Skip to main content

Ageing affects subtelomeric DNA methylation in blood cells from a large European population enrolled in the MARK-AGE study

Abstract

Ageing leaves characteristic traces in the DNA methylation make-up of the genome. However, the importance of DNA methylation in ageing remains unclear. The study of subtelomeric regions could give promising insights into this issue. Previously reported associations between susceptibility to age-related diseases and epigenetic instability at subtelomeres suggest that the DNA methylation profile of subtelomeres undergoes remodelling during ageing. In the present work, this hypothesis has been tested in the context of the European large-scale project MARK-AGE. In this cross-sectional study, we profiled the DNA methylation of chromosomes 5 and 21 subtelomeres, in more than 2000 age-stratified women and men recruited in eight European countries. The study included individuals from the general population as well as the offspring of nonagenarians and Down syndrome subjects, who served as putative models of delayed and accelerated ageing, respectively. Significant linear changes of subtelomeric DNA methylation with increasing age were detected in the general population, indicating that subtelomeric DNA methylation changes are typical signs of ageing. Data also show that, compared to the general population, the dynamics of age-related DNA methylation changes are attenuated in the offspring of centenarian, while they accelerate in Down syndrome individuals. This result suggests that subtelomeric DNA methylation changes reflect the rate of ageing progression. We next attempted to trace the age-related changes of subtelomeric methylation back to the influence of diverse variables associated with methylation variations in the population, including demographics, dietary/health habits and clinical parameters. Results indicate that the effects of age on subtelomeric DNA methylation are mostly independent of all other variables evaluated.

Introduction

Subtelomeres are transition DNA regions, ranging in size from 10 to 300 kb, which are found between chromosome-specific sequences and the telomeric repeats. Subtelomeres are poor in unique DNA sequences and genes. Instead, they are predominantly made up of a complex “patchwork” of blocks of sequences repeated in low copy numbers and characterised by a good intra- and inter-chromosomal sequence preservation [1,2,3]. Subtelomeric domains are considered heterochromatic regions, similar to telomeres. For instance, they contain HP1 protein and display histone modifications, such as H4K20me3 and H3K9me3, which are typical of heterochromatin. However, in contrast to the telomeres, the subtelomeres contain highly repetitive CpG dinucleotides, which make them prone to epigenetic regulation via DNA methylation [4, 5]. Telomere length is strongly affected by telomeric and subtelomeric chromatin modifications (reviewed in [4]). Subtelomeres tend to be strongly methylated both in humans and mice, and telomere elongation has been shown to be associated with subtelomeric hypomethylation, either following knockout of DNA methyltransferase enzymes [6] or in pathological conditions like cancer [7].

DNA methylation is among the epigenetic mechanisms that allow integration of intrinsic and environmental cues to shape genome functions [8]. Multiple interconnected pathways transduce these signals to the DNA methylation machinery, which can modify the cytosine base by the action of the DNA methyltransferase enzymes (DNMT1 or DNMT3A/B) to form 5-methylcytosine (5mC). 5mC, in turn, can be iteratively modified by the ten-eleven translocation (TET) family of proteins (TET1, TET2 and TET3) to produce the oxidation products 5-hydroxymethylcytosine (5hmC), 5-formylcytosine (5fC) and 5-carboxylcytosine (5caC). These 5mC oxidation products can act as intermediary compounds in the conversion of 5mC to unmodified cytosine, thus providing the first steps in the pathway for active DNA demethylation [9].

Rearrangements in the epigenetic landscape of the genome are recognized as being one of the major hallmarks of the ageing process [10], and the study of age-related DNA methylation changes is conceivably a promising way towards enhancing our understanding of the molecular mechanisms of ageing [11, 12]. While the bulk of the genome encounters a global loss of DNA methylation during ageing, a subset of CpG sites displays age-associated DNA methylation changes that are highly reproducible across individuals [11, 13]. This finding allowed the development of DNA methylation-based predictors of age, termed epigenetic clocks. First-generation epigenetic clocks were built as predictors of chronological age. However, it has been shown that the improved precision of epigenetic clock estimates was at the expense of their ability to detect departures from the physiological trajectories of ageing, possibly associated with age-related phenotypes and diseases [14, 15]. Therefore, attention has recently been devoted also to those CpG sites that do not necessarily display strong associations with chronological age but nevertheless are informative of the deviation of biological age from chronological age [13, 16].

In particular, the role of subtelomeric DNA methylation in ageing and age-related diseases is attracting an increasing level of interest [17]. Buxton et al. demonstrated that DNA methylation of subtelomeric sequences is associated with telomere length [18]. The mechanisms underlying the regulation of subtelomeric DNA methylation and its functional implications are yet to be fully understood. However, some previous reports have demonstrated the correlation between the subtelomeric DNA methylation and the development of neurodegenerative disorders (i.e. Alzheimer’s disease and Parkinson’s disease) [19,20,21,22], metabolic disorders (i.e. diabetes) [23] and some sporadic malignancies [7, 24,25,26,27,28]. Since these diseases are typically associated with ageing, these observations have led to the hypothesis that alterations in the status of subtelomeric methylation might be related to the ageing process.

This hypothesis is also supported by some initial evidence of an age-related change of subtelomeric DNA methylation in the white blood cells of healthy Japanese individuals [29]. However, the relationship between subtelomeric DNA methylation and ageing has not been investigated in large human populations so far.

Based on these premises, the present study has tested the association of subtelomeric methylation with ageing in the context of a large-scale European study, as part of the MARK-AGE project. MARK-AGE is a Europe-wide population study, supported by the European Commission (FP7), aiming to discover new biomarkers of ageing [30, 31]. MARK-AGE is mainly a cross-sectional study, in which age-stratified individuals (age range 35–75 years) were randomly recruited between 2008 and 2013 in seven European countries. The MARK-AGE study is largely representative of the general population, as the exclusion criteria included only seropositivity for HIV, HCV and HBV (except for seropositivity by vaccination) and the presence of actual cancer/current use of anti-cancer drugs or glucocorticoids. Furthermore, subjects born from a long-living parent belonging to a family with long-living sibling(s) and persons with progeroid syndromes were included as models of successful and unsuccessful ageing, respectively. Anthropometric, clinical and social data have been collected in a standardised manner, and a wide range of potential biomarkers of age was tested.

Here, we assessed the DNA methylation status of two subtelomeric regions. We analysed their variation with age in peripheral blood mononuclear cells (PBMC) from more than two thousand age-stratified donors (35–75 years), representative of the general population of eight European countries [31].

Our results indicate that age indeed influences the methylation level and patterns of the subtelomeres in PBMC. This association did not significantly depend on several nutritional, lifestyle or clinical variables, which influence subtelomeric DNA methylation in the population.

This study also took into consideration subtelomeric DNA methylation in models of successful (subjects born from a long-lived parent) and unsuccessful (subjects affected by Down syndrome, DS) ageing [31].

The study of these two subgroups provided further validation of the relationship between subtelomeric methylation and ageing, as the age-related methylation dynamic of the subtelomeres was consistent with their putative divergent rate of ageing.

Methods

Study design, recruitment, data and blood cell collection

The details of the MARK-AGE project have been the subject of previous publications, to which we refer for the study design [30, 31], data collection (i.e. demographic, anthropometric, clinical and social data) [32], the standard operating procedures (i.e. subject recruitment, collection, shipment and distribution of biological samples) [33] and management and processing of the MARK-AGE database [34, 35].

PBMC isolation procedure has been previously described [33, 36]. Briefly, the PBMC were isolated from EDTA whole blood, obtained by phlebotomy after overnight fasting, by discontinuous density gradient centrifugation in Percoll and subsequently cryopreserved to allow shipment, distribution and storage of the samples until analysis.

DNA extraction

The PBMC samples were thawed by incubation at 37 °C, followed by dropwise addition of RPMI containing 10% FCS to a final dilution of 1:20. Cells were collected by centrifugation and processed for DNA extraction.

Isolation of total DNA was performed using the QIAamp 96 DNA Blood Kit (Qiagen, Hilden, Germany) according to the manufacturer’s instructions. DNA concentration, purity and integrity were evaluated as previously described [37].

