Skip to main content

Advertisement

DNA methylation subgroups in melanoma are associated with proliferative and immunological processes

BMC Medical Genomicsvolume 8, Article number: 73 (2015) | Download Citation

Abstract

Background

DNA methylation at CpG dinucleotides is modified in tumorigenesis with potential impact on transcriptional activity.

Methods

We used the Illumina 450 K platform to evaluate DNA methylation patterns of 50 metastatic melanoma tumors, with matched gene expression data.

Results

We identified three different methylation groups and validated the groups in independent data from The Cancer Genome Atlas. One group displayed hypermethylation of a developmental promoter set, genome-wide demethylation, increased proliferation and activity of the SWI/SNF complex. A second group had a methylation pattern resembling stromal and leukocyte cells, over-expressed an immune signature and had improved survival rates in metastatic tumors (p < 0.05). A third group had intermediate methylation levels and expressed both proliferative and immune signatures. The methylation groups corresponded to some degree with previously identified gene expression phenotypes.

Conclusions

Melanoma consists of divergent methylation groups that are distinguished by promoter methylation, proliferation and content of immunological cells.

Open Peer Review reports

Background

The tumor phenotype is formed by genetic and epigenetic events and signals from the micro-environment. In melanoma, the landscape of somatic mutations and gene copy number changes has been explored [1–3], and the understanding of surrounding immunological cells has led to the development of new treatment options [4, 5]. Recurrently mutated genes discovered by recent exome sequencing studies are frequently involved in epigenetic modifications [6], e.g., ARID2 [1, 2], pointing to a yet under-appreciated driver role of epigenetic factors. Methylation of cytosine in the CpG context is an epigenetic mark that can directly influence transcriptional activity, and changes of DNA methylation pattern have been associated with tumorigenesis. In melanoma, a number of genes were found to harbor promoter CpG island methylation [7]. Consequently, melanomas hypermethylated at several CpG islands were termed CpG Island Methylator Phenotype (CIMP) [8], according to findings from other cancer types [9, 10]. Promoter methylation is reported to repress gene expression. Conversely, a small number of genes, such as MAGE, are activated by hypomethylation in melanoma [7]. High-throughput technology has enabled the assessment of DNA methylation of a wider spectrum of genomic locations in melanoma [11–23], often highlighting methylation events that discriminate melanoma from nevi/melanocytes. Genome-wide methylation patterns may reveal tumor subtypes of biological and clinical relevance. In this respect, Thomas et al. used the Illumina GoldenGate platform (1505 CpGs) and found three methylation subgroups in 47 primary cutaneous melanoma, with the hypermethylated groups having increased Breslow thickness [24]. Sigalotti et al. analyzed short-term cultures from 45 stage IIIC patients on Illumina 27 K BeadChips and identified one group with low and one with high average methylation, respectively; with the latter group having poor overall survival [25].

Previously, we introduced four gene expression subgroups in melanoma; one proliferative group (‘Proliferative’), one group with activated melanogenesis pathway (‘Pigmentation’), one group displaying elevated immune response (‘High-Immune’) and one with contribution from surrounding normal tissue (‘Normal-like’) [26]. The groups were also present in primary melanomas and had diverging clinical outcome [27]. In this study we aimed to characterize DNA methylation subtypes of melanoma, validate the findings in independent data, and to investigate the relationship of methylation and gene expression patterns.

Results

Identification of three methylation subtypes in melanoma

We determined the methylation status of more than 480,000 individual CpGs in 50 metastatic melanoma tumors, subsequently called ‘Bergen’ data, that were included in a previous discovery of gene expression phenotypes [26] (Table 1). The methylation measurements are β-values that range from 0, unmethylated to 1, fully methylated [28]. We defined a set of CpGs that is aberrantly methylated in melanoma as compared to melanocytes, with 9,886 melanoma-methylated CpGs and 5,236 melanoma-demethylated CpGs, respectively, as previously described [29]. Unsupervised clustering of the combined CpG sets identified three consensus groups in the Bergen melanomas, subsequently called methylation subtype 1, 2 and 3 (MS1, MS2, MS3) (Fig. 1a). As validation data, we used 242 samples from The Cancer Genome Atlas (TCGA) (Table 1). Unsupervised clustering of the TCGA data, which consists of primary and metastatic tumors, using the same CpG set, resulted in three groups with comparable methylation patterns to the Bergen data (Fig. 1a). Principal component analyses were performed to exclude that the groups are due to technical procedures at data generation, such as the use of different batches (Additional file 1: Figure S1A and B). The three groups were re-identified in both datasets when changing the number of CpGs to be included in the clustering procedure (Additional file 1: Figure S1C). We next classified the TCGA samples into MS1, MS2, and MS3 groups using Bergen-derived methylation centroids (Additional file 2: Table S1). Centroid classification was the dominant explainer of total variation in TCGA methylation data compared to histopathological and molecular factors (Additional file 1: Figure S1B). Furthermore, classification of TCGA tumors using Bergen-derived centroids, is in good agreement with the groups obtained from unsupervised clustering of the TCGA data (76 % sample co-occurence, P < 2x10−16, Additional file 1: Figure S1D and “MS classified” annotation in Fig. 1a), confirming that the methylation clusters of Bergen are re-identified in the TCGA data.

