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Age-associated epigenetic drift: implications, and a case of epigenetic thrift?

A. E. Teschendorff, J. West, S. Beck

Human Molecular Genetics · 2013 · Review

doi:10.1093/hmg/ddt375

Abstract

It is now well established that the genomic landscape of DNA methylation (DNAm) gets altered as a function of age, a process we here call 'epigenetic drift'. The biological, functional, clinical and evolutionary significance of this epigenetic drift, however, remains unclear. We here provide a brief review of epigenetic drift, focusing on the potential implications for ageing, stem cell biology and disease risk prediction. It has been demonstrated that epigenetic drift affects most of the genome, suggesting a global deregulation of DNAm patterns with age. A component of this drift is tissue-specific, allowing remarkably accurate age-predictive models to be constructed. Another component is tissue-independent, targeting stem cell differentiation pathways and affecting stem cells, which may explain the observed decline of stem cell function with age. Age-associated increases in DNAm target developmental genes, overlapping those associated with environmental disease risk factors and with disease itself, notably cancer. In particular, cancers and precursor cancer lesions exhibit aggravated age DNAm signatures. Epigenetic drift is also influenced by genetic factors. Thus, drift emerges as a promising biomarker for premature or biological ageing, and could potentially be used in geriatrics for disease risk prediction. Finally, we propose, in the context of human evolution, that epigenetic drift may represent a case of epigenetic thrift, or bet-hedging. In summary, this review demonstrates the growing importance of the 'ageing epigenome', with potentially far-reaching implications for understanding the effect of age on stem cell function and differentiation, as well as for disease prevention.

Full text

From PubMed Central, U.S. National Library of Medicine, as current on Oct 18, 2026. Paragraph numbers are ours, so an answer can point at one.

INTRODUCTION

DNA methylation (DNAm) is a key epigenetic mark of regulatory potential affecting mostly (but not exclusively) cytosines in a CpG context. The observation that DNAm in normal cells is altered as a function of age has a relatively long history, with early studies already reporting age-associated changes affecting a small number of individual gene loci, notably high CpG density promoters of important cancer genes such as IGF2 and ESR1 (; see also,). Global (genome-wide) hypomethylation with age was also noted early on, with subsequent confirmation in a longitudinal study of global DNAm patterns. It was also observed that monozygotic (MZ) twins exhibit epigenetic divergence in DNAm patterns that increases with age and differences in lifestyle. The advent of novel biotechnologies, allowing highly accurate assessment of DNAm levels across at least tens of thousands of CpG sites, have allowed more recent studies to test and confirm these earlier observations. For instance, using Illumina Infinium 27K arrays, in which probes map mainly to gene promoters, three separate studies have demonstrated that age-associated increases in DNAm happen preferentially at the promoters of key developmental genes, notably those bivalently marked in embryonic stem cells and which are often also marked by the Polycomb Repressive Complex (PRC2) and thus generally referred to as PolyComb Group Targets (PCGTs). Many of the bivalent genes/PCGTs encode known tumour-suppressors and transcription factors (TFs) necessary for differentiation. These data were derived from measuring DNAm in normal tissue, specifically in human whole-blood tissue, as well as in murine intestinal cells. Two more recent studies, using the more comprehensive and unbiased Illumina 450K arrays, have further confirmed that age-associated hypermethylation happens preferentially at high CpG density promoters, which often reside upstream of key developmental genes such as PCGTs. These studies have also confirmed that the majority of changes in the genome involve loss of methylation affecting CpG sites located in low CpG density regions, in line with the fact that most of these sites start out as methylated. Thus, it would appear that the machinery responsible for maintaining normal DNAm patterns becomes gradually deregulated with age, leading to deviations from a normal epigenetic state, a process we call epigenetic drift. Next, we briefly discuss the potential biological, functional, clinical and evolutionary significance of this age-associated epigenetic drift.

TISSUE-SPECIFIC AND TISSUE-INDEPENDENT AGE-ASSOCIATED DNAm SIGNATURES

One natural question that arises in the context of the observed epigenetic drift is whether this phenomenon is tissue-specific. Back in 2007, Issa and co-workers already noted that age-related DNAm changes affecting certain genes were only seen in specific tissues. In trying to fully address this question, it is important to appreciate the complex nature of the profiled tissues, which often encompass a variety of different cell types. Thus, if the cellular composition of tissues alters with age, then this could lead to age-associated DNAm signatures which purely reflect these underlying changes in cell type. Indeed, a number of studies have now shown that some of the age-associated DNAm changes seen in whole-blood tissue, especially those involving hypomethylation, can be related to an age-associated skew in blood cell-type proportions, specifically in the relative proportion of myeloid to lymphoid cells. This is consistent with reports of global hypomethylation as being associated with commitment to the myeloid lineage. Thus, age-associated DNAm signatures reflecting changes in tissue composition are likely to be tissue-specific, and indeed, these generally do not validate in other tissue types. Therefore, changing cellular composition is a major confounder when assessing DNAm changes, and, in response to this, statistical methods aimed at dissecting this cellular heterogeneity have recently emerged. Application of these methods will be key since effect sizes associated with age and with other EWAS phenotypes could be small. Indeed, these methods have already been shown to have a dramatic impact on statistical inference and significance estimates.

Interestingly, however, a number of recent studies have also demonstrated age-associated DNAm signatures that are largely independent of tissue type. For instance, a DNA hypermethylation signature consisting of 69 CpGs mapping to promoters of PCGTs was validated not only in whole blood but also in normal tissue from the cervix, lung and even in ovarian cancer cells. A separate study derived a similar signature, enriched for bivalently marked genes, which was then validated in purified CD4+ T-cells and CD14+ monocytes, thus effectively discarding changing blood cell-type composition as the underlying reason for these signatures. A recent meta-analysis focusing on brain and blood tissue also concluded that a large proportion of age-associated DNAm changes are common to both tissue types, with important implications for studying epigenetic effects in diseases like Alzheimer's disease. Another more recent study used a systems approach to identify interactome hotspots of age-associated differential methylation, which were found to target stem cell differentiation pathways and to be independent of tissue type (Fig. 1A). These age-associated interactome modules, derived with Illumina 27K arrays, have also been validated in data generated using Illumina 450K arrays (Fig. 1B and C). In summary, although it is hard to absolutely discard age-associated changes in tissue composition as the underlying mechanism of these common tissue-independent signatures, following Occam's Razor, the evidence does point towards the simplest explanation, which is that gradual age-associated accumulation of DNAm changes does occur independently of cell type.