Quantitative DNA methylation analysis

The EpiTYPER assay (Sequenom, San Diego, USA) [38] was used to quantitatively assess the DNA methylation of two subtelomeric regions located in the short arm of chromosome 5 (5p; chr5:12,038–12,237 in the GRCh37/hg19 assembly) and in the long arm of chromosome 21 (21q), respectively. DNA (1 μg) was bisulphite-converted using the EZ-96 DNA Methylation Kit (Zymo Research, Irvine, USA) with the following modifications: incubation in CT buffer for 21 cycles of 15 min at 55 °C and 30 s at 95 °C, elution of bisulphite-treated DNA in 100 μl of water. Bisulphite-specific primers were designed using the EpiDesigner software (https://www.epidesigner.com) and checked by SYBR Green-based melt curve to evaluate the specificity of the amplification. The selected primers amplified the following regions, annotated in the GRCh37/hg19 assembly: chr5:12,038–12,237 (5p Fw: aggaagagagTTTTTTTTATTATAGATGTTGGGGG; 5p Rv: cagtaatacgactcactatagggagaaggctCCCAAACCTTCCTTAAAAACATCT); chr21:48,081,403-48,081,721: 21q Fw: aggaagagagGTTTTGTTGTGGAAAGGTTTAGTT; 21q Rv: cagtaatacgactcactatagggagaaggctCCCTCAAAATCTAAATCAAACAAAT. PCR was performed on 10 ng of converted DNA.

Statistical analysis

Batch effect correction of methylation data was performed via the Partek Genomic Suite 6.6 implemented with the ANOVA tool (Partek Incorporated). We considered each EpiTYPER experimental plate (containing about 100 samples with study groups not evenly distributed across plates) as a batch.

For continuous variables, normal distribution of data was verified by the Kolmogorov–Smirnov and Shapiro–Wilk normality tests (data not shown) as previously described [36]. Identification and handling of outliers were performed as previously described [36].

The characteristics of the study population across age groups were analysed by the one-way-ANOVA (continuous variables) or chi-square test (categorical variables).

Associations between variables have been analysed by both parametric and non-parametric tests. The generalised linear model (GLM) method was used as a parametric approach for comparisons between groups. The GLM was also used to investigate the influence of confounding variables (tested as categorised and continuous variables). The Kruskal–Wallis (KW) method was used as a non-parametric approach to compare between groups. When a significant p value was found, pairwise comparisons (adjusted for multiple comparisons by Bonferroni’s and Dunn’s methods for the GLM and the KW tests, respectively) were used to identify significant differences between groups. The GLM and KW test included categorical and categorised continuous variables as predictors. Associations between continuous variables were also investigated by linear regression using both parametric (Pearson) and non-parametric (Spearman) correlations. Correlations were additionally investigated by stratified bootstrap sampling (1000 bootstrap samples). Effect sizes in the GLM and KW tests were estimated by the eta square (η2) and epsilon square (ε2) indexes (η2 values ≅ 0.01, ≅ 0.06 and > 0.14 indicate weak, moderate and strong effect sizes, respectively; ε2 values <0.04, <0.16, <0.36 and > 0.36 indicate weak, moderate, relatively strong and strong effect sizes, respectively).

For the generation of the Methylation Age of SubTelomere index (MAST), we adopted a strategy based on regression analysis for multiple biomarkers. Briefly, methylation levels of all CpG sites were combined by linear regression using age as dependent variable in the randomly recruited age-stratified individuals from the general population (RASIG). MAST was then calculated in GO, SGO and DS as the sum of the methylation levels of each CpG site multiplied by its corresponding coefficient derived from RASIG (MAST = Constant + ∑ linear regression coefficient of methylation level of CpG × methylation level of CpG).

All statistical analyses were carried out using SPSS software (IBM SPSS Statistics Version 23.0, New York, USA).

Results

Study population

The population under study consisted of 3155 individuals divided into three groups (Table 1). The largest group, representative of the “average” ageing population, consisted of randomly recruited age-stratified individuals from the general population (RASIG) of seven European countries covering the age range of 35–75 years. Stratification of RASIG into four consecutive 10-year age groups guaranteed an almost homogenous distribution of sample size, a balanced sex ratio and a broad area of origins across the whole age range studied.

Table 1 Study population

A second group represented a presumed model of successful or “retarded” ageing. It consisted of the offspring of nonagenarians, allegedly predisposed to longevity because of their genetic background. This group has been previously studied in the framework of the GEHA (Genetics of Healthy Ageing) project [39] and is hereafter referred to as GO (GEHA offspring). To check for lifestyle and environmental effects, the GO group was compared to the group of their spouses, which was named the SGO (spouses of the GO) [31] group. Both groups covered the age range of 55–75 years.

Finally, subjects affected by DS, a known segmental progeroid syndrome, were considered as a model of premature/accelerated ageing [31].

Being composed of quite rare individuals, the GO, SGO and DS groups show limited sample size, a not wholly balanced sex ratio in some age groups and a limited geographical distribution of sample origin.

The body mass index (BMI) appeared to increase with age in RASIG and is consistently higher in SGO compared to GO, indicating that the analysed population was effectively representative of a physiological ageing process.

Characteristics of the analysed subtelomeric regions

Subtelomeric DNA methylation was quantified in PBMC-derived genomic DNA using the EpiTYPER assay. This assay measures the methylation percentage of single CpG sites or groups of adjacent sites, termed CpG units, included in a target genomic sequence. Two target sequences were selected among the subtelomeres that have low structural variation and lack sequence gaps and large duplications [40, 41]: the first one is located on the short arm of chromosome 5 (5p) and includes 3 detectable CpG sites; the second one is located in the long arm of chromosome 21 (21q) and includes 18 detectable CpG sites, grouped in 10 CpG units. The localisation of the target genomic sequences and the CpG sites covered by the analysis are shown in Fig. 1.

Fig. 1
figure1

CpG distribution of the 5p and 21q subtelomeric regions. Schematic representation of CpG site distribution within the analysed regions. Green and red circles represent the analysed and non-analysed CpG sites, respectively. The dashed boxes indicate the CpG sites that were measured as single methylation units in the EpiTYPER assay. The genomic positions refer to the 2009 (GRCh37/hg19) assembly

Methylation changes of the subtelomeric CpG sites with age in the general population

The relationship between variation in subtelomeric methylation and physiological ageing was investigated in the RASIG group, representative of the general population in the chronological age range of 35–75 years.

The association between CpG methylation level and age was investigated both by an age stratification approach and by linear correlation analysis. By comparing the 10-year age groups, we observed a progressive increase in methylation with increasing age of most of the CpG sites on both subtelomeres, as well as an increase of the mean subtelomeric methylation calculated in each individual (Supplementary Table S1). The significance of these associations was confirmed by both non-parametric (Kruskal–Wallis, KW) and parametric (generalised linear model, GLM) tests, the latter accounting for the effects of sex and recruitment centre as potential confounding factors. One exception was the 21q CpG unit 1.2 which was significantly associated with age only in the GLM. Pairwise comparison tests indicated that the differences mainly concerned the most extreme age groups. These data are shown graphically in Fig. 2.

Fig. 2
figure2

DNA methylation level of the 5p and 21q subtelomeres in RASIG stratified by age. a Methylation percentage of the CpG sites in the 5p subtelomeric region. b Methylation percentage of the CpG sites in the 21q subtelomeric region. c Mean methylation percentage calculated from all the CpG sites of the 5p and 21q subtelomeres. Data are depicted by box-and-whisker plots. The horizontal line indicates the median. The lower and the upper edge of the box show the first and the third quartile, respectively. The whiskers show the maximum and the minimum data values. Pairwise comparisons resulting in a significant Kruskal–Wallis test are indicated by the asterisks. *p < 0.05, **p < 0.01, ***p < 0.001

All CpG sites showed a weak positive, albeit highly significant, linear correlation with age, both in non-parametric (Spearman) and parametric (Pearson) tests, which included a bootstrap stratified resampling in order to control for the effects of sex and recruitment centre (Supplementary Table S2 and Fig. 3).