Table 1 Patient and sample information
Full size table
Fig. 1
figure1

Three melanoma methylation subtypes. a Methylation lanes from left to right: 3 methylation subtypes (MS) from Bergen tumors, 9 cell lines, blood leucocytes, melanocytes (two lanes of each light, medium and dark melanocytes), dermal epidermis, dermal fibroblasts; and 3 unsupervised groups from TCGA tumors. Beta values in heatmap are from unmethylated, blue to methylated, yellow. Cluster lane displays the four main CpG probe clusters of the 9,886 melanoma-methylated and 5,236 melanoma-demethylated CpGs, using unsupervised hierarchical clustering in the Bergen data. Island lane: black = CpG island, dark grey = shore/shelf, light grey = open sea. Chromatin lane refers to embryonic stem cell chromatin states. GEX = gene expression. CDKN2Adel = homozygous deletion of the CDKN2A locus. b Mean beta value across MS subtypes in different genome-wide CpG sets. Promoter & Island = annotated as TSS200 or TSS1500 (i.e. up to 1500 bp from transcription start site) and annotated as CpG Island, n = 57,579 CpGs. Away from genes and Island = no annotation for gene and island, n = 42,728 CpGs. Poised promoter = embryonic stem cell chromatin state, see panel A, n = 59,901 CpGs. P-value from Kruskal-Wallis test

Full size image

We then restricted the analysis to a subset of CpGs located in CpG islands within 1500 bp upstream of transcription start sites. The vast majority of these promoter island CpGs were hyper-methylated in melanomas (930 of 947), in line with other tumor types. In both datasets, methylation levels spanned a continuous gradient from unmethylated melanomas to fully methylated melanomas, rather than forming a distinctive CIMP group (Additional file 1: Figure S2). We conclude that in melanomas the full range of CpGs provides additional information to the traditionally studied promoter island CpGs, and allowed for the identification of three reproducible methylation subtypes, MS1/2/3.

Biological processes shaping the methylation subtypes

Methylation levels at promoter islands are elevated in MS1 tumors in comparison to MS3 tumors (Fig. 1b, Kruskal-Wallis test). ‘Poised promoters’ are characterized by Polycomb-complex 2 (PRC2) induced H3K27 tri-methylation marks in addition to H3K4 tri-methylation marks, and are most prevalent in embryonic stem cells [30]. The poised promoter set of embryonic stem cells is important in developmental processes and found to be methylated in various cancer types [31, 32]. Notably, CpGs in this poised promoter set also displayed increased methylation levels in the MS1 group. Conversely, intergenic methylation levels away from genes and islands are reduced in MS1 tumors (Fig. 1b, Kruskal-Wallis test). The MS1 group showed a pattern similar to melanocytes but with hyper-methylation at many poised promoters. The nine melanoma cell lines also displayed the MS1 pattern (Fig. 1a). In contrast, the DNA methylation pattern of the MS3 group was similar to peripheral blood leukocytes. Finally, the MS2 group presents a mixture of MS1 and MS3 methylation patterns with intermediate methylation levels for the majority of CpGs.

