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Dried Blood Spots for Global Health Diagnostics and Surveillance: Opportunities and Challenges

Mark D. Lim

The American Journal of Tropical Medicine and Hygiene · 2018 · Review

doi:10.4269/ajtmh.17-0889

Abstract

There is increasing interest in using dried blood spot (DBS) cards to extend the reach of global health and disease surveillance programs to hard-to-reach populations. Conceptually, DBS offers a cost-effective solution for multiple use cases by simplifying logistics for collecting, preserving, and transporting blood specimens in settings with minimal infrastructure. This review describes methods to determine both the reliability of DBS-based bioanalysis for a defined use case and the optimal conditions that minimize pre-analytical sources of data variability. Examples by the newborn screening, drug development, and global health communities are provided in this review of published literature. Sources of variability are linked in most cases, emphasizing the importance of field-to-laboratory standard operating procedures that are evidence based and consider both stability and efficiency of recovery for a specified analyte in defining the type of DBS card, accessories, handling procedures, and storage conditions. Also included in this review are reports where DBS was determined to not be feasible because of technology limitations or physiological properties of a targeted analyte.

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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

Most diagnostics and surveillance programs rely on measurements from an individual’s blood specimen to guide a clinical or public health decision. To minimize pre-analytical sources of data variability, processes for venipuncture collection are standardized through devices such as analyte-specific blood collection tubes and evidence-based best practices, guidelines, and protocols., Global health settings often lack infrastructure for quality-assured venipuncture, sparking significant interest in the use of dried blood spot (DBS) cards as a universal solution.– The intent of this review is to underscore the need to assess the reliability of DBS-based bioanalysis in context to a specific biomarker and envisioned field-to-laboratory workflow, before applying this technology into a remote health or surveillance program.

Compared with venipuncture, the value proposition of DBS is simplified logistics for remote sampling through:Reduced workforce requirementsSmaller volumes of blood and components (plasma and serum)Direct heelprick/fingerprick-to-DBS or indirect capillary-to-DBS deposition of bloodCollection of nonblood biofluids such as salivaSimplified transport, shipment, and disposalSimplified biobanking for retrospective analysis

Reduced workforce requirements

Smaller volumes of blood and components (plasma and serum)

Direct heelprick/fingerprick-to-DBS or indirect capillary-to-DBS deposition of blood

Collection of nonblood biofluids such as saliva

Simplified transport, shipment, and disposal

Simplified biobanking for retrospective analysis

Commercially available DBS cards are not designed for the minimally resourced environments typical of remote health settings and instead are primarily used in newborn screening and preclinical drug development by highly proficient personnel within controlled clinical and laboratory environments. For instance, most DBS are susceptible to contamination by the user, patient, environment, insects, equipment, or contact with other cards. Health-care workers also have a risk of exposure to potentially infectious agents until blood is dried and contained in secure packaging. Most of these risks can be mitigated through standard operating procedures and accessories, but the impact of these variables on data quality needs to be assessed through careful studies simulating the pre-analytical workflow, starting with specimen acquisition to DBS preparation for analysis. Readers are advised to review the comprehensive review of mass spectrometry (MS) methods and the collection of reports compiled by Li and Lee discussing various use cases, techniques, and technologies for DBS-based bioanalysis.

Two primary global health applications envision that the use of DBS can extend either health-care services or research and surveillance studies into harder-to-reach populations. The clinical scenario aims to measure health-related diagnostic data to stratify at-risk individuals for additional confirmatory testing or to guide individual- or population-level treatment decisions. The other scenario aims to extend epidemiological surveillance that monitors population-level transmission of infection or tracks emerging or recrudescing disease. Both scenarios rely on tools that provide high-sensitivity analysis of individual samples to minimize the risk of missed positive cases, particularly in geographies where loss to follow-up remains a significant challenge. In other words, for both scenarios, false-negative test results typically have higher consequences for these programs than false-positive test results if there is an opportunity to further confirm the clinical or epidemiological status of test-positive individuals or populations.

The weakest link for sensitivity within a bioanalytical workflow is the quality of the specimen. The concept of DBS is appealing; however, these broad remote-sampling aspirations should consider the extensive literature evaluating the reliability of DBS for high-sensitivity analysis of specific biomarkers. In most instances, quantitative studies have demonstrated the feasibility of DBS if standardized collection and laboratory protocols are followed.,– However, there are examples where DBS fails to provide reliable results and this review includes a sample of these reports.

BACKGROUND

The concept of depositing fingerprick-derived blood on laboratory filter paper, the precursor of DBS, was first described in the 1860s for glucose measurements and in the 1960s for screening metabolic disorders in newborns using heelprick-derived blood. One of the popular DBS formats is the Whatman 903 card, which is composed of cotton-based filter paper within a rigid cardboard frame for handling and labeling. The paper is ink-printed with five half-inch circles that direct the user to the location for depositing a specimen. Blood-deposited cards are typically dried in an open environment by suspension in ambient air or under forced circulation in a laboratory or hospital. Dried blood spots are often stored for transport in a sealed bag with desiccant and archived under refrigerated or frozen conditions., Portions of the dried spot are “punched” out with a regular hole puncher or scissors, specialized DBS punchers and protocols are both available to reduce risk of contamination by card-to-card carryover.– The whole spot can also be used if there are no plans to re-analyze or archive the specimen.

The panel of diseases screened by newborn programs has significantly expanded since Guthrie’s first application of DBS with interest to use this technology in global health strategies.,,,– Given the implications of test results on treatment decisions or public health resources, published protocols and guidelines aiming to minimize the risk of pre-analytical variability are regularly evaluated and updated.,,,– Some assessments have found that a diagnostic cutoff determining one decision over another may be dependent on the type of platform used to analyze a DBS-derived specimen, such as those using human immunodeficiency virus (HIV) viral load measurements to determine treatment effectiveness,– or polymerase chain reaction (PCR) analysis of malarial DNA. These findings stress the importance of assessing and mitigating sources of data variability within a complete field-to-laboratory pre-analytical workflow, starting with the type of DBS and the platform used for downstream analysis of a specific biomarker (Figure 1).

The drug development sector is another early adopter, envisioning that DBS provides a simplified and cost-effective approach for measuring drug metabolites and toxicology biomarkers in preclinical animal studies.– This community published most of the quantitative evaluations in an effort to support claims on the equivalency of DBS-based data to data from venipuncture.,– Recent efforts to evaluate the feasibility of DBS for remote clinical trials have also been met with successes and challenges.,– One common conclusion from the newborn screening and drug development communities is the importance of storing DBS cards in refrigerated and desiccated conditions as soon as the specimen is dried to reduce data variability. The impact of these mitigation measures is dependent on the individual stability and physiological profiles of a specific analyte with frozen biobanking conditions still failing to provide sufficient stabilization over extended periods of time for many analytes. Some of the literature reviews summarizing the feasibility of DBS in global health applications include hepatitis B and C,,,– HIV,,,– and malaria.

