|Different measures of "genome-wide" DNA methylation exhibit unique properties in placental and somatic tissues.|
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|PMID: 22531475 Owner: NLM Status: MEDLINE|
|DNA methylation of CpGs located in two types of repetitive elements-LINE1 (L1) and Alu-is used to assess "global" changes in DNA methylation in studies of human disease and environmental exposure. L1 and Alu contribute close to 30% of all base pairs in the human genome and transposition of repetitive elements is repressed through DNA methylation. Few studies have investigated whether repetitive element DNA methylation is associated with DNA methylation at other genomic regions, or the biological and technical factors that influence potential associations. Here, we assess L1 and Alu DNA methylation by Pyrosequencing of consensus sequences and using subsets of probes included in the Illumina Infinium HumanMethylation27 BeadChip array. We show that evolutionary age and assay method affect the assessment of repetitive element DNA methylation. Additionally, we compare Pyrosequencing results for repetitive elements to average DNA methylation of CpG islands, as assessed by array probes classified into strong, weak and non-islands. We demonstrate that each of these dispersed sequences exhibits different patterns of tissue-specific DNA methylation. Correlation of DNA methylation suggests an association between L1 and weak CpG island DNA methylation in some of the tissues examined. We caution, however, that L1, Alu and CpG island DNA methylation are distinct measures of dispersed DNA methylation and one should not be used in lieu of another. Analysis of DNA methylation data is complex and assays may be influenced by environment and pathology in different or complementary ways.|
|E Magda Price; Allison M Cotton; Maria S Peñaherrera; Deborah E McFadden; Michael S Kobor; Wendy Robinson|
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|Type: Journal Article; Research Support, Non-U.S. Gov't Date: 2012-06-01|
|Title: Epigenetics : official journal of the DNA Methylation Society Volume: 7 ISSN: 1559-2308 ISO Abbreviation: Epigenetics Publication Date: 2012 Jun|
|Created Date: 2012-07-03 Completed Date: 2012-11-09 Revised Date: 2013-06-25|
Medline Journal Info:
|Nlm Unique ID: 101265293 Medline TA: Epigenetics Country: United States|
|Languages: eng Pagination: 652-63 Citation Subset: IM|
|Department of Obstetrics and Gynaecology, University of British Columbia, Vancouver, BC, Canada.|
|APA/MLA Format Download EndNote Download BibTex|
Blood / metabolism
Embryonic Development / genetics
Fetus / metabolism
Gene Expression Regulation, Developmental*
High-Throughput Nucleotide Sequencing
Long Interspersed Nucleotide Elements
Placenta / metabolism
|//Canadian Institutes of Health Research|
|Epigenetics. 2012 Jul;7(7):796
Journal ID (nlm-ta): Epigenetics
Journal ID (iso-abbrev): Epigenetics
Journal ID (publisher-id): EPI
Publisher: Landes Bioscience
Copyright © 2012 Landes Bioscience
Print publication date: Day: 01 Month: 6 Year: 2012
pmc-release publication date: Day: 01 Month: 6 Year: 2012
Volume: 7 Issue: 6
First Page: 652 Last Page: 663
PubMed Id: 22531475
Publisher Id: 2012EPI0053R
Publisher Item Identifier: 20221
|Different measures of “genome-wide” DNA methylation exhibit unique properties in placental and somatic tissues|
|E. Magda Price123|
|Allison M. Cotton2|
|Maria S. Peñaherrera23|
|Deborah E. McFadden24|
|Michael S. Kobor235|
1Department of Obstetrics and Gynaecology; University of British Columbia; Vancouver, BC Canada
2Department of Medical Genetics; University of British Columbia; Vancouver, BC Canada
3Child and Family Research Institute, British Columbia; Vancouver, BC Canada
4Department of Pathology, University of British Columbia; Vancouver, BC Canada
5Centre for Molecular Medicine and Therapeutics, Child and Family Research Institute; Vancouver, BC Canada
|*Correspondence to: Wendy Robinson, Email: email@example.com
The theory that the environment can affect gene expression has gained much attention in recent years. This has led to widespread interest in assessing the effects of environmental exposures on epigenetic changes, including DNA methylation, at targeted loci as well as across the genome. Repetitive elements (REs) have been used as a surrogate to measure “global” changes in DNA methylation1 associated with diverse factors including nutrition,2 pollutants3,4 and toxin exposure.5 Several approaches can be used to study the same families of REs, and each method may yield varying results depending on the population of elements that is analyzed. The degree to which RE DNA methylation relates to DNA methylation at other genomic sequences and how different measures are influenced by biological and technical variables remains unclear.