Fig. 3
figure3

Correlation between the DNA methylation level of the 5p and 21q subtelomeres and age in RASIG. a CpG methylation percentage and average methylation percentage of the 5p subtelomere. b CpG methylation percentage and average methylation percentage of the 21q subtelomere. Data are depicted by scatterplots, including the line of best fit

Generation of a cumulative epigenetic age predictor by combining the age-related DNA methylation changes on 5p and 21 q subtelomeric regions

Based on the highly concordant linear association of all the CpG sites with age, we chose to create a summary index that illustrates the cumulative importance of the DNA methylation of all sites in predicting age. Several multiple linear regression methods were tested in the RASIG population using the methylation value of all the 5p and 21q CpG sites as the predictor variables and age as the response variable (Supplementary Table S3, methods 1–8). Method 1 (linear regression based on enter method) outperformed all other methods in modelling the relationship between age and DNA methylation changes as it provided predicted values with the highest correlation vs age in both parametric (R = 0.176, p < 0.001) and non-parametric tests (R = 0.174 p < 0.001). Further details on this regression model are given in Supplementary Table S4. Notably, the coefficient of determination (R = 0.254) of the model was higher than the association with age of each of the CpG sites methylation in the binary correlation analyses (Supplementary Table S2). This indicated that the combined model was more informative for age prediction than the methylation values of each single CpG site. The linear predictor of the model was therefore used to combine the methylation status of all CpG sites into a single subtelomeric DNA methylation age index (from now on referred to as Methylation Age of SubTelomeres or MAST) for each individual. The linear regression coefficients, calculated from the RASIG group, were then used to compute MAST in all the other populations (GO, SGO, DS) included in this study.

Notably, given the relatively low coefficient of determination of the model, MAST should not be regarded as a DNA methylation-based predictor of age (in other words, MAST is not an epigenetic clock) but as a cumulative index measuring the combined age-related DNA methylation changes of the 5p and 21q subtelomeric regions.

Association of MAST with age and telomere length in the general population

Stratification analysis was used to further evaluate the association of MAST with age. As shown by a GLM test adjusted for sex and recruitment centre, a significant increase of MAST was detected with increasing age in RASIG (Table 2 and Fig. 4). Non-parametric tests confirmed this trend (Supplementary Table S5).

Table 2 GLM analysis of the methylation age of subtelomeres (MAST) by age in RASIG
Fig. 4
figure4

Level of MAST in RASIG stratified by age. Data are represented by mean ± S.D. Pairwise comparisons resulting in a significant GLM analysis, followed by Bonferroni post hoc test, are indicated by the asterisks. The GLM was adjusted for sex and recruitment centre. *p < 0.05, **p < 0.01, ***p < 0.001

In order to investigate the possible functional importance of subtelomeric DNA methylation, we next examined the relationship between MAST, telomere length and age. In fact, subtelomeric DNA methylation is known to be closely related to the control of telomere length, and telomere shortening is associated with the ageing process. A correlation analysis showed that the positive relationship between MAST and age was paralleled by an inverse association between telomere length and age (Supplementary Table S6). These findings indicated that the increase in MAST with age could be associated with telomere shortening. In fact, a significant, albeit very weak in magnitude, negative correlation between MAST and telomere length supported such a connection (Supplementary Table S6). The difference in the correlation coefficient of MAST with age from that reported in Supplementary Table S4 may be due to the limited number of subjects tested for the telomere length included in this last analysis.

Analysis of MAST in the offspring of nonagenarians and in persons affected by Down syndrome

To evaluate the association between subtelomeric DNA methylation and ageing progression, MAST was analysed in the GO and DS groups as models of decelerated and accelerated ageing, respectively.

We tested if MAST was able to distinguish GO from SGO. Age-matched RASIG individuals (55–75 years) were used as an additional normal ageing control group. As reported in Fig. 5, significant differences between the two age subgroups (55–64 and 65–75) were found in the RASIG and in the SGO groups, but not in the GO group. Furthermore, in the 65–75 age group, MAST was significantly lower in GO compared to SGO and RASIG. A GLM test adjusted for sex and recruitment centre, as well as non-parametric comparison tests, confirmed this result (Table 3 and Supplementary Table S5).

Fig. 5
figure5

Level of MAST in GO vs SGO and RASIG stratified by age. Data are represented by mean ± S.D. Pairwise comparisons resulting in a significant GLM analysis, followed by least significant difference (and Bonferroni) post hoc tests, are indicated by the asterisks. The GLM was adjusted for sex and recruitment centre. *p < 0.05, **p < 0.01, ***p < 0.001

Table 3 GLM analysis of MAST in GO vs SGO and RASIG in the population aged >54 years controlling for sex and recruitment centre

A similar analysis was performed on DS. Due to the limited sample size of the DS group, the analysis was limited to the age range of 35–54 years. Age- and recruitment centre–matched RASIG individuals were used as a control group. Again, significant differences in MAST between the two age subgroups (35–44 and 45–54) were found in the RASIG but not in the DS group (Fig. 6). MAST mean values in DS were significantly higher than those of 35–44-year-old RASIG. A GLM test adjusted for sex, as well as non-parametric comparison tests, confirmed this result (Table 4 and Supplementary Table S5).

Fig. 6
figure6

Level of MAST in DS vs RASIG stratified by age. Data are represented by mean ± S.D. Pairwise comparisons resulting in a significant GLM analysis, followed by least significant difference (and Bonferroni) post hoc tests, are indicated by the asterisks. The GLM was adjusted for sex and recruitment centre. *p < 0.05, **p < 0.01, ***p < 0.001

Table 4 GLM analysis of MAST in DS vs RASIG in the age range of 35–55 years

Investigation of factors associated with subtelomeric DNA methylation changes in the general population

An extensive set of data on demographics, anthropometric and clinical parameters have been collected from RASIG, GO and SGO subjects enrolled in the MARK-AGE study [30]. A subset of these parameters, possibly implicated in DNA methylation and telomere homeostasis, was evaluated for its association with MAST changes in RASIG. These included demographic and anthropometric data (Supplementary Table S7), self-reported dietary and lifestyle habits (Supplementary Table S8), cardiovascular/diabetes risk factors (Supplementary Table S9) and expression of components of the DNA methylation molecular machinery in PBMC (Supplementary Table S10). Moreover, differential white blood cell count data were used to monitor the effect of changes in the PBMC sample composition (Supplementary Table S11). The analysis was performed by comparing MAST levels between RASIG individuals stratified into consecutive subgroups according to the variable of interest. Comparisons were performed by both non-parametric (KW) and parametric (GLM) tests. The latter allowed for confounding variables adjustment (i.e. sex and recruitment centre). The magnitude of the difference in MAST between subgroups (effect size) was estimated by calculating the η2 and the ε2 for the GLM and KW tests, respectively.

Several associations were identified by the KW test but were disproved by the GLM. These included the BMI, French fries and whole bread consumption, serum levels of glucose, total cholesterol and free fatty acids. The connection of these factors to MAST seemed, therefore, to be spurious and strongly influenced by confounding factors (i.e. sex and recruitment centre). Conversely, the association of MAST with glycated haemoglobin A1c was proved only by the GLM, which indicated that sex and recruitment centre were acting as positive confounders.

Based on the congruence between the KW and GLM tests, several factors appeared to be significantly associated with MAST.

Among demographics, the recruitment centre had an impact, evidently due to the samples recruited in Austria (Supplementary Table S7).

An influence of dietary/lifestyle habits on MAST was attributable to the consumption of white bread and alcoholic beverages (Supplementary Table S8). In both cases, increased MAST was detectable between the moderate- and high-consumption groups. In the case of white bread consumption, the GLM attenuated the significance of the association detected by the KW, indicating a partial confounding effect by sex and recruitment centre.

Regarding cardiovascular risk biomarkers (Supplementary Table S9), serum triglycerides, low-density lipoprotein cholesterol (LDL-C) and fibrinogen showed a significant positive association with MAST, although the effect of the confounding variables attenuated the association of LDL-C in the GLM analysis.

In the analysis of the association of MAST with the expression of enzymes involved in the methylation/demethylation processes (Supplementary Table S10), a significant association was found for DNMT1, DNMT3A and TET3. MAST increased in the upper quantiles of DNMT1 and DNMT3A expression, while it decreased in the case of TET3.