DNAm-BASED AGE PREDICTORS

The observation that a number of age-associated DNAm signatures validate consistently across so many different tissue types is remarkable, given that analogous robust molecular signatures at the copy-number, mutational or transcriptomic levels have not been reported, or at least not at the same level of consistency as seen for DNAm. In fact, a meta-analysis of age-associated gene expression changes only reported marginal statistically significant agreement across studies, although, interestingly implicating genes with roles in metabolism and DNA repair. Telomere attrition and other molecular features such as T-cell DNA rearrangements can predict age, but the reported prediction accuracies are not high. More recently, a study reported mosaic copy-number changes with age, yet whether specific age-predictive copy-number-based signatures can be derived is unclear. In contrast, at least three separate studies have now reported DNAm -based age predictors. For instance, in Hannum et al., a DNAm-based age signature derived in whole blood could predict the age of independent blood samples with a median absolute deviation of only ±5 years. The authors further noted that this signature was highly correlated with age in other tissue types, but that highly accurate absolute age estimates could be achieved only if the parameters were retrained. It, therefore, seems likely that the high predictive accuracy attained by tissue-specific signatures is driven partly, if not entirely, by tissue-specific effects. Mechanistically, if changes in cell-type composition with age are highly certain and tissue-specific, then this would lead to corresponding highly accurate tissue-specific age predictors. This seems particularly relevant in the haematopoietic system where an age-associated skew towards the myeloid lineage has been observed. Thus, it remains to be seen whether tissue-independent age-associated DNA methylation signatures can achieve the predictive accuracy of tissue-specific DNAm signatures as reported in, e.g., Hannum et al.. Irrespective of the underlying biological mechanism, the high accuracy of some of the DNAm-based age predictors derived so far already promises some exciting novel applications, for instance in forensic science it has been suggested that they could be used to determine the approximate age of a suspect or victim from DNA samples collected at the crime scene. However, before this or other applications may be considered, it will be important to validate existing and novel DNAm-based age predictors more extensively, using truly independent cohorts. In doing so, particular care must also be taken in relation to technical confounding factors (e.g. batch effects), as these could easily skew or bias results.

Most of the age-predictive models reported so far are linear univariate or multivariate models, which assume that the rate at which age-associated DNAm changes accumulate is constant. This ageing rate has been shown to depend on genetic factors, and notably also on sex, with men exhibiting a faster rate. It remains to be seen, however, whether the rate of change is indeed constant, or whether instead a non-linear model could more accurately reflect how changes accumulate with age. For instance, a recent DNAm study performed on whole-blood samples from a paediatric population, consisting of boys aged between 3 and 17 years, showed that even at this young age, DNAm changes associated with age can be detected and, intriguingly, that these early changes account for most of the variation seen in the adult population. Thus, the authors of this study suggested a log-linear model to describe age-associated DNAm changes. However, not being a longitudinal study, and with the samples from the adult populations coming from different cohorts and generated by independent groups, this analysis could be subject to the usual caveats of confounding factors. A recent longitudinal twin study comparing buccal DNAm profiles of newborn twins with those at 18 months of age noted significant (3% differences at 12 months) age-associated DNAm changes. This is noteworthy in light of cross-sectional studies reporting typically 10% or at most 25% changes in DNAm across wider age ranges encompassing several decades. Thus, put together, the data from Alisch et al. and Martino et al. seem to suggest that age-associated epigenetic drift kicks in immediately after birth and may be particularly prominent during pre-puberty. These observations are surprising, yet also very interesting in light of studies proposing that the epigenome might be particularly sensitive to environmental stressors (e.g. nutrient deprivation) during pre-puberty. Thus, cumulative age-associated exposure to environmental factors during early life could be an important driver of epigenetic drift.

IMPLICATIONS OF AGE-ASSOCIATED DNAm FOR AGEING, STEM CELL BIOLOGY AND REPROGRAMMING

It is a striking observation that it is precisely the tissue-independent age DNAm signatures that also seem to validate in stem cell populations. For instance, an age-associated DNAm signature, derived from whole-blood tissue and enriched for PCGTs, was validated in bone marrow-derived mesenchymal stem cells (MSCs) from eight donors spanning a wide age range. A similar signature was also observed to be present in haematopoietic progenitor cells (HPCs). Other tissue-independent age signatures have also been validated in MSCs and in HPCs. Thus, it would appear that the generic epigenetic drift observed across all tissue types may be driven by changes in underlying long-lived stem cells, thus explaining why these age-associated changes can be seen in differentiated cell populations with a high turnover rate such as the haematopoietic system.

If epigenetic drift does indeed occur in stem cells, then this drift could, over time, affect stem cell function. Supporting this possibility, a recent bioinformatics study identified tissue-independent age-associated differential methylation interactome hotspots, specifically targeting a number of stem cell differentiation pathways (Fig. 1). One of these hotspots was enriched for stem cell TFs, including UTF1, SOX8 and SOX2, with their promoter CpGs gradually becoming hypermethylated with age. UTF1 is a TF necessary for the differentiation of human embryonic stem cells and has also recently been implicated as an important marker of reprogramming efficiency. Another age-associated network hotspot was found to be enriched in genes involved in WNT signalling, a pathway of key importance for normal differentiation of stem cells. Interestingly, age-associated changes in WNT-signalling activity are well documented, yet whether this is due to epigenetic deregulation is unclear. Interpretation is complicated by the fact that the promoters of both negative regulators and receptors of this pathway all become hypermethylated with age, hence the net effect of these changes is hard to predict.

