Ikkala O.; Belova L.; Berglund L. A. Clay Nanopaper with Tough Cellulose Nanofiber Matrix for Fire Retardancy and Gas Barrier Functions. Biomacromolecules 2011, 12, 633–641..

    Not in our library10.1021/bm101296z

  780. 780.

    Aulin C.; Salazar-Alvarez G.; Lindström T. High Strength, Flexible and Transparent Nanofibrillated Cellulose–Nanoclay Biohybrid Films with Tunable Oxygen and Water Vapor Permeability. Nanoscale 2012, 4, 6622–6628..

    Not in our library10.1039/c2nr31726e

  781. 781.

    Svagan A.; Bender Koch C.; Hedenqvist M.; Nilsson F.; Glasser G.; Baluschev S.; Andersen M. Liquid-Core Nanocellulose-Shell Capsules with Tunable Oxygen Permeability. Carbohydr. Polym. 2016, 136, 292–299..

    Not in our library10.1016/j.carbpol.2015.09.040

  782. 782.

    Lengowski E. C.; Bonfatti E. A. Jr.; Simon L.; de Muniz G. I. B.; de Andrade A. S.; Nisgoski S.; Klock U. Different Degree of Fibrillation: Strategy to Reduce Permeability in Nanocellulose-Starch Films. Cellulose 2020, 27, 10855–10872..

    Not in our library10.1007/s10570-020-03232-4

  783. 783.

    Wu C.-N.; Saito T.; Fujisawa S.; Fukuzumi H.; Isogai A. Ultrastrong and High Gas-Barrier Nanocellulose/Clay-Layered Composites. Biomacromolecules 2012, 13, 1927–1932..

    Not in our library10.1021/bm300465d

  784. 784.

    Rojo E.; Peresin M. S.; Sampson W. W.; Hoeger I. C.; Vartiainen J.; Laine J.; Rojas O. J. Comprehensive Elucidation of the Effect of Residual Lignin on the Physical, Barrier, Mechanical and Surface Properties of Nanocellulose Films. Green Chem. 2015, 17, 1853–1866..

    Not in our library10.1039/c4gc02398f

  785. 785.

    Liimatainen H.; Ezekiel N.; Sliz R.; Ohenoja K.; Sirviö J. A.; Berglund L.; Hormi O.; Niinimäki J. High-Strength Nanocellulose–Talc Hybrid Barrier Films. ACS Appl. Mater. Interfaces 2013, 5, 13412–13418..

    Not in our library10.1021/am4043273

  786. 786.

    Koppolu R.; Lahti J.; Abitbol T.; Swerin A.; Kuusipalo J.; Toivakka M. Continuous Processing of Nanocellulose and Polylactic Acid into Multilayer Barrier Coatings. ACS Appl. Mater. Interfaces 2019, 11, 11920–11927..

    Not in our library10.1021/acsami.9b00922

  787. 787.

    Mandal A.; Chakrabarty D. Studies on the Mechanical, Thermal, Morphological and Barrier Properties of Nanocomposites Based on Poly (Vinyl Alcohol) and Nanocellulose from Sugarcane Bagasse. J. Ind. Eng. Chem. 2014, 20, 462–473..

    Not in our library10.1016/j.jiec.2013.05.003

  788. 788.

    Garusinghe U. M.; Varanasi S.; Raghuwanshi V. S.; Garnier G.; Batchelor W. Nanocellulose-Montmorillonite Composites of Low Water Vapour Permeability. Colloids Surf., A 2018, 540, 233–241..

    Not in our library10.1016/j.colsurfa.2018.01.010

  789. 789.

    Espinosa E.; Bascón-Villegas I.; Rosal A.; Pérez-Rodríguez F.; Chinga-Carrasco G.; Rodríguez A. Pva/(Ligno) Nanocellulose Biocomposite Films. Effect of Residual Lignin Content on Structural, Mechanical, Barrier and Antioxidant Properties. Int. J. Biol. Macromol. 2019, 141, 197–206..

    Not in our library10.1016/j.ijbiomac.2019.08.262

  790. 790.

    Chi K.; Catchmark J. M. Improved Eco-Friendly Barrier Materials Based on Crystalline Nanocellulose/Chitosan/Carboxymethyl Cellulose Polyelectrolyte Complexes. Food Hydrocolloids 2018, 80, 195–205..

    Not in our library10.1016/j.foodhyd.2018.02.003

  791. 791.

    Maliha M.; Herdman M.; Brammananth R.; McDonald M.; Coppel R.; Werrett M.; Andrews P.; Batchelor W. Bismuth Phosphinate Incorporated Nanocellulose Sheets with Antimicrobial and Barrier Properties for Packaging Applications. J. Cleaner Prod. 2020, 246, 119016.

    Not in our library10.1016/j.jclepro.2019.119016

  792. 792.

    Bideau B.; Bras J.; Adoui N.; Loranger E.; Daneault C. Polypyrrole/Nanocellulose Composite for Food Preservation: Barrier and Antioxidant Characterization. Food Packag. Shelf Life 2017, 12, 1–8..

    Not in our library10.1016/j.fpsl.2017.01.007

  793. 793.

    Trifol J.; Plackett D.; Sillard C.; Szabo P.; Bras J.; Daugaard A. E. Hybrid Poly (Lactic Acid)/Nanocellulose/Nanoclay Composites with Synergistically Enhanced Barrier Properties and Improved Thermomechanical Resistance. Polym. Int. 2016, 65, 988–995..

    Not in our library10.1002/pi.5154

  794. 794.

    Lazić V.; Vivod V.; Peršin Z.; Stoiljković M.; Ratnayake I. S.; Ahrenkiel P. S.; Nedeljković J. M.; Kokol V. Dextran-Coated Silver Nanoparticles for Improved Barrier and Controlled Antimicrobial Properties of Nanocellulose Films Used in Food Packaging. Food Packag. Shelf Life 2020, 26, 100575.

    Not in our library10.1016/j.fpsl.2020.100575

  795. 795.

    Matsumoto M.; Kitaoka T. Ultraselective Gas Separation by Nanoporous Metal– Organic Frameworks Embedded in Gas-Barrier Nanocellulose Films. Adv. Mater. 2016, 28, 1765–1769..

    Not in our library10.1002/adma.201504784

  796. 796.

    Fukuzumi H.; Fujisawa S.; Saito T.; Isogai A. Selective Permeation of Hydrogen Gas Using Cellulose Nanofibril Film. Biomacromolecules 2013, 14, 1705–1709..

    Not in our library10.1021/bm400377e

  797. 797.

    Janakiram S.; Ansaloni L.; Jin S.-A.; Yu X.; Dai Z.; Spontak R. J.; Deng L. Humidity-Responsive Molecular Gate-Opening Mechanism for Gas Separation in Ultraselective Nanocellulose/Il Hybrid Membranes. Green Chem. 2020, 22, 3546–3557..

    Not in our library10.1039/d0gc00544d

  798. 798.

    Sharma S.; Zhang X.; Nair S. S.; Ragauskas A.; Zhu J.; Deng Y. Thermally Enhanced High Performance Cellulose Nano Fibril Barrier Membranes. RSC Adv. 2014, 4, 45136–45142..

    Not in our library10.1039/c4ra07469f

  799. 799.

    Li M.; Zong L.; Yang W.; Li X.; You J.; Wu X.; Li Z.; Li C. Biological Nanofibrous Generator for Electricity Harvest from Moist Air Flow. Adv. Funct. Mater. 2019, 29, 1901798.

    Not in our library10.1002/adfm.201901798

  800. 800.

    Rodionova G.; Lenes M.; Eriksen Ø.; Gregersen Ø. Surface Chemical Modification of Microfibrillated Cellulose: Improvement of Barrier Properties for Packaging Applications. Cellulose 2011, 18, 127–134..

    Not in our library10.1007/s10570-010-9474-y

  801. 801.

    Lu P.; Xiao H.; Zhang W.; Gong G. Reactive Coating of Soybean Oil-Based Polymer on Nanofibrillated Cellulose Film for Water Vapor Barrier Packaging. Carbohydr. Polym. 2014, 111, 524–529..

    Not in our library10.1016/j.carbpol.2014.04.071

  802. 802.

    Andersson C. New Ways to Enhance the Functionality of Paperboard by Surface Treatment–a Review. Packag. Technol. Sci. 2008, 21, 339–373..

    Not in our library10.1002/pts.823

  803. 803.

    Martínez-Sanz M.; Lopez-Rubio A.; Lagaron J. M. High-Barrier Coated Bacterial Cellulose Nanowhiskers Films with Reduced Moisture Sensitivity. Carbohydr. Polym. 2013, 98, 1072–1082..

    Not in our library10.1016/j.carbpol.2013.07.020

  804. 804.

    Spence K. L.; Venditti R. A.; Rojas O. J.; Pawlak J. J.; Hubbe M. A. Water Vapor Barrier Properties of Coated and Filled Microfibrillated Cellulose Composite Films. BioResources 2011, 6, 4370–4388..

    Not in our library10.15376/biores.6.4.4370-4388

  805. 805.

    Tayeb A. H.; Tajvidi M.; Bousfield D. Enhancing the Oxygen Barrier Properties of Nanocellulose at High Humidity: Numerical and Experimental Assessment. Sustain. Chem. 2020, 1, 198–208..

    Not in our library10.3390/suschem1030014

  806. 806.

    Chinga-Carrasco G.; Averianova N.; Gibadullin M.; Petrov V.; Leirset I.; Syverud K. Micro-Structural Characterisation of Homogeneous and Layered Mfc Nano-Composites. Micron 2013, 44, 331–338..

    Not in our library10.1016/j.micron.2012.08.005

  807. 807.

    Lagaron J.; Catalá R.; Gavara R. Structural Characteristics Defining High Barrier Properties in Polymeric Materials. Mater. Sci. Technol. 2004, 20, 1–7..

    Not in our library10.1179/026708304225010442

  808. 808.

    Vartiainen J.; Shen Y.; Kaljunen T.; Malm T.; Vähä-Nissi M.; Putkonen M.; Harlin A. Bio-Based Multilayer Barrier Films by Extrusion, Dispersion Coating and Atomic Layer Deposition. J. Appl. Polym. Sci. 2016, 133, 42260.

    Not in our library10.1002/app.42260

  809. 809.

    Vähä-Nissi M.; Koivula H. M.; Räisänen H. M.; Vartiainen J.; Ragni P.; Kenttä E.; Kaljunen T.; Malm T.; Minkkinen H.; Harlin A. Cellulose Nanofibrils in Biobased Multilayer Films for Food Packaging. J. Appl. Polym. Sci. 2017, 134, 44830.

    Not in our library10.1002/app.44830

  810. 810.

    Schade M.; Weinkötz S.; Assmann J. Lignocellulosic Materials Containing Defibrillated Cellulose. US US20160257814A1, 2016.

    Not in our library

  811. 811.

    Du L.; Yu H.; Zhang B.; Tang R.; Zhang Y.; Qi C.; Wolcott M. P.; Yu Z.; Wang J. Transparent Oxygen Barrier Nanocellulose Composite Films with a Sandwich Structure. Carbohydr. Polym. 2021, 268, 118206.

    Not in our library10.1016/j.carbpol.2021.118206

  812. 812.

    Fotie G.; Limbo S.; Piergiovanni L. Manufacturing of Food Packaging Based on Nanocellulose: Current Advances and Challenges. Nanomaterials 2020, 10, 1726.

    Not in our library10.3390/nano10091726

  813. 813.

    Yook S.; Park H.; Park H.; Lee S.-Y.; Kwon J.; Youn H. J. Barrier Coatings with Various Types of Cellulose Nanofibrils and Their Barrier Properties. Cellulose 2020, 27, 4509–4523..

    Not in our library10.1007/s10570-020-03061-5

  814. 814.

    Cranston E. D.; Eita M.; Johansson E.; Netrval J.; Salajkova M.; Arwin H.; Wagberg L. Determination of Young’s Modulus for Nanofibrillated Cellulose Multilayer Thin Films Using Buckling Mechanics. Biomacromolecules 2011, 12, 961–969..

    Not in our library10.1021/bm101330w

  815. 815.
  816. 816.

    Carpenter A. W.; de Lannoy C.-F.; Wiesner M. R. Cellulose Nanomaterials in Water Treatment Technologies. Environ. Sci. Technol. 2015, 49, 5277–5287..

    Not in our library10.1021/es506351r

  817. 817.

    Putro J. N.; Kurniawan A.; Ismadji S.; Ju Y.-H. Nanocellulose Based Biosorbents for Wastewater Treatment: Study of Isotherm, Kinetic, Thermodynamic and Reusability. Environ. Nanotechnol. Monit. Manage. 2017, 8, 134–149..

    Not in our library10.1016/j.enmm.2017.07.002

  818. 818.

    Zhu J.; Xie S.; Yang Z.; Li X.; Chen J.; Zhang X.; Zheng N. A Review of Recent Advances and Prospects on Nanocellulose Properties and Its Applications in Oil and Gas Production. J. Nat. Gas Sci. Eng. 2021, 96, 104253.

    Not in our library10.1016/j.jngse.2021.104253

  819. 819.

    Pei A.; Butchosa N.; Berglund L. A.; Zhou Q. Surface Quaternized Cellulose Nanofibrils with High Water Absorbency and Adsorption Capacity for Anionic Dyes. Soft Matter 2013, 9, 2047–2055..

    Not in our library10.1039/c2sm27344f

  820. 820.

    Zhou Y.; Fu S.; Zhang L.; Zhan H.; Levit M. V. Use of Carboxylated Cellulose Nanofibrils-Filled Magnetic Chitosan Hydrogel Beads as Adsorbents for Pb (Ii). Carbohydr. Polym. 2014, 101, 75–82..

    Not in our library10.1016/j.carbpol.2013.08.055

  821. 821.

    Zha R.; Shi T.; He L.; Zhang M. Chemistry and Nanotechnology-Oriented Strategies toward Nanocellulose for Human Water Treatment. Adv. Sustainable Syst. 2022, 6, 2100302.

    Not in our library10.1002/adsu.202100302

  822. 822.

    Xiong Y.; Wang C.; Wang H.; Jin C.; Sun Q.; Xu X. Nano-Cellulose Hydrogel Coated Flexible Titanate-Bismuth Oxide Membrane for Trinity Synergistic Treatment of Super-Intricate Anion/Cation/Oily-Water. Chem. Eng. J. 2018, 337, 143–151..

    Not in our library10.1016/j.cej.2017.12.080

  823. 823.