Evaluations of discordant DBS results identified sources of variability that includeInterindividual differences, with a particular emphasis on hematocrit (Hct)Differences in analyte abundance between capillary and venous systemsType of DBS cardHeterogeneity within a single dried spot, particularly if only a portion is used for analysisStorage conditions during transport and archiveSample preparation methods

Interindividual differences, with a particular emphasis on hematocrit (Hct)

Differences in analyte abundance between capillary and venous systems

Type of DBS card

Heterogeneity within a single dried spot, particularly if only a portion is used for analysis

Storage conditions during transport and archive

Sample preparation methods

It is important to note that sources of variability are often interconnected. As discussed later, Hct and homogeneity of a dried spot are linked and the impact of these variables on test results might also depend on the type of DBS card and the chemical and physical properties of an analyte. The possibility of multiparametric sources of variability reinforces the need for analyte-specific quantitative evaluations that define the conditions, processes, and tools that will be locked down as described within a standard operating procedure and reinforced through quality assessments during and after implementation.

Few improvements to the paper-based backbone of DBS have been pursued other than the development of cellulose-based formats to enhance extraction of some classes of analytes or addition of embedded chemicals to increase nucleic acid stability. There are recent efforts to improve the field-ability of DBS through accessories that reduce the risk of cross contamination or improve desiccation of the collected sample and Table 1 provides examples of commercially available technologies.

Hematocrit.

The predominant source of interindividual variability studied in the DBS literature is Hct, a measurement representing the percentage of red blood cells in a known volume of blood., These clinical measurements are used to determine if a patient has anemia and can vary by age, gender, health, living environment, and nutritional status. From a chemical and materials perspective, a blood sample with an elevated Hct would have increased viscosity because of the higher percentage of red blood cells. As described in several reports, a viscous blood drop would have a less homogenous spread across a piece of filter paper compared with a sample with lower Hct.,– These physical dynamics introduce at least three potential interlinked sources of variability: material composition of DBS, location of the “punch” within a heterogenous spot, and extraction method. The latter is likely to be dependent on the physical density of the dried blood as determined in part by an individual’s Hct. De Kesel et al. provide a comprehensive review of different drug development studies evaluating the implications of Hct on DBS-derived data. Across these reports, the degree of variability from different Hct was dependent on the properties of a specific analyte and the type of DBS used, complicating possibilities for a simple Hct correction factor.

The impact of Hct on newborn screening results was evaluated by the U.S. Centers for Disease Control and Prevention. Similar to a study conducted by a U.K. newborn screening network, Hall et al. observed that the total volume of dried blood within each spot increased with higher Hct. The opposite effect was noted for dried serum where higher Hct was associated with lower per-punch volumes of serum. The physical diameter of the DBS was related to the total volume of blood but not significantly affected by Hct. In addition, per-punch volumes of whole blood, red blood cells, and serum were differentially impacted by Hct level, potentially affecting reliability of test results if targeted analytes naturally partition between these blood components.

In addition to physical dynamics, several studies evaluated the impact of Hct on the measurement of individual markers. For instance, most newborn screening panels include congenital hypothyroidism, a condition with no visible symptoms and without immediate treatment that could result in mental retardation. The risk of a newborn developing this condition is determined by quantitation of thyroid-stimulating hormone (TSH, thyrotropin), a peptide of approximately 200 amino acids. Butler et al. reported that an increase in Hct resulted in an artificial and clinically significant decrease in TSH concentration, using DBS samples collected as part of a newborn screening program. Although the opposite effect (decreased Hct, increased TSH) was also observed, false-negative test results caused by an Hct-influenced decrease of TSH have greater health implications, particularly if this measurement is the basis of a primary screen.

Unfortunately, there is no direct method to determine Hct directly from a DBS sample. As mentioned earlier, the diameter of the total blood spot has been shown to have little change over a range of Hct and an endogenous or exogenous marker has yet to be validated.,– One suggestion is to control the total volume of blood deposited on a DBS using a volumetric capillary or fixed-volume accessory.– Another possible mitigation is to ensure that the complete dried spot, including colorless plasma, is used for analysis rather an aliquoted punch. If the whole DBS circle is not used, location of punch relative to the whole spot should remain consistent along with annotation of an individual’s Hct., These additional procedures and accessories to mitigate this source of data variability increase logistical requirements in the field and laboratory, representing one of many trade-offs that should be assessed before scaling the use of DBS within remote health and surveillance strategies.

Analyte abundance in venous versus capillary blood.

There are several reports describing a difference in the natural abundance of biomarkers between capillary and venous blood,– some of which are described in Table 2. For low-abundant analytes, the impact of this variability on test results is likely to be amplified, given that smaller volumes of blood collected in DBS increase the probability of false-negative detection., Unlike venous blood draw, there is also a higher risk for inconsistent volumes with static fingerprick- or heelprick-drawn blood; “milking” the skin puncture to increase volume through direct pressure also increases risk for hemoconcentration.

Different hemoglobin concentrations were measured when fingerprick blood was extracted from either the left or right hand of the same individual. Bond and Richards-Kortum also reported higher degrees of variability in hemoglobin, white blood cell, and platelet count measurements from fingerprick-derived blood compared with venous-derived blood. In that study, collecting larger volumes of blood did not reduce the difference in total variability between capillary- and venous-derived blood (i.e., increased fingerprick volumes did not align the magnitude of variability with venous-derived blood). The authors also reported different degrees of drop-to-drop variability between patients, sharing that these results indicate interindividual physiological differences in the abundance of these analytes between the two circulatory pathways. Adding to the complexity, Hct levels were reportedly higher in capillary blood compared with venous blood in neonatal and young infants.

As demonstrated by these examples, partitioning between venous and capillary circulation is likely analyte specific and cannot be simply rationalized by smaller diameters of peripheral capillaries or mitigated by larger volumes of collected blood. Higher concentrations of some analytes in capillary blood can be attributed to hemoconcentration effects or, alternatively, lower concentrations may be due to the presence of extracellular fluid., This physiological basis for biomarker partitioning needs to be considered in guiding the clinical relevance of bioanalytical data, particularly if reported clinical correlations are based on a different source or component of blood. Assessments of analytical and clinical equivalence for any biomarker measured by capillary- and venous-derived samples should be conducted before implementing DBS within a research study or clinical workflow.

Type of DBS.

As shown in Table 1, different DBS formats are commercially available with some claiming improved extraction efficiency or stability for specific classes of analytes. The appropriate selection of the card should be based on the analyte properties and its stabilization requirements, extraction efficiency, and method of analysis. Basic DBS formats include the paper-based Whatman 903 and Ahlstrom 226 cards, and specialized cards include the Flinders Technology Associates (FTA) Drug Metabolism and Pharmacokinetics (DMPK) cards that are impregnated with cell lysis and analyte-stabilizing materials. Flinders Technology Associates DMPK-A cards contain sodium dodecyl sulfate and tris- (hydroxymethyl)aminomethane, and FTA DMPK-B cards contain guanidium thiocyanate. Some of these chemicals have been reported to leach from DBS during sample preparation and potentially interfere with some analytical platforms through a “matrix effect,” a risk that has been evaluated extensively by the drug development community.,

Analyte- and DBS-specific data variability was found between different FTA DMPK cards used for the measurement of small-molecule drugs in whole blood by liquid chromatography/MS., In addition to the matrix effect caused by impregnated chemicals, the type of paper can also influence spreading dynamics of blood across the DBS, as mentioned earlier.,, Distribution of antibodies across a DBS spot was found to be heterogenous and not predictable with authors suggesting that greater than 15% variability between different punches of the same spot. The impact of Hct and concentration on the recovery of small drug analytes were also dependent on the type of DBS.