Although there are numerous methods for measuring DNA methylation across the genome, one of the most widely used is high performance liquid chromatography (HPLC). Using HPLC, individual nucleotides are counted and a total measure of 5-methyl-cytosine (5-mC) content is obtained.6 5-mC-specific antibody kits have been developed as a less expensive and less labor intensive alternative to HPLC.7,8 While both HPLC and antibody kits provide a measure of average global methylation, the distribution of 5-mCs within the genome cannot be determined with these methods. Alternatively, array-based methods sacrifice some genomic coverage for the ability to detect the specific location of 5-mCs. Methylated DNA immunoprecipitation (MeDIP) captures methylated fragments of DNA with a 5-mC-specific antibody and is used in combination with a microarray for comparison against a differentially labeled control.9 Another array-based method, the Illumina Infinium HumanMethylation27 BeadChip array, allows single-nucleotide resolution of the DNA methylation status of 27,578 CpG sites in over 14,000 gene promoters.10
DNA methylation of two RE families, LINE1 (L1) and Alu, has recently been used to assess genome-wide DNA methylation because L1 and Alu sequences account for close to 30% of the total number of base pairs in the human genome;11 about 12% of all CpG dinucleotides fall within L1s while about 25% fall within Alu sequences.12,13 Alu and L1 transposable elements integrated into the ancestral genome more than 80 and 150 million years ago respectively, and over time, lineages have diverged significantly from the original DNA sequences.14 Alu and L1s amplify by a copy-and-paste mechanism that reverse transcribes the repeat sequence into a new location.11 The reverse transcriptase machinery is not robust: whereas the short Alu sequences of about 300 bps can be entirely transcribed,15 full L1s are much longer (up to about 6,000 bps) and thus are 5′ truncated at many insertion sites.16 Phylogenetic analyses divide the existing 500,000 copies of L1 and 1,000,000 copies of Alu14 each into three large subfamilies based on evolutionary age.15,17,18 REs can have diverse effects on local genomic environment including altering gene expression and acting as sites for crossover, leading to duplications or deletions (reviewed in Kazazian, 200419). Full-length L1 elements contain a sense and antisense promoter close to their 5′ end, in addition to a sense promoter in the 3′UTR20 that can act as alternative promoters.21 It is hypothesized that the host genome methylates RE DNA9,22 as a defense mechanism to limit detrimental transcription. However, these DNA methylation patterns differ based on the evolutionary age of the RE examined.23 Given their copy number and the diversity of subfamily sequences, it is unlikely that different techniques used to measure RE DNA methylation, such as Pyrosequencing,1,24 MethyLight25 and COBRA1 measure the same population of Alu or L1 elements.
There is evidence that REs are particularly prone to changes in DNA methylation with exposure to environmental toxins. In mice, feeding mothers the xenoestrogen bisphenol A (BPA) during pregnancy results in hypomethylation of the RE upstream of the Avy gene26 and a coordinated change in coat color in the offspring.27 Furthermore, supplying the mother with a methyl donor-rich diet partially counteracts the effects of BPA-induced hypomethylation.26 In humans, several studies have reported small reductions in L1 and/or Alu DNA methylation in adults exposed to benzene,28 particulate air pollution,3,29 DDT4 and PCBs.4
Since REs are present throughout the genome and sensitive to environmental exposures, measuring the DNA methylation status of Alu and L1 sequences is an attractive method to rapidly and economically assess the DNA methylation status of many CpGs.1 There is however, little evidence in direct support of L1 and Alu DNA methylation as surrogates for genome-wide DNA methylation25,30 or DNA methylation of other groups of genomic sequences. The self-replication of REs in addition to their evolutionary age and parasitic relationship with the human genome makes L1 and Alu DNA methylation particularly interesting yet difficult to study. In order to design and compare experiments, there is a need to understand what L1 and Alu DNA methylation assays measure, how RE DNA methylation relates to other DNA methylation assays and the conditions that influence L1 and Alu assessment.