    Korhonen J. T.; Kettunen M.; Ras R. H.; Ikkala O. Hydrophobic Nanocellulose Aerogels as Floating, Sustainable, Reusable, and Recyclable Oil Absorbents. ACS Appl. Mater. Interfaces 2011, 3, 1813–1816..

    Not in our library10.1021/am200475b

  824. 824.

    Jiang F.; Hsieh Y.-L. Amphiphilic Superabsorbent Cellulose Nanofibril Aerogels. J. Mater. Chem. A 2014, 2, 6337–6342..

    Not in our library10.1039/c4ta00743c

  825. 825.

    Qiao A.; Huang R.; Penkova A.; Qi W.; He Z.; Su R. Superhydrophobic, Elastic and Anisotropic Cellulose Nanofiber Aerogels for Highly Effective Oil/Water Separation. Sep. Purif. Technol. 2022, 295, 121266.

    Not in our library10.1016/j.seppur.2022.121266

  826. 826.

    Wang Y.; Yadav S.; Heinlein T.; Konjik V.; Breitzke H.; Buntkowsky G.; Schneider J. J.; Zhang K. Ultra-Light Nanocomposite Aerogels of Bacterial Cellulose and Reduced Graphene Oxide for Specific Absorption and Separation of Organic Liquids. RSC Adv. 2014, 4, 21553–21558..

    Not in our library10.1039/c4ra02168a

  827. 827.

    Gholami Derami H.; Jiang Q.; Ghim D.; Cao S.; Chandar Y. J.; Morrissey J. J.; Jun Y.-S.; Singamaneni S. A Robust and Scalable Polydopamine/Bacterial Nanocellulose Hybrid Membrane for Efficient Wastewater Treatment. ACS Appl. Nano Mater. 2019, 2, 1092–1101..

    Not in our library10.1021/acsanm.9b00022

  828. 828.

    Cunha A. G.; Lundahl M.; Ansari M. F.; Johansson L.-S.; Campbell J. M.; Rojas O. J. Surface Structuring and Water Interactions of Nanocellulose Filaments Modified with Organosilanes toward Wearable Materials. ACS Appl. Nano Mater. 2018, 1, 5279–5288..

    Not in our library10.1021/acsanm.8b01268

  829. 829.

    Wang X.; Yao C.; Wang F.; Li Z. Cellulose-Based Nanomaterials for Energy Applications. Small 2017, 13, 1702240.

    Not in our library10.1002/smll.201702240

  830. 830.

    Agate S.; Joyce M.; Lucia L.; Pal L. Cellulose and Nanocellulose-Based Flexible-Hybrid Printed Electronics and Conductive Composites–a Review. Carbohydr. Polym. 2018, 198, 249–260..

    Not in our library10.1016/j.carbpol.2018.06.045

  831. 831.
  832. 832.

    Ding Q.; Xu X.; Yue Y.; Mei C.; Huang C.; Jiang S.; Wu Q.; Han J. Nanocellulose-Mediated Electroconductive Self-Healing Hydrogels with High Strength, Plasticity, Viscoelasticity, Stretchability, and Biocompatibility toward Multifunctional Applications. ACS Appl. Mater. Interfaces 2018, 10, 27987–28002..

    Not in our library10.1021/acsami.8b09656

  833. 833.

    Ram F.; Velayutham P.; Sahu A. K.; Lele A. K.; Shanmuganathan K. Enhancing Thermomechanical and Chemical Stability of Polymer Electrolyte Membranes Using Polydopamine Coated Nanocellulose. ACS Appl. Energy Mater. 2020, 3, 1988–1999..

    Not in our library10.1021/acsaem.9b02417

  834. 834.

    Lasrado D.; Ahankari S.; Kar K. Nanocellulose-Based Polymer Composites for Energy Applications—a Review. J. Appl. Polym. Sci. 2020, 137, 48959.

    Not in our library10.1002/app.48959

  835. 835.

    Xu T.; Du H.; Liu H.; Liu W.; Zhang X.; Si C.; Liu P.; Zhang K. Advanced Nanocellulose-Based Composites for Flexible Functional Energy Storage Devices. Adv. Mater. 2021, 33, 2101368.

    Not in our library10.1002/adma.202101368

  836. 836.

    Dias O. A. T.; Konar S.; Leão A. L.; Yang W.; Tjong J.; Sain M. Current State of Applications of Nanocellulose in Flexible Energy and Electronic Devices. Front. Chem. 2020, 8, 420.

    Not in our library10.3389/fchem.2020.00420

  837. 837.

    Lv P.; Lu X.; Wang L.; Feng W. Nanocellulose-Based Functional Materials: From Chiral Photonics to Soft Actuator and Energy Storage. Adv. Funct. Mater. 2021, 31, 2104991.

    Not in our library10.1002/adfm.202104991

  838. 838.

    Lokhande P.; Singh P. P.; Vo D.-V. N.; Kumar D.; Balasubramanian K.; Mubayi A.; Srivastava A.; Sharma A. Bacterial Nanocellulose: Green Polymer Materials for High Performance Energy Storage Applications. J. Environ. Chem. Eng. 2022, 10, 108176.

    Not in our library10.1016/j.jece.2022.108176

  839. 839.

    Gladen A.; Bajwa D. A Novel Composite Material of Hygroscopic Salt Stabilized by Nanocellulose for Thermochemical Energy Storage. In Proceedings of the ASME 2021 15th International Conference on Energy Sustainability collocated with the ASME 2021 Heat Transfer Summer Conference, June 16–18, 2021, Virtual, Online; ASME, 2021.

    Not in our library

  840. 840.

    Gladen A. C.; Bajwa D. An Improved Thermochemical Energy Storage Material Using Nanocellulose to Stabilize Calcium Chloride Salt. J. Sol. Energy Eng. 2022, 144, 030905.

    Not in our library10.1115/1.4053904

  841. 841.

    Salviati S.; Carosio F.; Cantamessa F.; Medina L.; Berglund L. A.; Saracco G.; Fina A. Ice-Templated Nanocellulose Porous Structure Enhances Thermochemical Storage Kinetics in Hydrated Salt/Graphite Composites. Renewable Energy 2020, 160, 698–706..

    Not in our library10.1016/j.renene.2020.07.036

  842. 842.

    Chen C.; Hu L. Nanocellulose toward Advanced Energy Storage Devices: Structure and Electrochemistry. Acc. Chem. Res. 2018, 51, 3154–3165..

    Not in our library10.1021/acs.accounts.8b00391

  843. 843.

    Lizundia E.; Kundu D. Advances in Natural Biopolymer-Based Electrolytes and Separators for Battery Applications. Adv. Funct. Mater. 2021, 31, 2005646.

    Not in our library10.1002/adfm.202005646

  844. 844.

    Mittal N.; Tien S.; Lizundia E.; Niederberger M. Hierarchical Nanocellulose-Based Gel Polymer Electrolytes for Stable Na Electrodeposition in Sodium Ion Batteries. Small 2022, 18, 2107183.

    Not in our library10.1002/smll.202107183

  845. 845.

    Lu H.; Behm M.; Leijonmarck S.; Lindbergh G.; Cornell A. Flexible Paper Electrodes for Li-Ion Batteries Using Low Amount of Tempo-Oxidized Cellulose Nanofibrils as Binder. ACS Appl. Mater. Interfaces 2016, 8, 18097–18106..

    Not in our library10.1021/acsami.6b05016

  846. 846.

    Kim H.; Guccini V.; Lu H.; Salazar-Alvarez G.; Lindbergh G.; Cornell A. Lithium Ion Battery Separators Based on Carboxylated Cellulose Nanofibers from Wood. ACS Appl. Energy Mater. 2019, 2, 1241–1250..

    Not in our library10.1021/acsaem.8b01797

  847. 847.

    Kim H.; Mattinen U.; Guccini V.; Liu H.; Salazar-Alvarez G.; Lindström R. W.; Lindbergh G.; Cornell A. Feasibility of Chemically Modified Cellulose Nanofiber Membranes as Lithium-Ion Battery Separators. ACS Appl. Mater. Interfaces 2020, 12, 41211–41222..

    Not in our library10.1021/acsami.0c08820

  848. 848.

    Leijonmarck S.; Cornell A.; Lindbergh G.; Wågberg L. Single-Paper Flexible Li-Ion Battery Cells through a Paper-Making Process Based on Nano-Fibrillated Cellulose. J. Mater. Chem. A 2013, 1, 4671–4677..

    Not in our library10.1039/c3ta01532g

  849. 849.

    Jabbour L.; Destro M.; Chaussy D.; Gerbaldi C.; Penazzi N.; Bodoardo S.; Beneventi D. Flexible Cellulose/Lifepo 4 Paper-Cathodes: Toward Eco-Friendly All-Paper Li-Ion Batteries. Cellulose 2013, 20, 571–582..

    Not in our library10.1007/s10570-012-9834-x

  850. 850.

    Jabbour L.; Bongiovanni R.; Chaussy D.; Gerbaldi C.; Beneventi D. Cellulose-Based Li-Ion Batteries: A Review. Cellulose 2013, 20, 1523–1545..

    Not in our library10.1007/s10570-013-9973-8

  851. 851.

    Jeong S.; Böckenfeld N.; Balducci A.; Winter M.; Passerini S. Natural Cellulose as Binder for Lithium Battery Electrodes. J. Power Sources 2012, 199, 331–335..

    Not in our library10.1016/j.jpowsour.2011.09.102

  852. 852.

    Bayer T.; Cunning B. V.; Selyanchyn R.; Nishihara M.; Fujikawa S.; Sasaki K.; Lyth S. M. High Temperature Proton Conduction in Nanocellulose Membranes: Paper Fuel Cells. Chem. Mater. 2016, 28, 4805–4814..

    Not in our library10.1021/acs.chemmater.6b01990

  853. 853.

    Jiang G.-p.; Zhang J.; Qiao J.-l.; Jiang Y.-m.; Zarrin H.; Chen Z.; Hong F. Bacterial Nanocellulose/Nafion Composite Membranes for Low Temperature Polymer Electrolyte Fuel Cells. J. Power Sources 2015, 273, 697–706..

    Not in our library10.1016/j.jpowsour.2014.09.145

  854. 854.

    Gadim T. D.; Vilela C.; Loureiro F. J.; Silvestre A. J.; Freire C. S.; Figueiredo F. M. Nafion® and Nanocellulose: A Partnership for Greener Polymer Electrolyte Membranes. Ind. Crops Prod. 2016, 93, 212–218..

    Not in our library10.1016/j.indcrop.2016.01.028

  855. 855.

    Guccini V.; Carlson A.; Yu S.; Lindbergh G.; Lindström R. W.; Salazar-Alvarez G. Highly Proton Conductive Membranes Based on Carboxylated Cellulose Nanofibres and Their Performance in Proton Exchange Membrane Fuel Cells. J. Mater. Chem. A 2019, 7, 25032–25039..

    Not in our library10.1039/c9ta04898g

  856. 856.

    Jankowska I.; Pankiewicz R.; Pogorzelec-Glaser K.; Ławniczak P.; Łapiński A.; Tritt-Goc J. Comparison of Structural, Thermal and Proton Conductivity Properties of Micro-and Nanocelluloses. Carbohydr. Polym. 2018, 200, 536–542..

    Not in our library10.1016/j.carbpol.2018.08.033

  857. 857.

    Zhang Z.; Li X.; Yin J.; Xu Y.; Fei W.; Xue M.; Wang Q.; Zhou J.; Guo W. Emerging Hydrovoltaic Technology. Nat. Nanotechnol. 2018, 13, 1109–1119..

    Not in our library10.1038/s41565-018-0228-6

  858. 858.

    Bai J.; Huang Y.; Cheng H.; Qu L. Moist-Electric Generation. Nanoscale 2019, 11, 23083–23091..

    Not in our library10.1039/c9nr06113d

  859. 859.

    Xu Y.; Chen P.; Peng H. Generating Electricity from Water through Carbon Nanomaterials. Chem.–Eur. J. 2018, 24, 6287–6294..

    Not in our library10.1002/chem.201704638

  860. 860.

    Cao S.; Rathi P.; Wu X.; Ghim D.; Jun Y. S.; Singamaneni S. Cellulose Nanomaterials in Interfacial Evaporators for Desalination: A “Natural” Choice. Adv. Mater. 2021, 33, 2000922.

    Not in our library10.1002/adma.202000922

  861. 861.

    Zhu H.; Luo W.; Ciesielski P. N.; Fang Z.; Zhu J.; Henriksson G.; Himmel M. E.; Hu L. Wood-Derived Materials for Green Electronics, Biological Devices, and Energy Applications. Chem. Rev. 2016, 116, 9305–9374..

    Not in our library10.1021/acs.chemrev.6b00225

  862. 862.

    Li Z.; Yao C.; Yu Y.; Cai Z.; Wang X. Highly Efficient Capillary Photoelectrochemical Water Splitting Using Cellulose Nanofiber-Templated TiO2 Photoanodes. Adv. Mater. 2014, 26, 2262–2267..

    Not in our library10.1002/adma.201303369

  863. 863.

    Fujishima A.; Honda K. Electrochemical Photolysis of Water at a Semiconductor Electrode. Nature 1972, 238, 37–38..

    Not in our library10.1038/238037a0

  864. 864.

    Wang F.; Seo J.-H.; Li Z.; Kvit A. V.; Ma Z.; Wang X. Cl-Doped Zno Nanowires with Metallic Conductivity and Their Application for High-Performance Photoelectrochemical Electrodes. ACS Appl. Mater. Interfaces 2014, 6, 1288–1293..

    Not in our library10.1021/am405141s

  865. 865.

    Li Z.; Yao C.; Wang F.; Cai Z.; Wang X. Cellulose Nanofiber-Templated Three-Dimension TiO2 Hierarchical Nanowire Network for Photoelectrochemical Photoanode. Nanotechnology 2014, 25, 504005.

    Not in our library10.1088/0957-4484/25/50/504005

  866. 866.

    Ke D.; Liu S.; Dai K.; Zhou J.; Zhang L.; Peng T. Cds/Regenerated Cellulose Nanocomposite Films for Highly Efficient Photocatalytic H2 Production under Visible Light Irradiation. J. Phys. Chem. C 2009, 113, 16021–16026..

    Not in our library10.1021/jp903378q

  867. 867.

    Lee M.; Kim J. H.; Lee S. H.; Lee S. H.; Park C. B. Biomimetic Artificial Photosynthesis by Light-Harvesting Synthetic Wood. ChemSusChem 2011, 4, 581–586..

    Not in our library10.1002/cssc.201100074

  868. 868.