Importantly, a number of experimental studies have shown that the age-associated DNAm changes seen in stem cells may underlie the observed decline in stem cell function, for instance in the case of MSCs and myogenic stem cells. Further important support for this hypothesis was recently provided by a study showing that DNAm changes associated with haematopoietic stem cell (HSC) ontogeny happen preferentially at PRC2 targets, and in particular at genes that would normally be expressed in differentiated progeny. In fact, this study also reported silencing (through DNA hypermethylation) of key TFs needed for cell-lineage specification in aged HSCs, although the overall genome-wide correlation between DNAm and gene expression was very low, suggesting that most DNAm changes at PRC2 targets in HSCs only affect their transcriptional competency when passed on to downstream progeny. In summary, age-associated DNAm changes in adult stem cells possibly underpins the observed decline in stem cell function (Fig. 2), including the observed myeloid skewing of the ageing haematopoietic system and immunosenescence.

Reprogramming of adult differentiated cells into induced pluripotent stem cells (iPSC) is accompanied by widespread changes in the DNAm landscape. Interestingly, loci undergoing age-associated DNAm changes have been observed to overlap significantly with those undergoing changes in reprogramming experiments. Thus, an intriguing and exciting possibility, suggested now by a number of studies and reviewed in Rando et al., is that of ‘epigenetic rejuvenation’, whereby age-driven accumulation of DNAm changes could be rewound and reset to zero, thus resembling the DNAm patterns of embryonic stem cells.

AGE-ASSOCIATED DNAm, DISEASE RISK AND CAUSALITY

Age-associated DNAm targeting the promoters of key tumour-suppressor genes in normal tissue has long been noted. Moreover, age-associated epigenetic divergence has been observed in MZ twins, with the drift proportional to the environmental divergence as measured by differences in lifestyle and time spent apart, suggesting that epigenetic drift could underlie their observed disease discordancy. Using Illumina beadarrays, a recent study demonstrated a highly statistically significant overlap between genes undergoing age-associated hypermethylation in their promoters and gene promoters undergoing hypermethylation in cancer, both involving preferentially PRC2 targets. Furthermore, one also observes strong overlaps of these genes with gene promoters characterized by DNAm changes associated with specific cancer risk factors [e.g. smoking, inflammation, obesity and viral oncoprotein expression]. Thus, age, cancer and cancer risk factor DNA hypermethylation signatures all seem commonly enriched for bivalent marks and PCGTs. However, not all DNAm changes associated with known cancer risk factors correlate with those seen in ageing—for instance, this seems to be the case for sunlight/UV exposure. In contrast to DNAm, it is only more recently that the age-associated mutational burden in normal tissue has been assessed, and therefore it is yet unclear if age- and cancer-associated mutational signatures overlap to the same degree as observed at the DNAm level.

Given that (i) age-associated DNAm changes are seen in normal tissue, (ii) that these are shared with those associated with cancer risk factors and (iii) that age is the strongest demographic risk factor for cancer, it is thus entirely plausible that these DNAm changes could predispose to cancer and thus be used for early detection or risk prediction. Supporting this, an age-associated DNAm signature enriched for PCGTs was found to be aggravated in intraepithelial neoplasias of the cervix, a pre-invasive cancer lesion. In a subsequent study that used a novel statistical risk-prediction algorithm based on epigenetic variable outliers, DNAm profiles measured in cytologically normal cervical swabs collected 3 years in advance of morphological transformation were shown to predict the future risk of a high-grade cervical intraepithelial neoplasia (CIN2+) with a low, yet statistically significant, AUC of approximately 0.64. Importantly, the CpG sites making up this risk classifier were shown to be associated with age in normal cervix and other normal tissue types including blood, as well as being highly differentially variable between individuals at different risk of developing CIN2+. Supporting this, inter-individual variable DNAm sites have also been shown to correlate with disease predisposition and to be enriched for bivalent/PCGT genes.

The overlap between DNAm changes associated with age in normal tissue with those conferring risk of cervical cancer is intriguing. Interestingly, overexpression of an HPV-associated viral oncoprotein has recently been shown to lead to widespread DNA hypermethylation at promoters of PRC2 targets. This suggests that at least some of the DNAm changes associated with the risk of cervical cancer are likely to have been caused by HPV infection. In this regard, it is important to recall, however, that HPV infection, although necessary, is not a sufficient factor for cervical cancer. Hence, it is possible that age-associated epigenetic drift, possibly linked with a cumulative exposure to other risk factors, contributes to disease predisposition and that further HPV-induced epigenetic alterations then synergize with these to allow initiation of morphological transformation.

The intriguing link between age-associated epigenetic drift and the changes seen in cancer and in precursor cancer lesions suggests a causal contributing role for DNAm in disease initiation and may also extend to other diseases. Indeed, a recent study analysing DNAm profiles of patients with Hutchinson–Gilford Progeria and Werner Syndrome, a premature ageing condition, concluded that DNAm changes may play a key causal or mediating role in these diseases. In fact, in those patients where the syndrome could be linked to genetic mutations in known causal genes (LMNA and WRN), aberrant DNAm profiles showed a remarkable overlap with those associated with age. Interestingly, DNAm changes, although distinct ones, were also observed in those patients not carrying the causal genetic mutation, suggesting that DNAm changes could play a causal role in these subsets of patients. Further support for a causal role of DNAm in mediating disease risk was provided by a recent EWAS study, which identified a number of methylation quantitative trait loci associated with rheumatoid arthritis. Finally, a number of epidemiological studies have also linked epigenetic changes with overall stress levels, itself a major risk factor for neurological diseases.