In this study, we use the term representative dispersed sequences (ReDS) to describe subsets of five targets—L1, Alu, strong CpG islands, weak CpG islands and non-islands—which were examined to determine “dispersed DNA methylation” in a set of placental chorionic villi at three gestational ages (1st trimester villi, 2nd trimester villi and term villi) and in four somatic tissues (fetal brain, fetal kidney, fetal muscle and adult blood; Fig. 1). Alu and L1 DNA methylation was assessed by Pyrosequencing of consensus sequences in addition to examining groups of probes on the Illumina Infinium HumanMethylation27 BeadChip array that map to REs. DNA methylation of three categories of CpG islands was also examined using probes from the Illumina Infinium HumanMethylation27 BeadChip array: (1) strong island probes (map to high density CpG islands); (2) weak island probes (map to intermediate density CpG islands) and; (3) non-island probes (map to CpGs outside of islands) (see Methods for a full description of each assay).9 Assessment of RE DNA methylation was compared between assays and correlation of DNA methylation was assessed between the five ReDS. Our analyses have highlighted that DNA methylation at CpG sites in L1 and Alu generally follow patterns distinct from other genomic sequences in the control tissues examined here.
Characteristics that may bias the assessment of RE DNA methylation include evolutionary age,13,23 genomic location13,31 and assay method. DNA methylation of L1 and Alu sequences assessed by Pyrosequencing was compared with subsets of probes from the Illumina Infinium HumanMethylation27 BeadChip array that we identified as mapping to REs. Subfamily consensus sequences are used to design L1 and Alu Pyrosequencing primers and thus multiple primer sets are available for each family. Here, we used a primer set that measures four CpGs in the 5′ CpG island promoter of the L1H consensus sequence and three CpGs in the body of the AluSx consensus sequence, since these primer sets have been widely used in recent years.1,3,4,28,29,32 While there are about 130,000 copies of AluSx in the human genome,15 there are only about 1,200 copies of L1H,33 and up to 70% of these are expected to be 5′ truncated.16 Thus, the L1 and Alu Pyrosequencing assays sample only a small portion of each subfamily and are only representative of these dispersed sequences. RE array probes cover a variety of evolutionary age groups but, due to the design of the array, the population we could examine was biased toward REs incorporated into gene promoters. A variable number of array probes mapped to each of the Alu and L1 subfamilies: old Alu (AluJ; n = 153), intermediate Alu (AluS; n = 392), young Alu (AluY; n = 78) and old L1 (L1M; n = 192), intermediate L1 (L1P; n = 26), young L1 (L1H; n = 4). This sample represents approximately 0.52% of all AluJ, 0.11% of all AluS, 0.08% of all AluY and 0.23% of all L1H, 0.01% of all L1P and 0.03% of all L1M.
Analyses of element age were conducted in two tissue groups: (1) merged villi (placental villi from all three gestational ages) and (2) merged somatic tissues (fetal brain, fetal kidney, fetal muscle and adult blood), since DNA methylation of each subfamily of Alu or L1 did not differ between the tissues included in each of these groups (data not shown). There was a significant trend for hypomethylation of older L1 and Alu subfamilies in comparison to intermediate and young in both the merged villi and somatic groups (Fig. 2). We next compared the level of RE DNA methylation assessed by Pyrosequencing to array probe assessment. After correction for multiple comparisons, mean L1 methylation by Pyrosequencing was not different from L1H methylation assessed by array probes in the merged villi group (Fig. 2B). All other comparisons of DNA methylation between L1/Alu Pyrosequencing and array probes were significantly different in both tissue groups (Fig. 2A and B, all p < 0.001). Assessment by Pyrosequencing of L1 DNA methylation was correlated with array results in the somatic tissue group (L1M, r = 0.55; L1P, r = 0.58; both p < 0.0001) but in neither tissue group for Alu methylation. Thus, DNA methylation of REs is dependent on both evolutionary age and assay method.
Correlation analyses were performed to determine how L1 and Alu DNA methylation assessed by Pyrosequencing compare with each other and to DNA methylation of other ReDS. Using average DNA methylation assessed by the array, samples clustered most strongly by placental vs. somatic origin (Fig. S1), and then by tissue type; thus, inter-method comparisons were conducted within each somatic tissue (fetal brain, kidney and muscle and adult blood) and then collectively in the merged somatic group. Gestational age was previously found to have a significant effect on villi DNA methylation,34,35 therefore, inter-method comparisons of villi were performed within each gestational age group. RE DNA methylation was compared with three groups of Illumina Infinium HumanMethylation27 BeadChip array probes categorized based on CpG island density: strong, weak and non-island probes. Table S1 summarizes average DNA methylation by tissue group for each of the five ReDS. There were no significant differences in DNA methylation by sex for any tissue or for any ReDS; thus, males and females were considered together for all analyses (Fig. S2).