    Zhang Y.; Ge L.; Ge S.; Yan M.; Yan J.; Zang D.; Lu J.; Yu J.; Song X. TiO2–Graphene Complex Nanopaper for Paper-Based Label-Free Photoelectrochemical Immunoassay. Electrochim. Acta 2013, 112, 620–628..

    Not in our library10.1016/j.electacta.2013.09.009

  869. 869.

    Rooke J. C.; Meunier C.; Léonard A.; Su B.-L. Energy from Photobioreactors: Bioencapsulation of Photosynthetically Active Molecules, Organelles, and Whole Cells within Biologically Inert Matrices. Pure Appl. Chem. 2008, 80, 2345–2376..

    Not in our library10.1351/pac200880112345

  870. 870.

    Giese M.; Blusch L. K.; Khan M. K.; MacLachlan M. J. Functional Materials from Cellulose-Derived Liquid-Crystal Templates. Angew. Chem., Int. Ed. 2015, 54, 2888–2910..

    Not in our library10.1002/anie.201407141

  871. 871.

    Shopsowitz K. E.; Qi H.; Hamad W. Y.; MacLachlan M. J. Free-Standing Mesoporous Silica Films with Tunable Chiral Nematic Structures. Nature 2010, 468, 422–425..

    Not in our library10.1038/nature09540

  872. 872.

    Qi H.; Shopsowitz K. E.; Hamad W. Y.; MacLachlan M. J. Chiral Nematic Assemblies of Silver Nanoparticles in Mesoporous Silica Thin Films. J. Am. Chem. Soc. 2011, 133, 3728–3731..

    Not in our library10.1021/ja110369d

  873. 873.

    Li Z.; Ahadi K.; Jiang K.; Ahvazi B.; Li P.; Anyia A. O.; Cadien K.; Thundat T. Freestanding Hierarchical Porous Carbon Film Derived from Hybrid Nanocellulose for High-Power Supercapacitors. Nano Res. 2017, 10, 1847–1860..

    Not in our library10.1007/s12274-017-1573-8

  874. 874.

    Xu S.; Yao Y.; Guo Y.; Zeng X.; Lacey S. D.; Song H.; Chen C.; Li Y.; Dai J.; Wang Y.; et al. Textile Inspired Lithium–Oxygen Battery Cathode with Decoupled Oxygen and Electrolyte Pathways. Adv. Mater. 2018, 30, 1704907.

    Not in our library10.1002/adma.201704907

  875. 875.

    Jost K.; Dion G.; Gogotsi Y. Textile Energy Storage in Perspective. J. Mater. Chem. A 2014, 2, 10776–10787..

    Not in our library10.1039/c4ta00203b

  876. 876.

    Bao L.; Li X. Towards Textile Energy Storage from Cotton T-Shirts. Adv. Mater. 2012, 24, 3246–3252..

    Not in our library10.1002/adma.201200246

  877. 877.

    Leijonmarck S.; Cornell A.; Lindbergh G.; Wågberg L. Flexible Nano-Paper-Based Positive Electrodes for Li-Ion Batteries—Preparation Process and Properties. Nano Energy 2013, 2, 794–800..

    Not in our library10.1016/j.nanoen.2013.02.002

  878. 878.

    Chen W.; Yu H.; Lee S.-Y.; Wei T.; Li J.; Fan Z. Nanocellulose: A Promising Nanomaterial for Advanced Electrochemical Energy Storage. Chem. Soc. Rev. 2018, 47, 2837–2872..

    Not in our library10.1039/c7cs00790f

  879. 879.

    Muhd Julkapli N.; Bagheri S. Nanocellulose as a Green and Sustainable Emerging Material in Energy Applications: A Review. Polym. Adv. Technol. 2017, 28, 1583–1594..

    Not in our library10.1002/pat.4074

  880. 880.

    Su Y.; Zhao Y.; Zhang H.; Feng X.; Shi L.; Fang J. Polydopamine Functionalized Transparent Conductive Cellulose Nanopaper with Long-Term Durability. J. Mater. Chem. C 2017, 5, 573–581..

    Not in our library10.1039/c6tc04928a

  881. 881.

    Nizam P.; Gopakumar D. A.; Pottathara Y. B.; Pasquini D.; Nzihou A.; Thomas S. Nanocellulose-Based Composites: Fundamentals and Applications in Electronics. In Nanocellulose Based Composites for Electronics; Thomas S., Pottathara Y. B., Eds.; Elsevier: Amsterdam, 2021; pp 15–29.

    Not in our library

  882. 882.

    Yu H.; Chen P.; Chen W.; Liu Y. Effect of Cellulose Nanofibers on Induced Polymerization of Aniline and Formation of Nanostructured Conducting Composite. Cellulose 2014, 21, 1757–1767..

    Not in our library10.1007/s10570-014-0189-3

  883. 883.

    Thunberg J.; Kalogeropoulos T.; Kuzmenko V.; Hägg D.; Johannesson S.; Westman G.; Gatenholm P. In Situ Synthesis of Conductive Polypyrrole on Electrospun Cellulose Nanofibers: Scaffold for Neural Tissue Engineering. Cellulose 2015, 22, 1459–1467..

    Not in our library10.1007/s10570-015-0591-5

  884. 884.

    Du X.; Zhang Z.; Liu W.; Deng Y. Nanocellulose-Based Conductive Materials and Their Emerging Applications in Energy Devices-a Review. Nano Energy 2017, 35, 299–320..

    Not in our library10.1016/j.nanoen.2017.04.001

  885. 885.

    Wang Z.; Carlsson D. O.; Tammela P.; Hua K.; Zhang P.; Nyholm L.; Strømme M. Surface Modified Nanocellulose Fibers Yield Conducting Polymer-Based Flexible Supercapacitors with Enhanced Capacitances. ACS Nano 2015, 9, 7563–7571..

    Not in our library10.1021/acsnano.5b02846

  886. 886.

    Zhang X.; Wu X.; Lu C.; Zhou Z. Dialysis-Free and in Situ Doping Synthesis of Polypyrrole@ Cellulose Nanowhiskers Nanohybrid for Preparation of Conductive Nanocomposites with Enhanced Properties. ACS Sustainable Chem. Eng. 2015, 3, 675–682..

    Not in our library10.1021/sc500853m

  887. 887.

    Wu X.; Chabot V. L.; Kim B. K.; Yu A.; Berry R. M.; Tam K. C. Cost-Effective and Scalable Chemical Synthesis of Conductive Cellulose Nanocrystals for High-Performance Supercapacitors. Electrochim. Acta 2014, 138, 139–147..

    Not in our library10.1016/j.electacta.2014.06.089

  888. 888.

    Tang L.; Han J.; Jiang Z.; Chen S.; Wang H. Flexible Conductive Polypyrrole Nanocomposite Membranes Based on Bacterial Cellulose with Amphiphobicity. Carbohydr. Polym. 2015, 117, 230–235..

    Not in our library10.1016/j.carbpol.2014.09.049

  889. 889.

    Wang H.; Bian L.; Zhou P.; Tang J.; Tang W. Core–Sheath Structured Bacterial Cellulose/Polypyrrole Nanocomposites with Excellent Conductivity as Supercapacitors. J. Mater. Chem. A 2013, 1, 578–584..

    Not in our library10.1039/c2ta00040g

  890. 890.

    Razaq A.; Nyström G.; Strømme M.; Mihranyan A.; Nyholm L. High-Capacity Conductive Nanocellulose Paper Sheets for Electrochemically Controlled Extraction of DNA Oligomers. PLoS One 2011, 6, e29243.

    Not in our library10.1371/journal.pone.0029243

  891. 891.

    Yang B.; Yao C.; Yu Y.; Li Z.; Wang X. Nature Degradable, Flexible, and Transparent Conductive Substrates from Green and Earth-Abundant Materials. Sci. Rep. 2017, 7, 4936.

    Not in our library10.1038/s41598-017-04969-y

  892. 892.

    Khoshkava V.; Kamal M. Effect of Drying Conditions on Cellulose Nanocrystal (CNC) Agglomerate Porosity and Dispersibility in Polymer Nanocomposites. Powder Technol. 2014, 261, 288–298..

    Not in our library10.1016/j.powtec.2014.04.016

  893. 893.

    Fairman E. Avoiding Aggregation During Drying and Rehydration of Nanocellulose. M.Sc. Thesis. University of Maine, 2014.

    Not in our library

  894. 894.

    Huang D.; Wu M.; Wang C.; Kuga S.; Huang Y. Effect of Partial Dehydration on Freeze-Drying of Aqueous Nanocellulose Suspension. ACS Sustainable Chem. Eng. 2020, 8, 11389–11395..

    Not in our library10.1021/acssuschemeng.0c03688

  895. 895.

    Hanif Z.; Jeon H.; Tran T. H.; Jegal J.; Park S.-A.; Kim S.-M.; Park J.; Hwang S. Y.; Oh D. X. Butanol-Mediated Oven-Drying of Nanocellulose with Enhanced Dehydration Rate and Aqueous Re-Dispersion. J. Polym. Res. 2018, 25, 191.

    Not in our library10.1007/s10965-017-1343-z

  896. 896.

    Nadeem H.; Naseri M.; Shanmugam K.; Browne C.; Garnier G.; Batchelor W. Impact of Heat Drying on the Physical and Environmental Characteristics of the Nanocellulose-Based Films Produced Via Spray Deposition Technique. Cellulose 2020, 27, 10225–10239..

    Not in our library10.1007/s10570-020-03473-3

  897. 897.

    Chen Y.; Zhang L.; Yang Y.; Pang B.; Xu W.; Duan G.; Jiang S.; Zhang K. Recent Progress on Nanocellulose Aerogels: Preparation, Modification, Composite Fabrication, Applications. Adv. Mater. 2021, 33, 2005569.

    Not in our library10.1002/adma.202005569

  898. 898.

    Sinquefield S.; Ciesielski P. N.; Li K.; Gardner D. J.; Ozcan S. Nanocellulose Dewatering and Drying: Current State and Future Perspectives. ACS Sustainable Chem. Eng. 2020, 8, 9601–9615..

    Not in our library10.1021/acssuschemeng.0c01797

  899. 899.

    Wang X.; Zhang Y.; Jiang H.; Song Y.; Zhou Z.; Zhao H. Fabrication and Characterization of Nano-Cellulose Aerogels Via Supercritical Co2 Drying Technology. Mater. Lett. 2016, 183, 179–182..

    Not in our library10.1016/j.matlet.2016.07.081

  900. 900.

    Lewis L.; Hatzikiriakos S. G.; Hamad W. Y.; MacLachlan M. J. Freeze–Thaw Gelation of Cellulose Nanocrystals. ACS Macro Lett. 2019, 8, 486–491..

    Not in our library10.1021/acsmacrolett.9b00140

  901. 901.

    Gromovykh T. I.; Pigaleva M. A.; Gallyamov M. O.; Ivanenko I. P.; Ozerova K. E.; Kharitonova E. P.; Bahman M.; Feldman N. B.; Lutsenko S. V.; Kiselyova O. I. Structural Organization of Bacterial Cellulose: The Origin of Anisotropy and Layered Structures. Carbohydr. Polym. 2020, 237, 116140.

    Not in our library10.1016/j.carbpol.2020.116140

  902. 902.

    Munier P.; Gordeyeva K.; Bergström L.; Fall A. B. Directional Freezing of Nanocellulose Dispersions Aligns the Rod-Like Particles and Produces Low-Density and Robust Particle Networks. Biomacromolecules 2016, 17, 1875–1881..

    Not in our library10.1021/acs.biomac.6b00304

  903. 903.

    Sehaqui H.; Zhou Q.; Berglund L. A. High-Porosity Aerogels of High Specific Surface Area Prepared from Nanofibrillated Cellulose (NFC). Compos. Sci. Technol. 2011, 71, 1593–1599..

    Not in our library10.1016/j.compscitech.2011.07.003

  904. 904.

    Wan C.; Lu Y.; Jiao Y.; Jin C.; Sun Q.; Li J. Ultralight and Hydrophobic Nanofibrillated Cellulose Aerogels from Coconut Shell with Ultrastrong Adsorption Properties. J. Appl. Polym. Sci. 2015, 132, 42037.

    Not in our library10.1002/app.42037

  905. 905.

    Saito T.; Uematsu T.; Kimura S.; Enomae T.; Isogai A. Self-Aligned Integration of Native Cellulose Nanofibrils Towards Producing Diverse Bulk Materials. Soft Matter 2011, 7, 8804–8809..

    Not in our library10.1039/c1sm06050c

  906. 906.

    Kontturi E.; Vuorinen T. Indirect Evidence of Supramolecular Changes within Cellulose Microfibrils of Chemical Pulp Fibers Upon Drying. Cellulose 2009, 16, 65–74..

    Not in our library10.1007/s10570-008-9235-3

  907. 907.

    Liao J.; Pham K. A.; Breedveld V. Dewatering Cellulose Nanomaterial Suspensions and Preparing Concentrated Polymer Composite Gels Via Reverse Dialysis. ACS Sustainable Chem. Eng. 2021, 9, 9671–9679..

    Not in our library10.1021/acssuschemeng.1c01169

  908. 908.

    Fall A.; Henriksson M.; Karppinen A.; Opstad A.; Heggset E. B.; Syverud K. The Effect of Ionic Strength and Ph on the Dewatering Rate of Cellulose Nanofibril Dispersions. Cellulose 2022, 29, 7649–7662..

    Not in our library10.1007/s10570-022-04719-y

  909. 909.

    Chi K.; Catchmark J. M. Enhanced Dispersion and Interface Compatibilization of Crystalline Nanocellulose in Polylactide by Surfactant Adsorption. Cellulose 2017, 24, 4845–4860..

    Not in our library10.1007/s10570-017-1479-3

  910. 910.

    Kargarzadeh H.; Huang J.; Lin N.; Ahmad I.; Mariano M.; Dufresne A.; Thomas S.; Gałęski A. Recent Developments in Nanocellulose-Based Biodegradable Polymers, Thermoplastic Polymers, and Porous Nanocomposites. Prog. Polym. Sci. 2018, 87, 197–227..

    Not in our library10.1016/j.progpolymsci.2018.07.008

  911. 911.

    Kuo P.-Y.; de Assis Barros L.; Yan N.; Sain M.; Qing Y.; Wu Y. Nanocellulose Composites with Enhanced Interfacial Compatibility and Mechanical Properties Using a Hybrid-Toughened Epoxy Matrix. Carbohydr. Polym. 2017, 177, 249–257..