AGE-ASSOCIATED EPIGENETIC DRIFT: FUTURE DIRECTIONS

It is clear that the epigenome is altered by an age-associated epigenetic drift, whereby normal methylation patterns become deregulated with age. High CpG density promoters, and in particular those mapping to developmental genes, acquire methylation, whereas CpGs located outside these regions tend to lose methylation with age. However, a number of key questions require urgent attention. First, what is the precise biological mechanism (or mechanisms) leading to the deregulation of the normal DNAm patterns? While age-dependent expression of DNA methyltransferase genes has been reported, other epigenetic modulators (e.g. Sirtuins) may likely play an equally or even more important role. Methyl-binding domain proteins (e.g. MBD4) also seem implicated in modulating the rate of epigenetic drift. More fundamentally, it has been proposed that long-term deregulation of DNAm patterns occurs in response to spontaneous loss of histone modifications that happen on shorter timescales and in direct proportion to the number of cell divisions. To elucidate the mechanisms of regulation, it might help to investigate the degree of spatial stochasticity of age-associated DNAm changes. Besides CpG density, fairly little is known as to which other DNA sequence features may effect these age-related changes. Thus, it would be interesting to see whether age-associated methylation changes ‘cluster’ spatially as is observed, for instance, in cancer, or if instead they implicate a higher proportion of ‘singleton CpGs’, i.e. those that exhibit solitary DNAm changes and which are, therefore, less likely to be of functional significance. Heyn et al. reported an overall loss of spatial correlations in the DNA methylome of centenarians, yet another study did report finding extended age-associated DMRs (aDMRs). How frequent aDMRs are and how they compare with cancer DMRs in terms of their spatial correlative patterns remain to be seen. The precise pattern of CG dinucleotides in sequences affected by age-associated DNAm may also point to which epigenetic enzymes might be implicated. Alternatively, does one observe preferential enrichment of specific TF motifs among the sites that acquire age-associated DNAm changes, which would then point to the importance of specific TFs in mediating this age-associated deregulation of DNAm patterns, analogous to the TF-mediated redistribution of DNAm patterns one observes in response to stem cell differentiation and disease.

A second pressing question relates to the functional consequences of epigenetic drift, since it would appear that the association between age-driven DNAm and gene expression changes is, at the very best, only marginal. Moreover, it could well be that the weak association between DNAm and gene expression observed in whole blood is entirely driven by underlying changes in blood cell-type composition with no direct effect on cell function. Thus, it will be interesting to perform comprehensive paired DNAm and transcriptomic profiling of specific genes/pathways (e.g. WNT-signalling pathway) undergoing age-associated DNAm changes in a large number of cell-purified samples to assess the functional impact of the epigenetic changes. It is very likely that only a very small fraction of the age-associated epigenetic drift is of functional consequence, with the few functional changes ultimately affecting key transcriptional regulators, thus compromising stem cell differentiation or predisposing cells to neoplastic transformation.

A third key outstanding question is the dissection of age-associated DNAm changes that grow with ‘chronological age’, reflecting the number of cell divisions of long-lived stem cell populations, from the age-associated DNAm changes that may result from cumulative exposure to environmental risk factors, as well as from the changes that may accumulate with age in response to underlying genetic risk factors (Fig. 2). Two longitudinal studies, one on MZ twins and another involving families from an Icelandic cohort, have shown the importance of genotype in influencing the DNAm changes seen with age. Considerations of these separate components thus lead to the notion of a ‘biological’ age, as measured by the overall deregulation of DNAm in the genome of an individual, and which may be indicative of an overall prospective disease risk (Fig. 2). Epigenetic studies in model organisms where (isogenic) animals can be kept under controlled environmental conditions, allowing, for instance, a sustained and constant exposure to risk factors, seem key in order to help dissect the relative contributions of the intrinsic and extrinsic ‘epigenetic clocks’ in determining the biological age of the organism. Although Beerman et al. studied DNAm changes during HSC ontogeny and concluded that most of the age-associated hypermethylation at PRC2 targets was determined by the proliferative history of the HSCs (i.e. the intrinsic clock), these were not cells that had been exposed to the effects of environmental risk factors, as it might happen, for instance, under inflammatory conditions.

A fourth key question concerns the relative importance of epigenetic drift in comparison with other age-associated biological effects, most notably the well-known shortening of telomeres with age. Curiously, age-associated epigenetic drift and telomere shortening share many similar properties: both processes are influenced by genotype, both have been proposed to lead to stem cell dysfunction, both are aggravated in men compared with women, both are tissue-independent phenomena, and both have been linked to disease, disease risk and disease risk factors. For instance, a recent study reported seven genetic variants associated with leucocyte telomere length (LTL), with inter-individual variation in LTL being associated with cancer and other age-related diseases. Thus, both age-associated epigenetic drift and telomere shortening have been proposed as markers of biological ageing. In this regard, it is important to note that although epigenetic drift seems to outperform telomere length as a predictor of chronological age, it is the estimated deviations between predicted (i.e. biological) and chronological age that are potentially of most interest and which may account for the observed variation in disease risk. Thus, it remains to be seen whether epigenetic drift or telomere attrition is a more relevant marker of biological ageing. Matched LTL and DNAm data for MZ twin pairs discordant for disease status or for exposure to environmental risk factors could elucidate the relative contributions of these two biological processes to the biological ageing and disease risk phenotype.

EPIGENETIC DRIFT: A CASE OF EPIGENETIC THRIFT?

Finally, it is of interest to discuss the potential evolutionary significance of age-associated epigenetic drift. One attractive framework in which to interpret epigenetic drift is in the context of evolutionary theories of ageing. One competing theory argues that ageing emerged early in evolution as a means of controlling population size. It is conceivable that during times of limited resources or famine, which would have been frequent in early living history, overpopulation could lead to resource depletion and severe risk of mass extinction. Thus, in our ancestral species, natural ‘group’ selection could have favoured genetic and epigenetic mechanisms that promote ageing, with the damaging effects of these mechanisms only kicking in after the reproductive period, thus allowing new improved gene pools to take over and keeping overall populations at a stable and sustainable level. This viewpoint is supported by a related idea, grounded on evolutionary mathematical principles, and referred to as highly optimized tolerance. This evolutionary theory proposes that biological organisms, and multi-cellular species in particular, represent states of highly optimized tolerance, providing robustness to common perturbations, but simultaneously, and also inevitably, implicating costly trade-offs, such as an increase in fragility, as exemplified by the ageing phenotype. Thus, it is tempting to speculate that epigenetic drift is one possible mechanism contributing to the ageing phenotype (e.g. through a decline in stem cell function) and to an associated increased risk of disease and death (e.g. through increased predisposition to cancer or other age-related diseases, and possibly mediated by immunosenescence). As mentioned earlier, another mechanism could be telomere shortening, and so both telomere shortening and epigenetic drift may be seen as providing an evolutionary benefit to the species as a whole, by managing population dynamics through ageing and increased fragility.