L1 and weak island probe methylation were correlated in 2nd trimester villi (Table 1; r = 0.68, p = 0.025) and in brain (Table 1; r = 0.88, p = 0.007); however, these correlations did not withstand correction for multiple comparisons. Weak and non-island probe methylation were significantly correlated after correction for multiple comparisons in 1st trimester villi (Table 1; r = 0.94, p < 0.001) and 2nd trimester villi (Table 1; r = 0.80, p = 0.005). In the merged somatic group, weak island probe methylation was also correlated with L1 DNA methylation (Table 1; r = 0.48, p = 0.002) and with non-island probe methylation (Table 1; r = 0.91, p < 0.0001). L1 and Alu DNA methylation were correlated in 1st trimester villi (Table 1; r = 0.64, p = 0.054) and in brain (Table 1; r = 0.74, p = 0.046), but neither of these was significant after correction for multiple comparisons. Detailed correlation analyses within each tissue can be found in Figures S3–10. Since the correlation of DNA methylation between weak islands and non-islands in addition to weak islands and L1s was present in several individual tissues and the merged somatic group, the association between these two pairs of ReDS may be more than inter-individual variation. However, the inconsistency of correlation between DNA methylation of the other pairs of ReDS suggests that each measure targets a genomic sequence with different trends in DNA methylation.
The five ReDS examined here are functionally different and thus trends in tissue-specific DNA methylation at these regions may also be distinct. Second trimester tissues (villi, brain, kidney and muscle) and adult blood were used to compare tissue-specific DNA methylation at each ReDS (Fig. 3). After correction for multiple comparisons, there were no significant tissue-to-tissue differences in average Alu DNA methylation (Fig. 3A). However, average L1 DNA methylation in villi (62.52% ± 4.60) was significantly lower than in somatic tissues (Fig. 3B; brain, 84.89% ± 3.32; muscle, 82.82% ± 2.44 and blood, 85.79% ± 1.92; all p < 0.001). Reduced average non-island probe methylation was also observed in villi (49.60% ± 1.20) compared with somatic tissues (Fig. 3E; brain, 60.89% ± 1.48; kidney, 57.91% ± 0.93 and blood, 63.64% ± 0.58; all p < 0.001) and at weak island probes (Fig. 3D; villi, 37.44% ± 0.65 vs. brain, 41.31% ± 0.49; kidney 38.83% ± 0.47 and blood, 43.53% ± 0.36; all p < 0.001). Interestingly, strong island DNA methylation in villi (11.21% ± 0.49) was greater than in other tissues (Fig. 3C; muscle, 9.83% ± 0.32 and kidney, 9.80% ± 0.47; all p < 0.0001), although these small differences in DNA methylation may not be biologically significant. The similarity in the patterns of tissue-specific DNA methylation assessed by L1, weak island and non-island probe methylation further suggest that these ReDS may follow similar trends in DNA methylation.