    Not in our library10.1016/j.carbpol.2017.08.091

  912. 912.

    Fumagalli M.; Berriot J.; de Gaudemaris B.; Veyland A.; Putaux J.-L.; Molina-Boisseau S.; Heux L. Rubber Materials from Elastomers and Nanocellulose Powders: Filler Dispersion and Mechanical Reinforcement. Soft Matter 2018, 14, 2638–2648..

    Not in our library10.1039/c8sm00210j

  913. 913.

    Kedzior S. A.; Graham L.; Moorlag C.; Dooley B. M.; Cranston E. D. Poly (Methyl Methacrylate)-Grafted Cellulose Nanocrystals: One-Step Synthesis, Nanocomposite Preparation, and Characterization. Can. J. Chem. Eng. 2016, 94, 811–822..

    Not in our library10.1002/cjce.22456

  914. 914.

    Liu Y.; Zhou L.; Wang L.; Pan X.; Wang K.; Shu J.; Liu L.; Zhang H.; Lin L.; Shi X.; et al. Air-Dried Porous Powder of Polymethyl Methacrylate Modified Cellulose Nanocrystal Nanocomposite and Its Diverse Applications. Compos. Sci. Technol. 2020, 188, 107985.

    Not in our library10.1016/j.compscitech.2019.107985

  915. 915.

    Yang X.; Ku T.-H.; Biswas S. K.; Yano H.; Abe K. Uv Grafting: Surface Modification of Cellulose Nanofibers without the Use of Organic Solvents. Green Chem. 2019, 21, 4619–4624..

    Not in our library10.1039/c9gc02035g

  916. 916.

    Wang Z.; Zhao S.; Zhang W.; Qi C.; Zhang S.; Li J. Bio-Inspired Cellulose Nanofiber-Reinforced Soy Protein Resin Adhesives with Dopamine-Induced Codeposition of “Water-Resistant” Interphases. Appl. Surf. Sci. 2019, 478, 441–450..

    Not in our library10.1016/j.apsusc.2019.01.154

  917. 917.

    Hu Z.; Berry R. M.; Pelton R.; Cranston E. D. One-Pot Water-Based Hydrophobic Surface Modification of Cellulose Nanocrystals Using Plant Polyphenols. ACS Sustainable Chem. Eng. 2017, 5, 5018–5026..

    Not in our library10.1021/acssuschemeng.7b00415

  918. 918.

    Gopakumar D. A.; Pai A. R.; Pottathara Y. B.; Pasquini D.; Carlos de Morais L. s.; Luke M.; Kalarikkal N.; Grohens Y.; Thomas S. Cellulose Nanofiber-Based Polyaniline Flexible Papers as Sustainable Microwave Absorbers in the X-Band. ACS Appl. Mater. Interfaces 2018, 10, 20032–20043..

    Not in our library10.1021/acsami.8b04549

  919. 919.

    Yuan H.; Nishiyama Y.; Wada M.; Kuga S. Surface Acylation of Cellulose Whiskers by Drying Aqueous Emulsion. Biomacromolecules 2006, 7, 696–700..

    Not in our library10.1021/bm050828j

  920. 920.

    Chen Q.-H.; Zheng J.; Xu Y.-T.; Yin S.-W.; Liu F.; Tang C.-H. Surface Modification Improves Fabrication of Pickering High Internal Phase Emulsions Stabilized by Cellulose Nanocrystals. Food Hydrocolloids 2018, 75, 125–130..

    Not in our library10.1016/j.foodhyd.2017.09.005

  921. 921.

    Ávila Ramírez J. A.; Fortunati E.; Kenny J. M.; Torre L.; Foresti M. L. Simple Citric Acid-Catalyzed Surface Esterification of Cellulose Nanocrystals. Carbohydr. Polym. 2017, 157, 1358–1364..

    Not in our library10.1016/j.carbpol.2016.11.008

  922. 922.

    Wei L.; Agarwal U. P.; Hirth K. C.; Matuana L. M.; Sabo R. C.; Stark N. M. Chemical Modification of Nanocellulose with Canola Oil Fatty Acid Methyl Ester. Carbohydr. Polym. 2017, 169, 108–116..

    Not in our library10.1016/j.carbpol.2017.04.008

  923. 923.

    Shojaeiarani J.; Bajwa D. S.; Stark N. M. Green Esterification: A New Approach to Improve Thermal and Mechanical Properties of Poly (Lactic Acid) Composites Reinforced by Cellulose Nanocrystals. J. Appl. Polym. Sci. 2018, 135, 46468.

    Not in our library10.1002/app.46468

  924. 924.

    Isogai A. Emerging Nanocellulose Technologies: Recent Developments. Adv. Mater. 2021, 33, 2000630.

    Not in our library10.1002/adma.202000630

  925. 925.

    Sain M.; Oksman K. Introduction to Cellulose Nanocomposites. ACS Symp. Ser. 2006, 938, 2–8..

    Not in our library10.1021/bk-2006-0938.ch001

  926. 926.

    Puglia D.; Fortunati E.; Kenny J. M. Multifunctional Polymeric Nanocomposites Based on Cellulosic Reinforcements; Elsevier: Amsterdam, 2016.

    Not in our library

  927. 927.

    Kalia S.; Kaith B.; Kaur I. Cellulose Fibers: Bio- and Nano-Polymer Composites; Springer: Berlin, 2011.

    Not in our library

  928. 928.

    Thiruvengadam V.; Vitta S. Bacterial Cellulose and its Multifunctional Composites: Synthesis and Properties. In Nanocellulose Polymer Nanocomposites; Thakur V. K., Ed.; Scrivener: Salem, MA, 2014; pp 479–506.

    Not in our library

  929. 929.

    Oksman K.; Aitomäki Y.; Mathew A. P.; Siqueira G.; Zhou Q.; Butylina S.; Tanpichai S.; Zhou X.; Hooshmand S. Review of the Recent Developments in Cellulose Nanocomposite Processing. Composites, Part A 2016, 83, 2–18..

    Not in our library10.1016/j.compositesa.2015.10.041

  930. 930.

    Kim J.-H.; Shim B. S.; Kim H. S.; Lee Y.-J.; Min S.-K.; Jang D.; Abas Z.; Kim J. Review of Nanocellulose for Sustainable Future Materials. Int. J. Precis. Eng. Manuf. 2015, 2, 197–213..

    Not in our library10.1007/s40684-015-0024-9

  931. 931.

    Ilyas R.; Sapuan S.; Sanyang M. L.; Ishak M. R.; Zainudin E. Nanocrystalline Cellulose as Reinforcement for Polymeric Matrix Nanocomposites and Its Potential Applications: A Review. Curr. Anal. Chem. 2018, 14, 203–225..

    Not in our library10.2174/1573411013666171003155624

  932. 932.

    Benítez A.; Walther A. Cellulose Nanofibril Nanopapers and Bioinspired Nanocomposites: A Review to Understand the Mechanical Property Space. J. Mater. Chem. A 2017, 5, 16003–16024..

    Not in our library10.1039/c7ta02006f

  933. 933.

    Ferreira F.; Dufresne A.; Pinheiro I.; Souza D.; Gouveia R.; Mei L.; Lona L. How Do Cellulose Nanocrystals Affect the Overall Properties of Biodegradable Polymer Nanocomposites: A Comprehensive Review. Eur. Polym. J. 2018, 108, 274–285..

    Not in our library10.1016/j.eurpolymj.2018.08.045

  934. 934.

    Sharma A.; Thakur M.; Bhattacharya M.; Mandal T.; Goswami S. Commercial Application of Cellulose Nano-Composites-a Review. Biotechnol. Rep 2019, 21, e00316.

    Not in our library10.1016/j.btre.2019.e00316

  935. 935.

    Poothanari M. A.; Schreier A.; Missoum K.; Bras J.; Leterrier Y. Photocured Nanocellulose Composites: Recent Advances. ACS Sustainable Chem. Eng. 2022, 10, 3131–3149..

    Not in our library10.1021/acssuschemeng.1c07631

  936. 936.

    Parambath Kanoth B.; Claudino M.; Johansson M.; Berglund L. A.; Zhou Q. Biocomposites from Natural Rubber: Synergistic Effects of Functionalized Cellulose Nanocrystals as Both Reinforcing and Cross-Linking Agents Via Free-Radical Thiol–Ene Chemistry. ACS Appl. Mater. Interfaces 2015, 7, 16303–16310..

    Not in our library10.1021/acsami.5b03115

  937. 937.

    Yao J.; Ji P.; Sheng N.; Guan F.; Zhang M.; Wang B.; Chen S.; Wang H. Hierarchical Core-Sheath Polypyrrole@ Carbon Nanotube/Bacterial Cellulose Macrofibers with High Electrochemical Performance for All-Solid-State Supercapacitors. Electrochim. Acta 2018, 283, 1578–1588..

    Not in our library10.1016/j.electacta.2018.07.086

  938. 938.

    Xiong J.; Lin M. F.; Wang J.; Gaw S. L.; Parida K.; Lee P. S. Wearable All-Fabric-Based Triboelectric Generator for Water Energy Harvesting. Adv. Energy Mater. 2017, 7, 1701243.

    Not in our library10.1002/aenm.201701243

  939. 939.

    Li S.; Warzywoda J.; Wang S.; Ren G.; Fan Z. Bacterial Cellulose Derived Carbon Nanofiber Aerogel with Lithium Polysulfide Catholyte for Lithium–Sulfur Batteries. Carbon 2017, 124, 212–218..

    Not in our library10.1016/j.carbon.2017.08.062

  940. 940.

    Carrillo C. A.; Nypelö T.; Rojas O. J. Double Emulsions for the Compatibilization of Hydrophilic Nanocellulose with Non-Polar Polymers and Validation in the Synthesis of Composite Fibers. Soft Matter 2016, 12, 2721–2728..

    Not in our library10.1039/c5sm02578h

  941. 941.

    Lee W. J.; Clancy A. J.; Kontturi E.; Bismarck A.; Shaffer M. S. Strong and Stiff: High-Performance Cellulose Nanocrystal/Poly (Vinyl Alcohol) Composite Fibers. ACS Appl. Mater. Interfaces 2016, 8, 31500–31504..

    Not in our library10.1021/acsami.6b11578

  942. 942.

    Lyubimova O.; Stoyanov S. R.; Gusarov S.; Kovalenko A. Electric Interfacial Layer of Modified Cellulose Nanocrystals in Aqueous Electrolyte Solution: Predictions by the Molecular Theory of Solvation. Langmuir 2015, 31, 7106–7116..

    Not in our library10.1021/acs.langmuir.5b00680

  943. 943.

    Wei Z.; Sinko R.; Keten S.; Luijten E. Effect of Surface Modification on Water Adsorption and Interfacial Mechanics of Cellulose Nanocrystals. ACS Appl. Mater. Interfaces 2018, 10, 8349–8358..

    Not in our library10.1021/acsami.7b18803

  944. 944.

    Palange C.; Johns M. A.; Scurr D. J.; Phipps J. S.; Eichhorn S. J. The Effect of the Dispersion of Microfibrillated Cellulose on the Mechanical Properties of Melt-Compounded Polypropylene–Polyethylene Copolymer. Cellulose 2019, 26, 9645–9659..

    Not in our library10.1007/s10570-019-02756-8

  945. 945.

    Naseri N.; Deepa B.; Mathew A. P.; Oksman K.; Girandon L. Nanocellulose-Based Interpenetrating Polymer Network (IPN) Hydrogels for Cartilage Applications. Biomacromolecules 2016, 17, 3714–3723..

    Not in our library10.1021/acs.biomac.6b01243

  946. 946.

    Liu Y.; Sui Y.; Liu C.; Liu C.; Wu M.; Li B.; Li Y. A Physically Crosslinked Polydopamine/Nanocellulose Hydrogel as Potential Versatile Vehicles for Drug Delivery and Wound Healing. Carbohydr. Polym. 2018, 188, 27–36..

    Not in our library10.1016/j.carbpol.2018.01.093

  947. 947.

    Zheng C.; Lu K.; Lu Y.; Zhu S.; Yue Y.; Xu X.; Mei C.; Xiao H.; Wu Q.; Han J. A Stretchable, Self-Healing Conductive Hydrogels Based on Nanocellulose Supported Graphene Towards Wearable Monitoring of Human Motion. Carbohydr. Polym. 2020, 250, 116905.

    Not in our library10.1016/j.carbpol.2020.116905

  948. 948.

    Cao L.; Huang J.; Fan J.; Gong Z.; Xu C.; Chen Y. Nanocellulose-a Sustainable and Efficient Nanofiller for Rubber Nanocomposites: From Reinforcement to Smart Soft Materials. Polym. Rev. 2022, 62, 549–584..

    Not in our library10.1080/15583724.2021.2001004

  949. 949.

    Ilyas R.; Sapuan S.; Norrrahim M. N. F.; Yasim-Anuar T. A. T.; Kadier A.; Kalil M. S.; Atikah M.; Ibrahim R.; Asrofi M.; Abral H. Nanocellulose/Starch Biopolymer Nanocomposites: Processing, Manufacturing, and Applications. In Advanced Processing, Properties, and Applications of Starch and Other Bio-Based Polymers; Al-Oqla F. M., Sapuan S. M., Eds.; Elsevier: Amsterdam, 2020; pp 65–88.

    Not in our library

  950. 950.

    Spoljaric S.; Salminen A.; Luong N. D.; Seppälä J. Crosslinked Nanofibrillated Cellulose: Poly (Acrylic Acid) Nanocomposite Films; Enhanced Mechanical Performance in Aqueous Environments. Cellulose 2013, 20, 2991–3005..

    Not in our library10.1007/s10570-013-0061-x

  951. 951.

    Lu P.; Hsieh Y.-L. Cellulose Nanocrystal-Filled Poly (Acrylic Acid) Nanocomposite Fibrous Membranes. Nanotechnology 2009, 20, 415604.

    Not in our library10.1088/0957-4484/20/41/415604

  952. 952.

    Heiner A. P.; Kuutti L.; Teleman O. Comparison of the Interface between Water and Four Surfaces of Native Crystalline Cellulose by Molecular Dynamics Simulations. Carbohydr. Res. 1998, 306, 205–220..

    Not in our library10.1016/s0008-6215(97)10053-2

  953. 953.

    Bergenstråhle-Wohlert M.; Brady J. W. Overview of Computer Modeling of Cellulose. In Biomass Conversion; Himmel M. E., Ed.; Springer: Berlin, 2012; pp 11–22.

    Not in our library10.1007/978-1-61779-956-3_2

  954. 954.