The CpG set used for group discovery consisted of four functional clusters (Fig. 1a). First, one CpG cluster (Fig. 1a, black cluster “Cl. 1 + 2”) was highly enriched in the aforementioned Polycomb-targeted poised promoters. This CpG cluster was hypermethylated in melanoma compared to melanocytes with gradually increasing methylation levels from MS3 to MS1 tumors. Second, genome-wide hypomethylation was observed in repetitive, heterochromatic regions, that had gradually decreasing methylation levels from MS3 to MS1 tumors (Fig. 1a, grey cluster “Cl. 5”). Third, a heterogeneous CpG cluster was found that had opposite methylation status in melanocytes and blood leukocytes, with melanoma samples spanning the gradient in between (Fig. 1a, green cluster “Cl. 3 + 4”). The fourth cluster of CpGs could not be assigned to a biological function (Fig. 1a, ‘mixed’, pale blue cluster “Cl. 6”). As the third cluster seemed to contain methylation signals from non-tumoral cells, we used the ESTIMATE algorithm to further investigate the cellular composition of the tumors [33]. Evidence of elevated stromal and immune cell content was observed in MS2/3 compared to MS1 samples (Fig. 2a, Kruskal-Wallis test). Overall, tumor purity was estimated to be lowest in MS3 samples and highest in MS1 samples (Fig. 2a, Kruskal-Wallis test). Furthermore, MS1 and MS2 over-expressed mitotic gene signatures, whereas MS2 and MS3 over-expressed an immune response signature (Fig. 2b, ANOVA). These observations were validated in TCGA data (Additional file 1: Figure S3). In conclusion, the molecular subtypes are shaped by various degrees of promoter hypermethylation, genome-wide hypomethylation, and cell-type specific methylation signatures from the micro-environment.

Fig. 2
figure2

Immunological and proliferative signature expression across methylation subtypes. a ESTIMATE scores and tumor purity. P-value from Kruskal-Wallis test. b Mean expression values of melanoma gene modules and GO-term ‘cell cycle’. P-value from anova. Bergen tumor data

Full size image

Methylation processes of melanoma in comparison to other cancer types

To set the methylation processes of melanoma in context to other cancer types, we used TCGA data from colon cancer (295 tumors, 38 normal tissues), breast cancer (201 tumors, 40 normal tissues) and lung cancer (lung adenocarcinoma, 452 tumors, 32 normal tissues). For these cancer types, we derived tumor-methylated and tumor-demethylated CpGs in the same way as for our melanoma data. The majority of methylated and demethylated CpGs occurred in only one cancer-type (Additional file 1: Figure S4A). Yet, at the gene level the agreement across cancer types was larger, particularly the agreement of methylated genes was considerable (Additional file 1: Figure S4A). Importantly, for all investigated cancer types, the methylated CpGs were located within poised promoters (i.e. PRC2 target genes), and the demethylated CpGs located within heterochromatic regions of ES cells chromatin (Additional file 1: Figure S4B). Similarly, for melanocyte chromatin states, methylated CpGs were situated in bivalently marked chromatin regions, and demethylated CpGs in quiescent/repressed regions (Additional file 1: Figure S4C). In an aim to find melanoma-specific mechanisms of methylation, we compared genes hypermethylated exclusively in melanoma to genes hypermethylated in colon, lung and breast cancer. Genes exclusively methylated in melanoma were significantly enriched for the GO-terms “catalytic activity”, “nucleoside-triphosphatase regulator activity” and “GTPase regulator activity” (false discovery rate (fdr) < 5 %). This may allow speculating that a metabolic process exists in melanocytes that is connected to the MAPK pathway via regulation of GTPase (e.g., Ras) activity, with methylation of the regulators emerging at tumorigenesis. In summary, aberrant methylation in tumors preferentially occurs at genes with “poised promoters” and demethylation in heterochromatin, however, the exact stretches of DNA that get aberrantly methylated are cancer-type specific. This resembles findings from Sproul et al., who however had not included melanomas in their study [34].

Correlation to histopathology, mutation data and clinical outcome

Overall the proportions of the three methylation groups were comparable between the Bergen and TCGA samples. However, the TCGA distant metastasis samples contained more MS1 samples than the Bergen cohort (Fig. 3a, Fisher’s exact test). We did not observe any significant associations of gender, age, primary tumor features (Breslow thickness, Clark’s level, SSM/NM), LDH, lymph-node/subcutaneous, CD3 or CD20 IHC with the methylation groups in the Bergen data. Furthermore, in our data, neither BRAF nor NRAS mutation status was clearly associated with either subgroup (Fig. 1a). Homozygous deletions of the CDKN2A locus seemed to be more frequent in MS1 (p = 0.02). We repeated the mutation analysis for TCGA exome-sequencing data. The total number of mutations in tumors was equally distributed across subtypes (Additional file 1: Figure S5A). For mutations in 15 known melanoma driver genes [1, 2] we did not observe any subtype association, with an fdr < 10 % (Additional file 1: Figure S5B). IDH1 hotspot mutations at R132 correlate with a glioblastoma hypermethylation phenotype [35] and have been reported in melanoma [36]. IDH1 hotspot mutation was more prevalent in the hypermethylated MS1 group (6 of 11 mutated cases), however, not reaching significance.