There are a number of other important observations which further support a role for epigenetic drift in human evolution. For instance, a recent study has shown that epigenetic drift does not happen randomly in the context of the human interactome, but that it preferentially affects genes of low connectivity and centrality. Thus, genes carrying out integral housekeeping and cellular functions, and which are generally of high connectivity and centrality, appear to be more protected from epigenetic drift. Since epigenetic drift kicks in straight after birth and is prominent even in paediatric populations (i.e. well before the reproductive period), it is tempting to speculate that drift affecting highly integral and essential genes would be weeded out by natural selection. In contrast, natural selection would not be able to efficiently weed out the epigenetic drift targeting the non-essential and less integral genes, since the main effects of drift at these genes only show up after the reproductive age. Indeed, as argued earlier, epigenetic drift targeting non-essential genes may even be selected for as a mechanism underlying ageing and increased fragility, which are necessary for population control.

The observation that epigenetic drift is prominent in early life, and that associated epigenetic changes could be heritable, further suggests that epigenetic drift may represent another example of ‘thrift’, a term first coined by James Neel in the genetic context, whereby genes that would have conveyed an evolutionary advantage to our ancestral species would now lead to an opposing, apparently detrimental, effect in today's resource-rich society. Indeed, the genetic thrift hypothesis has recently been invoked to explain the current obesity and metabolic disease epidemics, according to which, genes favouring our ancestors, for instance, in promoting fat storage in anticipation of possible famines, would now have detrimental effects. Interestingly, epigenetic (or phenotype) thrift has also been proposed as the underlying mechanism to explain the increased incidence of diabetes and cardiovascular disease among people born during the 1944 Dutch Winter Famine. A compromised resource-depleted in utero environment could lead to epigenetic deregulation of metabolic genes to promote a more favourable metabolic state, which in a food-rich environment, however, would only be detrimental. Thus, if epigenetic changes are heritable, this would allow epigenetic drift to quickly shape phenotypes and evolution.

In summary, it is tempting to speculate that DNAm changes associated with epigenetic drift, which may be heritable, represent a case of epigenetic thrift, or perhaps even a case of evolutionary bet-hedging, contributing to both phenotypic diversity and the ageing phenotype, in a way that optimized evolutionary adaptation and species survival in the face of potential uncertain adversities.

Conflict of Interest statement. None declared.

FUNDING

A.E.T. is supported by a Heller Research Fellowship. J.W. is supported by an EPSRC/BBSRC PhD studentship awarded to CoMPLEX. S.B. was supported by the Wellcome Trust (WT084071) and a Royal Society Wolfson Research Merit Award (WM100023). Funding to pay the Open Access publication charges for this article was provided by the Wellcome Trust (WT084071).

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    Sandoval J., Heyn H.A., Moran S., Serra-Musach J., Pujana M.A., Bibikova M., Esteller M. Validation of a DNA methylation microarray for 450,000 CpG sites in the human genome. Epigenetics. 2011;6:692-702.

    Not in our library10.4161/epi.6.6.16196

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    Kwabi-Addo B., Chung W., Shen L., Ittmann M., Wheeler T., Jelinek J., Issa J.P. Age-related DNA methylation changes in normal human prostate tissues. Clin. Cancer Res. 2007;13:3796-3802.

    Not in our library10.1158/1078-0432.ccr-07-0085

  21. 21.
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    Langevin S.M., Houseman E.A., Christensen B.C., Wiencke J.K., Nelson H.H., Karagas M.R., Marsit C.J., Kelsey K.T. The influence of aging, environmental exposures and local sequence features on the variation of DNA methylation in blood. Epigenetics. 2011;6:908-919.

    Not in our library10.4161/epi.6.7.16431

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    Ji H., Ehrlich L.I., Seita J., Murakami P., Doi A., Lindau P., Lee H., Aryee M.J., Irizarry R.A., Kim K., et al. Comprehensive methylome map of lineage commitment from haematopoietic progenitors. Nature. 2010;467:338-342.

    Not in our library10.1038/nature09367

  25. 25.

    West J., Beck S., Wang X., Teschendorff A.E. An integrative network algorithm identifies age-associated differential methylation interactome hotspots targeting stem-cell differentiation pathways. Sci. Rep. 2013;3:1630.

    Not in our library10.1038/srep01630

  26. 26.

    Quon G., Haider S., Deshwar A.G., Cui A., Boutros P.C., Morris Q. Computational purification of individual tumor gene expression profiles leads to significant improvements in prognostic prediction. Genome Med. 2013;5:29.

    Not in our library10.1186/gm433

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    Rakyan V.K., Down T.A., Balding D.J., Beck S. Epigenome-wide association studies for common human diseases. Nat. Rev. Genet. 2011;12:529-541.

    Not in our library10.1038/nrg3000

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    Liu Y., Aryee M.J., Padyukov L., Fallin M.D., Hesselberg E., Runarsson A., Reinius L., Acevedo N., Taub M., Ronninger M., et al. Epigenome-wide association data implicate DNA methylation as an intermediary of genetic risk in rheumatoid arthritis. Nat. Biotechnol. 2013;31:142-147.

    Not in our library10.1038/nbt.2487

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    de Magalhaes J.P., Curado J., Church G.M. Meta-analysis of age-related gene expression profiles identifies common signatures of aging. Bioinformatics. 2009;25:875-881.

    Not in our library10.1093/bioinformatics/btp073

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    Aubert G., Lansdorp P.M. Telomeres and aging. Physiol. Rev. 2008;88:557-579.

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  32. 32.

    Meissner C., Ritz-Timme S. Molecular pathology and age estimation. Forensic Sci. Int. 2010;203:34-43.

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    Zubakov D., Liu F., van Zelm M.C., Vermeulen J., Oostra B.A., van Duijn C.M., Driessen G.J., van Dongen J.J., Kayser M., Langerak A.W. Estimating human age from T-cell DNA rearrangements. Curr. Biol. 2010;20:R970-R971.

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    Lin J., Epel E., Blackburn E. Telomeres and lifestyle factors: roles in cellular aging. Mutat. Res. 2012;730:85-89.

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    Laurie C.C., Laurie C.A., Rice K., Doheny K.F., Zelnick L.R., McHugh C.P., Ling H., Hetrick K.N., Pugh E.W., Amos C., et al. Detectable clonal mosaicism from birth to old age and its relationship to cancer. Nat. Genet. 2012;44:642-650.