    Zhang Y.; He H.; Liu Y.; Wang Y.; Huo F.; Fan M.; Adidharma H.; Li X.; Zhang S. Recent Progress in Theoretical and Computational Studies on the Utilization of Lignocellulosic Materials. Green Chem. 2019, 21, 9–35..

    Not in our library10.1039/c8gc02059k

  955. 955.

    Zhou S.; Jin K.; Buehler M. J. Understanding Plant Biomass Via Computational Modeling. Adv. Mater. 2021, 33, 2003206.

    Not in our library10.1002/adma.202003206

  956. 956.

    Xia W.; Song J.; Jeong C.; Hsu D. D.; Phelan F. R. Jr; Douglas J. F.; Keten S. Energy-Renormalization for Achieving Temperature Transferable Coarse-Graining of Polymer Dynamics. Macromolecules 2017, 50, 8787–8796..

    Not in our library10.1021/acs.macromol.7b01717

  957. 957.

    Noid W. G. Perspective: Coarse-Grained Models for Biomolecular Systems. J. Chem. Phys. 2013, 139, 090901.

    Not in our library10.1063/1.4818908

  958. 958.

    Guvench O.; Greene S. N.; Kamath G.; Brady J. W.; Venable R. M.; Pastor R. W.; Mackerell A. D. Jr Additive Empirical Force Field for Hexopyranose Monosaccharides. J. Comput. Chem. 2008, 29, 2543–2564..

    Not in our library10.1002/jcc.21004

  959. 959.

    Guvench O.; Hatcher E.; Venable R. M.; Pastor R. W.; MacKerell A. D. Jr Charmm Additive All-Atom Force Field for Glycosidic Linkages between Hexopyranoses. J. Chem. Theory Comput. 2009, 5, 2353–2370..

    Not in our library10.1021/ct900242e

  960. 960.

    Kirschner K. N.; Yongye A. B.; Tschampel S. M.; González-Outeiriño J.; Daniels C. R.; Foley B. L.; Woods R. J. Glycam06: A Generalizable Biomolecular Force Field. Carbohydrates. J. Comput. Chem. 2008, 29, 622–655..

    Not in our library10.1002/jcc.20820

  961. 961.

    Hansen H. S.; Hünenberger P. H. A Reoptimized Gromos Force Field for Hexopyranose-Based Carbohydrates Accounting for the Relative Free Energies of Ring Conformers, Anomers, Epimers, Hydroxymethyl Rotamers, and Glycosidic Linkage Conformers. J. Comput. Chem. 2011, 32, 998–1032..

    Not in our library10.1002/jcc.21675

  962. 962.

    Damm W.; Frontera A.; Tirado-Rives J.; Jorgensen W. L. Opls All-Atom Force Field for Carbohydrates. J. Comput. Chem. 1997, 18, 1955–1970..

    Not in our library10.1002/(sici)1096-987x(199712)18:16<1955::aid-jcc1>3.0.co;2-l

  963. 963.

    Berendsen H.; Postma J.; Van Gunsteren W.; Hermans J. Interaction Models for Water in Relation to Protein Hydration. In Intermolecular Forces; Pullman B., Ed.; Springer: Dordrecht, The Netherlands, 1981; pp 331–342.

    Not in our library

  964. 964.

    Jorgensen W. L.; Chandrasekhar J.; Madura J. D.; Impey R. W.; Klein M. L. Comparison of Simple Potential Functions for Simulating Liquid Water. J. Chem. Phys. 1983, 79, 926–935..

    Not in our library10.1063/1.445869

  965. 965.

    Stenqvist B.; Wernersson E.; Lund M. Cellulose-Water Interactions: Effect of Electronic Polarizability. Nordic Pulp Pap. Res. J. 2015, 30, 26–31..

    Not in our library10.3183/npprj-2015-30-01-p026-031

  966. 966.

    Vega C.; Abascal J. L. Simulating Water with Rigid Non-Polarizable Models: A General Perspective. Phys. Chem. Chem. Phys. 2011, 13, 19663–19688..

    Not in our library10.1039/c1cp22168j

  967. 967.

    Medronho B.; Romano A.; Miguel M. G.; Stigsson L.; Lindman B. Rationalizing Cellulose (in) Solubility: Reviewing Basic Physicochemical Aspects and Role of Hydrophobic Interactions. Cellulose 2012, 19, 581–587..

    Not in our library10.1007/s10570-011-9644-6

  968. 968.

    Lindman B.; Medronho B.; Alves L.; Norgren M.; Nordenskiöld L. Hydrophobic Interactions Control the Self-Assembly of DNA and Cellulose. Q. Rev. Biophys. 2021, 54, E3.

    Not in our library10.1017/s0033583521000019

  969. 969.

    Bergenstråhle-Wohlert M.; Angles d’Ortoli T.; Sjöberg N. A.; Widmalm G.; Wohlert J. On the Anomalous Temperature Dependence of Cellulose Aqueous Solubility. Cellulose 2016, 23, 2375–2387..

    Not in our library10.1007/s10570-016-0991-1

  970. 970.

    Bergenstråhle M.; Wohlert J.; Himmel M. E.; Brady J. W. Simulation Studies of the Insolubility of Cellulose. Carbohydr. Res. 2010, 345, 2060–2066..

    Not in our library10.1016/j.carres.2010.06.017

  971. 971.

    Gross A. S.; Bell A. T.; Chu J.-W. Entropy of Cellulose Dissolution in Water and in the Ionic Liquid 1-Butyl-3-Methylimidazolim Chloride. Phys. Chem. Chem. Phys. 2012, 14, 8425–8430..

    Not in our library10.1039/c2cp40417f

  972. 972.

    Tolonen L. K.; Bergenstråhle-Wohlert M.; Sixta H.; Wohlert J. Solubility of Cellulose in Supercritical Water Studied by Molecular Dynamics Simulations. J. Phys. Chem. B 2015, 119, 4739–4748..

    Not in our library10.1021/acs.jpcb.5b01121

  973. 973.

    Wernersson E.; Stenqvist B.; Lund M. The Mechanism of Cellulose Solubilization by Urea Studied by Molecular Simulation. Cellulose 2015, 22, 991–1001..

    Not in our library10.1007/s10570-015-0548-8

  974. 974.

    Chen P.; Nishiyama Y.; Wohlert J.; Lu A.; Mazeau K.; Ismail A. E. Translational Entropy and Dispersion Energy Jointly Drive the Adsorption of Urea to Cellulose. J. Phys. Chem. B 2017, 121, 2244–2251..

    Not in our library10.1021/acs.jpcb.6b11914

  975. 975.

    Bu L.; Beckham G. T.; Crowley M. F.; Chang C. H.; Matthews J. F.; Bomble Y. J.; Adney W. S.; Himmel M. E.; Nimlos M. R. The Energy Landscape for the Interaction of the Family 1 Carbohydrate-Binding Module and the Cellulose Surface Is Altered by Hydrolyzed Glycosidic Bonds. J. Phys. Chem. B 2009, 113, 10994–11002..

    Not in our library10.1021/jp904003z

  976. 976.

    Bu L.; Himmel M. E.; Crowley M. F. The Molecular Origins of Twist in Cellulose Iβ. Carbohydr. Polym. 2015, 125, 146–152..

    Not in our library10.1016/j.carbpol.2015.02.023

  977. 977.

    Devarajan A.; Markutsya S.; Lamm M. H.; Cheng X.; Smith J. C.; Baluyut J. Y.; Kholod Y.; Gordon M. S.; Windus T. L. Ab Initio Study of Molecular Interactions in Cellulose Iα. J. Phys. Chem. B 2013, 117, 10430–10443..

    Not in our library10.1021/jp406266u

  978. 978.

    Hadden J. A.; French A. D.; Woods R. J. Unraveling Cellulose Microfibrils: A Twisted Tale. Biopolymers 2013, 99, 746–756..

    Not in our library10.1002/bip.22279

  979. 979.

    Matthews J. F.; Bergenstråhle M.; Beckham G. T.; Himmel M. E.; Nimlos M. R.; Brady J. W.; Crowley M. F. High-Temperature Behavior of Cellulose I. J. Phys. Chem. B 2011, 115, 2155–2166..

    Not in our library10.1021/jp1106839

  980. 980.

    Matthews J. F.; Beckham G. T.; Bergenstrahle-Wohlert M.; Brady J. W.; Himmel M. E.; Crowley M. F. Comparison of Cellulose Iβ Simulations with Three Carbohydrate Force Fields. J. Chem. Theory Comput. 2012, 8, 735–748..

    Not in our library10.1021/ct2007692

  981. 981.

    Nishiyama Y.; Johnson G. P.; French A. D.; Forsyth V. T.; Langan P. Neutron Crystallography, Molecular Dynamics, and Quantum Mechanics Studies of the Nature of Hydrogen Bonding in Cellulose Iβ. Biomacromolecules 2008, 9, 3133–3140..

    Not in our library10.1021/bm800726v

  982. 982.

    Wohlert J.; Berglund L. A. A Coarse-Grained Model for Molecular Dynamics Simulations of Native Cellulose. J. Chem. Theory Comput. 2011, 7, 753–760..

    Not in our library10.1021/ct100489z

  983. 983.

    Yui T.; Nishimura S.; Akiba S.; Hayashi S. Swelling Behavior of the Cellulose Iβ Crystal Models by Molecular Dynamics. Carbohydr. Res. 2006, 341, 2521–2530..

    Not in our library10.1016/j.carres.2006.04.051

  984. 984.

    Willhammar T.; Daicho K.; Johnstone D. N.; Kobayashi K.; Liu Y.; Midgley P. A.; Bergström L.; Saito T. Local Crystallinity in Twisted Cellulose Nanofibers. ACS Nano 2021, 15, 2730–2737..

    Not in our library10.1021/acsnano.0c08295

  985. 985.

    Hanley S. J.; Revol J.-F.; Godbout L.; Gray D. G. Atomic Force Microscopy and Transmission Electron Microscopy of Cellulose from Micrasterias Denticulata; Evidence for a Chiral Helical Microfibril Twist. Cellulose 1997, 4, 209–220..

    Not in our library10.1023/a:1018483722417

  986. 986.

    Arcari M.; Zuccarella E.; Axelrod R.; Adamcik J.; Sánchez-Ferrer A.; Mezzenga R.; Nyström G. Nanostructural Properties and Twist Periodicity of Cellulose Nanofibrils with Variable Charge Density. Biomacromolecules 2019, 20, 1288–1296..

    Not in our library10.1021/acs.biomac.8b01706

  987. 987.

    Zhao Z.; Shklyaev O. E.; Nili A.; Mohamed M. N. A.; Kubicki J. D.; Crespi V. H.; Zhong L. Cellulose Microfibril Twist, Mechanics, and Implication for Cellulose Biosynthesis. J. Phys. Chem. A 2013, 117, 2580–2589..

    Not in our library10.1021/jp3089929

  988. 988.

    Wang D.; Ámundadóttir M. L.; van Gunsteren W. F.; Hünenberger P. H. Intramolecular Hydrogen-Bonding in Aqueous Carbohydrates as a Cause or Consequence of Conformational Preferences: A Molecular Dynamics Study of Cellobiose Stereoisomers. Eur. Biophys. J. 2013, 42, 521–537..

    Not in our library10.1007/s00249-013-0901-5

  989. 989.

    Berglund J.; Angles d’Ortoli T.; Vilaplana F.; Widmalm G.; Bergenstråhle-Wohlert M.; Lawoko M.; Henriksson G.; Lindström M.; Wohlert J. A Molecular Dynamics Study of the Effect of Glycosidic Linkage Type in the Hemicellulose Backbone on the Molecular Chain Flexibility. Plant J. 2016, 88, 56–70..

    Not in our library10.1111/tpj.13259

  990. 990.

    Kannam S. K.; Oehme D. P.; Doblin M. S.; Gidley M. J.; Bacic A.; Downton M. T. Hydrogen Bonds and Twist in Cellulose Microfibrils. Carbohydr. Polym. 2017, 175, 433–439..

    Not in our library10.1016/j.carbpol.2017.07.083

  991. 991.

    Paajanen A.; Ceccherini S.; Maloney T.; Ketoja J. A. Chirality and Bound Water in the Hierarchical Cellulose Structure. Cellulose 2019, 26, 5877–5892..

    Not in our library10.1007/s10570-019-02525-7

  992. 992.

    Gross A. S.; Chu J.-W. On the Molecular Origins of Biomass Recalcitrance: The Interaction Network and Solvation Structures of Cellulose Microfibrils. J. Phys. Chem. B 2010, 114, 13333–13341..

    Not in our library10.1021/jp106452m

  993. 993.

    Malaspina D. C.; Faraudo J. Molecular Insight into the Wetting Behavior and Amphiphilic Character of Cellulose Nanocrystals. Adv. Colloid Interface Sci. 2019, 267, 15–25..

    Not in our library10.1016/j.cis.2019.02.003

  994. 994.

    Bergenstråhle M.; Mazeau K.; Berglund L. A. Molecular Modeling of Interfaces between Cellulose Crystals and Surrounding Molecules: Effects of Caprolactone Surface Grafting. Eur. Polym. J. 2008, 44, 3662–3669..

    Not in our library10.1016/j.eurpolymj.2008.08.029

  995. 995.

    Chen P.; Terenzi C.; Furo I.; Berglund L. A.; Wohlert J. Quantifying Localized Macromolecular Dynamics within Hydrated Cellulose Fibril Aggregates. Macromolecules 2019, 52, 7278–7288..

    Not in our library10.1021/acs.macromol.9b00472

  996. 996.

    Petridis L.; O’Neill H. M.; Johnsen M.; Fan B.; Schulz R.; Mamontov E.; Maranas J.; Langan P.; Smith J. C. Hydration Control of the Mechanical and Dynamical Properties of Cellulose. Biomacromolecules 2014, 15, 4152–4159..

    Not in our library10.1021/bm5011849

  997. 997.

    Chandler D. Interfaces and the Driving Force of Hydrophobic Assembly. Nature 2005, 437, 640–647..

    Not in our library10.1038/nature04162

  998. 998.

    Miyamoto H.; Schnupf U.; Brady J. W. Water Structuring over the Hydrophobic Surface of Cellulose. J. Agric. Food Chem. 2014, 62, 11017–11023..

    Not in our library10.1021/jf501763r

  999. 999.

    Kuribayashi T.; Ogawa Y.; Rochas C.; Matsumoto Y.; Heux L.; Nishiyama Y. Hydrothermal Transformation of Wood Cellulose Crystals into Pseudo-Orthorhombic Structure by Cocrystallization. ACS Macro Lett. 2016, 5, 730–734..