Among haematological parameters (Supplementary Table S11), MAST was associated with peripheral blood lymphocyte and neutrophil count and with the lymphocyte to monocyte count ratio. Differences mainly concerned the 1st vs the 4th quartiles. This association was positive for the lymphocyte count and the lymphocyte/monocyte count ratio, while it was negative for neutrophils count.

Most of the reported MAST associations showed weak effect sizes, except for TET3 and DNMT3A expression that showed moderate and relatively strong effect sizes, respectively.

The contribution of selected variables on age-related changes in MAST in the RASIG and GO/SGO population

The variables found to be associated with MAST were next studied as potential causative factors in the association of MAST with age in RASIG and in its difference between the GO, SGO and RASIG groups.

Due to sample size limitations, data on DNMT3A, TET and TDG expression were excluded from the analyses.

The effect on the relationship between MAST and age in RASIG was examined by GLM analysis. The model tested MAST differences between the 10-year age strata, adjusted for all the factors that significantly affected MAST level as previously shown by both KW and GLM analyses (see Supplementary Tables S7–S11).

As shown in Table 5, none of the variables confounded the association of MAST with age groups, which, in fact, retained a highly significant p value (p < 0.001, see Table 2 for comparison) despite the inclusion of all the covariates. However, the DNMT1 transcript level and alcohol consumption seemed to have a certain weight in the model (Table 5).

Table 5 Contribution of selected variables and covariates on age-related changes of MAST in RASIG

Similar results were obtained by running several additional GLM models with the progressive inclusion of all the MAST-associated variables, categorised on the basis of having any significant association with MAST (i.e. also including variables showing significant interaction after the KW or GLM only) (Supplementary Table S12).

The crude models (models 1–4) included “standard” adjustment variables (recruitment centre, sex and lymphocyte to monocyte ratio). We next added to these crude models all the variables—one by one—associated with MAST either by both the GLM and KW tests (models 5–12) or by only one of the tests (models 14–19). The order in which the variables were added followed the criterion of obtaining the minimum reduction in the number of cases included in the model. Models 13, 20 and 21 accounted for the effect of all the potential confounding variables simultaneously. Models 20 and 21 differ for the inclusion of DNMT1 expression, which was the variable causing the greatest reduction in sample size.

No significant confounding effect on MAST variation across age groups was observed by any of the covariates. In fact, the association of MAST with age groups remained highly significant in all the tested models. Nevertheless, based on their significant p values, DNMT1, glucose, glycated haemoglobin and alcohol were found to be explanatory variables in the cumulative model (model 21) that contained all the other factors.

Conversely, the significance showed by other covariates (e.g. recruitment centre, sex, BMI, fibrinogen and LDL-C) in some of the models was dependent on the effect of other adjusting variables. In fact, their p value became non-significant in the cumulative models.

The same analyses were performed to test the variation of MAST between GO, SGO and RASIG.

The confounding effect of the factors associated with MAST in both the KW and GLM tests was negligible, both in the cumulative (Table 6) and in the stepwise analysis (Supplementary Table S13, models 1–14). The expression of DNMT1 and the lymphocyte to monocyte ratio were the covariates partially affecting MAST differences across subject groups (Table 6 and Supplementary Table S13, model 14). However, the significance of the association between MAST and subject groups was partially affected by the combination of all factors rather than by a single one (see the subject group p value in models 1–13 with respect to model 14 in the Supplementary Table S13).

Table 6 Contribution of selected variables and covariates on group-related (GO, SGO and RASIG) changes of MAST in individuals aged >54 years

Similar conclusions could be drawn from the analysis of factors associated with MAST by the KW or the GLM tests. Each additional factor was, by itself, ineffective in explaining MAST association with subject groups (Supplementary Table S13, models 15–20), but the inclusion of all factors made this relationship not significant (p value = 0.065 in model 22).

The loss of significance of subject groups seemed to be driven by two factors: (i) a drop in the sample size when DNMT1 expression was entered in the model and/or (ii) to a synergy between DNMT1 expression and other variables, such as the lymphocyte/monocyte ratio (see model 21 vs model 22).

After the removal of DNMT1, the association of MAST with the subject groups regained a borderline significance (p value = 0.045 in model 21). Compared to previous models, the decrease in significance for the subject groups in this model could be due to the confounding effect of BMI, glycated haemoglobin, French fries and glucose, as well as to a smaller sample size.

Discussion

Previous studies indicate the possibility that epigenetic changes occur at subtelomeric DNA regions in both physiological and abnormal ageing [19,20,21,22,23, 29, 42]. Here, this hypothesis has been tested in the context of a large-scale population-based study, which also provides a reference framework for factors that are associated with subtelomeric DNA methylation variation in the general population including demographics, clinical laboratory parameters, dietary and health habits. Furthermore, this study adopts the innovative approach of validating the identified putative subtelomeric methylation signature of ageing in highly informative groups represented by offspring of nonagenarians and subjects affected by Down syndrome, representing models of healthy ageing [43] and premature/accelerated ageing [44], respectively.

The method adopted for methylation analysis (EpiTYPER [38]) enabled us to get a quantitative measure of subtelomeric DNA methylation in blood mononucleated cells, largely at single-nucleotide resolution. Data obtained provided an unprecedented opportunity to systematically analyse the subtelomeric methylation profile and its variation with age in the general population.

The CpGs showed an intermediate level of methylation possibly reflecting an epigenetic heterogeneity across principal immune cells that form the PBMC population. However, this heterogeneity may also conform to variation within cell types, since varying degrees of subtelomeric methylation were reported in other studies even in cultured primary cells [45].

Nevertheless, each CpG site showed a limited range of methylation variation, thus forming a methylation pattern that appeared to be specific to the subtelomeric region. The methylation profile of subtelomeres seems therefore to be controlled by specific mechanisms and might reflect certain functions as it has recently been proposed for other regions showing intermediate methylation states in the human genome [46]. CpG methylation levels increased with age at almost all the assessed CpG sites. Moreover, the rate of increase of methylation with age seems to be similar across the different CpG sites. Consequently, the average methylation of the entire subtelomeric region increases without significant changes in its variability. This suggests that age-related hypermethylation of subtelomeres does not evolve randomly, unlike many other age-associated differentially methylated regions, where ageing is associated with an entropic decay of the epigenetic profile [47].

Overall, these findings contrast with previous results showing an age-related hypomethylation of global subtelomeric regions in blood from healthy individuals [29] and patients affected by age-related diseases such as Parkinson’s disease [21]. There are several possible explanations for this discrepancy. Firstly, compared to Maeda et al. [29], our cohort of cases was significantly more extensive and representative of a different and more heterogeneous geographical area. Secondly, we adopted an analytical method that has an advantage over the methylation-sensitive Southern blot assay used by Maeda et al., both in terms of quantitative accuracy and the number of CpG sites that can be assessed individually. Finally, we focused on two specific subtelomeric regions, while Maeda et al. evaluated the global methylation status of subtelomeres. This last point is of particular relevance since the methylation status of a subtelomeric region and its variation with age may depend on its specific chromosomal context, including the length of the adjacent telomere end. It is, therefore, possible that the increase in methylation with age reported here for 5p and 21q subtelomeric regions reflects their specific chromosomal context and represents the trend of a specific subset of the telomeres.

DNA methylation appears to change at a constant rate across age groups, indicating a linear relationship with chronological age. Regression analyses actually show a significant direct correlation between age and methylation level for all CpG sites. However, the proportion of methylation variation explained by age was small for every single site. By contrast, a subtelomeric DNA methylation index (MAST) based on the aggregate methylation status of all CpG sites provided a better fit with age and outperformed every single site in discriminating between age groups. Biologically, this suggests that the amount that each CpG methylation contributes to age is additive and/or that additional information may come from the effects of age on the DNA methylation pattern of the whole subtelomeric region.

This point should also be taken into account when interpreting the negative correlation between MAST and the average length of the bulk telomere population shown in Supplementary Table S6. These results are consistent with previous observations linking a loss of subtelomeric methylation to telomere elongation [6, 7] and suggest that subtelomeric DNA hypermethylation is related to telomere shortening in ageing. However, this association might not involve all of the subtelomeres. In fact, it has been suggested that the correlation between subtelomeric methylation and telomere length is variable, in terms of both strength and direction, across different chromosomes and/or different regions of the same subtelomere [27]. This insight could also offer a plausible explanation for the observation that the amount of the telomere length variation explained by MAST is relatively small.