Of relevance to global health applications, the variability of HIV viral load measurements was evaluated in three different types of DBS, and across different RNA analysis platforms. These studies observed variable genotyping efficiencies and drug susceptibility test results from samples derived from different DBS cards; some of the authors suggest that storage conditions might mitigate paper-dependent bias. Dried blood spot–based samples were also found to result in test results that overestimate HIV incidence when compared with test results from plasma samples.

The recovery and stability of malaria-related histidine-rich protein 2 (HRP2) and mRNA were also reported to be dependent on the type of DBS., In a report by Miguel et al., none of the three commercially available reagents were able to reliably extract DNA associated with Plasmodium falciparum or Plasmodium vivax infection from blood stored on cotton-based filter paper, although others have shown a dependence on the type of DBS., The use of cards designed to preserve nucleic acids was found to provide sufficient stability for detecting single-species malaria infection but failed to diagnose individuals with mixed P. vivax/falciparum infections. Addressing these limitations, a method for the simultaneous extraction of nucleic acids indicating P. vivax and P. falciparum infections was developed and field-evaluated with slight differences in analytical performance reported between two types of DBS cards. Different sample preparation methods resulted in discordant results when using PCR to detect malaria parasites, particularly if only a single aliquot/punch was used. These reports reinforce the need to carefully select the type of DBS card with criteria based on the properties of a specific biomarker, method for analysis, and physiochemical interactions with the card materials, in context of optimized stabilization and sample preparation.

STORAGE CONDITIONS

The impact of post-collection storage conditions on data quality has been extensively evaluated by multiple communities, focused on the type of card, time, temperature, humidity, and storage methods.,– These conditions include storage in the field, conditions during transport, storage before sample preparation, and longer term biobanking. The effects of these parameters are often dependent on the properties of the analyte and DBS, with a general recommendation that many of these impacts can be mitigated by storing dried cards in desiccated and frozen conditions as soon as possible.–

As mentioned earlier, biobanking in frozen conditions can fail to stabilize some analytes over extended period. For example, standard protocol for HIV viral load measurements calls for the immediate storage of DBS to less than −20°C or no longer than 14 days at ambient temperature. Even if stored at −20°C, DBS cards are only reliable if these measurements are made within 2 years. Similar recommendations are also described for storing DBS used in newborn screening and other clinical tests.,,,

Temperature and humidity conditions directly affect the ability to detect specific amino acids and metabolites routinely measured for newborn screening., Gene transcriptomics analysis of newborn DBS was more consistent if samples were stored at temperatures less than −20°C immediately after specimen acquisition, with time and temperature imparting various degrees of degradation for specific mRNA profiling targets and housekeeping genes. Lower temperatures is not the solution for all analytes; three polyunsaturated fatty acids used to screen newborns for neural development and visual function were found to have significant degradation after 10 days of storage at −28°C, with a high degree of intraindividual variability, when measured from umbilical blood dried on Ahlstrom 226 cards.–

For function-based bioanalysis, DBS storage temperatures greater than 4°C reduced the activity of all five enzymes measured to diagnose newborns at risk of lysosomal storage disorders, with the degree of variability dependent on the properties of a specific enzyme.– Quantitative measurements of glucose-6-phosphate dehydrogenase (G6PD) are used by both malaria and newborn screening programs to identify individuals deficient of this essential enzyme. Two studies showed that temperature and humidity impacted quantitative measurements of G6PD activity, a source of variability that can be mitigated if DBS was stored under desiccated and refrigerated conditions.,

There is emerging literature describing the pre-analytical impact of DBS storage conditions on bioanalytical test results for other diseases of global health interest such as hepatitis B and C,–,– and dengue., DNA measurements of P. falciparum were affected by type of DBS, drying time, and humidity, with an overall inferior sensitivity compared with frozen whole blood.,– Incomplete drying, storage temperature, and humidity affected measurements of malaria gametocyte mRNA more significantly on samples derived from FTA DBS compared with Whatman 903 cards., Type of DBS and storage temperature and humidity affected stability and recovery of antibodies for malarial serological surveys. For HRP2 measurements on Whatman 903 cards, storage at temperatures less than −20°C significantly reduced the variability of test results from archived samples.

For HIV drug resistance testing, HIV-1 nucleic acids were stable in DBS if stored in desiccated conditions at temperatures less than 4°C and were not recoverable if stored at 37°C under high humidity.,– Another report found that the rate of nucleic acid degradation because of storage conditions was dependent on a patient’s total viral load and preservation as dried blood or plasma., Similar to the malaria studies, drying time and handling of the specimen before biobanking affected the stability of HIV-1 RNA.,

Storage environment is not just one variable and includes temperature, humidity, and time within field, transport, and laboratory settings, all in context to the stability of a specific analyte. In many instances, the type of DBS was an important consideration. Storage procedures and conditions optimizing the stability of one biomarker are likely not optimal for a different analyte. This consideration is important for those developing multiplexed detection of a panel of analytes as trade-offs in analytical performance are likely and should be evaluated in the construction of a rigorous standard operating procedure.

DISCUSSION

Dried blood spot offers several logistical advantages for remote health and surveillance programs, particularly for screening and surveying hard-to-reach populations. For many of these tests, a highly sensitive biomarker analysis is important for reducing the risk of missed positive cases. Analytical sensitivity not only includes the performance of a downstream platform but also the pre-analytical workflow that starts with the collection of a specimen from an individual. Quality assurance should not be the compromise of simplified logistics if incorrect test results have significant health implications or result in unnecessary expenditure of research and programmatic resources.

Although this review focused on evaluations of validated biomarkers, there is also significant interest in the use of DBS for biomarker discovery. Given current challenges of biomarker validation,, DBS introduces interlinked sources of data variability that should be considered in any experimental design and statistical plan. As described in this review, significant effort is required to determine optimal conditions for specific analytes making broad standard operating procedures in the absence of an identified analyte overly simplistic. Field-collected DBS should be used sparingly in biomarker research or, at-minimum, in parallel with quality-assured venipuncture.

Several opportunities for improving the technology behind DBS should consider trade-offs with roll-to-roll DBS manufacturing processes, lower per-card cost, and simplified implementation logistics. In addition to direct measurements of Hct from DBS, there still lacks methods to determine the total volume of blood deposited on a card in the absence of a volumetric accessory. Simple field-appropriate technologies are also needed to control specimen drying and maintain desiccation of a blood spot on various types of DBS until storage in controlled conditions. Technologies that prevent contamination from other DBS cards, instrumentation, or environment would also be beneficial for the community.