Since 98% of the array probes examined in the strong, weak and non-island groups were within 1500 bps from a known transcription start site (TSS), they are considered to be in gene promoters. We investigated whether probe distance to a TSS within each of the CpG island groups affected average DNA methylation. We present here the data from the merged somatic tissues; however, merged villi yielded similar results. Probes were binned into six 500 bp windows based on distance to nearest TSS: (1) -1500 to -1001 bps (n = 575), (2) -1000 to -501 bps (n = 1,989), (3) -500 to 0 bps (n = 8,628), (4) 1 to 500 bps (n = 8,707), (5) 501 to 1000 bps (n = 2,036) and (6) 1001 to 1500 bps (n = 558) (Fig. 4A). DNA methylation was significantly different between strong, weak and non island CpGs within each bin (p<0.0001) but was not dependent on probe direction to TSS (upstream vs. downstream, p = 0.73); thus, direction to TSS was not considered in further analyses. We next assessed tissue-specific patterns of DNA methylation in 2nd trimester tissues and adult blood for probes of each CpG island density within each of the three TSS bins: (1) ± 0 to 500 bps, (2) ± 501 to 1000 bps and (3) ± 1001 to 1500 bps. Average DNA methylation of tissues followed the same rank-order within each of the three TSS groups for strong, weak, and non-island probes (data shown for strong islands (Fig. 4B-D). These patterns were also the same as those observed when probes were not separated by distance to closest TSS (Fig. 3C, D and E). Between-tissue differences in strong-islands were largest at CpGs distal to a TSS (Fig. 4D; villi 16.91% ± 0.7 vs. kidney 15.00% ± 0.63, p p<0.0001; blood 18.10% ± 0.74, vs. brain 16.13% ± 0.64, kidney 15.00% ± 0.63 and muscle 16.20% ± 0.42, all p<0.05) and smallest at CpGs close to TSS (Fig. 4B; villi 9.63% ± 0.67 vs. kidney 8.27%± 0.46, and muscle 8.10% ± 0.32, all p<0.001).To test for an association between distance to nearest TSS and CpG island density, we compared the observed to expected number of array probes in each of the three TSS bins (Fig. S11). There was an overrepresentation of strong island probes and underrepresentation of non-island probes close to TSS (± 0 to 500 bps). Conversely, there was an overrepresentation of non-island probes and an underrepresentation of strong island probes distal to TSS (± 1001 to 1500 bps). Taken together, these results imply that within promoters, distance to nearest TSS is linked to CpG island density, which influences DNA methylation of promoters.
After examining tissue-specific patterns of dispersed DNA methylation, we investigated whether there were within-individual trends at each of the five ReDS. This is of particular interest in studies of environmental exposure and pathological conditions, to determine if changes in DNA methylation are localized to one tissue or are more widespread. The 2nd trimester fetal samples including villi, brain, kidney and muscle were obtained from 12 fetuses and were thus used to investigate intra-individual DNA methylation. None of the ReDS was universally significantly correlated across all four tissues analyzed within an individual (Fig. S12A-E). However, weak island probe methylation was significantly correlated in villi and kidney (Fig. S12D; r = 0.70, p = 0.03) and villi and brain (Fig. S12D; r = 0.89, p = 0.01). Additionally, Alu DNA methylation was correlated in villi and kidney (Fig. S12A; r = 0.82, p = 0.01). Overall, we observed more positive than negative correlation coefficients (Fig. S12; 18 vs. 7). In particular, there were more comparisons with r > 0.5 than for r < -0.5 (Fig. S12; 8 vs. 1). These results suggest a general trend for correlation of DNA methylation between tissues; however, conclusions are limited by the small sample size.
We previously reported an increase in villi gene promoter methylation throughout gestation using the Illumina Infinium HumanMethylation27 BeadChip array data for 1st trimester, 2nd trimester and term villi.35 Here, we evaluated gestational age changes in villi DNA methylation with the addition of L1 and Alu DNA methylation, and further subdivision of array probes into strong, weak and non-islands (Fig. 5A-E). After correction for multiple comparisons, there was a significant increase in non-island probe methylation from 1st trimester (46.99% ± 1.75) to term (52.01% ± 0.91) (Fig. 5E; p < 0.0001) and weak island probe methylation from 1st trimester (36.12% ± 0.99) to term (38.10% ± 0.68) (Fig. 5D; p < 0.0001) while strong island probe methylation was not altered between gestations (Fig. 5C; 1st trimester, 11.15% ± 0.61; 2nd trimester, 11.21% ± 0.49 and term 11.82% ± 0.63). Mean L1 DNA methylation did not change throughout gestation, although variation did decrease (Fig. 5B; 1st trimester, 62.69% ± 7.00; 2nd trimester, 62.52% ± 4.60 and term, 62.54% ± 2.78). Thus, villi gain in DNA methylation throughout gestation occurs at specific ReDS.
The phrase “global DNA methylation” has been widely and indiscriminately used in the literature to describe DNA methylation measured by a variety of techniques. Arguably, the only true global measures of DNA methylation assess genome-wide total 5-mC content. However, both L1 and Alu DNA methylation are commonly used as surrogates for “global DNA methylation,” implying that the status of the genome is being examined comprehensively. In this study, we examined representative members of five targets for DNA methylation (ReDS)—L1, Alu, strong CpG island promoters, weak CpG island promoters and non-island promoter CpGs—in placental villi, fetal organ tissues and adult blood. We have shown that the assessment of L1 and Alu DNA methylation is affected by assay method, evolutionary age composition of REs and tissue type. Additionally, distinct inter-tissue patterns of DNA methylation were observed at each of the ReDS. The subdivision of Illumina Infinium HumanMethylation27 BeadChip array probes into strong, weak and non-island probes, showed that the gestational age-related gain in villi DNA methylation observed in other studies35-37 predominantly occurred at weak CpG island and non-island regions.