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    Pang W.W., Price E.A., Sahoo D., Beerman I., Maloney W.J., Rossi D.J., Schrier S.L., Weissman I.L. Human bone marrow hematopoietic stem cells are increased in frequency and myeloid-biased with age. Proc. Natl Acad. Sci. USA. 2011;108:20012-20017.

    Not in our library10.1073/pnas.1116110108

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    Rossi D.J., Bryder D., Zahn J.M., Ahlenius H., Sonu R., Wagers A.J., Weissman I.L. Cell intrinsic alterations underlie hematopoietic stem cell aging. Proc. Natl Acad. Sci. USA. 2005;102:9194-9199.

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    Beerman I., Bhattacharya D., Zandi S., Sigvardsson M., Weissman I.L., Bryder D., Rossi D.J. Functionally distinct hematopoietic stem cells modulate hematopoietic lineage potential during aging by a mechanism of clonal expansion. Proc. Natl Acad. Sci. USA. 2010;107:5465-5470.

    Not in our library10.1073/pnas.1000834107

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    Leek J.T., Scharpf R.B., Bravo H.C., Simcha D., Langmead B., Johnson W.E., Geman D., Baggerly K., Irizarry R.A. Tackling the widespread and critical impact of batch effects in high-throughput data. Nat. Rev. Genet. 2010;11:733-739.

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    Teschendorff A.E., Zhuang J., Widschwendter M. Independent surrogate variable analysis to deconvolve confounding factors in large-scale microarray profiling studies. Bioinformatics. 2011;27:1496-1505.

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    Alisch R.S., Barwick B.G., Chopra P., Myrick L.K., Satten G.A., Conneely K.N., Warren S.T. Age-associated DNA methylation in pediatric populations. Genome Res. 2012;22:623-632.

    Not in our library10.1101/gr.125187.111

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    Pembrey M.E. Time to take epigenetic inheritance seriously. Eur. J. Hum. Genet. 2002;10:669-671.

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    Pembrey M.E., Bygren L.O., Kaati G., Edvinsson S., Northstone K., Sjostrom M., Golding J. Sex-specific, male-line transgenerational responses in humans. Eur. J. Hum. Genet. 2006;14:159-166.

    Not in our library10.1038/sj.ejhg.5201538

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    Bocker M.T., Hellwig I., Breiling A., Eckstein V., Ho A.D., Lyko F. Genome-wide promoter DNA methylation dynamics of human hematopoietic progenitor cells during differentiation and aging. Blood. 2011;117:e182-e189.

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    van den Boom V., Kooistra S.M., Boesjes M., Geverts B., Houtsmuller A.B., Monzen K., Komuro I., Essers J., Drenth-Diephuis L.J., Eggen B.J. UTF1 is a chromatin-associated protein involved in ES cell differentiation. J. Cell Biol. 2007;178:913-924.

    Not in our library10.1083/jcb.200702058

  50. 50.

    Baylin S.B., Ohm J.E. Epigenetic gene silencing in cancer – a mechanism for early oncogenic pathway addiction? Nat. Rev. Cancer. 2006;6:107-116.

    Not in our library10.1038/nrc1799

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    Brack A.S., Conboy M.J., Roy S., Lee M., Kuo C.J., Keller C., Rando T.A. Increased Wnt signaling during aging alters muscle stem cell fate and increases fibrosis. Science. 2007;317:807-810.

    Not in our library10.1126/science.1144090

  52. 52.

    Maiese K., Li F., Chong Z.Z., Shang Y.C. The Wnt signaling pathway: aging gracefully as a protectionist. Pharmacol. Ther. 2008;118:58-81.

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    Brack A.S., Rando T.A. Intrinsic changes and extrinsic influences of myogenic stem cell function during aging. Stem Cell Rev. 2007;3:226-237.

    Not in our library10.1007/s12015-007-9000-2

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    Beerman I., Bock C., Garrison B.S., Smith Z.D., Gu H., Meissner A., Rossi D.J. Proliferation-dependent alterations of the DNA methylation landscape underlie hematopoietic stem cell aging. Cell Stem Cell. 2013;12:413-425.

    Not in our library10.1016/j.stem.2013.01.017

  56. 56.

    Grolleau-Julius A., Ray D., Yung R.L. The role of epigenetics in aging and autoimmunity. Clin. Rev. Allergy Immunol. 2010;39:42-50.

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    Doi A., Park I.H., Wen B., Murakami P., Aryee M.J., Irizarry R., Herb B., Ladd-Acosta C., Rho J., Loewer S., et al. Differential methylation of tissue- and cancer-specific CpG island shores distinguishes human induced pluripotent stem cells, embryonic stem cells and fibroblasts. Nat. Genet. 2009;41:1350-1353.

    Not in our library10.1038/ng.471

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    Stricker S.H., Feber A., Engstrom P.G., Caren H., Kurian K.M., Takashima Y., Watts C., Way M., Dirks P., Bertone P., et al. Widespread resetting of DNA methylation in glioblastoma-initiating cells suppresses malignant cellular behavior in a lineage-dependent manner. Genes Dev. 2013;27:654-669.

    Not in our library10.1101/gad.212662.112

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    Rando T.A., Chang H.Y. Aging, rejuvenation, and epigenetic reprogramming: resetting the aging clock. Cell. 2012;148:46-57.

    Not in our library10.1016/j.cell.2012.01.003

  60. 60.

    Bell J.T., Spector T.D. DNA methylation studies using twins: what are they telling us? Genome Biol. 2012;13:172.

    Not in our library10.1186/gb-2012-13-10-172

  61. 61.
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    Widschwendter M., Fiegl H., Egle D., Mueller-Holzner E., Spizzo G., Marth C., Weisenberger D.J., Campan M., Young J., Jacobs I., et al. Epigenetic stem cell signature in cancer. Nat. Genet. 2007;39:157-158.

    Not in our library10.1038/ng1941

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    Schlesinger Y., Straussman R., Keshet I., Farkash S., Hecht M., Zimmerman J., Eden E., Yakhini Z., Ben-Shushan E., Reubinoff B.E., et al. Polycomb-mediated methylation on Lys27 of histone H3 pre-marks genes for de novo methylation in cancer. Nat. Genet. 2007;39:232-236.