Broad lessons learned include the importance of evaluating the physiological, chemical, and physical properties of each analyte in context to a conceptual pre-analytical workflow that includes DBS type, collection methods, and storage conditions. The newborn screening and drug development communities, in addition to an emerging community of global health researchers, continue to build on literature evaluating the reliability of DBS. These reports provide a foundation of methods for validating of DBS-based bioanalysis and for defining standardized procedures that ensure quality and reproducible data.

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    Zida S 2016 Estimation of HIV-1 DNA level interfering with reliability of HIV-1 RNA quantification performed on dried blood spots collected from successfully treated patients. J Clin Microbiol 54: 1641–1643.

    Not in our library10.1128/jcm.03372-15

  38. 38.

    Sawadogo S Shiningavamwe A Chang J Maher AD Zhang G Yang C Gaeb E Kaura H Ellenberger D Lowrance DW, 2014 Limited utility of dried-blood- and plasma spot-based screening for antiretroviral treatment failure with Cobas Ampliprep/TaqMan HIV-1 version 2.0. J Clin Microbiol 52: 3878–3883.

    Not in our library10.1128/jcm.02063-14

  39. 39.

    Chang J 2017 Performance characteristics of finger-stick dried blood spots (DBS) on the determination of human immunodeficiency virus (HIV) treatment failure in a pediatric population in Mozambique. PLoS One 12: e0181054.

    Not in our library10.1371/journal.pone.0181054

  40. 40.

    Schmitz ME et al.; for VL-DBS Study Group, 2017 Field evaluation of dried blood spots for HIV-1 viral load monitoring in adults and children receiving antiretroviral treatment in Kenya: implications for scale-up in resource-limited settings. J Acquir Immune Defic Syndr 74: 399–406.

    Not in our library10.1097/qai.0000000000001275

  41. 41.

    Baidjoe A 2013 Combined DNA extraction and antibody elution from filter papers for the assessment of malaria transmission intensity in epidemiological studies. Malar J 12: 272.

    Not in our library10.1186/1475-2875-12-272

  42. 42.

    Burnett JE, 2011 Dried blood spot sampling: practical considerations and recommendation for use with preclinical studies. Bioanalysis 3: 1099–1107.

    Not in our library10.4155/bio.11.68

  43. 43.

    Cobb Z 2013 In-depth study of homogeneity in DBS using two different techniques: results from the EBF DBS-microsampling consortium. Bioanalysis 5: 2161–2169.

    Not in our library10.4155/bio.13.171

  44. 44.

    Caron A Lelong C Pascual M-H Benning V, 2015 Miniaturized blood sampling techniques to benefit reduction in mice and refinement in nonhuman primates: applications to bioanalysis in toxicity studies with antibody-drug conjugates. J Am Assoc Lab Anim Sci 54: 145–152.

    Not in our library

  45. 45.

    Spooner N Lad R Barfield M, 2009 Dried blood spots as a sample collection technique for the determination of pharmacokinetics in clinical studies: considerations for the validation of a quantitative bioanalytical method. Anal Chem 81: 1557–1563.

    Not in our library10.1021/ac8022839

  46. 46.

    Chapman K Chivers S Gliddon D Mitchell D Robinson S Sangster T Sparrow S Spooner N Wilson A, 2014 Overcoming the barriers to the uptake of nonclinical microsampling in regulatory safety studies. Drug Discov Today 19: 528–532.

    Not in our library10.1016/j.drudis.2014.01.002

  47. 47.

    Nilsson LB Ahnoff M Jonsson O, 2013 Capillary microsampling in the regulatory environment: validation and use of bioanalytical capillary microsampling methods. Bioanalysis 5: 731–738.

    Not in our library10.4155/bio.13.27

  48. 48.

    Amara AB Else LJ Carey D Khoo S Back DJ Amin J Emery S Puls RL, 2017 Comparison of dried blood spots versus conventional plasma collection for the characterization of efavirenz pharmacokinetics in a large-scale global clinical trial-the ENCORE1 study. Ther Drug Monit 39: 654–658.

    Not in our library10.1097/ftd.0000000000000448

  49. 49.

    Kothare PA Bateman KP Dockendorf M Stone J Xu Y Woolf E Shipley LA, 2016 An integrated strategy for implementation of dried blood spots in clinical development programs. AAPS J 18: 519–527.

    Not in our library10.1208/s12248-015-9860-3

  50. 50.

    Antunes MV Charão MF Linden R, 2016 Dried blood spots analysis with mass spectrometry: potentials and pitfalls in therapeutic drug monitoring. Clin Biochem 49: 1035–1046.

    Not in our library10.1016/j.clinbiochem.2016.05.004

  51. 51.

    Edelbroek PM van der Heijden J Stolk LML, 2009 Dried blood spot methods in therapeutic drug monitoring: methods, assays, and pitfalls. Ther Drug Monit 31: 327–336.

    Not in our library10.1097/ftd.0b013e31819e91ce

  52. 52.

    Enderle Y Foerster K Burhenne J, 2016 Clinical feasibility of dried blood spots: analytics, validation, and applications. J Pharm Biomed Anal 130: 231–243.

    Not in our library10.1016/j.jpba.2016.06.026

  53. 53.

    Panchal T Spooner N Barfield M, 2017 Ensuring the collection of high-quality dried blood spot samples across multisite clinical studies. Bioanalysis 9: 209–213.

    Not in our library10.4155/bio-2016-0189

  54. 54.

    Li C-C 2017 Population PK analyses of Ubrogepant (MK-1602), a CGRP receptor antagonist: enriching in-clinic plasma PK sampling with outpatient dried blood spot sampling. J Clin Pharmacol 58: 294–303.

    Not in our library10.1002/jcph.1021

  55. 55.

    Guerra Valero YC Wallis SC Lipman J Stove C Roberts JA Parker SL, 2018 Clinical application of microsampling versus conventional sampling techniques in the quantitative bioanalysis of antibiotics: a systematic review. Bioanalysis 10: 407–423.

    Not in our library10.4155/bio-2017-0269

  56. 56.

    Wilhelm AJ den Burger JCG Swart EL, 2014 Therapeutic drug monitoring by dried blood spot: progress to date and future directions. Clin Pharmacokinet 53: 961–973.

    Not in our library10.1007/s40262-014-0177-7

  57. 57.

    Muzembo BA Mbendi NC Nakayama SF, 2017 Systematic review with meta-analysis: performance of dried blood spots for hepatitis C antibodies detection. Public Health 153: 128–136.

    Not in our library10.1016/j.puhe.2017.08.008

  58. 58.

    Greenman J Roberts T Cohn J Messac L, 2015 Dried blood spot in the genotyping, quantification and storage of HCV RNA: a systematic literature review. J Viral Hepat 22: 353–361.

    Not in our library10.1111/jvh.12345

  59. 59.

    Lange B 2017 Diagnostic accuracy of detection and quantification of HBV-DNA and HCV-RNA using dried blood spot (DBS) samples—a systematic review and meta-analysis. BMC Infect Dis 17 (Suppl 1): 693.

    Not in our library10.1186/s12879-017-2776-z

  60. 60.