L1 and Alu sequences account for about 17% and 11% of the human genome, respectively,14 and only a subset of these can be interrogated by any given technique. Although many studies use both L1 and Alu as surrogate measures for “global DNA methylation,” few have examined the question of whether L1 and Alu DNA methylation correlate with each other and with total 5-mC levels. Choi et al. reported a correlation of L1 with Alu DNA methylation in neuroendocrine tumors but not in control samples.38 Given that REs may be sensitive sites in the genome for changes in DNA methylation, the correlation of L1 and Alu DNA methylation may be stronger under pathological conditions. This theory is supported by two additional studies in cancer cells39,40 as well as our negative findings in control human tissues. Wang et al. found no correlation of total 5-mC, measured by Methylamp with mean L1 DNA methylation in human nervous tissue.30 However, a study by Weisenberger et al. in blood identified a strong association of both L1 and Alu DNA methylation with total 5-mC content measured by HPLC.25 Some of this study-to-study variation may be attributed to the use of different methods for measuring RE DNA methylation as well as total 5-mC content. Our comparison of RE DNA methylation obtained by Pyrosequencing vs. array probes suggests that the assessment of L1 and Alu DNA methylation is assay-dependent and thus may contribute to how these ReDS correlate with a genome-wide measure of 5-mC.
Using DNA methylation of different ReDS revealed that tissue to tissue DNA methylation was most variable at L1, non-islands and weak CpG islands and that the pattern of DNA methylation across tissues was similar at these three ReDS. Correlations between L1, weak CpG island and non-island methylation also suggest that these measures of dispersed DNA methylation may be associated with each other. Studies examining the genomic distribution of REs have demonstrated an enrichment of L1 in low GC content regions and on the X chromosome,14 in addition to an underrepresentation near genes, where Alu elements are overrepresented.41 L1s may be sites of de novo DNA methylation in the developing embryo from which DNA methylation silencing is spread TSS.42 However, this spread into CpG island promoters may be buffered by Alus, which are enriched near TSSs associated with CpG islands.31 We observed lower levels of DNA methylation in CpG island promoters close to TSS across all tissue types and increased DNA methylation at CpGs in island promoters further away from TSS. Kang et al. proposed a model of counteracting forces in the spread of DNA methylation toward promoters that leads to a transitional area of DNA methylation bordering CpG island promoters.31 However, Kang et al. use a definition for CpG islands that falls in between the weak and strong CpG islands identified in our study. The spreading model of DNA methylation from L1 sequences suggests an explanation for the correlation we observed between L1 and weak CpG island DNA methylation.
Studies using HPLC have determined that the placenta has the lowest 5-mC content in comparison to other normal tissues.36,43,44 Thus, the placenta is often described as hypomethylated compared with other fetal and adult tissues. Specific regions have also been shown to have decreased DNA methylation in the placenta, including Alu,45 L1 and regions on the X chromosome.46 Our study confirmed previous reports that L1s are hypomethylated in the placenta vs. other tissues. Some active L1 and Alu elements may play a functional role in the placenta, contributing to its invasive and proliferative properties. Placental-specific gene expression has been shown from both L121 and Alu47 sequences and may be more common in the placenta due to the lower levels of L1 and Alu DNA methylation. Syncytin is a classic example of another type of transposable element expressed exclusively in the placenta throughout gestation48 and plays a critical role in the fusion of pluripotent cytotrophoblast into differentiated syncytiotrophoblast cells.49 Interestingly, we found that there were not large differences in the DNA methylation of placenta compared with somatic tissues at strong CpG islands or close to TSS, in support of previous findings on the X chromosome.46 Since L1 and Alu elements make up almost 30% of the genome,14 REs may bias genome-wide tissue comparisons of DNA methylation based on total 5-mC content.