Remarkably, MAST was more correlated with age than with telomere length. This finding suggests that part of the DNA methylation ‘signature’ of age in subtelomeres is not related to telomere length control. DNA methylation could also affect the expression of genes related to ageing via the telomere position effect (TPE) [48] and/or by controlling transcription of the non-coding telomeric RNAs (TERRA), recently described as trans-acting epigenetic modulators of multiple genes throughout the genome [49].

The trend of MAST in the GO and DS with respect to RASIG further supports a link of subtelomeric methylation and the ageing process. Higher MAST in DS is compatible with the accelerated ageing phenotype of this syndrome and mirrors previous data indicating that telomere length maintenance processes are impaired in DS [50, 51]. In contrast, lower MAST in GO is in agreement with the notion that offspring of long-lived parents show slower ageing [43, 52] and improved telomere length maintenance [53,54,55] compared to normal ageing subjects.

To investigate possible sources of variation of MAST in the general population, we next adopted a multidimensional approach that integrates demographic, dietary/lifestyle and clinical data.

Concerning demographic variables, a variation of MAST was found by country. This association, which was predominantly driven by samples from Austria, seems to be spurious and generated by the effect of third variables (e.g. age, BMI, alcohol and white bread consumption; see Table S12).

Although nutritional and lifestyle factors are believed to be significant modifiers of epigenetic patterns, MAST was independent of most of them except for the consumption of white bread and alcoholic beverages.

The positive relationship between white bread consumption and MAST is difficult to interpret since there are no previous reports regarding this association. However, there is initial evidence that dietary patterns, typified by higher intakes of refined grains, are associated with DNA methylation alterations [56] and telomere shortening [57]. The possible underlying mechanisms include epigenetic alterations induced by higher oxidative stress or an imbalanced supply of nutrients that act as methyl donors or cofactors in the one-carbon metabolism pathway.

The association of MAST with alcohol consumption is in line with previous observations [58, 59] and further supports the idea that chronic alcohol consumption influences genomic DNA methylation pattern. Within subtelomeric DNA, alcohol-induced hypermethylation is likely to have an impact on the telomere length homeostasis. In fact, subtelomeric DNA hypermethylation has been associated with telomere shortening in ethanol-treated cells [60].

A multitude of studies indicate a relationship between telomere shortening in blood cells and dyslipidaemia- and hyperglycaemia-related diseases (reviewed in [61]). Furthermore, recent follow-up studies have advocated that telomere shortening is a long-term marker of cellular ageing, illustrating a chronic deterioration of a person’s metabolic health [62]. In this context, the positive association of MAST with total blood triglycerides and LDL cholesterol is likely to be a reflection of an underlying mechanism translating the increased cell damage and turnover that are secondary to elevated blood lipid levels, to shortened telomere length [62,63,64].

Similarly, the positive association of MAST with fibrinogen levels is in agreement with previous studies that report shorter telomeres in the blood cells of individuals with higher levels of fibrinogen, an association that probably reflects cardiovascular ageing [65, 66].

The positive association of MAST with DNMT1 and DNMT3A and its negative association with TET3 transcript levels suggest that the age-associated methylation increase of the two subtelomeric regions reflects in part expression changes of components of the DNA methylation/demethylation machinery [36, 67]. This possibility is in line with previous data showing that the modulation of the DNMT and TET expression has an impact on subtelomeric methylation status [6, 68,69,70].

Finally, the association of MAST with specific white blood cell counts may reflect pieces of evidence that white blood cell types have different rates of telomere length changes with age, which would imply differential age-related subtelomeric methylation changes in individual cell types. Specifically, the positive association of MAST with lymphocyte counts agrees with previous findings showing that this leucocyte subpopulation (especially the B-cells) exhibits higher rates of telomere loss with ageing compared to other components of the PBMC [71]. It cannot be ruled out, however, that associations between MAST and white blood cell counts are also influenced by the effect of ageing on lymphocyte subpopulation numbers. The age-related decrease of lymphocyte counts [71, 72] may be an additional mediating factor in the MAST–lymphocyte count association. The inverse association of MAST with neutrophils, which are not part of the PBMC fraction where MAST was measured, may reflect their decrease in numbers with ageing [72].

After the identification of factors associated with MAST variations in the general population, we then sought to determine their impact on the differences in MAST between age groups. The results showed that, although all the critical variables were taken into account in the analysis, the differences of MAST between the age groups were still significant (Supplementary Table S12). This would indicate that age predicts subtelomeric DNA methylation changes in PBMC as an almost independent variable with respect to all other variables and factors evaluated here. This result may be reminiscent of recent data showing that age-related changes of specific CpGs in blood, which are part of Horvath’s epigenetic ageing clock (Horvath’s pan tissue 353 CpG site clock [73]), primarily reflect cell-intrinsic properties [74, 75]. In contrast, the influence of “extrinsic” factors is weak, but it is nevertheless driven by multiple environmental and lifestyle factors [76]. Nevertheless, none of Horvath’s epigenetic clock CpGs is located in or near the subtelomeric regions here analysed. This points to the existence of different pathways/mechanisms underlying the clock and the epigenetic ageing of the subtelomeres, as suggested by the observation that the length of telomeres and the Horvath’s epigenetic clock are independently associated with chronological age and do not correlate with each other [77].

This analysis also confirmed alcohol consumption, the expression of DNMT1, blood levels of glycated haemoglobin and glucose as important explanatory factors. All other factors were not associated with MAST in the GLM or olny indirectly linked to it. For example, recruitment centre and sex seem to have an effect on MAST through other exogenous variables, including dietary/lifestyle factors (i.e. alcohol and white bread consumption), markers of carbohydrates (i.e. serum glucose level) and lipid metabolism (i.e. blood levels of LDL cholesterol, triglycerides and free fatty acids).

On the other hand, the differences in MAST between GO, SGO and RASIG seem to depend on multiple factors, ranging from dietary habits (i.e. French fries consumption) and metabolic fitness markers (i.e. BMI and blood levels of glycated haemoglobin and glucose) to molecular markers (i.e. DNMT1 expression).

These data suggest that if a more efficient control of the epigenetic status of the subtelomeres represents a further element of the advantages that predispose the GO to healthy ageing, this could be related to a peculiar physiology that confers to the offspring of long-lived subjects favourable body anthropometrical characteristics [78] and better glucose handling [79, 80].

Collectively, results from this study confirm in large-scale population settings that ageing has an impact on the methylation profile of subtelomeric DNA. These data, together with the identification of factors that are associated with subtelomeric DNA methylation variation, could be helpful for future research aimed at understanding the mechanisms underlying the ageing process.

Data availability

The data that support the findings of this study are available from the authors upon reasonable request.

References

  1. 1.

    Linardopoulou EV, Williams EM, Fan Y, Friedman C, Young JM, Trask BJ. Human subtelomeres are hot spots of interchromosomal recombination and segmental duplication. Nature. 2005;437(7055):94–100.

    CAS  PubMed  PubMed Central  Google Scholar 

  2. 2.

    Mefford HC, Trask BJ. The complex structure and dynamic evolution of human subtelomeres. Nature reviews. 2002;3(2):91–102.

    CAS  PubMed  Google Scholar 

  3. 3.

    Riethman H, Ambrosini A, Paul S. Human subtelomere structure and variation. Chromosom Res. 2005;13(5):505–15.

    CAS  Google Scholar 

  4. 4.

    Blasco MA. The epigenetic regulation of mammalian telomeres. Nature reviews. 2007;8(4):299–309.

    CAS  PubMed  Google Scholar 

  5. 5.

    Mikkelsen TS, Ku M, Jaffe DB, Issac B, Lieberman E, Giannoukos G, et al. Genome-wide maps of chromatin state in pluripotent and lineage-committed cells. Nature. 2007;448(7153):553–60.

    CAS  PubMed  PubMed Central  Google Scholar 

  6. 6.