    Not in our library10.1021/acsmacrolett.6b00273

  1000. 1000.

    Chen P.; Wohlert J.; Berglund L.; Furó I. Water as an Intrinsic Structural Element in Cellulose Fibril Aggregates. J. Phys. Chem. Lett. 2022, 13, 5424–5430..

    Not in our library10.1021/acs.jpclett.2c00781

  1001. 1001.

    Zhang C.; Keten S.; Derome D.; Carmeliet J. Hydrogen Bonds Dominated Frictional Stick-Slip of Cellulose Nanocrystals. Carbohydr. Polym. 2021, 258, 117682.

    Not in our library10.1016/j.carbpol.2021.117682

  1002. 1002.

    Hou Y.; Guan Q.-F.; Xia J.; Ling Z.-C.; He Z.; Han Z.-M.; Yang H.-B.; Gu P.; Zhu Y.; Yu S.-H.; Wu H-A. Strengthening and Toughening Hierarchical Nanocellulose Via Humidity-Mediated Interface. ACS Nano 2021, 15, 1310–1320..

    Not in our library10.1021/acsnano.0c08574

  1003. 1003.

    Li Y.; Lin M.; Davenport J. W. Ab Initio Studies of Cellulose I: Crystal Structure, Intermolecular Forces, and Interactions with Water. J. Phys. Chem. C 2011, 115, 11533–11539..

    Not in our library10.1021/jp2006759

  1004. 1004.

    Nawrocki G.; Cazade P.-A.; Thompson D.; Cieplak M. Peptide Recognition Capabilities of Cellulose in Molecular Dynamics Simulations. J. Phys. Chem. C 2015, 119, 24404–24416..

    Not in our library10.1021/acs.jpcc.5b07118

  1005. 1005.

    Trentin L. N.; Pereira C. S.; Silveira R. L.; Hill S.; Sorieul M.; Skaf M. S. Nanoscale Wetting of Crystalline Cellulose. Biomacromolecules 2021, 22, 4251–4261..

    Not in our library10.1021/acs.biomac.1c00801

  1006. 1006.

    Karna N. K.; Wohlert J.; Lidén A.; Mattsson T.; Theliander H. Wettability of Cellulose Surfaces under the Influence of an External Electric Field. J. Colloid Interface Sci. 2021, 589, 347–355..

    Not in our library10.1016/j.jcis.2021.01.003

  1007. 1007.

    Maurer R. J.; Sax A. F.; Ribitsch V. Molecular Simulation of Surface Reorganization and Wetting in Crystalline Cellulose I and II. Cellulose 2013, 20, 25–42..

    Not in our library10.1007/s10570-012-9835-9

  1008. 1008.

    Ogawa Y.; Nishiyama Y.; Mazeau K. Drying-Induced Bending Deformation of Cellulose Nanocrystals Studied by Molecular Dynamics Simulations. Cellulose 2020, 27, 9779–9786..

    Not in our library10.1007/s10570-020-03451-9

  1009. 1009.

    Bourassa P.; Bouchard J.; Robert S. Quantum Chemical Calculations of Pristine and Modified Crystalline Cellulose Surfaces: Benchmarking Interactions and Adsorption of Water and Electrolyte. Cellulose 2014, 21, 71–86..

    Not in our library10.1007/s10570-013-0150-x

  1010. 1010.
  1011. 1011.

    Nishiyama Y.; Sugiyama J.; Chanzy H.; Langan P. Crystal Structure and Hydrogen Bonding System in Cellulose Iα from Synchrotron X-Ray and Neutron Fiber Diffraction. J. Am. Chem. Soc. 2003, 125, 14300–14306..

    Not in our library10.1021/ja037055w

  1012. 1012.

    Cosgrove D. J. Re-Constructing Our Models of Cellulose and Primary Cell Wall Assembly. Curr. Opin. Plant Biol. 2014, 22, 122–131..

    Not in our library10.1016/j.pbi.2014.11.001

  1013. 1013.

    Martínez-Sanz M.; Gidley M. J.; Gilbert E. P. Application of X-Ray and Neutron Small Angle Scattering Techniques to Study the Hierarchical Structure of Plant Cell Walls: A Review. Carbohydr. Polym. 2015, 125, 120–134..

    Not in our library10.1016/j.carbpol.2015.02.010

  1014. 1014.

    Tenhunen T.-M.; Peresin M. S.; Penttilä P. A.; Pere J.; Serimaa R.; Tammelin T. Significance of Xylan on the Stability and Water Interactions of Cellulosic Nanofibrils. React. Funct. Polym. 2014, 85, 157–166..

    Not in our library10.1016/j.reactfunctpolym.2014.08.011

  1015. 1015.

    Belbekhouche S.; Bras J.; Siqueira G.; Chappey C.; Lebrun L.; Khelifi B.; Marais S.; Dufresne A. Water Sorption Behavior and Gas Barrier Properties of Cellulose Whiskers and Microfibrils Films. Carbohydr. Polym. 2011, 83, 1740–1748..

    Not in our library10.1016/j.carbpol.2010.10.036

  1016. 1016.

    Natarajan B.; Emiroglu C.; Obrzut J.; Fox D. M.; Pazmino B.; Douglas J. F.; Gilman J. W. Dielectric Characterization of Confined Water in Chiral Cellulose Nanocrystal Films. ACS Appl. Mater. Interfaces 2017, 9, 14222–14231..

    Not in our library10.1021/acsami.7b01674

  1017. 1017.

    Hatakeyama T.; Inui Y.; Iijima M.; Hatakeyama H. Bound Water Restrained by Nanocellulose Fibres. J. Therm. Anal. Calorim. 2013, 113, 1019–1025..

    Not in our library10.1007/s10973-012-2823-3

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    Gelin K.; Bodin A.; Gatenholm P.; Mihranyan A.; Edwards K.; Strømme M. Characterization of Water in Bacterial Cellulose Using Dielectric Spectroscopy and Electron Microscopy. Polymer 2007, 48, 7623–7631..

    Not in our library10.1016/j.polymer.2007.10.039

  1019. 1019.

    Ahola S.; Salmi J.; Johansson L.-S.; Laine J.; Österberg M. Model Films from Native Cellulose Nanofibrils. Preparation, Swelling, and Surface Interactions. Biomacromolecules 2008, 9, 1273–1282..

    Not in our library10.1021/bm701317k

  1020. 1020.

    Ducker W. A.; Senden T. J.; Pashley R. M. Direct Measurement of Colloidal Forces Using an Atomic Force Microscope. Nature 1991, 353, 239–241..

    Not in our library10.1038/353239a0

  1021. 1021.

    Farooq M.; Zou T.; Riviere G.; Sipponen M. H.; Osterberg M. Strong, Ductile, and Waterproof Cellulose Nanofibril Composite Films with Colloidal Lignin Particles. Biomacromolecules 2019, 20, 693–704..

    Not in our library10.1021/acs.biomac.8b01364

  1022. 1022.

    Huhtamäki T.; Tian X.; Korhonen J. T.; Ras R. H. Surface-Wetting Characterization Using Contact-Angle Measurements. Nat. Protoc. 2018, 13, 1521–1538..

    Not in our library10.1038/s41596-018-0003-z

  1023. 1023.

    Emelyanenko A.; Ermolenko N.; Boinovich L. Contact Angle and Wetting Hysteresis Measurements by Digital Image Processing of the Drop on a Vertical Filament. Colloids Surf., A 2004, 239, 25–31..

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    Tretinnikov O. N.; Ikada Y. Dynamic Wetting and Contact Angle Hysteresis of Polymer Surfaces Studied with the Modified Wilhelmy Balance Method. Langmuir 1994, 10, 1606–1614..

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  1025. 1025.

    Barber A. H.; Cohen S. R.; Wagner H. D. Static and Dynamic Wetting Measurements of Single Carbon Nanotubes. Phys. Rev. Lett. 2004, 92, 186103.

    Not in our library10.1103/physrevlett.92.186103

  1026. 1026.

    Eral H. B.; ’t Mannetje D. J. C. M.; Oh J. M. Contact Angle Hysteresis: A Review of Fundamentals and Applications. Colloid Polym. Sci. 2013, 291, 247–260..

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  1027. 1027.

    Atefi E.; Mann J. A. Jr; Tavana H. A Robust Polynomial Fitting Approach for Contact Angle Measurements. Langmuir 2013, 29, 5677–5688..

    Not in our library10.1021/la4002972

  1028. 1028.

    Stalder A. F.; Melchior T.; Müller M.; Sage D.; Blu T.; Unser M. Low-Bond Axisymmetric Drop Shape Analysis for Surface Tension and Contact Angle Measurements of Sessile Drops. Colloids Surf., A 2010, 364, 72–81..

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  1029. 1029.

    Marmur A. A Guide to the Equilibrium Contact Angles Maze. In Contact Angle Wettability and Adhesion; Mittal K. L., Ed.; CRC Press: London, 2009; Vol. 6, Chapter 1.

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  1030. 1030.

    Karim Z.; Hakalahti M.; Tammelin T.; Mathew A. P. In Situ Tempo Surface Functionalization of Nanocellulose Membranes for Enhanced Adsorption of Metal Ions from Aqueous Medium. RSC Adv. 2017, 7, 5232–5241..

    Not in our library10.1039/c6ra25707k

  1031. 1031.

    De Gennes P.-G. Wetting: Statics and Dynamics. Rev. Mod. Phys. 1985, 57, 827.

    Not in our library10.1103/revmodphys.57.827

  1032. 1032.

    Dankovich T. A.; Gray D. G. Contact Angle Measurements on Smooth Nanocrystalline Cellulose (I) Thin Films. J. Adhes. Sci. Technol. 2011, 25, 699–708..

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    Kontturi K. S.; Holappa S.; Kontturi E.; Johansson L.-S.; Hyvärinen S.; Peltonen S.; Laine J. Arrangements of Cationic Starch of Varying Hydrophobicity on Hydrophilic and Hydrophobic Surfaces. J. Colloid Interface Sci. 2009, 336, 21–29..

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  1034. 1034.

    Hejda F.; Solar P.; Kousal J. Surface Free Energy Determination by Contact Angle Measurements–A Comparison of Various Approaches. In 19th Annual Conference of Doctoral Students, WDS’10 “Week of Doctoral Students 2010", June 1–4, 2010, Prague, Czech Republic; Matfyzpress: Praha, 2010.

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    Fowkes F. M. Attractive Forces at Interfaces. Ind. Eng. Chem. 1964, 56, 40–52..

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    Blake T. D. The Physics of Moving Wetting Lines. J. Colloid Interface Sci. 2006, 299, 1–13..

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  1037. 1037.

    Peršin Z.; Stana-Kleinschek K.; Sfiligoj-Smole M.; Kre T.; Ribitsch V. Determining the Surface Free Energy of Cellulose Materials with the Powder Contact Angle Method. Text. Res. J. 2004, 74, 55–62..

    Not in our library10.1177/004051750407400110

  1038. 1038.

    Dang-Vu T.; Hupka J. Characterization of Porous Materials by Capillary Rise Method. Physicochem. Probl. Miner. Process. 2005, 39, 47–65.

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    Van Oss C.; Giese R.; Li Z.; Murphy K.; Norris J.; Chaudhury M.; Good R. Determination of Contact Angles and Pore Sizes of Porous Media by Column and Thin Layer Wicking. J. Adhes. Sci. Technol. 1992, 6, 413–428..

    Not in our library10.1163/156856192x00755

  1040. 1040.

    Holysz L.; Chibowski E. Surface Free Energy Components Of. Alpha.-Alumina from Thin-Layer Wicking. Langmuir 1992, 8, 717–721..

    Not in our library10.1021/la00038a067

  1041. 1041.

    Hołysz L. Investigation of the Effect of Substrata on the Surface Free Energy Components of Silica Gel Determined by Thin Layer Wicking Method. J. Mater. Sci. 2000, 35, 6081–6091..

    Not in our library10.1023/a:1026779816279

  1042. 1042.

    Simončič B.; Černe L.; Tomšič B.; Orel B. Surface Properties of Cellulose Modified by Imidazolidinone. Cellulose 2008, 15, 47–58..

    Not in our library10.1007/s10570-007-9151-y

  1043. 1043.

    Kontturi E.; Meriluoto A.; Penttilä P. A.; Baccile N.; Malho J. M.; Potthast A.; Rosenau T.; Ruokolainen J.; Serimaa R.; Laine J.; Sixta H. Degradation and Crystallization of Cellulose in Hydrogen Chloride Vapor for High-Yield Isolation of Cellulose Nanocrystals. Angew. Chem., Int. Ed. 2016, 55, 14455–14458..

    Not in our library10.1002/anie.201606626

  1044. 1044.

    Schreiber H. P.; Lloyd D. R. Overview of Inverse Gas Chromatography. ACS Symp. Ser. 1989, 391, 1–10..

    Not in our library10.1021/bk-1989-0391.ch001

  1045. 1045.

    Mohammadi-Jam S.; Waters K. Inverse Gas Chromatography Applications: A Review. Adv. Colloid Interface Sci. 2014, 212, 21–44..

    Not in our library10.1016/j.cis.2014.07.002

  1046. 1046.

    Thielmann F. Introduction into the Characterisation of Porous Materials by Inverse Gas Chromatography. J. Chromatogr. A 2004, 1037, 115–123..

    Not in our library10.1016/j.chroma.2004.03.060

  1047. 1047.

    Wålinder M. E.; Gardner D. J. Surface Energy of Extracted and Non-Extracted Norway Spruce Wood Particles Studied by Inverse Gas Chromatography (IGC). Wood Fiber Sci. 2007, 32, 478–488.

    Not in our library

  1048. 1048.

    Gamelas J. A. The Surface Properties of Cellulose and Lignocellulosic Materials Assessed by Inverse Gas Chromatography: A Review. Cellulose 2013, 20, 2675–2693..

    Not in our library10.1007/s10570-013-0066-5

  1049. 1049.

    Jacob P. N.; Berg J. C. Acid-Base Surface Energy Characterization of Microcrystalline Cellulose and Two Wood Pulp Fiber Types Using Inverse Gas Chromatography. Langmuir 1994, 10, 3086–3093..

    Not in our library10.1021/la00021a036

  1050. 1050.

    Planinšek O.; Buckton G. Inverse Gas Chromatography: Considerations About Appropriate Use for Amorphous and Crystalline Powders. J. Pharm. Sci. 2003, 92, 1286–1294..