Fig. 3
figure3

Clinical evaluation of methylation subtypes. a Distribution of methylation subtypes in Bergen and TCGA cohorts. P-values from Fisher’s exact test. b, c, d Survival analyses. P-values from Cox regression

Full size image

Disease-specific survival analysis indicated more aggressive behavior of MS1 melanomas compared to MS2/3 melanomas, although not reaching significance (p = 0.2 log-rank test, Fig. 3b). This trend was further supported in metastatic TCGA tumors, with MS1 patients having inferior survival outcome (p = 5x10−5, Fig. 3c). As samples from distant metastases are over-represented in the MS1 subtype, we repeated the survival analysis using only the regional lymph node metastasis from TCGA, and again observed inferior survival of MS1 patients (p = 0.008, Fig. 3d). The primary TCGA cohort size (n = 27) was too small to allow for survival analysis.

A link between methylation and gene expression phenotypes

The MAPK and PI(3)K pathways are instrumental in melanoma [37, 38]. However, these pathways did not seem to be differentially expressed across methylation subtypes in Bergen and TCGA data, with the exception of DUSP genes (Additional file 1: Figure S6A). Genes that promote the cell cycle, such as MDM2, CDK4, CDK6, CCND1, CCNE1 and E2F3 are up-regulated in MS1 samples; as well as genes that directly modify CpG methylation, such as de-novo methyltransferase DNMT3A and 5-hydroxy converting TET1 (fdr < 5 %, Fig. 4a, ANOVA with Benjamini-Hochberg fdr). Histone modifiers were generally not differentially expressed across methylation subtypes, again with an exception, the H3K4 de-methylation enzyme JARID1B. Recently, members of the SWI/SNF chromatin remodeling complex have been found to carry loss-of-function mutations across cancer types, implying a tumor suppressor role [39, 40]. Interestingly, several SWI/SNF members are up-regulated in MS1 tumors (Fig. 4a).

Fig. 4
figure4

Association between transcription and methylation landscapes. a Expression of genes involved in cancer-driving pathways and processes, across methylation subtypes. fdr = false discovery rate for p-values from anova using Benjamini-Hochberg adjustment. b Heatmap of association between gene expression and methylation subtypes. P-values from Fisher’s exact test. c Summary cartoon. Check sign = presence, up-arrow = up-regulation, down-arrow = down-regulation. MS = Methylation subtype. GEX = Gene expression. Prolif. = Proliferative subtype. Pigm. = Pigmentation subtype

Full size image

To further investigate the relationship of methylation to gene expression patterns, we compared the methylation subtypes to the four gene expression phenotypes previously defined in the Bergen cohort [26]. MS1 consisted of ‘Proliferative’ and ‘Pigmentation’–type tumors (Fig. 4b), suggesting a link between proliferation and hyper-methylation. The MS3 subgroup is dominated by ‘High-immune’ and ‘Normal-like’ tumors. The agreement of gene expression subtypes and methylation subtypes is statistically significant (p = 0.0001, Fisher’s exact test, Cross-table Additional file 1: Figure S6B), with methylation subtypes providing additional stratification beyond gene expression subtypes. The co-occurrence of methylation and gene expression phenotypes was also observed in the TCGA data (p = 6x10−14, Fisher’s exact test, Fig. 4b and Additional file 1: Figure S6B). Together, these findings provide a link between the transcriptional and DNA methylation landscapes in melanoma.

Discussion

In the present study, we have identified three groups of melanoma specimens with different methylation patterns. The MS1 group fits the paradigm of genome-wide de-methylation and focal promoter hyper-methylation in tumors [41]. Most cancer types studied by the TCGA consortium, contained a subgroup with high methylation levels [42]. Hypermethylated subgroups in colon and endometrial cancer were associated with MLH1 inactivation and increased mutation rate. In other cancer types hypermethylated subgroups were associated with IDH1 mutations (AML, glioblastoma), or EBV virus (gastric cancer). For breast cancer, lung squamous cell carcinoma and lung adenocarcinoma, there has been no clear association of the methylated group to such a factor. Likewise, our melanoma hypermethylated group MS1 was not significantly associated with a mutated gene or overall mutation rate. Hyper-methylation is primarily directed towards the embryonic PRC2 target gene set. These genes are pre-marked by histone H3K27 tri-methylation in addition to a H3K4 mark in embryonic stem cells [43]. DNA methylation of these ‘poised promoters’ has emerged as a general process across tumor types [31, 44]. Genome-wide de-methylation in melanoma occurs in repetitive regions, distant from CpG islands. A relatively small number of de-methylated CpGs are captured on the array, which is likely due to difficulties with designing probes in repetitive regions.Cell line methylation patterns differed from normal melanocytes and matched well with the MS1 group. Moreover, methylation subtypes seemed to be influenced by the cellular composition of the tumor, in particular, the MS3 methylation pattern is closely related to blood leukocytes and has a reduced tumor cell content compared to MS1. In the future, single-cell sequencing may clarify the methylation pattern of pure MS3 tumor cells. However, for prediction of immune therapy success, information from both tumor and surrounding cells has been valuable [45–48]. Therefore, methylation signals from the micro-environment may prove useful for decision making in melanoma.