Although REs are widespread elements that can be rapidly and inexpensively assessed, our results suggest that L1s and Alus are sequences in the genome with distinct trends in DNA methylation. In fact, L1 DNA methylation may be more closely associated with weak CpG island methylation than “global DNA methylation.” Despite our findings, it should not be ruled out that under significant environmental changes or pathological conditions, DNA methylation of different ReDS may be more strongly associated and there may be greater intra-individual correlation. Conversely, DNA methylation of one type of dispersed sequence may be affected by a given condition while others are spared. Thus, the DNA methylation status of multiple ReDS are valuable measures to consider. We propose that L1 and Alu DNA methylation not be extrapolated to represent trends at other ReDS; they should be reported as a measure of methylation at CpG sites in the consensus sequence of specific REs. Additionally, we recommend that DNA methylation results only be compared when elements are measured by the same technique. The findings of our study reveal that the interpretation of dispersed DNA methylation data collected via a diverse range of assays is complex and the true power of these individual measurements and their relationship to each other should be scrutinized.
Samples were collected through the BC Women’s Hospital pathology department and previously described in Yuen et al.50,51 The study was approved by the ethics committees of the University of British Columbia and the Children’s and Women’s Health Centre of British Columbia (H04–70488, H06–70085). First trimester placenta (male n = 8, female n = 2) were obtained anonymously from elective terminations between 8–12 weeks gestation. Second trimester placenta (male n = 5, female n = 6) and fetal tissues (kidney, male n = 5, female n = 6; brain, male n = 4, female n = 4; muscle, male n = 4, female n = 6) were obtained from anonymous chromosomally normal pregnancies terminated for medical reasons such as premature rupture of membranes or placental abruption between 17–24 weeks gestation. Term placenta (38–41 weeks gestation, male n = 5, female n = 5) and adult female blood (n = 10) were samples used for previous studies of DNA methylation in the placenta.34 After collection, a 1 cm3 piece was sampled from the fetal side of each placenta to avoid maternal decidual contamination. The amniotic membrane and chorion were removed and then DNA was extracted from one quarter of the piece of chorionic villi. A similar sized piece of each fetal tissue was also taken for DNA extraction. The remainder of each sample was stored at -80 C for future use. Extraction was performed by standard salt method for all samples and DNA was stored at -20 C.
Methylation of L1 and Alu elements was measured by Pyrosequencing. 300 ng of genomic DNA was bisulfite converted using the EZ DNA Methylation Gold Kit (Zymo Research). L1 and Alu elements were amplified using published primer sets designed to complement the L1H and AluSx consensus sequences and cycling conditions used were as previously published.28 PCR products were subsequently sequenced by a PyroMark MD system (Biotage). The DNA methylation status for each CpG dinucleotide was evaluated using PyroQ-CpG software (Biotage) and the average for all CpG sites was calculated as a percentage for each sample. Correlation of distinct bisulfite conversions for the L1 and Alu assays were r = 0.99 and r = 0.51 respectively. The lower Alu correlation is in part due to the small range of methylation values measured for the Alu assay. There was an average difference of only 1.6% methylation between Alu technical replicates.
All samples were run on the Illumina Infinium HumanMethylation27 BeadChip array. Data for villi, fetal tissues and blood samples were previously published in an analysis of gestational-age changes in DNA methylation35 and for identification of novel differentially methylated regions between fetal tissues and blood.51 Briefly, genomic DNA was bisulfite converted using the EZ DNA Methylation Kit (Zymo Research), digested and then hybridized to the Inifinium HumanMethylation27 BeadChip array (Illumina). The Illumina Infinium HumanMethylation27 BeadChip array is a robust assay and technical replicates were highly correlated (r = 0.99). Using GenomeStudio 2008 1.0.5 software (Illumina), sex chromosome probes were removed from analysis to reduce sex-bias (n = 1,092). Poor quality probes (n = 32), defined as probes with detection p-value of > 0.05, in > 10% of samples were removed. Additionally we removed probes that were polymorphic at the target CpG (n = 263). Signal intensity output from genome studio was read in R (www.R-project.org) with the Bioconductor methylumi package to calculate an M value based on the ratio of the intensity of the methylated to unmethylated probes.52 The lumi Bioconductor package was used to correct color biases from chip to chip and then a β value was calculated for each probe.