    Villar LM de Oliveira JC Cruz HM Yoshida CFT Lampe E Lewis-Ximenez LL, 2011 Assessment of dried blood spot samples as a simple method for detection of hepatitis B virus markers. J Med Virol 83: 1522–1529.

    Not in our library10.1002/jmv.22138

  61. 61.

    Jardi R Rodriguez-Frias F Buti M Schaper M Valdes A Martinez M Esteban R Guardia J, 2004 Usefulness of dried blood samples for quantification and molecular characterization of HBV-DNA. Hepatology 40: 133–139.

    Not in our library10.1002/hep.20275

  62. 62.

    Bertagnolio S Parkin NT Jordan M Brooks J García-Lerma JG, 2010 Dried blood spots for HIV-1 drug resistance and viral load testing: a review of current knowledge and WHO efforts for global HIV drug resistance surveillance. AIDS Rev 12: 195–208.

    Not in our library

  63. 63.

    Hamers RL Smit PW Stevens W Schuurman R Rinke de Wit TF, 2009 Dried fluid spots for HIV type-1 viral load and resistance genotyping: a systematic review. Antivir Ther 14: 619–629.

    Not in our library

  64. 64.

    Parkin NT, 2014 Measurement of HIV-1 viral load for drug resistance surveillance using dried blood spots: literature review and modeling of contribution of DNA and RNA. AIDS Rev 16: 160–171.

    Not in our library

  65. 65.

    Adawaye C Kamangu E Moussa AM Tchoumbou B Vaira D Moutschen M, 2013 Use of dried blood spot to improve the diagnosis and management of HIV in resource-limited settings. World J AIDS 3: 251–256.

    Not in our library

  66. 66.

    Johannessen A, 2010 Dried blood spots in HIV monitoring:applications in resource-limited settings. Bioanalysis 2: 1893–1908.

    Not in our library10.4155/bio.10.120

  67. 67.

    Denniff P Spooner N, 2010 The effect of hematocrit on assay bias when using DBS samples for the quantitative bioanalysis of drugs. Bioanalysis 2: 1385–1395.

    Not in our library10.4155/bio.10.103

  68. 68.

    De Kesel PM Sadones N Capiau S Lambert WE Stove CP, 2013 Hemato-critical issues in quantitative analysis of dried blood spots: challenges and solutions. Bioanalysis 5: 2023–2041.

    Not in our library10.4155/bio.13.156

  69. 69.

    Chao TC Trybala A Starov V Das DB, 2014 Influence of haematocrit level on the kinetics of blood spreading on thin porous medium during dried blood spot sampling. Colloids Surf A Physicochem Eng Asp 451: 38–47.

    Not in our library

  70. 70.

    O’Mara M Hudson-Curtis B Olson K Yueh Y Dunn J Spooner N, 2011 The effect of hematocrit and punch location on assay bias during quantitative bioanalysis of dried blood spot samples. Bioanalysis 3: 2335–2347.

    Not in our library10.4155/bio.11.220

  71. 71.

    Hall EM Flores SR De Jesús VR, 2015 Influence of hematocrit and total-spot volume on performance characteristics of dried blood spots for newborn screening. Int J Neonatal Screen 1: 69–78.

    Not in our library10.3390/ijns1020069

  72. 72.

    Lawson AJ Bernstone L Hall SK, 2016 Newborn screening blood spot analysis in the UK: influence of spot size, punch location and haematocrit. J Med Screen 23: 7–16.

    Not in our library10.1177/0969141315593571

  73. 73.

    Butler AM Charoensiriwatana W Krasao P Pankanjanato R Thong-Ngao P Polson RC Snow G Ehrenkranz J, 2017 Newborn thyroid screening: influence of pre-analytic variables on dried blood spot thyrotropin measurement. Thyroid 27: 1128–1134.

    Not in our library10.1089/thy.2016.0452

  74. 74.

    Fan L Lee JA, 2012 Managing the effect of hematocrit on DBS analysis in a regulated environment. Bioanalysis 4: 345–347.

    Not in our library10.4155/bio.11.337

  75. 75.

    den Burger JCG Wilhelm AJ Chahbouni AC Vos RM Sinjewel A Swart EL, 2015 Haematocrit corrected analysis of creatinine in dried blood spots through potassium measurement. Anal Bioanal Chem 407: 621–627.

    Not in our library10.1007/s00216-014-8291-9

  76. 76.

    Abu-Rabie P Denniff P Spooner N Chowdhry BZ Pullen FS, 2015 Investigation of different approaches to incorporating internal standard in DBS quantitative bioanalytical workflows and their effect on nullifying hematocrit-based assay bias. Anal Chem 87: 4996–5003.

    Not in our library10.1021/acs.analchem.5b00908

  77. 77.

    Spooner N Olatunji A Webbley K, 2018 Investigation of the effect of blood hematocrit and lipid content on the blood volume deposited by a disposable dried blood spot collection device. J Pharm Biomed Anal 149: 419–424.

    Not in our library10.1016/j.jpba.2017.11.036

  78. 78.

    Polley SD Bell D Oliver J Tully F Perkins MD Chiodini PL González IJ, 2015 The design and evaluation of a shaped filter collection device to sample and store defined volume dried blood spots from finger pricks. Malar J 14: 45.

    Not in our library10.1186/s12936-015-0558-x

  79. 79.

    Fang K Bowen CL Kellie JF Karlinsey MZ Evans CA, 2018 Drug monitoring by volumetric absorptive microsampling: method development considerations to mitigate hematocrit effects. Bioanalysis 10: 241–255.

    Not in our library10.4155/bio-2017-0221

  80. 80.

    Aylward LL Hays SM Smolders R Koch HM Cocker J Jones K Warren N Levy L Bevan R, 2014 Sources of variability in biomarker concentrations. J Toxicol Environ Health B Crit Rev 17: 45–61.

    Not in our library10.1080/10937404.2013.864250

  81. 81.

    Tang R 2017 Capillary blood for point-of-care testing. Crit Rev Clin Lab Sci 54: 294–308.

    Not in our library10.1080/10408363.2017.1343796

  82. 82.

    Kupke IR Kather B Zeugner S, 1981 On the composition of capillary and venous blood serum. Clin Chim Acta 112: 177–185.

    Not in our library10.1016/0009-8981(81)90376-4

  83. 83.

    Canier L 2015 Malaria PCR detection in Cambodian low-transmission settings: dried blood spots versus venous blood samples. Am J Trop Med Hyg 92: 573–577.

    Not in our library10.4269/ajtmh.14-0614

  84. 84.

    Bond MM Richards-Kortum RR, 2015 Drop-to-drop variation in the cellular components of fingerprick blood: implications for point-of-care diagnostic development. Am J Clin Pathol 144: 885–894.

    Not in our library10.1309/ajcp1l7dkmpchpeh

  85. 85.

    Morris SS Ruel MT Cohen RJ Dewey KG de la Brière B Hassan MN, 1999 Precision, accuracy, and reliability of hemoglobin assessment with use of capillary blood. Am J Clin Nutr 69: 1243–1248.