    Not in our library10.1038/ng1950

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    Ohm J.E., McGarvey K.M., Yu X., Cheng L., Schuebel K.E., Cope L., Mohammad H.P., Chen W., Daniel V.C., Yu W., et al. A stem cell-like chromatin pattern may predispose tumor suppressor genes to DNA hypermethylation and heritable silencing. Nat. Genet. 2007;39:237-242.

    Not in our library10.1038/ng1972

  65. 65.

    Selamat S.A., Chung B.S., Girard L., Zhang W., Zhang Y., Campan M., Siegmund K.D., Koss M.N., Hagen J.A., Lam W.L., et al. Genome-scale analysis of DNA methylation in lung adenocarcinoma and integration with mRNA expression. Genome Res. 2012;22:1197-1211.

    Not in our library10.1101/gr.132662.111

  66. 66.

    Suzuki H., Toyota M., Kondo Y., Shinomura Y. Inflammation-related aberrant patterns of DNA methylation: detection and role in epigenetic deregulation of cancer cell transcriptome. Methods Mol. Biol. 2009;512:55-69.

    Not in our library10.1007/978-1-60327-530-9_5

  67. 67.

    Issa J.P., Ahuja N., Toyota M., Bronner M.P., Brentnall T.A. Accelerated age-related CpG island methylation in ulcerative colitis. Cancer Res. 2001;61:3573-3577.

    Not in our library

  68. 68.

    Issa J.P. Epigenetic variation and cellular Darwinism. Nat. Genet. 2011;43:724-726.

    Not in our library10.1038/ng.897

  69. 69.

    Xu X., Su S., Barnes V.A., De Miguel C., Pollock J., Ownby D., Shi H., Zhu H., Snieder H., Wang X. A genome-wide methylation study on obesity: differential variability and differential methylation. Epigenetics. 2013;8.

    Not in our library10.4161/epi.24506

  70. 70.

    Lechner M., Fenton T., West J., Wilson G., Feber A., Henderson S., Thirlwell C., Dibra H.K., Jay A., Butcher L., et al. Identification and functional validation of HPV-mediated hypermethylation in head and neck squamous cell carcinoma. Genome Med. 2013;5:15.

    Not in our library10.1186/gm419

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    Tomasetti C., Vogelstein B., Parmigiani G. Half or more of the somatic mutations in cancers of self-renewing tissues originate prior to tumor initiation. Proc. Natl Acad. Sci. USA. 2013;110:1999-2004.

    Not in our library10.1073/pnas.1221068110

  73. 73.

    Hoeijmakers J.H. DNA damage, aging, and cancer. N. Engl. J. Med. 2009;361:1475-1485.

    Not in our library10.1056/nejmra0804615

  74. 74.
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    Gemma C., Ramagopalan S.V., Down T.A., Beyan H., Hawa M.I., Holland M.L., Hurd P.J., Giovannoni G., Leslie R.D., Ebers G.C., et al. Inactive or moderately active human promoters are enriched for inter-individual epialleles. Genome Biol. 2013;14:R43.

    Not in our library10.1186/gb-2013-14-5-r43

  77. 77.

    Heyn H., Moran S., Esteller M. Aberrant DNA methylation profiles in the premature aging disorders Hutchinson-Gilford Progeria and Werner syndrome. Epigenetics. 2013;8:28-33.

    Not in our library10.4161/epi.23366

  78. 78.

    Nestler E.J. Epigenetics: stress makes its molecular mark. Nature. 2012;490:171-172.

    Not in our library10.1038/490171a

  79. 79.

    Xiao Y., Word B., Starlard-Davenport A., Haefele A., Lyn-Cook B.D., Hammons G. Age and gender affect DNMT3a and DNMT3b expression in human liver. Cell Biol. Toxicol. 2008;24:265-272.

    Not in our library10.1007/s10565-007-9035-9

  80. 80.

    Donadini A., Rosano C., Felli L., Ponassi M. Human sirtuins: an overview of an emerging drug target in age-related diseases and cancer. Curr. Drug Targets. 2013;14:653-661.

    Not in our library10.2174/1389450111314060006

  81. 81.

    Longo V.D., Kennedy B.K. Sirtuins in aging and age-related disease. Cell. 2006;126:257-268.

    Not in our library10.1016/j.cell.2006.07.002

  82. 82.

    Saunders L.R., Verdin E. Sirtuins: critical regulators at the crossroads between cancer and aging. Oncogene. 2007;26:5489-5504.

    Not in our library10.1038/sj.onc.1210616

  83. 83.

    Przybilla J., Galle J., Rohlf T. Is adult stem cell aging driven by conflicting modes of chromatin remodeling. BioEssays. 2012;34:841-848.

    Not in our library10.1002/bies.201100190

  84. 84.

    Hansen K.D., Timp W., Bravo H.C., Sabunciyan S., Langmead B., McDonald O.G., Wen B., Wu H., Liu Y., Diep D., et al. Increased methylation variation in epigenetic domains across cancer types. Nat. Genet. 2011;43:768-775.

    Not in our library10.1038/ng.865

  85. 85.

    Irizarry R.A., Ladd-Acosta C., Carvalho B., Wu H., Brandenburg S.A., Jeddeloh J.A., Wen B., Feinberg A.P. Comprehensive high-throughput arrays for relative methylation (CHARM). Genome Res. 2008;18:780-790.

    Not in our library10.1101/gr.7301508

  86. 86.

    Glass J.L., Fazzari M.J., Ferguson-Smith A.C., Greally J.M. CG dinucleotide periodicities recognized by the Dnmt3a-Dnmt3L complex are distinctive at retroelements and imprinted domains. Mamm. Genome. 2009;20:633-643.

    Not in our library10.1007/s00335-009-9232-3

  87. 87.
  88. 88.

    Hogart A., Lichtenberg J., Ajay S.S., Anderson S., Margulies E.H., Bodine D.M. Genome-wide DNA methylation profiles in hematopoietic stem and progenitor cells reveal overrepresentation of ETS transcription factor binding sites. Genome Res. 2012;22:1407-1418.

    Not in our library10.1101/gr.132878.111

  89. 89.

    Blackburn E.H. Cell biology: telomeres sans frontières. Nature. 1990;343:122.

    Not in our library10.1038/343122a0

  90. 90.

    Mitteldorf J. The future of aging pathways to human life extension. 2010;87-126.