Together, the methylation data reveals two tumor strategies (Fig. 4c). First, a proliferative strategy that co-occurs with hypermethylation of poised promoters. Poised promoters are located in differentiation genes, some of them potentially negative for tumor fitness. It is therefore tempting to speculate that methylation of poised promoters is aimed at removing the brakes of tumor proliferation. Sequential methylation of the poised promoter set may inactivate repressive developmental genes, resulting in a small advantage in tumor growth. Therefore, clones with ever-increasing poised promoter methylation may be preferred in tumor evolution. Accordingly, instead of a clear CIMP group, we observe a gradual increase in promoter methylation. This proliferation strategy also seems to act independently from the MAPK and PI(3)K signaling pathways (Additional file 1: Figure S6A). The second strategy is based on an interplay of tumor cells with immune cells. The composition of the immune cells in the melanoma samples was preserved across cohorts, as the methylation subtypes could be validated in the independent TCGA data. The precise interplay of tumor and immune cells is still unclear. The knowledge of this interplay may reveal the basis of improved survival of MS3 patients, and could greatly benefit the development of further immune therapies. Importantly, immunomodulating agents have demonstrated significant clinical benefit in melanoma and include immune checkpoint blockade agents such as anti-CTLA4 and anti-PD1/PDL1 [4, 5]. In contrast, tumor-associated macrophages, regulatory T-cells and myeloid-derived suppressor cells can blunt anti-tumor effector functions and promote tumor growth and invasiveness, highlighting the complexity of the interplay between the tumor and the immune system.

A major limitation of the current study is that DNA methylation is the only investigated epigenetic mark. Characterization of a broad spectrum of epigenetic marks will most likely enhance insight into melanoma. In addition, a better understanding of the functional role of the SWI/SNF chromatin remodeling complex and its impact on the epigenetic landscape will be very useful.

Conclusions

Herein, we identified three methylation subgroups in melanoma, with distinct biological properties and disease outcome. The methylation groups are in good agreement with gene expression phenotypes, and highlight two different mechanisms underlying this disease, a proliferative strategy and a strategy based on the presence of immune cells.

Methods

Generation of genome-wide methylation data

We determined genome-wide methylation levels in 50 tumors from Haukeland University Hospital in Bergen [26], 9 melanoma cell lines (A2058, A7, CHL1, HT144, MM383, SKMEL3, SKMEL5, WM239A, WM852), light, medium, dark melanocytes, dermal epidermis and fibroblasts (Science Cell Research, USA), and peripheral blood leukocytes (Promega), using Illumina Infinium HumanMethylation450K BeadChips. Informed consent was obtained from all patients. The study was approved by the local ethics committee. DNA was extracted as described previously [26]. Bisulfite conversion and hybridization to Infinium HumanMethylation450K BeadChips was performed following the manufacturer’s instructions, with samples being processed as one batch. Methylation data had been deposited at Gene Expression Omnibus as series GSE51547, and gene expression data as GSE22153.

Processing of Bergen methylation and gene expression data

Beta-values were calculated from methylated (M) and unmethylated (U) signal, as beta = M/(M + U). A total of 496 missing values were imputed using k-nearest neighbor imputation (k = 10) [49]. For each sample we performed a peak-based correction of Illumina I and II chemical assays similar to Dedeurwaerder et al. [50]. For each assay the beta values were smoothened (Epanechnikov kernel) to estimate unmethylated and methylated peaks, respectively. The unmethylated peak was moved to 0 and the methylated peak to 1 using linear scaling, with beta-values in between stretched accordingly and capped at 0 and 1. CpGs of chromosomes X and Y were removed.

The matched gene expression data was processed as described previously [26]. Multiple probes for a gene (based on gene symbol) were median-merged.