    Gonzalo S, Jaco I, Fraga MF, Chen T, Li E, Esteller M, et al. DNA methyltransferases control telomere length and telomere recombination in mammalian cells. Nat Cell Biol. 2006;8(4):416–24.

    CAS  PubMed  Google Scholar 

  7. 7.

    Vera E, Canela A, Fraga MF, Esteller M, Blasco MA. Epigenetic regulation of telomeres in human cancer. Oncogene. 2008;27(54):6817–33.

    CAS  PubMed  Google Scholar 

  8. 8.

    Feil R, Fraga MF. Epigenetics and the environment: emerging patterns and implications. Nature reviews. 2012;13(2):97–109.

    CAS  PubMed  Google Scholar 

  9. 9.

    Schubeler D. Function and information content of DNA methylation. Nature. 2015;517(7534):321–6.

    CAS  PubMed  Google Scholar 

  10. 10.

    Lopez-Otin C, Blasco MA, Partridge L, Serrano M, Kroemer G. The hallmarks of aging. Cell. 2013;153(6):1194–217.

    CAS  PubMed  PubMed Central  Google Scholar 

  11. 11.

    Ciccarone F, Tagliatesta S, Caiafa P, Zampieri M. DNA methylation dynamics in aging: how far are we from understanding the mechanisms? Mech Ageing Dev. 2018;174:3–17.

    CAS  PubMed  Google Scholar 

  12. 12.

    Pal S, Tyler JK. Epigenetics and aging. Sci Adv. 2016;2(7):e1600584.

    PubMed  PubMed Central  Google Scholar 

  13. 13.

    Bell CG, Lowe R, Adams PD, Baccarelli AA, Beck S, Bell JT, et al. DNA methylation aging clocks: challenges and recommendations. Genome Biol. 2019;20(1):249.

    PubMed  PubMed Central  Google Scholar 

  14. 14.

    Horvath S, Raj K. DNA methylation-based biomarkers and the epigenetic clock theory of ageing. Nature reviews. 2018;19(6):371–84.

    CAS  PubMed  Google Scholar 

  15. 15.

    Zhang Q, Vallerga CL, Walker RM, Lin T, Henders AK, Montgomery GW, et al. Improved precision of epigenetic clock estimates across tissues and its implication for biological ageing. Genome medicine. 2019;11(1):54.

    CAS  PubMed  PubMed Central  Google Scholar 

  16. 16.

    Levine ME, Lu AT, Quach A, Chen BH, Assimes TL, Bandinelli S, et al. An epigenetic biomarker of aging for lifespan and healthspan. Aging. 2018;10(4):573–91.

    PubMed  PubMed Central  Google Scholar 

  17. 17.

    Hu H, Li B, Duan S. The alteration of subtelomeric DNA methylation in aging-related diseases. Front Genet. 2019;9:697.

    PubMed  PubMed Central  Google Scholar 

  18. 18.

    Buxton JL, Suderman M, Pappas JJ, Borghol N, McArdle W, Blakemore AI, et al. Human leukocyte telomere length is associated with DNA methylation levels in multiple subtelomeric and imprinted loci. Sci Rep. 2014;4:4954.

    CAS  PubMed  PubMed Central  Google Scholar 

  19. 19.

    Guan JZ, Guan WP, Maeda T, Makino N. The subtelomere of short telomeres is hypermethylated in Alzheimer’s disease. Aging Dis. 2012;3(2):164–70.

    PubMed  Google Scholar 

  20. 20.

    Guan JZ, Guan WP, Maeda T, Makino N. Analysis of telomere length and subtelomeric methylation of circulating leukocytes in women with Alzheimer’s disease. Aging Clin Exp Res. 2013;25(1):17–23.

    PubMed  Google Scholar 

  21. 21.

    Maeda T, Guan JZ, Koyanagi M, Higuchi Y, Makino N. Aging-associated alteration of telomere length and subtelomeric status in female patients with Parkinson’s disease. J Neurogenet. 2012;26(2):245–51.

    CAS  PubMed  Google Scholar 

  22. 22.

    Maeda T, Guan JZ, Oyama J, Higuchi Y, Makino N. Aging-associated alteration of subtelomeric methylation in Parkinson’s disease. J Gerontol A Biol Sci Med Sci. 2009;64(9):949–55.

    PubMed  Google Scholar 

  23. 23.

    Makino N, Maeda T, Abe N. Short telomere subtelomeric hypomethylation is associated with telomere attrition in elderly diabetic patients. Can J Physiol Pharmacol. 2019;97(4):335–9.

    CAS  PubMed  Google Scholar 

  24. 24.

    Choudhury SR, Cui Y, Milton JR, Li J, Irudayaraj J. Selective increase in subtelomeric DNA methylation: an epigenetic biomarker for malignant glioma. Clin Epigenetics. 2015;7:107.

    PubMed  PubMed Central  Google Scholar 

  25. 25.

    Han Y, Xu J, Kim J, Wu X, Gu J. Methylation of subtelomeric repeat D4Z4 in peripheral blood leukocytes is associated with biochemical recurrence in localized prostate cancer patients. Carcinogenesis. 2017;38(8):821–6.

    CAS  PubMed  PubMed Central  Google Scholar 

  26. 26.

    Lee ME, Rha SY, Jeung HC, Chung HC, Oh BK. Subtelomeric DNA methylation and telomere length in human cancer cells. Cancer Lett. 2009;281(1):82–91.

    CAS  PubMed  Google Scholar 

  27. 27.

    Oh BK, Um TH, Choi GH, Park YN. Frequent changes in subtelomeric DNA methylation patterns and its relevance to telomere regulation during human hepatocarcinogenesis. Int J Cancer. 2011;128(4):857–68.

    CAS  PubMed  Google Scholar 

  28. 28.

    Xu J, Tsai CW, Chang WS, Han Y, Bau DT, Pettaway CA, et al. Methylation of global DNA repeat LINE-1 and subtelomeric DNA repeats D4Z4 in leukocytes is associated with biochemical recurrence in African American prostate cancer patients. Carcinogenesis. 2019;40:1055–60.

    CAS  Google Scholar 

  29. 29.

    Maeda T, Guan JZ, Oyama J, Higuchi Y, Makino N. Age-related changes in subtelomeric methylation in the normal Japanese population. J Gerontol A Biol Sci Med Sci. 2009;64(4):426–34.

    PubMed  Google Scholar 

  30. 30.

    Burkle A, Moreno-Villanueva M, Bernhard J, Blasco M, Zondag G, Hoeijmakers JH, et al. MARK-AGE biomarkers of ageing. Mech Ageing Dev. 2015;151:2–12.

    PubMed  Google Scholar 

  31. 31.

    Capri M, Moreno-Villanueva M, Cevenini E, Pini E, Scurti M, Borelli V, et al. MARK-AGE population: from the human model to new insights. Mech Ageing Dev. 2015;151:13–7.

    PubMed  Google Scholar 

  32. 32.

    Moreno-Villanueva M, Kotter T, Sindlinger T, Baur J, Oehlke S, Burkle A, et al. The MARK-AGE phenotypic database: structure and strategy. Mech Ageing Dev. 2015;151:26–30.

    PubMed  Google Scholar 

  33. 33.

    Moreno-Villanueva M, Capri M, Breusing N, Siepelmeyer A, Sevini F, Ghezzo A, et al. MARK-AGE standard operating procedures (SOPs): a successful effort. Mech Ageing Dev. 2015;151:18–25.

    PubMed  Google Scholar 

  34. 34.

    Baur J, Kotter T, Moreno-Villanueva M, Sindlinger T, Berthold MR, Burkle A, et al. The MARK-AGE extended database: data integration and pre-processing. Mech Ageing Dev. 2015;151:31–7.

    CAS  PubMed  Google Scholar 

  35. 35.

    Baur J, Moreno-Villanueva M, Kotter T, Sindlinger T, Burkle A, Berthold MR, et al. MARK-AGE data management: cleaning, exploration and visualization of data. Mech Ageing Dev. 2015;151:38–44.

    PubMed  Google Scholar 

  36. 36.

    Ciccarone F, Malavolta M, Calabrese R, Guastafierro T, Bacalini MG, Reale A, et al. Age-dependent expression of DNMT1 and DNMT3B in PBMCs from a large European population enrolled in the MARK-AGE study. Aging Cell. 2016;15(4):755–65.