    Not in our library

  91. 91.

    Benetos A., Okuda K., Lajemi M., Kimura M., Thomas F., Skurnick J., Labat C., Bean K., Aviv A. Telomere length as an indicator of biological aging: the gender effect and relation with pulse pressure and pulse wave velocity. Hypertension. 2001;37:381-385.

    Not in our library10.1161/01.hyp.37.2.381

  92. 92.

    Codd V., Nelson C.P., Albrecht E., Mangino M., Deelen J., Buxton J.L., Hottenga J.J., Fischer K., Esko T., Surakka I., et al. Identification of seven loci affecting mean telomere length and their association with disease. Nat. Genet. 2013;45:422-427.

    Not in our library10.1038/ng.2528

  93. 93.

    Broer L., Codd V., Nyholt D.R., Deelen J., Mangino M., Willemsen G., Albrecht E., Amin N., Beekman M., de Geus E.J., et al. Meta-analysis of telomere length in 19 713 subjects reveals high heritability, stronger maternal inheritance and a paternal age effect. Eur. J. Hum. Genet. 2013.

    Not in our library10.1038/ejhg.2012.303

  94. 94.

    Blasco M.A. Telomere length, stem cells and aging. Nat. Chem. Biol. 2007;3:640-649.

    Not in our library10.1038/nchembio.2007.38

  95. 95.

    Wilson W.R., Herbert K.E., Mistry Y., Stevens S.E., Patel H.R., Hastings R.A., Thompson M.M., Williams B. Blood leucocyte telomere DNA content predicts vascular telomere DNA content in humans with and without vascular disease. Eur. Heart J. 2008;29:2689-2694.

    Not in our library10.1093/eurheartj/ehn386

  96. 96.

    Blackburn E.H., Epel E.S. Telomeres and adversity: too toxic to ignore. Nature. 2012;490:169-171.

    Not in our library10.1038/490169a

  97. 97.

    Blackburn E.H., Greider C.W., Szostak J.W. Telomeres and telomerase: the path from maize, tetrahymena and yeast to human cancer and aging. Nat. Med. 2006;12:1133-1138.

    Not in our library10.1038/nm1006-1133

  98. 98.

    Petronis A. Epigenetics as a unifying principle in the aetiology of complex traits and diseases. Nature. 2010;465:721-727.

    Not in our library10.1038/nature09230

  99. 99.

    Huda N., Tanaka H., Herbert B.S., Reed T., Gilley D. Shared environmental factors associated with telomere length maintenance in elderly male twins. Aging Cell. 2007;6:709-713.

    Not in our library10.1111/j.1474-9726.2007.00330.x

  100. 100.

    Valdes A.M., Andrew T., Gardner J.P., Kimura M., Oelsner E., Cherkas L.F., Aviv A., Spector T.D. Obesity, cigarette smoking, and telomere length in women. Lancet. 2005;366:662-664.

    Not in our library10.1016/s0140-6736(05)66630-5

  101. 101.

    Samani N.J., van der Harst P. Biological ageing and cardiovascular disease. Heart. 2008;94:537-539.

    Not in our library10.1136/hrt.2007.136010

  102. 102.

    Mitteldorf J. Chaotic population dynamics and the evolution of ageing. Evol. Ecol. Res. 2006;8:561-574.

    Not in our library

  103. 103.

    Mitteldorf J. Aging is not a process of wear and tear. Rejuvenation Res. 2010;13:322-326.

    Not in our library10.1089/rej.2009.0967

  104. 104.

    Goldsmith T.C. Aging, evolvability, and the individual benefit requirement; medical implications of aging theory controversies. J. Theor. Biol. 2008;252:764-768.

    Not in our library10.1016/j.jtbi.2008.02.035

  105. 105.

    Kriete A. Robustness and aging—a systems-level perspective. Biosystems. 2013;112:37-48.

    Not in our library10.1016/j.biosystems.2013.03.014

  106. 106.

    West J., Widschwendter M., Teschendorff A.E. The distinctive topology of age-associated epigenetic drift in the human interactome. Proc. Natl Acad. Sci. USA. 2013.

    Not in our library10.1073/pnas.1307242110

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    Radford E.J., Isganaitis E., Jimenez-Chillaron J., Schroeder J., Molla M., Andrews S., Didier N., Charalambous M., McEwen K., Marazzi G., et al. An unbiased assessment of the role of imprinted genes in an intergenerational model of developmental programming. PLoS Genet. 2012;8:e1002605.

    Not in our library10.1371/journal.pgen.1002605

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    Carone B.R., Rando O.J. Rewriting the epigenome. Cell. 2012;149:1422-1423.

    Not in our library10.1016/j.cell.2012.06.008

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    Carone B.R., Fauquier L., Habib N., Shea J.M., Hart C.E., Li R., Bock C., Li C., Gu H., Zamore P.D., et al. Paternally induced transgenerational environmental reprogramming of metabolic gene expression in mammals. Cell. 2010;143:1084-1096.

    Not in our library10.1016/j.cell.2010.12.008

  110. 110.
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    Neel J.V. Diabetes mellitus: a ‘thrifty’ genotype rendered detrimental by ‘progress. Am. J. Hum. Genet. 1962;14:353-362.

    Not in our library

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    Wells J.C. Thrift: a guide to thrifty genes, thrifty phenotypes and thrifty norms. Int. J. Obes. (Lond.). 2009;33:1331-1338.

    Not in our library10.1038/ijo.2009.175

  113. 113.

    Hales C.N., Barker D.J. Type 2 (non-insulin-dependent) diabetes mellitus: the thrifty phenotype hypothesis. Diabetologia. 1992;35:595-601.

    Not in our library10.1007/bf00400248

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    Stoger R. The thrifty epigenotype: an acquired and heritable predisposition for obesity and diabetes. BioEssays. 2008;30:156-166.

    Not in our library10.1002/bies.20700

  115. 115.

    Veening J.W., Stewart E.J., Berngruber T.W., Taddei F., Kuipers O.P., Hamoen L.W. Bet-hedging and epigenetic inheritance in bacterial cell development. Proc. Natl Acad. Sci. USA. 2008;105:4393-4398.

    Not in our library10.1073/pnas.0700463105

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