Processing of TCGA methylation and gene expression data

Methylation data for 242 samples from the TCGA data portal https://tcga-data.nci.nih.gov/tcga/ were processed as described for the Bergen data. For a subset of 214 samples we downloaded normalized RSEM gene counts from ‘level 3’ RNA sequencing data. The data was quantile-normalized using limma [51], added an offset of 32, capped to a maximum value of 65,000, log2 transformed, and genes were median-centered. The samples were classified using reported gene expression phenotype centroids as described [26]. TCGA methylation data for colon cancer (COAD, 295 tumors, 38 solid normal tissues), breast cancer (BRCA, 201 tumors, 40 solid normal tissues, constituting the first six TCGA batches) and lung adenocarcinoma (LUAD, 452 tumors, 32 solid normal tissues) were processed as described for the Bergen data.

Clustering procedure to obtain consensus clusters

The set of 9,886 melanoma-methylated CpGs was defined as β < 0.1 in melanocytes and β > 0.5 in at least 20 % of tumors (n = 10). The set of 5,236 melanoma-demethylated CpGs was defined as β > 0.9 in melanocytes and β < 0.5 in at least 20 % of tumors (n = 10), respectively. The CpG sets were combined for the clustering procedure. Hierarchical Clustering Analysis (HCA) with Euclidean distance and Ward’s algorithm for agglomeration, was performed for 1000 bootstrapped versions of the data [44]. At each bootstrap HCA the dendrogram is cut into either 2 or 3 clusters. For all sample pairs, the frequency with which the two samples have clustered into the same group is calculated. The co-clustering frequency matrix is then reordered by HCA (Pearson correlation distance, Ward agglomeration) to obtain the consensus methylation groups, i.e. subsets of samples that repeatedly cluster together.

Nearest Centroid Classification

The centroids of the methylation subgroups were defined as the mean methylation values of the 9,886 melanoma-methylated and 5,236 melanoma-demethylated CpGs, across each subgroup of the Bergen samples. Therefore, we obtained three centroids, one for MS1, one for MS2, and one for MS3, presenting the mean beta-values of the subgroups. The centroids were deposited as Additional file 2: Table S1. To classify a sample from the TCGA HumanMethylation450K data, the beta-values of the centroid CpGs were extracted. The Euclidean distance of the TCGA beta-values to each of the three centroids was calculated and the sample was assigned to the MS subgroup to whose centroid it had the shortest distance. Using this classification system we assigned each TCGA tumor as being either MS1, MS2 or MS3.

Statistical analysis

We used chromatin predictions for H1 embryonic stem cells [52], and melanoma gene co-expression modules for ‘Immune Response’ and ‘Cell Cycle’ from an independent cohort [53]. All statistical analysis was performed in R 3.1.1. Survival analysis was performed using the survival package, principal component analysis was performed using the swamp package [54], ESTIMATE scores were derived using the estimate package [33].

Abbreviations

CIMP:

CpG island methylator phenotype

TCGA:

The cancer genome atlas

HCA:

Hierarchical clustering analysis

MS:

Methylation subtype

NM:

Nodular melanoma

SSM:

Superficial spreading melanoma

LDH:

Lactate dehydrogenase

IHC:

Immunohistochemistry

SWI/SNF:

SWItch/Sucrose nonfermentable

PRC2:

Polycomb repressive complex 2

References

  1. 1.

    Hodis E, Watson IR, Kryukov GV, Arold ST, Imielinski M, Theurillat J-P, et al. A landscape of driver mutations in melanoma. Cell. 2012;150:251–63.

  2. 2.

    Krauthammer M, Kong Y, Ha BH, Evans P, Bacchiocchi A, McCusker JP, et al. Exome sequencing identifies recurrent somatic RAC1 mutations in melanoma. Nat Genet. 2012;44:1006–14.

  3. 3.

    Pleasance ED, Cheetham RK, Stephens PJ, McBride DJ, Humphray SJ, Greenman CD, et al. A comprehensive catalogue of somatic mutations from a human cancer genome. Nature. 2010;463:191–6.

  4. 4.

    Robert C, Thomas L, Bondarenko I, O’Day S, M D JW, Garbe C, et al. Ipilimumab plus dacarbazine for previously untreated metastatic melanoma. N Engl J Med. 2011;364:2517–26.

  5. 5.

    Wolchok JD, Kluger H, Callahan MK, Postow MA, Rizvi NA, Lesokhin AM, et al. Nivolumab plus ipilimumab in advanced melanoma. N Engl J Med. 2013;369:122–33.

  6. 6.

    Kandoth C, McLellan MD, Vandin F, Ye K, Niu B, Lu C, et al. Mutational landscape and significance across 12 major cancer types. Nature. 2013;502:333–9.

  7. 7.

    van den Hurk K, Niessen HEC, Veeck J, van den Oord JJ, van Steensel MAM, Zur HA, et al. Genetics and epigenetics of cutaneous malignant melanoma: A concert out of tune. Biochimica Et Biophysica Acta. 2012;1826:89–102.