GpGIE2.053 was used to annotate the genome with the location, size and density of CpG islands based on Weber’s definition.9 This annotation was intersected with the genomic location of array probes in Galaxy (http://galaxyproject.org/) to group probes into three categories based on the density of the CpG island in which they fell. Strong island probes (n = 14,391) were defined as those that mapped to CpG islands with > 55% GC content, > 0.75 observed/expected GC ratio and > 500 bps in length. Weak island probes (n = 2,786) were defined as those that mapped to CpG islands with > 50% GC content, > 0.48 observed/expected GC ratio and > 200 bps in length. Probes in weak islands that bordered strong islands (n = 2,229) were not included since they may act like CpG island shores and thus confound analyses. Non-island probes (n = 5,805) were all remaining probes. Probes that mapped to Alu (n = 623) and L1 (n = 222) were removed from CpG island groups and used for evolutionary age comparison of DNA methylation of REs. An estimate of the representation of all Alu and L1 sequences was obtained by dividing the number of probes on the array by the total number of sequences in each subfamily. The total number of Alu sequences was estimated based on supporting data in Price et al.54 whereas the total number of L1 sequences was estimated base on counts from the UCSC RepeatMasker track (hg18).
Binning of probes into distance to nearest TSS was accomplished using distances provided in the Illumina Infinium HumanMethylation27 BeadChip array annotation file. Strong, weak and non-island probes were initially grouped separately into each of six non-overlapping bins: (1) -1500 to -1001 bps, (2) -1000 to -501 bps, (3) -500 to 0 bps, (4) 1 to 500 bps, (5) 501 to 1000 bps and (6) 1001 to 1500 bps. Average DNA methylation was calculated for probes in three groups based on CpG island density within each of the six TSS bin. Error bars give the standard deviation of this average between somatic tissue samples. Given that we found no difference in DNA methylation based on direction to TSS, probes were not separated into upstream/downstream in later TSS analyses.
Total 5-mC content of each sample was measured using the MethylFlash Methylated DNA Quantification Kit (Colorimetric) (Epigentek Group Inc.) following the manufacturerr’s protocol. As our results were variable and correlation of technical replicates was not significant, these data were not included in this publication.
Comparison of methylation between tissue groups, gestational ages and RE evolutionary age was performed using the non-parametric ANOVA, Kruskal-Wallis test, followed by Dunn’s multiple comparison tests. Averages of DNA methylation are stated for tissue groups ± standard deviation. Spearman’s rank order correlation (r) was used to compare DNA methylation of different ReDS within each tissue group and within an individual, followed by Benjamini-Hochberg correction for multiple comparisons. A chi-square test was used to compare the observed vs. expected number of probes in each of the TSS bins. Statistics were performed in GraphPad Prism 5 (GraphPad Software, Inc.). Graphs were produced in R and GraphPad Prism 5. For box plots, boxes represent the interquartile range (IQR), whiskers the last data point within ± 1.5 x IQR, bars the median and dots outliers.
Previously published online: www.landesbioscience.com/journals/epigenetics/article/20221
The authors would like to thank Ruby Jiang for technical assistance, Courtney Hanna and Dr. Kirsten Hogg for their constructive comments, Lucia Lam and Sarah Neumann for aid in microarray processing and analysis, Dr. Angela Devlin for use of the Biotage PyroMarkTM MD machine, Dr. Dixie Mager for useful conversations and Katarzyna Stepien for her figure illustrations. This work was supported by funds from the BC Clinical Genomics Network, a grant from the Canadian Institute for Health Research to WPR, and a training fellowship from the Child and Family Research Institute to EMP. MSK is a Scholar of the Michael Smith Foundation for Health Research and the Canadian Institute for Advanced Research. Sources of support include BC Clinical Genomics Network, Canadian Institute for Health Research and the Child and Family Research Institute
|Villi||placental chorionic villi|
|L1||long interspersed nuclear element (LINE1)|
|ReDS||representative dispersed sequences|
|TSS||transcription start site|
No potential conflicts of interest were disclosed.
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|villi - 1st trimester||villi - 2nd trimester||villi - term||brain||kidney||muscle||blood||merged somatic|
Spearman correlation values (r) are stated; *indicates correlations with p ≤ 0.05; † indicates significant correlations (p ≤ 0.05) after Benjamini-Hochberg correction for multiple comparisons
Keywords: Keywords: Alu, CpG island, DNA Methylation, L1, epigenetics, placenta, repetitive elements.
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