    Not in our library10.1093/ajcn/69.6.1243

  86. 86.

    Kayiran SM Ozbek N Turan M Gürakan B, 2003 Significant differences between capillary and venous complete blood counts in the neonatal period. Clin Lab Haematol 25: 9–16.

    Not in our library10.1046/j.1365-2257.2003.00484.x

  87. 87.

    Zanet DL Saberi S Oliveira L Sattha B Gadawski I Côté HCF, 2013 Blood and dried blood spot telomere length measurement by qPCR: assay considerations. PLoS One 8: e57787.

    Not in our library10.1371/journal.pone.0057787

  88. 88.

    Emmons G Rowland M, 2010 Pharmacokinetic considerations as to when to use dried blood spot sampling. Bioanalysis 2: 1791–1796.

    Not in our library10.4155/bio.10.159

  89. 89.

    Chen X Zhao H Hatsis P Amin J, 2012 Investigation of dried blood spot card-induced interferences in liquid chromatography/mass spectrometry. J Pharm Biomed Anal 61: 30–37.

    Not in our library10.1016/j.jpba.2011.11.015

  90. 90.

    Matuszewski BK Constanzer ML Chavez-Eng CM, 2003 Strategies for the assessment of matrix effect in quantitative bioanalytical methods based on HPLC-MS/MS. Anal Chem 75: 3019–3030.

    Not in our library10.1021/ac020361s

  91. 91.

    Li W Tse FLS, 2010 Dried blood spot sampling in combination with LC-MS/MS for quantitative analysis of small molecules. Biomed Chromatogr 24: 49–65.

    Not in our library10.1002/bmc.1367

  92. 92.

    Ren X Paehler T Zimmer M Guo Z Zane P Emmons GT, 2010 Impact of various factors on radioactivity distribution in different DBS papers. Bioanalysis 2: 1469–1475.

    Not in our library10.4155/bio.10.96

  93. 93.

    Lenk G Hansson J Beck O Roxhed N, 2015 The effect of drying on the homogeneity of DBS. Bioanalysis 7: 1977–1985.

    Not in our library10.4155/bio.15.135

  94. 94.

    Koster RA Botma R Greijdanus B Uges DRA Kosterink JGW Touw DJ Alffenaar J-WC, 2015 The performance of five different dried blood spot cards for the analysis of six immunosuppressants. Bioanalysis 7: 1225–1235.

    Not in our library10.4155/bio.15.63

  95. 95.

    Rottinghaus EK Beard RS Bile E Modukanele M Maruping M Mine M Nkengasong J Yang C, 2014 Evaluation of dried blood spots collected on filter papers from three manufacturers stored at ambient temperature for application in HIV-1 drug resistance monitoring. PLoS One 9: e109060.

    Not in our library10.1371/journal.pone.0109060

  96. 96.

    Rottinghaus E Bile E Modukanele M Maruping M Mine M Nkengasong J Yang C, 2013 Comparison of Ahlstrom grade 226, Munktell TFN, and Whatman 903 filter papers for dried blood spot specimen collection and subsequent HIV-1 load and drug resistance genotyping analysis. J Clin Microbiol 51: 55–60.

    Not in our library10.1128/jcm.02002-12

  97. 97.

    Levine M Beck I Styrchak S Pepper G Frenkel L, 2016 Comparison of matrix-based and filter paper-based systems for transport of plasma for HIV-1 RNA quantification and amplicon preparation for genotyping. J Clin Microbiol 54: 1899–1901.

    Not in our library10.1128/jcm.00541-16

  98. 98.
    Comparison of cross-sectional HIV incidence assay results from dried blood spots and plasma. · 2017
    Not checked
  99. 99.

    Gibson LE Markwalter CF Kimmel DW Mudenda L Mbambara S Thuma PE Wright DW, 2017 Plasmodium falciparum HRP2 ELISA for analysis of dried blood spot samples in rural Zambia. Malar J 16: 350.

    Not in our library10.1186/s12936-017-1996-4

  100. 100.

    Jones S 2012 Filter paper collection of Plasmodium falciparum mRNA for detecting low-density gametocytes. Malar J 11: 266.

    Not in our library10.1186/1475-2875-11-266

  101. 101.

    Mlambo G Vasquez Y LeBlanc R Sullivan D Kumar N, 2008 A filter paper method for the detection of Plasmodium falciparum gametocytes by reverse transcription polymerase chain reaction. Am J Trop Med Hyg 78: 114–116.

    Not in our library

  102. 102.

    Miguel RB Coura JR Samudio F Suárez-Mutis MC, 2013 Evaluation of three different DNA extraction methods from blood samples collected in dried filter paper in Plasmodium subpatent infections from the Amazon region in Brazil. Rev Inst Med Trop São Paulo 55: pii: S0036-46652013000300205.

    Not in our library10.1590/s0036-46652013000300012

  103. 103.

    Bereczky S Mårtensson A Gil JP Färnert A, 2005 Short report: rapid DNA extraction from archive blood spots on filter paper for genotyping of Plasmodium falciparum. Am J Trop Med Hyg 72: 249–251.

    Not in our library

  104. 104.

    Zhong KJ Salas CJ Shafer R Gubanov A Gasser RA Magill AJ Forney JR Kain KC, 2001 Comparison of IsoCode STIX and FTA gene guard collection matrices as whole-blood storage and processing devices for diagnosis of malaria by PCR. J Clin Microbiol 39: 1195–1196.

    Not in our library10.1128/jcm.39.3.1195-1196.2001

  105. 105.

    Zainabadi K Adams M Han ZY Lwin HW Han KT Ouattara A Thura S Plowe CV Nyunt MM, 2017 A novel method for extracting nucleic acids from dried blood spots for ultrasensitive detection of low-density Plasmodium falciparum and Plasmodium vivax infections. Malar J 16: 377.

    Not in our library10.1186/s12936-017-2025-3

  106. 106.

    Bowen CL Dopson W Kemp DC Lewis M Lad R Overvold C, 2011 Investigations into the environmental conditions experienced during ambient sample transport: impact to dried blood spot sample shipments. Bioanalysis 3: 1625–1633.

    Not in our library10.4155/bio.11.128

  107. 107.

    Denniff P Spooner N, 2010 Effect of storage conditions on the weight and appearance of dried blood spot samples on various cellulose-based substrates. Bioanalysis 2: 1817–1822.

    Not in our library10.4155/bio.10.144

  108. 108.

    Adam BW Haynes CA Chafin DL De Jesus VR, 2014 Stabilities of intact hemoglobin molecules and hemoglobin peptides in dried blood samples. Clin Chim Acta 429: 59–60.

    Not in our library10.1016/j.cca.2013.11.019

  109. 109.

    Björkesten J 2017 Stability of proteins in dried blood spot Biobanks. Mol Cell Proteomics 16: 1286–1296.

    Not in our library10.1074/mcp.ra117.000015

  110. 110.

    Kyle JE 2017 Comparing identified and statistically significant lipids and polar metabolites in 15-year old serum and dried blood spot samples for longitudinal studies. Rapid Commun Mass Spectrom 31: 447–456.