  8. 8.

    Tanemura A, Terando AM, Sim M-S, van Hoesel AQ, de Maat MFG, Morton DL, et al. CpG island methylator phenotype predicts progression of malignant melanoma. Clin Cancer Res. 2009;15:1801–7.

  9. 9.

    Noushmehr H, Weisenberger DJ, Diefes K, Phillips HS, Pujara K, Berman BP, et al. Identification of a CpG island methylator phenotype that defines a distinct subgroup of glioma. Cancer Cell. 2010;17:510–22.

  10. 10.

    Weisenberger DJ, Siegmund KD, Campan M, Young J, Long TI, Faasse MA, et al. CpG island methylator phenotype underlies sporadic microsatellite instability and is tightly associated with BRAF mutation in colorectal cancer. Nat Genet. 2006;38:787–93.

  11. 11.

    Furuta J, Nobeyama Y, Umebayashi Y, Otsuka F, Kikuchi K, Ushijima T. Silencing of Peroxiredoxin 2 and aberrant methylation of 33 CpG islands in putative promoter regions in human malignant melanomas. Cancer Res. 2006;66:6080–6.

  12. 12.

    Koga Y, Pelizzola M, Cheng E, Krauthammer M, Sznol M, Ariyan S, et al. Genome-wide screen of promoter methylation identifies novel markers in melanoma. Genome Res. 2009;19:1462–70.

  13. 13.

    Conway K, Edmiston SN, Khondker ZS, Groben PA, Zhou X, Chu H, et al. DNA-methylation profiling distinguishes malignant melanomas from benign nevi. Pigment Cell Melanoma Res. 2011;24:352–60.

  14. 14.

    Bonazzi VF, Nancarrow DJ, Stark MS, Moser RJ, Boyle GM, Aoude LG, et al. Cross-platform array screening identifies COL1A2, THBS1, TNFRSF10D and UCHL1 as genes frequently silenced by methylation in melanoma. PLoS One. 2011;6:e26121.

  15. 15.

    Gao L, Smit MA, van den Oord JJ, Goeman JJ, Verdegaal EME, van der Burg SH, et al. Genome-wide promoter methylation analysis identifies epigenetic silencing of MAPK13 in primary cutaneous melanoma. Pigment Cell Melanoma Res. 2013;26:542–54.

  16. 16.

    Hou P, Liu D, Dong J, Xing M. The BRAF(V600E) causes widespread alterations in gene methylation in the genome of melanoma cells. Cell Cycle. 2012;11:286–95.

  17. 17.

    Lian CG, Xu Y, Ceol C, Wu F, Larson A, Dresser K, et al. Loss of 5-hydroxymethylcytosine is an epigenetic hallmark of melanoma. Cell. 2012;150:1135–46.

  18. 18.

    Marzese DM, Scolyer RA, Roqué M, Vargas-Roig LM, Huynh JL, Wilmott JS, et al. DNA methylation and gene deletion analysis of brain metastases in melanoma patients identifies mutually exclusive molecular alterations. Neuro Oncol. 2014;16:1499–509.

  19. 19.

    Marzese DM, Scolyer RA, Huynh JL, Huang SK, Hirose H, Chong KK, et al. Epigenome-wide DNA methylation landscape of melanoma progression to brain metastasis reveals aberrations on homeobox D cluster associated with prognosis. Hum Mol Genet. 2014;23:226–38.

  20. 20.

    Ecsedi S, Hernandez-Vargas H, Lima SC, Vizkeleti L, Toth R, Lazar V, et al. DNA methylation characteristics of primary melanomas with distinct biological behaviour. PLoS One. 2014;9:e96612.

  21. 21.

    Li J-L, Mazar J, Zhong C, Faulkner GJ, Govindarajan SS, Zhang Z, et al. Genome-wide methylated CpG island profiles of melanoma cells reveal a melanoma coregulation network. Sci Rep. 2013;3:2962.

  22. 22.

    Dahl C, Abildgaard C, Riber-Hansen R, Steiniche T, Lade-Keller J, Guldberg P. KIT Is a Frequent Target for Epigenetic Silencing in Cutaneous Melanoma. J Invest Dermatol. 2015;135:516–24.

  23. 23.

    Gao L, van den Hurk K, Moerkerk PTM, Goeman JJ, Beck S, Gruis NA, et al. Promoter CpG Island Hypermethylation in Dysplastic Nevus and Melanoma: CLDN11 as an Epigenetic Biomarker for Malignancy. J Invest Dermatol. 2014;134(12):2957–66.