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  1051. 1051.

    Osterberg M.; Vartiainen J.; Lucenius J.; Hippi U.; Seppala J.; Serimaa R.; Laine J. A Fast Method to Produce Strong Nfc Films as a Platform for Barrier and Functional Materials. ACS Appl. Mater. Interfaces 2013, 5, 4640–4647..

    Not in our library10.1021/am401046x

  1052. 1052.

    ASTM Standard Test Method for Water Vapor Transmission of Materials; ASTM E96-95; ASTM, 1995.

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  1053. 1053.

    Gennadios A.; Weller C. L.; Gooding C. H. Measurement Errors in Water Vapor Permeability of Highly Permeable, Hydrophilic Edible Films. J. Food Eng. 1994, 21, 395–410..

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  1054. 1054.

    Hu Y.; Topolkaraev V.; Hiltner A.; Baer E. Measurement of Water Vapor Transmission Rate in Highly Permeable Films. J. Appl. Polym. Sci. 2001, 81, 1624–1633..

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  1055. 1055.

    Spence K. L.; Venditti R. A.; Rojas O. J.; Habibi Y.; Pawlak J. J. The Effect of Chemical Composition on Microfibrillar Cellulose Films from Wood Pulps: Water Interactions and Physical Properties for Packaging Applications. Cellulose 2010, 17, 835–848..

    Not in our library10.1007/s10570-010-9424-8

  1056. 1056.

    Saxena A.; Ragauskas A. J. Water Transmission Barrier Properties of Biodegradable Films Based on Cellulosic Whiskers and Xylan. Carbohydr. Polym. 2009, 78, 357–360..

    Not in our library10.1016/j.carbpol.2009.03.039

  1057. 1057.

    Song Z.; Xiao H.; Zhao Y. Hydrophobic-Modified Nano-Cellulose Fiber/Pla Biodegradable Composites for Lowering Water Vapor Transmission Rate (Wvtr) of Paper. Carbohydr. Polym. 2014, 111, 442–448..

    Not in our library10.1016/j.carbpol.2014.04.049

  1058. 1058.

    Sehaqui H.; Liu A.; Zhou Q.; Berglund L. A. Fast Preparation Procedure for Large, Flat Cellulose and Cellulose/Inorganic Nanopaper Structures. Biomacromolecules 2010, 11, 2195–2198..

    Not in our library10.1021/bm100490s

  1059. 1059.

    Sethi J.; Visanko M.; Österberg M.; Sirviö J. A. A Fast Method to Prepare Mechanically Strong and Water Resistant Lignocellulosic Nanopapers. Carbohydr. Polym. 2019, 203, 148–156..

    Not in our library10.1016/j.carbpol.2018.09.037

  1060. 1060.

    Hakalahti M.; Mautner A.; Johansson L. S.; Hanninen T.; Setala H.; Kontturi E.; Bismarck A.; Tammelin T. Direct Interfacial Modification of Nanocellulose Films for Thermoresponsive Membrane Templates. ACS Appl. Mater. Interfaces 2016, 8, 2923–2927..

    Not in our library10.1021/acsami.5b12300

  1061. 1061.

    Hjärtstam J.; Hjertberg T. Studies of the Water Permeability and Mechanical Properties of a Film Made of an Ethyl Cellulose–Ethanol–Water Ternary Mixture. J. Appl. Polym. Sci. 1999, 74, 2056–2062..

    Not in our library10.1002/(sici)1097-4628(19991121)74:8<2056::aid-app21>3.0.co;2-y

  1062. 1062.

    Canadian Standard Method, Freeness of Pulp; T 227 om-17, 2017.

    Not in our library

  1063. 1063.

    Chemical Pulp: Water Retention Values; Scan-C 62:00; Scandinavian Pulp, Paper and Board Testing Committee: Stockholm, 2000.

    Not in our library

  1064. 1064.

    TAPPI Water Absorptiveness of Sized (Non-Bibulous) Paper, Paperboard, and Corrugated Fiberboard (Cobb Test); T 441 om-20; TAPPI, 2020.

    Not in our library

  1065. 1065.

    Driemeier C.; Mendes F. M.; Oliveira M. M. Dynamic Vapor Sorption and Thermoporometry to Probe Water in Celluloses. Cellulose 2012, 19, 1051–1063..

    Not in our library10.1007/s10570-012-9727-z

  1066. 1066.

    Hill C. A. S.; Norton A.; Newman G. The Water Vapor Sorption Behavior of Natural Fibers. J. Appl. Polym. Sci. 2009, 112, 1524–1537..

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  1067. 1067.

    Garg M.; Apostolopoulou-Kalkavoura V.; Linares M.; Kaldéus T.; Malmström E.; Bergström L.; Zozoulenko I. Moisture Uptake in Nanocellulose: The Effects of Relative Humidity, Temperature and Degree of Crystallinity. Cellulose 2021, 28, 9007–9021..

    Not in our library10.1007/s10570-021-04099-9

  1068. 1068.

    Lahtinen P.; Liukkonen S.; Pere J.; Sneck A.; Kangas H. A Comparative Study of Fibrillated Fibers from Different Mechanical and Chemical Pulps. BioResources 2014, 9, 2115–2127.

    Not in our library

  1069. 1069.

    Hanhikoski S.; Solala I.; Lahtinen P.; Niemelä K.; Vuorinen T. Fibrillation and Characterization of Lignin-Containing Neutral Sulphite (NS) Pulps Rich in Hemicelluloses and Anionic Charge. Cellulose 2020, 27, 7203–7214..

    Not in our library10.1007/s10570-020-03237-z

  1070. 1070.

    Herrick F. W.; Casebier R. L.; Hamilton J. K.; Sandberg K. R. Microfibrillated Cellulose: Morphology and Accessibility. J. Appl. Polym. Sci.: Appl. Polym. Symp. 1983, 37, 797–813.

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  1071. 1071.

    Ferrer A.; Quintana E.; Filpponen I.; Solala I.; Vidal T.; Rodríguez A.; Laine J.; Rojas O. J. Effect of Residual Lignin and Heteropolysaccharides in Nanofibrillar Cellulose and Nanopaper from Wood Fibers. Cellulose 2012, 19, 2179–2193..

    Not in our library10.1007/s10570-012-9788-z

  1072. 1072.

    Ceccon Claro F.; Jordão C.; Massa de Viveiros B.; Egio Isaka L. J.; Villanova J. A. Jr.; Estaves Magalhães W. L. Low Cost Membrane of Wood Nanocellulose Obtained by Mechanical Defibrillation for Potential Applications as Wound Dressing. Cellulose 2020, 27, 10765–10779..

    Not in our library10.1007/s10570-020-03129-2

  1073. 1073.

    Gu F.; Wang W.; Cai Z.; Xue F.; Jin Y.; Zhu J. Water Retention Value for Characterizing Fibrillation Degree of Cellulosic Fibers at Micro and Nanometer Scales. Cellulose 2018, 25, 2861–2871..

    Not in our library10.1007/s10570-018-1765-8

  1074. 1074.

    Maloney T. C. Network Swelling of Tempo-Oxidized Nanocellulose. Holzforschung 2015, 69, 207–213..

    Not in our library10.1515/hf-2014-0013

  1075. 1075.

    Schrecker S.; Gostomski P. Determining the Water Holding Capacity of Microbial Cellulose. Biotechnol. Lett. 2005, 27, 1435–1438..

    Not in our library10.1007/s10529-005-1465-y

  1076. 1076.

    Rautkari L.; Hill C. A.; Curling S.; Jalaludin Z.; Ormondroyd G. What Is the Role of the Accessibility of Wood Hydroxyl Groups in Controlling Moisture Content?. J. Mater. Sci. 2013, 48, 6352–6356..

    Not in our library10.1007/s10853-013-7434-2

  1077. 1077.

    Lundahl M. J.; Cunha A. G.; Rojo E.; Papageorgiou A. C.; Rautkari L.; Arboleda J. C.; Rojas O. J. Strength and Water Interactions of Cellulose I Filaments Wet-Spun from Cellulose Nanofibril Hydrogels. Sci. Rep. 2016, 6, 30695.

    Not in our library10.1038/srep30695

  1078. 1078.

    Pönni R.; Rautkari L.; Hill C. A. S.; Vuorinen T. Accessibility of Hydroxyl Groups in Birch Kraft Pulps Quantified by Deuterium Exchange in D2O Vapor. Cellulose 2014, 21, 1217–1226..

    Not in our library10.1007/s10570-014-0166-x

  1079. 1079.

    Thommes M.; Kaneko K.; Neimark A. V.; Olivier J. P.; Rodriguez-Reinoso F.; Rouquerol J.; Sing K. S. Physisorption of Gases, with Special Reference to the Evaluation of Surface Area and Pore Size Distribution (IUPAC Technical Report). Pure Appl. Chem. 2015, 87, 1051–1069..

    Not in our library10.1515/pac-2014-1117

  1080. 1080.

    Foster E. J.; Moon R. J.; Agarwal U. P.; Bortner M. J.; Bras J.; Camarero-Espinosa S.; Chan K. J.; Clift M. J. D.; Cranston E. D.; Eichhorn S. J.; et al. Current Characterization Methods for Cellulose Nanomaterials. Chem. Soc. Rev. 2018, 47, 2609–2679..

    Not in our library10.1039/c6cs00895j

  1081. 1081.

    Eyholzer C.; Bordeanu N.; Lopez-Suevos F.; Rentsch D.; Zimmermann T.; Oksman K. Preparation and Characterization of Water-Redispersible Nanofibrillated Cellulose in Powder Form. Cellulose 2010, 17, 19–30..

    Not in our library10.1007/s10570-009-9372-3

  1082. 1082.

    Hietala M.; Sain S.; Oksman K. Highly Redispersible Sugar Beet Nanofibers as Reinforcement in Bionanocomposites. Cellulose 2017, 24, 2177–2189..

    Not in our library10.1007/s10570-017-1245-6

  1083. 1083.

    Posada P.; Velásquez-Cock J.; Gómez-Hoyos C.; Serpa Guerra A.; Lyulin S.; Kenny J.; Gañán P.; Castro C.; Zuluaga R. Drying and Redispersion of Plant Cellulose Nanofibers for Industrial Applications: A Review. Cellulose 2020, 27, 10649–10670..

    Not in our library10.1007/s10570-020-03348-7

  1084. 1084.

    Rodahl M.; Höök F.; Krozer A.; Brzezinski P.; Kasemo B. Quartz Crystal Microbalance Setup for Frequency and Q-Factor Measurements in Gaseous and Liquid Environments. Rev. Sci. Instrum. 1995, 66, 3924–3930..

    Not in our library10.1063/1.1145396

  1085. 1085.

    Kontturi K. S.; Tammelin T.; Johansson L.-S.; Stenius P. Adsorption of Cationic Starch on Cellulose Studied by Qcm-D. Langmuir 2008, 24, 4743–4749..

    Not in our library10.1021/la703604j

  1086. 1086.

    Sauerbrey G. The Use of Quarts Oscillators for Weighing Thin Layers and for Microweighing. Z. Phys. 1959, 155, 206–222..

    Not in our library10.1007/bf01337937

  1087. 1087.

    Höök F.; Rodahl M.; Brzezinski P.; Kasemo B. Energy Dissipation Kinetics for Protein and Antibody– Antigen Adsorption under Shear Oscillation on a Quartz Crystal Microbalance. Langmuir 1998, 14, 729–734..

    Not in our library10.1021/la970815u

  1088. 1088.

    Fält S.; Wågberg L.; Vesterlind E.-L. Swelling of Model Films of Cellulose Having Different Charge Densities and Comparison to the Swelling Behavior of Corresponding Fibers. Langmuir 2003, 19, 7895–7903..

    Not in our library10.1021/la026984i

  1089. 1089.

    Hakalahti M.; Faustini M.; Boissiere C.; Kontturi E.; Tammelin T. Interfacial Mechanisms of Water Vapor Sorption into Cellulose Nanofibril Films as Revealed by Quantitative Models. Biomacromolecules 2017, 18, 2951–2958..

    Not in our library10.1021/acs.biomac.7b00890

  1090. 1090.

    Kontturi E.; Thüne P. C.; Niemantsverdriet J. Cellulose Model Surfaces Simplified Preparation by Spin Coating and Characterization by X-Ray Photoelectron Spectroscopy, Infrared Spectroscopy, and Atomic Force Microscopy. Langmuir 2003, 19, 5735–5741..

    Not in our library10.1021/la0340394

  1091. 1091.

    Gunnars S.; Wågberg L.; Cohen Stuart M. A. Model Films of Cellulose: I. Method Development and Initial Results. Cellulose 2002, 9, 239–249..

    Not in our library10.1023/a:1021196914398

  1092. 1092.

    Holmberg M.; Berg J.; Stemme S.; Ödberg L.; Rasmusson J.; Claesson P. Surface Force Studies of Langmuir–Blodgett Cellulose Films. J. Colloid Interface Sci. 1997, 186, 369–381..

    Not in our library10.1006/jcis.1996.4657

  1093. 1093.

    Rehfeldt F.; Tanaka M. Hydration Forces in Ultrathin Films of Cellulose. Langmuir 2003, 19, 1467–1473..

    Not in our library10.1021/la0261702

  1094. 1094.

    Delepierre G.; Vanderfleet O. M.; Niinivaara E.; Zakani B.; Cranston E. D. Benchmarking Cellulose Nanocrystals Part Ii: New Industrially Produced Materials. Langmuir 2021, 37, 8393–8409..

    Not in our library10.1021/acs.langmuir.1c00550

  1095. 1095.

    Foston M. Advances in Solid-State Nmr of Cellulose. Curr. Opin. Biotechnol. 2014, 27, 176–184..

    Not in our library10.1016/j.copbio.2014.02.002

  1096. 1096.

    Newman R. H.; Hemmingson J. A. Carbon-13 Nmr Distinction between Categories of Molecular Order and Disorder in Cellulose. Cellulose 1995, 2, 95–110..

    Not in our library10.1007/bf00816383

  1097. 1097.

    Park S.; Johnson D. K.; Ishizawa C. I.; Parilla P. A.; Davis M. F. Measuring the Crystallinity Index of Cellulose by Solid State 13 C Nuclear Magnetic Resonance. Cellulose 2009, 16, 641–647..

    Not in our library10.1007/s10570-009-9321-1

  1098. 1098.

    Hult E.-L.; Larsson P.; Iversen T. Cellulose Fibril Aggregation—an Inherent Property of Kraft Pulps. Polymer 2001, 42, 3309–3314..