    CAS  PubMed  PubMed Central  Google Scholar 

  37. 37.

    Zampieri M, Ciccarone F, Palermo R, Cialfi S, Passananti C, Chiaretti S, et al. The epigenetic factor BORIS/CTCFL regulates the NOTCH3 gene expression in cancer cells. Biochim Biophys Acta. 2014;1839(9):813–25.

    CAS  PubMed  Google Scholar 

  38. 38.

    Suchiman HE, Slieker RC, Kremer D, Slagboom PE, Heijmans BT, Tobi EW. Design, measurement and processing of region-specific DNA methylation assays: the mass spectrometry-based method EpiTYPER. Front Genet. 2015;6:287.

    PubMed  PubMed Central  Google Scholar 

  39. 39.

    Franceschi C, Bezrukov V, Blanche H, Bolund L, Christensen K, de Benedictis G, et al. Genetics of healthy aging in Europe: the EU-integrated project GEHA (GEnetics of Healthy Aging). Ann N Y Acad Sci. 2007;1100:21–45.

    CAS  PubMed  Google Scholar 

  40. 40.

    Ambrosini A, Paul S, Hu S, Riethman H. Human subtelomeric duplicon structure and organization. Genome Biol. 2007;8(7):R151.

    PubMed  PubMed Central  Google Scholar 

  41. 41.

    Young E, Abid HZ, Kwok PY, Riethman H, Xiao M. Comprehensive analysis of human subtelomeres by whole genome mapping. PLoS Genet. 2020;16(1):e1008347.

    PubMed  PubMed Central  Google Scholar 

  42. 42.

    Maeda T, Guan JZ, Higuchi Y, Oyama J, Makino N. Aging-related alterations of subtelomeric methylation in sarcoidosis patients. J Gerontol A Biol Sci Med Sci. 2009;64(7):752–60.

    PubMed  Google Scholar 

  43. 43.

    Atzmon G, Rincon M, Rabizadeh P, Barzilai N. Biological evidence for inheritance of exceptional longevity. Mech Ageing Dev. 2005;126(2):341–5.

    CAS  PubMed  Google Scholar 

  44. 44.

    Patterson D, Cabelof DC. Down syndrome as a model of DNA polymerase beta haploinsufficiency and accelerated aging. Mech Ageing Dev. 2012;133(4):133–7.

    CAS  PubMed  Google Scholar 

  45. 45.

    Yehezkel S, Rebibo-Sabbah A, Segev Y, Tzukerman M, Shaked R, Huber I, et al. Reprogramming of telomeric regions during the generation of human induced pluripotent stem cells and subsequent differentiation into fibroblast-like derivatives. Epigenetics. 2011;6(1):63–75.

    CAS  PubMed  PubMed Central  Google Scholar 

  46. 46.

    Elliott G, Hong C, Xing X, Zhou X, Li D, Coarfa C, et al. Intermediate DNA methylation is a conserved signature of genome regulation. Nat Commun. 2015;6:6363.

    CAS  PubMed  PubMed Central  Google Scholar 

  47. 47.

    Slieker RC, van Iterson M, Luijk R, Beekman M, Zhernakova DV, Moed MH, et al. Age-related accrual of methylomic variability is linked to fundamental ageing mechanisms. Genome Biol. 2016;17(1):191.

    PubMed  PubMed Central  Google Scholar 

  48. 48.

    Robin JD, Ludlow AT, Batten K, Magdinier F, Stadler G, Wagner KR, et al. Telomere position effect: regulation of gene expression with progressive telomere shortening over long distances. Genes Dev. 2014;28(22):2464–76.

    PubMed  PubMed Central  Google Scholar 

  49. 49.

    Chu HP, Cifuentes-Rojas C, Kesner B, Aeby E, Lee HG, Wei C, et al. TERRA RNA antagonizes ATRX and protects telomeres. Cell. 2017;170(1):86–101 e16.

    CAS  PubMed  PubMed Central  Google Scholar 

  50. 50.

    Brando B, Longo A, Beltrami B, Passoni D, Verna R, Licastro F, et al. Determination of telomere length by flow-fluorescence in situ hybridization in Down’s syndrome patients. Int J Tissue React. 2004;26(1–2):61–4.

    CAS  PubMed  Google Scholar 

  51. 51.

    Vaziri H, Schachter F, Uchida I, Wei L, Zhu X, Effros R, et al. Loss of telomeric DNA during aging of normal and trisomy 21 human lymphocytes. Am J Hum Genet. 1993;52(4):661–7.

    CAS  PubMed  PubMed Central  Google Scholar 

  52. 52.

    Horvath S, Pirazzini C, Bacalini MG, Gentilini D, Di Blasio AM, Delledonne M, et al. Decreased epigenetic age of PBMCs from Italian semi-supercentenarians and their offspring. Aging. 2015;7(12):1159–70.

    CAS  PubMed  PubMed Central  Google Scholar 

  53. 53.

    Arai Y, Martin-Ruiz CM, Takayama M, Abe Y, Takebayashi T, Koyasu S, et al. Inflammation, but not telomere length, predicts successful ageing at extreme old age: a longitudinal study of semi-supercentenarians. EBioMedicine. 2015;2(10):1549–58.

    PubMed  PubMed Central  Google Scholar 

  54. 54.

    Atzmon G, Cho M, Cawthon RM, Budagov T, Katz M, Yang X, et al. Evolution in health and medicine Sackler colloquium: genetic variation in human telomerase is associated with telomere length in Ashkenazi centenarians. Proc Natl Acad Sci U S A. 2010;107(Suppl 1):1710–7.

    CAS  PubMed  Google Scholar 

  55. 55.

    Tedone E, Arosio B, Gussago C, Casati M, Ferri E, Ogliari G, et al. Leukocyte telomere length and prevalence of age-related diseases in semisupercentenarians, centenarians and centenarians’ offspring. Exp Gerontol. 2014;58:90–5.

    CAS  PubMed  Google Scholar 

  56. 56.

    Colacino JA, Arthur AE, Dolinoy DC, Sartor MA, Duffy SA, Chepeha DB, et al. Pretreatment dietary intake is associated with tumor suppressor DNA methylation in head and neck squamous cell carcinomas. Epigenetics. 2012;7(8):883–91.

    CAS  PubMed  PubMed Central  Google Scholar 

  57. 57.

    Garcia-Calzon S, Moleres A, Martinez-Gonzalez MA, Martinez JA, Zalba G, Marti A. Dietary total antioxidant capacity is associated with leukocyte telomere length in a children and adolescent population. Clin Nutr. 2015;34(4):694–9.

    CAS  PubMed  Google Scholar 

  58. 58.

    Liu C, Marioni RE, Hedman AK, Pfeiffer L, Tsai PC, Reynolds LM, et al. A DNA methylation biomarker of alcohol consumption. Mol Psychiatry. 2018;23(2):422–33.

    CAS  PubMed  Google Scholar 

  59. 59.

    Wilson LE, Xu Z, Harlid S, White AJ, Troester MA, Sandler DP, et al. Alcohol and DNA methylation: an epigenome-wide association study in blood and normal breast tissue. Am J Epidemiol. 2019;188(6):1055–65.

    PubMed  PubMed Central  Google Scholar 

  60. 60.

    Harpaz T, Abumock H, Beery E, Edel Y, Lahav M, Rozovski U, et al. The effect of ethanol on telomere dynamics and regulation in human cells. Cells. 2018;7(10).

  61. 61.

    Kirchner H, Shaheen F, Kalscheuer H, Schmid SM, Oster H, Lehnert H. The telomeric complex and metabolic disease. Genes (Basel). 2017;8(7).

  62. 62.

    Revesz D, Milaneschi Y, Verhoeven JE, Penninx BW. Telomere length as a marker of cellular aging is associated with prevalence and progression of metabolic syndrome. J Clin Endocrinol Metab. 2014;99(12):4607–15.

    CAS  PubMed  Google Scholar 

  63. 63.

    Harte AL, da Silva NF, Miller MA, Cappuccio FP, Kelly A, O’Hare JP, et al. Telomere length attrition, a marker of biological senescence, is inversely correlated with triglycerides and cholesterol in South Asian males with type 2 diabetes mellitus. Exp Diabetes Res. 2012;2012:895185.