    Not in our library10.1002/rcm.7808

  111. 111.

    Adam BW Chafin DL De Jesús VR, 2013 Stabilities of hemoglobins A and S in dried blood spots stored under controlled conditions. Clin Biochem 46: 1089–1092.

    Not in our library10.1016/j.clinbiochem.2013.05.043

  112. 112.

    Lin Y-Q Zhang Y Li C Li L Zhang K Li S, 2012 Evaluation of dry blood spot technique for quantification of an anti-CD20 monoclonal antibody drug in human blood samples. J Pharmacol Toxicol Methods 65: 44–48.

    Not in our library10.1016/j.vascn.2011.11.003

  113. 113.

    Mei JV Alexander JR Adam BW Hannon WH, 2001 Use of filter paper for the collection and analysis of human whole blood specimens. J Nutr 131: 1631S–1636S.

    Not in our library10.1093/jn/131.5.1631s

  114. 114.

    Adam BW Hall EM Sternberg M Lim TH Flores SR O’Brien S Simms D Li LX De Jesus VR Hannon WH, 2011 The stability of markers in dried-blood spots for recommended newborn screening disorders in the United States. Clin Biochem 44: 1445–1450.

    Not in our library10.1016/j.clinbiochem.2011.09.010

  115. 115.

    Han J Higgins R Lim MD Lin K Yang J Borchers CH, 2017 Short-term stabilities of 21 amino acids in dried blood spots. Clin Chem 64: 400–402.

    Not in our library10.1373/clinchem.2017.278457

  116. 116.

    Golbahar J Altayab DD Carreon E, 2014 Short-term stability of amino acids and acylcarnitines in the dried blood spots used to screen newborns for metabolic disorders. J Med Screen 21: 5–9.

    Not in our library10.1177/0969141314525367

  117. 117.

    Grauholm J Khoo SK Nickolov RZ Poulsen JB Bækvad-Hansen M Hansen CS Hougaard DM Hollegaard MV, 2015 Gene expression profiling of archived dried blood spot samples from the Danish Neonatal Screening Biobank. Mol Genet Metab 116: 119–124.

    Not in our library10.1016/j.ymgme.2015.06.011

  118. 118.

    Ho NT Busik JV Resau JH Paneth N Khoo SK, 2016 Effect of storage time on gene expression data acquired from unfrozen archived newborn blood spots. Mol Genet Metab 119: 207–213.

    Not in our library10.1016/j.ymgme.2016.08.001

  119. 119.

    Pupillo D Simonato M Cogo PE Lapillonne A Carnielli VP, 2016 Short-term stability of whole blood polyunsaturated fatty acid content on filter paper during storage at −28 °C. Lipids 51: 193–198.

    Not in our library10.1007/s11745-015-4111-z

  120. 120.

    Supriya M De T Christopher R, 2018 Effect of temperature on lysosomal enzyme activity during preparation and storage of dried blood spots. J Clin Lab Anal 32: e22220.

    Not in our library10.1002/jcla.22220

  121. 121.

    Elbin CS Olivova P Marashio CA Cooper SK Cullen E Keutzer JM Zhang XK, 2011 The effect of preparation, storage and shipping of dried blood spots on the activity of five lysosomal enzymes. Clin Chim Acta 412: 1207–1212.

    Not in our library10.1016/j.cca.2011.03.012

  122. 122.

    Adam BW Orsini JJ Martin M Hall EM Zobel SD Caggana M Hannon WH, 2011 The preparation and storage of dried-blood spot quality control materials for lysosomal storage disease screening tests. Clin Biochem 44: 704–710.

    Not in our library10.1016/j.clinbiochem.2011.02.014

  123. 123.

    De Jesus VR Zhang XK Keutzer J Bodamer OA Mühl A Orsini JJ Caggana M Vogt RF Hannon WH, 2009 Development and evaluation of quality control dried blood spot materials in newborn screening for lysosomal storage disorders. Clin Chem 55: 158–164.

    Not in our library10.1373/clinchem.2008.111864

  124. 124.

    Flores SR Hall EM De Jesús VR, 2017 Glucose-6-phosphate dehydrogenase enzyme stability in filter paper dried blood spots. Clin Biochem 50: 878–881.

    Not in our library10.1016/j.clinbiochem.2017.05.003

  125. 125.

    Jalil N Azma RZ Mohamed E Ithnin A Alauddin H Baya SN Othman A, 2016 Evaluation of glucose-6-phosphate dehydrogenase stability in stored blood samples. EXCLI J 15: 155–162.

    Not in our library10.17179/excli2015-604

  126. 126.

    McAllister G Shepherd S Templeton K Aitken C Gunson R, 2015 Long term stability of HBsAg, anti-HBc and anti-HCV in dried blood spot samples and eluates. J Clin Virol 71: 10–17.

    Not in our library10.1016/j.jcv.2015.07.303

  127. 127.

    Ndiaye O 2017 Usefulness of dried blood spots (DBS) to perform hepatitis C virus genotyping in drug users in Senegal. J Med Virol 89: 484–488.

    Not in our library10.1002/jmv.24460

  128. 128.

    Parr JB 2018 An efficient, large-scale survey of hepatitis C viremia in the Democratic Republic of the Congo using dried blood spots. Clin Infect Dis 66: 254–260.

    Not in our library10.1093/cid/cix771

  129. 129.

    Tejada-Strop A Drobeniuc J Mixson-Hayden T Forbi JC Le N-T Li L Mei J Terrault N Kamili S, 2015 Disparate detection outcomes for anti-HCV IgG and HCV RNA in dried blood spots. J Virol Methods 212: 66–70.

    Not in our library10.1016/j.jviromet.2014.10.018

  130. 130.

    Marques BL Brandão CU Silva EF Marques VA Villela-Nogueira CA Do Ó KM de Paula MT Lewis-Ximenez LL Lampe E Villar LM, 2012 Dried blood spot samples: optimization of commercial EIAs for hepatitis C antibody detection and stability under different storage conditions. J Med Virol 84: 1600–1607.

    Not in our library10.1002/jmv.23379

  131. 131.

    Dauner AL Gilliland TC Mitra I Pal S Morrison AC Hontz RD Wu S-JL, 2015 Evaluation of nucleic acid stabilization products for ambient temperature shipping and storage of viral RNA and antibody in a dried whole blood format. Am J Trop Med Hyg 93: 46–53.

    Not in our library10.4269/ajtmh.15-0110

  132. 132.

    Ruangturakit S Rojanasuphot S Srijuggravanvong A Duangchanda S Nuangplee S Igarashi A, 1994 Storage stability of dengue IgM and IgG antibodies in whole blood and serum dried on filter paper strips detected by ELISA. Southeast Asian J Trop Med Public Health 25: 560–564.

    Not in our library

  133. 133.

    Schwartz A Baidjoe A Rosenthal PJ Dorsey G Bousema T Greenhouse B, 2015 The effect of storage and extraction methods on amplification of Plasmodium falciparum DNA from dried blood spots. Am J Trop Med Hyg 92: 922–925.

    Not in our library10.4269/ajtmh.14-0602

  134. 134.