    Not in our library10.1016/s0032-3861(00)00774-6

  1099. 1099.

    Wormald P.; Wickholm K.; Larsson P. T.; Iversen T. Conversions between Ordered and Disordered Cellulose. Effects of Mechanical Treatment Followed by Cyclic Wetting and Drying. Cellulose 1996, 3, 141–152..

    Not in our library10.1007/bf02228797

  1100. 1100.

    Vittadini E.; Dickinson L.; Chinachoti P. 1h and 2h Nmr Mobility in Cellulose. Carbohydr. Polym. 2001, 46, 49–57..

    Not in our library10.1016/s0144-8617(00)00282-4

  1101. 1101.

    Li T. Q.; Henriksson U.; Eriksson J. C.; Oedberg L. Water-Cellulose Interaction in Wood Pulp Fiber Suspensions Studied by Oxygen-17 and Deuterium Nmr Relaxation. The Effect of Beating. Langmuir 1992, 8, 680–686..

    Not in our library10.1021/la00038a063

  1102. 1102.

    Radloff D.; Boeffel C.; Spiess H. W. Cellulose and Cellulose/Poly (Vinyl Alcohol) Blends. 2. Water Organization Revealed by Solid-State NMR Spectroscopy. Macromolecules 1996, 29, 1528–1534..

    Not in our library10.1021/ma950405h

  1103. 1103.

    Lindh E. L. Cellulose–Water Interaction: A Spectroscopic Study. Ph.D. Thesis. KTH Royal Institute of Technology, 2016.

    Not in our library

  1104. 1104.

    Einfeldt J.; Meißner D.; Kwasniewski A. Polymerdynamics of Cellulose and Other Polysaccharides in Solid State-Secondary Dielectric Relaxation Processes. Prog. Polym. Sci. 2001, 26, 1419–1472..

    Not in our library10.1016/s0079-6700(01)00020-x

  1105. 1105.

    Schmidt-Rohr K.; Clauss J.; Spiess H. Correlation of Structure, Mobility, and Morphological Information in Heterogeneous Polymer Materials by Two-Dimensional Wideline-Separation NMR Spectroscopy. Macromolecules 1992, 25, 3273–3277..

    Not in our library10.1021/ma00038a037

  1106. 1106.

    Froix M. F.; Nelson R. The Interaction of Water with Cellulose from Nuclear Magnetic Resonance Relaxation Times. Macromolecules 1975, 8, 726–730..

    Not in our library10.1021/ma60048a011

  1107. 1107.

    Froix M. F.; Goedde A. O. The Effect of Temperature on the Cellulose/Water Interaction from NMR Relaxation Times. Macromolecules 1976, 9, 428–430..

    Not in our library10.1021/ma60051a009

  1108. 1108.

    Terenzi C.; Prakobna K.; Berglund L. A.; Furó I. Nanostructural Effects on Polymer and Water Dynamics in Cellulose Biocomposites: 2H and 13C NMR Relaxometry. Biomacromolecules 2015, 16, 1506–1515..

    Not in our library10.1021/acs.biomac.5b00330

  1109. 1109.

    Felby C.; Thygesen L. G.; Kristensen J. B.; Jørgensen H.; Elder T. Cellulose–Water Interactions During Enzymatic Hydrolysis as Studied by Time Domain NMR. Cellulose 2008, 15, 703–710..

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    Fengel D. Influence of Water on the OH Valency Range in Deconvoluted FTIR Spectra of Cellulose. Holzforschung 1993, 47, 103–108..

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    Guo X.; Liu L.; Wu J.; Fan J.; Wu Y. Qualitatively and Quantitatively Characterizing Water Adsorption of a Cellulose Nanofiber Film Using Micro-FTIR Spectroscopy. RSC Adv. 2018, 8, 4214–4220..

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    Pereda M.; Amica G.; Rácz I.; Marcovich N. E. Structure and Properties of Nanocomposite Films Based on Sodium Caseinate and Nanocellulose Fibers. J. Food Eng. 2011, 103, 76–83..

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    Jayaramudu J.; Reddy D. J. P.; Guduri B.; Rajulu A. V. Properties of Natural Fabric Polyalthia Cerasoides. Fibers Polym. 2009, 10, 338–342..

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    Abraham E.; Deepa B.; Pothan L.; Jacob M.; Thomas S.; Cvelbar U.; Anandjiwala R. Extraction of Nanocellulose Fibrils from Lignocellulosic Fibres: A Novel Approach. Carbohydr. Polym. 2011, 86, 1468–1475..

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    Lee C. M.; Kubicki J. D.; Fan B.; Zhong L.; Jarvis M. C.; Kim S. H. Hydrogen-Bonding Network and OH Stretch Vibration of Cellulose: Comparison of Computational Modeling with Polarized IR and SFG Spectra. J. Phys. Chem. B 2015, 119, 15138–15149..

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    Horikawa Y.; Sugiyama J. Accessibility and Size of Valonia Cellulose Microfibril Studied by Combined Deuteration/Rehydrogenation and FTIR Technique. Cellulose 2008, 15, 419–424..

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    Jafarpour G.; Roig F.; Dantras E.; Boudet A.; Lacabanne C. Influence of Water on Localized and Delocalized Molecular Mobility of Cellulose. J. Non-Cryst. Solids 2009, 355, 1669–1672..

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    Crofton D. J.; Pethrick R. A. Dielectric Studies of Proton Migration and Relaxation in Wet Cellulose and Its Derivatives. Polymer 1981, 22, 1048–1053..

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    Ek R.; Hill R.; Newton J. Low Frequency Dielectric Spectroscopy Characterization of Microcrystalline Cellulose, Tablets and Paper. J. Mater. Sci. 1997, 32, 4807–4814..

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    Bain C. D. Sum-Frequency Vibrational Spectroscopy of the Solid/Liquid Interface. J. Chem. Soc., Faraday Trans. 1995, 91, 1281–1296..

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    Tyrode E.; Rutland M. W.; Bain C. D. Adsorption of Ctab on Hydrophilic Silica Studied by Linear and Nonlinear Optical Spectroscopy. J. Am. Chem. Soc. 2008, 130, 17434–17445..

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    Kontturi E.; Thüne P.; Niemantsverdriet J. Novel Method for Preparing Cellulose Model Surfaces by Spin Coating. Polymer 2003, 44, 3621–3625..

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    Eriksson J.; Malmsten M.; Tiberg F.; Callisen T. H.; Damhus T.; Johansen K. S. Enzymatic Degradation of Model Cellulose Films. J. Colloid Interface Sci. 2005, 284, 99–106..

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    Ogieglo W.; Wormeester H.; Eichhorn K.-J.; Wessling M.; Benes N. E. In Situ Ellipsometry Studies on Swelling of Thin Polymer Films: A Review. Prog. Polym. Sci. 2015, 42, 42–78..

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    Popov K.; Tikhonravov A.; Campmany J.; Bertran E.; Bosch S.; Canillas A. Spectroscopic Ellipsometric Characterization of Transparent Thin Film Amorphous Electronic Materials: Integrated Analysis. Thin Solid Films 1998, 313, 379–383..

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    Flesch H. G.; Werzer O.; Weis M.; Jakabovič J.; Kováč J.; Haško D.; Jakopič G.; Wondergem H. J.; Resel R. A Combined X-Ray, Ellipsometry and Atomic Force Microscopy Study on Thin Parylene-C Films. Phys. Status Solidi A 2009, 206, 1727–1730..

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    Kontturi E.; Tammelin T.; Österberg M. Cellulose—Model Films and the Fundamental Approach. Chem. Soc. Rev. 2006, 35, 1287–1304..

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    Liedberg B.; Nylander C.; Lundström I. Biosensing with Surface Plasmon Resonance—How It All Started. Biosens. Bioelectron. 1995, 10, i–ix..

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    Geddes N.; Martin A.; Caruso F.; Urquhart R.; Furlong D.; Sambles J.; Than K.; Edgar J. Immobilisation of Igg onto Gold Surfaces and Its Interaction with Anti-Igg Studied by Surface Plasmon Resonance. J. Immunol. Methods 1994, 175, 149–160..

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    Cranston E. D.; Gray D. G. Morphological and Optical Characterization of Polyelectrolyte Multilayers Incorporating Nanocrystalline Cellulose. Biomacromolecules 2006, 7, 2522–2530..

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    Ahola S.; Myllytie P.; Österberg M.; Teerinen T.; Laine J. Effect of Polymer Adsorption on Cellulose Nanofibril Water Binding Capacity and Aggregation. BioResources 2008, 3, 1315–1328.

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    Eronen P.; Junka K.; Laine J.; Österberg M. Interaction between Water Soluble Polysaccharides and Native Nanofibrillar Cellulose Thin Films. BioResources 2011, 6, 4200–4217..

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    Nelson R. A. The Determination of Moisture Transitions in Cellulosic Materials Using Differential Scanning Calorimetry. J. Appl. Polym. Sci. 1977, 21, 645–654..

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    Talik P.; Hubicka U. The DSC Approach to Study Non-Freezing Water Contents of Hydrated Hydroxypropylcellulose (HPC). J. Therm. Anal. Calorim. 2018, 132, 445–451..

    Not in our library10.1007/s10973-017-6889-9

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    Brett C. J.; Mittal N.; Ohm W.; Gensch M.; Kreuzer L. P.; Körstgens V.; Månsson M.; Frielinghaus H.; Müller-Buschbaum P.; Söderberg L. D.; Roth S. V. Water-Induced Structural Rearrangements on the Nanoscale in Ultrathin Nanocellulose Films. Macromolecules 2019, 52, 4721–4728..

    Not in our library10.1021/acs.macromol.9b00531

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    Liu W. G.; Yao K. D. What Causes the Unfrozen Water in Polymers: Hydrogen Bonds between Water and Polymer Chains?. Polymer 2001, 42, 3943–3947..

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    Nechyporchuk O.; Belgacem M. N.; Pignon F. d. r. Current Progress in Rheology of Cellulose Nanofibril Suspensions. Biomacromolecules 2016, 17, 2311–2320..

    Not in our library10.1021/acs.biomac.6b00668

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    Schütz C.; Van Rie J.; Eyley S.; Gençer A.; van Gorp H.; Rosenfeldt S.; Kang K.; Thielemans W. Effect of Source on the Properties and Behavior of Cellulose Nanocrystal Suspensions. ACS Sustainable Chem. Eng. 2018, 6, 8317–8324..

    Not in our library10.1021/acssuschemeng.8b00334

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    Tanaka R.; Kuribayashi T.; Ogawa Y.; Saito T.; Isogai A.; Nishiyama Y. Ensemble Evaluation of Polydisperse Nanocellulose Dimensions: Rheology, Electron Microscopy, X-Ray Scattering and Turbidimetry. Cellulose 2017, 24, 3231–3242..

    Not in our library10.1007/s10570-017-1334-6

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    Mao Y.; Liu K.; Zhan C.; Geng L.; Chu B.; Hsiao B. S. Characterization of Nanocellulose Using Small-Angle Neutron, X-Ray, and Dynamic Light Scattering Techniques. J. Phys. Chem. B 2017, 121, 1340–1351..

    Not in our library10.1021/acs.jpcb.6b11425

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    De France K. J.; Yager K. G.; Hoare T.; Cranston E. D. Cooperative Ordering and Kinetics of Cellulose Nanocrystal Alignment in a Magnetic Field. Langmuir 2016, 32, 7564–7571..

    Not in our library10.1021/acs.langmuir.6b01827

  1147. 1147.

    Rosén T.; Wang R.; Zhan C.; He H.; Chodankar S.; Hsiao B. S. Cellulose Nanofibrils and Nanocrystals in Confined Flow: Single-Particle Dynamics to Collective Alignment Revealed through Scanning Small-Angle X-Ray Scattering and Numerical Simulations. Phys. Rev. E 2020, 101, 032610.

    Not in our library10.1103/physreve.101.032610

  1148. 1148.

    Mittal N.; Ansari F.; Gowda V K.; Brouzet C.; Chen P.; Larsson P. T.; Roth S. V.; Lundell F.; Wagberg L.; Kotov N. A.; Söderberg L. D. Multiscale Control of Nanocellulose Assembly: Transferring Remarkable Nanoscale Fibril Mechanics to Macroscale Fibers. ACS Nano 2018, 12, 6378–6388..

    Not in our library10.1021/acsnano.8b01084

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    Liu Y.; Agthe M.; Salajková M.; Gordeyeva K.; Guccini V.; Fall A.; Salazar-Alvarez G.; Schütz C.; Bergström L. Assembly of Cellulose Nanocrystals in a Levitating Drop Probed by Time-Resolved Small Angle X-Ray Scattering. Nanoscale 2018, 10, 18113–18118..

    Not in our library10.1039/c8nr05598j

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    Uhlig M.; Fall A.; Wellert S.; Lehmann M.; Prévost S.; Wågberg L.; von Klitzing R.; Nyström G. Two-Dimensional Aggregation and Semidilute Ordering in Cellulose Nanocrystals. Langmuir 2016, 32, 442–450..

    Not in our library10.1021/acs.langmuir.5b04008

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    Valencia L.; Kumar S.; Jalvo B.; Mautner A.; Salazar-Alvarez G.; Mathew A. P. Fully Bio-Based Zwitterionic Membranes with Superior Antifouling and Antibacterial Properties Prepared Via Surface-Initiated Free-Radical Polymerization of Poly (Cysteine Methacrylate). J. Mater. Chem. A 2018, 6, 16361–16370..

    Not in our library10.1039/c8ta06095a

  1152. 1152.

    Berrod Q.; Lagrené K.; Ollivier J.; Zanotti J.-M. Inelastic and Quasi-Elastic Neutron Scattering. Application to Soft Matter. In JDN 23—French–Swedish Winterschool on Neutron Scattering: Applications to Soft Matter, December 6-9, 2016, Uppsala, Sweden; EPJ, Web of Conferences, 188, 05001; EDP Sciences, 2018; Vol. 188.

    Not in our library

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    Guccini V.; Yu S.; Meng Z.; Kontturi E.; Demmel F.; Salazar-Alvarez G. The Impact of Surface Charges of Carboxylated Cellulose Nanofibrils on the Water Motions in Hydrated Films. Biomacromolecules 2022, 23, 3104–3115..

    Not in our library10.1021/acs.biomac.1c01517

  1154. 1154.

    Lei L.; Li S.; Gu Y. Cellulose Synthase Complexes: Composition and Regulation. Front. Plant Sci. 2012, 3, 75.

    Not in our library10.3389/fpls.2012.00075

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