    PubMed  PubMed Central  Google Scholar 

  64. 64.

    Weischer M, Bojesen SE, Cawthon RM, Freiberg JJ, Tybjaerg-Hansen A, Nordestgaard BG. Short telomere length, myocardial infarction, ischemic heart disease, and early death. Arterioscler Thromb Vasc Biol. 2012;32(3):822–9.

    CAS  PubMed  Google Scholar 

  65. 65.

    Masi S, Nightingale CM, Day IN, Guthrie P, Rumley A, Lowe GD, et al. Inflammation and not cardiovascular risk factors is associated with short leukocyte telomere length in 13- to 16-year-old adolescents. Arterioscler Thromb Vasc Biol. 2012;32(8):2029–34.

    CAS  PubMed  Google Scholar 

  66. 66.

    von Kanel R, Malan NT, Hamer M, van der Westhuizen FH, Malan L. Leukocyte telomere length and hemostatic factors in a South African cohort: the SABPA Study. J Thromb Haemost. 2014;12(12):1975–85.

    Google Scholar 

  67. 67.

    Valentini E, Zampieri M, Malavolta M, Bacalini MG, Calabrese R, Guastafierro T, et al. Analysis of the machinery and intermediates of the 5hmC-mediated DNA demethylation pathway in aging on samples from the MARK-AGE Study. Aging. 2016;8(9):1896–922.

    CAS  PubMed  PubMed Central  Google Scholar 

  68. 68.

    El-Maarri O, Kareta MS, Mikeska T, Becker T, Diaz-Lacava A, Junen J, et al. A systematic search for DNA methyltransferase polymorphisms reveals a rare DNMT3L variant associated with subtelomeric hypomethylation. Hum Mol Genet. 2009;18(10):1755–68.

    CAS  PubMed  Google Scholar 

  69. 69.

    Yang J, Guo R, Wang H, Ye X, Zhou Z, Dan J, et al. Tet enzymes regulate telomere maintenance and chromosomal stability of mouse ESCs. Cell Rep. 2016;15(8):1809–21.

    CAS  PubMed  Google Scholar 

  70. 70.

    Yehezkel S, Segev Y, Viegas-Pequignot E, Skorecki K, Selig S. Hypomethylation of subtelomeric regions in ICF syndrome is associated with abnormally short telomeres and enhanced transcription from telomeric regions. Hum Mol Genet. 2008;17(18):2776–89.

    CAS  PubMed  Google Scholar 

  71. 71.

    Lin Y, Damjanovic A, Metter EJ, Nguyen H, Truong T, Najarro K, et al. Age-associated telomere attrition of lymphocytes in vivo is co-ordinated with changes in telomerase activity, composition of lymphocyte subsets and health conditions. Clin Sci (Lond). 2015;128(6):367–77.

    CAS  Google Scholar 

  72. 72.

    Valiathan R, Ashman M, Asthana D. Effects of ageing on the immune system: infants to elderly. Scand J Immunol. 2016;83(4):255–66.

    CAS  PubMed  Google Scholar 

  73. 73.

    Horvath S. DNA methylation age of human tissues and cell types. Genome Biol. 2013;14(10):R115.

    PubMed  PubMed Central  Google Scholar 

  74. 74.

    Matsuyama M, WuWong DJ, Horvath S, Matsuyama S. Epigenetic clock analysis of human fibroblasts in vitro: effects of hypoxia, donor age, and expression of hTERT and SV40 largeT. Aging. 2019;11(10):3012–22.

    CAS  PubMed  PubMed Central  Google Scholar 

  75. 75.

    Soraas A, Matsuyama M, de Lima M, Wald D, Buechner J, Gedde-Dahl T, et al. Epigenetic age is a cell-intrinsic property in transplanted human hematopoietic cells. Aging Cell. 2019;18(2):e12897.

    PubMed  PubMed Central  Google Scholar 

  76. 76.

    Quach A, Levine ME, Tanaka T, Lu AT, Chen BH, Ferrucci L, et al. Epigenetic clock analysis of diet, exercise, education, and lifestyle factors. Aging. 2017;9(2):419–46.

    CAS  PubMed  PubMed Central  Google Scholar 

  77. 77.

    Marioni RE, Harris SE, Shah S, McRae AF, von Zglinicki T, Martin-Ruiz C, et al. The epigenetic clock and telomere length are independently associated with chronological age and mortality. Int J Epidemiol. 2018;45(2):424–32.

    PubMed  Google Scholar 

  78. 78.

    Bucci L, Ostan R, Cevenini E, Pini E, Scurti M, Vitale G, et al. Centenarians’ offspring as a model of healthy aging: a reappraisal of the data on Italian subjects and a comprehensive overview. Aging. 2016;8(3):510–9.

    PubMed  PubMed Central  Google Scholar 

  79. 79.

    Rozing MP, Westendorp RG, de Craen AJ, Frolich M, de Goeij MC, Heijmans BT, et al. Favorable glucose tolerance and lower prevalence of metabolic syndrome in offspring without diabetes mellitus of nonagenarian siblings: the Leiden longevity study. J Am Geriatr Soc. 2010;58(3):564–9.

    PubMed  Google Scholar 

  80. 80.

    Wijsman CA, Rozing MP, Streefland TC, le Cessie S, Mooijaart SP, Slagboom PE, et al. Familial longevity is marked by enhanced insulin sensitivity. Aging Cell. 2011;10(1):114–21.

    CAS  Google Scholar 

Download references

Acknowledgements

The authors thank the MARK-AGE subjects for participating in this study and all members of the MARK-AGE Consortium for fruitful discussion and collaboration.

Code availability

Not applicable.

Funding

Open access funding provided by Università  degli Studi di Roma La Sapienza within the CRUI-CARE Agreement. This work was financially supported by the European Union’s Seventh Framework Program, grant no. HEALTH-F4-2008-200880 MARK-AGE.

Author information

Affiliations

Authors

Contributions

MZ, PC and MGB designed the research; MGB, FC and MMB carried out the laboratory analyses; BGL recruited subjects from Austria, OT and FDC from Belgium, CS and JB from Germany, PES from the Netherlands, ESG from Greece, MC and CF from Italy, ES from Poland, AH and MH from Finland; NB and TG managed the Biobank; MZ, PC, MM, AR, FC, METD, EJ, MAB and MGB analysed and discussed the data; MM, ST and VA performed the statistical analysis; MMV was involved in database management; MZ and AR wrote the manuscript; AB coordinated the MARK-AGE project and edited the manuscript.

Corresponding authors

Correspondence to Paola Caiafa or Michele Zampieri.

Ethics declarations

Ethics approval

The study was approved by the local ethics committees of each recruiting centre. The local ethics committees’ approval for the recruitment of Italian participants in the MARK-AGE project was obtained by S. Orsola-Malipighi Hospital Committee (approved the project on 24/06/2008 code no. 75/2008/U/Tess) and AUSL—Independent Ethical Committee (Emilia-Romagna Region) approved on 01/04/2009—Prot num 346/CE; CE: 09007.

Consent to participate

Not applicable.

Consent for publication

All the authors provided written consent for publication.

Competing interests

The authors declare no competing interests.

Additional information

Publisher’s note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Olivier Toussaint is deceased.

Supplementary information

ESM 1

(DOCX 15 kb)

ESM 2

(PDF 537 kb)

Rights and permissions

This article is published under an open access license. Please check the 'Copyright Information' section either on this page or in the PDF for details of this license and what re-use is permitted. If your intended use exceeds what is permitted by the license or if you are unable to locate the licence and re-use information, please contact the Rights and Permissions team.

About this article

Verify currency and authenticity via CrossMark

Cite this article

Bacalini, M.G., Reale, A., Malavolta, M. et al. Ageing affects subtelomeric DNA methylation in blood cells from a large European population enrolled in the MARK-AGE study. GeroScience 43, 1283–1302 (2021). https://doi.org/10.1007/s11357-021-00347-9

Download citation

Keywords

  • Ageing
  • Subtelomere
  • Epigenetics
  • DNA methylation
  • Down syndrome
  • Centenarian offspring