    Strøm GEA Moyo S Fataki M Langeland N Blomberg B, 2014 PCR targeting Plasmodium mitochondrial genome of DNA extracted from dried blood on filter paper compared to whole blood. Malar J 13: 137.

    Not in our library10.1186/1475-2875-13-137

  135. 135.

    Chaorattanakawee S Natalang O Hananantachai H Nacher M Brockman A Krudsood S Looareesuwan S Patarapotikul J, 2003 Storage duration and polymerase chain reaction detection of Plasmodium falciparum from blood spots on filter paper. Am J Trop Med Hyg 69: 42–44.

    Not in our library

  136. 136.

    Hwang J Jaroensuk J Leimanis ML Russell B McGready R Day N Snounou G Nosten F Imwong M, 2012 Long-term storage limits PCR-based analyses of malaria parasites in archival dried blood spots. Malar J 11: 339.

    Not in our library10.1186/1475-2875-11-339

  137. 137.

    Strøm GEA Tellevik MG Hanevik K Langeland N Blomberg B, 2014 Comparison of four methods for extracting DNA from dried blood on filter paper for PCR targeting the mitochondrial Plasmodium genome. Trans R Soc Trop Med Hyg 108: 488–494.

    Not in our library10.1093/trstmh/tru084

  138. 138.

    Pritsch M Wieser A Soederstroem V Poluda D Eshetu T Hoelscher M Schubert S Shock J Loescher T Berens-Riha N, 2012 Stability of gametocyte-specific Pfs25-mRNA in dried blood spots on filter paper subjected to different storage conditions. Malar J 11: 138.

    Not in our library10.1186/1475-2875-11-138

  139. 139.
    Dried blood spots as a source of anti-malarial antibodies for epidemiological studies · 2008
    No notice
  140. 140.

    García-Lerma JG McNulty A Jennings C Huang D Heneine W Bremer JW, 2009 Rapid decline in the efficiency of HIV drug resistance genotyping from dried blood spots (DBS) and dried plasma spots (DPS) stored at 37 degrees C and high humidity. J Antimicrob Chemother 64: 33–36.

    Not in our library10.1093/jac/dkp150

  141. 141.

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    Not in our library10.1093/jac/dkn100

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    Not in our library10.1371/journal.pone.0131541

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    Parry CM 2014 Field study of dried blood spot specimens for HIV-1 drug resistance genotyping. J Clin Microbiol 52: 2868–2875.

    Not in our library10.1128/jcm.00544-14

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    Mitchell C et al.; Dried Blood Spot Working Group of the Infant Maternal Pediatric Adolescent AIDS Clinical Trials Network, 2008 Diminished human immunodeficiency virus type 1 DNA yield from dried blood spots after storage in a humid incubator at 37 degrees C compared to −20 degrees C. J Clin Microbiol 46: 2945–2949.

    Not in our library10.1128/jcm.00359-08

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    Monleau M Butel C Delaporte E Boillot F Peeters M, 2010 Effect of storage conditions of dried plasma and blood spots on HIV-1 RNA quantification and PCR amplification for drug resistance genotyping. J Antimicrob Chemother 65: 1562–1566.

    Not in our library10.1093/jac/dkq205

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    Amellal B Katlama C Calvez V, 2007 Evaluation of the use of dried spots and of different storage conditions of plasma for HIV-1 RNA quantification. HIV Med 8: 396–400.

    Not in our library10.1111/j.1468-1293.2007.00484.x

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    Wei X Smith AJ Forrest DW Cardenas GA Beck DW LaLota M Metsch LR Sionean C Owen SM Johnson JA, 2016 Incident infection and resistance mutation analysis of dried blood spots collected in a field study of HIV risk groups, 2007–2010. PLoS One 11: e0159266.

    Not in our library10.1371/journal.pone.0159266

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    Begley CG Ellis LM, 2012 Raise standards for preclinical cancer research. Nature 483: 531–533.

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    Luckwell J 2013 Assessment of the within- and between-lot variability of Whatman™ FTA(®) DMPK and 903(®) DBS papers and their suitability for the quantitative bioanalysis of small molecules. Bioanalysis 5: 2613–2630.

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    Matheus S de Laval F Moua D N’Guyen C Martinez E Rousset D Briolant S, 2017 Zika virus persistence and higher viral loads in cutaneous capillaries than in venous blood. Emerg Infect Dis 23: 1910–1911.

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    Boghani S Mei Z Perry GS Brittenham GM Cogswell ME, 2017 Accuracy of capillary hemoglobin measurements for the detection of anemia among U.S. low-income toddlers and pregnant women. Nutrients 9: pii: E253.

    Not in our library10.3390/nu9030253

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    Daae LN Halvorsen S Mathisen PM Mironska K, 1988 A comparison between haematological parameters in “capillary” and venous blood from healthy adults. Scand J Clin Lab Invest 48: 723–726.

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    Bancone G Chu CS Chowwiwat N Somsakchaicharoen R Wilaisrisak P Charunwatthana P Bansil P McGray S Domingo GJ Nosten FH, 2015 Suitability of capillary blood for quantitative assessment of G6PD activity and performances of G6PD point-of-care tests. Am J Trop Med Hyg 92: 818–824.

    Not in our library10.4269/ajtmh.14-0696

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    Kocisko DA Walsh DS Eamsila C Edstein MD, 2000 Measurement of tafenoquine (WR 238605) in human plasma and venous and capillary blood by high-pressure liquid chromatography. Ther Drug Monit 22: 184–189.

    Not in our library10.1097/00007691-200004000-00008

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    Ashley EA Stepniewska K Lindegardh N Annerberg A Tarning J McGready R Phaiphun L Singhasivanon P White NJ Nosten F, 2010 Comparison of plasma, venous and capillary blood levels of piperaquine in patients with uncomplicated falciparum malaria. Eur J Clin Pharmacol 66: 705–712.

    Not in our library10.1007/s00228-010-0804-7

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    Diaw PA Daneau G Coly AA Ndiaye BP Wade D Camara M Mboup S Kestens L Dieye TN, 2011 Multisite evaluation of a point-of-care instrument for CD4(+) T-cell enumeration using venous and finger-prick blood: the PIMA CD4. J Acquir Immune Defic Syndr 58: e103–e111.

    Not in our library10.1097/qai.0b013e318235b378

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    Steinmetzer K Seidel T Stallmach A Ermantraut E, 2010 HIV load testing with small samples of whole blood. J Clin Microbiol 48: 2786–2792.

    Not in our library10.1128/jcm.02276-09

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    Bruns T Steinmetzer K Ermantraut E Stallmach A, 2009 Hepatitis C virus RNA quantitation in venous and capillary small-volume whole-blood samples. J Clin Microbiol 47: 3231–3240.

    Not in our library10.1128/jcm.00925-09

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    Descloux E La Fuentez C Roca Y De Lamballerie X, 2014 Clinical significance of intra-host variability of dengue-1 virus in venous and capillary blood. Clin Microbiol Infect 20: O167–O175.

    Not in our library10.1111/1469-0691.12368

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