  24. 24.

    Thomas NE, Slater NA, Edmiston SN, Zhou X, Kuan P-F, Groben PA, et al. DNA methylation profiles in primary cutaneous melanomas are associated with clinically significant pathologic features. Pigment Cell Melanoma Res. 2014;27:1097–105.

  25. 25.

    Sigalotti L, Covre A, Fratta E, Parisi G, Sonego P, Colizzi F, et al. Whole genome methylation profiles as independent markers of survival in stage IIIC melanoma patients. J Transl Med. 2012;10:185.

  26. 26.

    Jönsson G, Busch C, Knappskog S, Geisler J, Miletic H, Ringnér M, et al. Gene expression profiling-based identification of molecular subtypes in stage IV melanomas with different clinical outcome. Clin Cancer Res. 2010;16:3356–67.

  27. 27.

    Harbst K, Staaf J, Lauss M, Karlsson A, Måsbäck A, Johansson I, et al. Molecular profiling reveals low- and high-grade forms of primary melanoma. Clin Cancer Res. 2012;18:4026–36.

  28. 28.

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

  29. 29.

    Lauss M, Haq R, Cirenajwis H, Phung B, Harbst K, Staaf J, et al. Genome-Wide DNA Methylation Analysis in Melanoma Reveals the Importance of CpG Methylation in MITF Regulation. J Invest Dermatol. 2015;135(7):1820–8.

  30. 30.

    Roadmap Epigenomics Consortium, Kundaje A, Meuleman W, Ernst J, Bilenky M, Yen A, et al. Integrative analysis of 111 reference human epigenomes. Nature. 2015;518:317–30.

  31. 31.

    Easwaran H, Johnstone SE, Van Neste L, Ohm J, Mosbruger T, Wang Q, et al. A DNA hypermethylation module for the stem/progenitor cell signature of cancer. Genome Res. 2012;22:837–49.

  32. 32.

    Widschwendter M, Fiegl H, Egle D, Mueller-Holzner E, Spizzo G, Marth C, et al. Epigenetic stem cell signature in cancer. Nat Genet. 2007;39:157–8.

  33. 33.

    Yoshihara K, Shahmoradgoli M, Martínez E, Vegesna R, Kim H, Torres-Garcia W, et al. Inferring tumour purity and stromal and immune cell admixture from expression data. Nat Commun. 2013;4:2612.

  34. 34.

    Sproul D, Kitchen RR, Nestor CE, Dixon JM, Sims AH, Harrison DJ, et al. Tissue of origin determines cancer-associated CpG island promoter hypermethylation patterns. Genome Biol. 2012;13:R84.

  35. 35.

    Turcan S, Rohle D, Goenka A, Walsh LA, Fang F, Yilmaz E, et al. IDH1 mutation is sufficient to establish the glioma hypermethylator phenotype. Nature. 2012;483:479–83.

  36. 36.

    Shibata T, Kokubu A, Miyamoto M, Sasajima Y, Yamazaki N. Mutant IDH1 confers an in vivo growth in a melanoma cell line with BRAF mutation. Am J Pathol. 2011;178:1395–402.

  37. 37.

    Long GV, Stroyakovskiy D, Gogas H, Levchenko E, de Braud F, Larkin J, et al. Combined BRAF and MEK Inhibition versus BRAF Inhibition Alone in Melanoma. N Engl J Med. 2014;371:1877–88.

  38. 38.

    Kwong LN, Davies MA. Navigating the therapeutic complexity of PI3K pathway inhibition in melanoma. Clin Cancer Res. 2013;19:5310–9.

  39. 39.

    Shain AH, Pollack JR. The spectrum of SWI/SNF mutations, ubiquitous in human cancers. PLoS One. 2013;8:e55119.

  40. 40.

    Helming KC, Wang X, Roberts CWM. Vulnerabilities of Mutant SWI/SNF Complexes in Cancer. Cancer Cell. 2014;26:309–17.

  41. 41.

    Ehrlich M. DNA methylation in cancer: too much, but also too little. Oncogene. 2002;21:5400–13.

  42. 42.

    Witte T, Plass C, Gerhauser C. Pan-cancer patterns of DNA methylation. Genome Med. 2014;6:66.

  43. 43.

    Bernstein BE, Mikkelsen TS, Xie X, Kamal M, Huebert DJ, Cuff J, et al. A bivalent chromatin structure marks key developmental genes in embryonic stem cells. Cell. 2006;125:315–26.

  44. 44.

    Lauss M, Aine M, Sjödahl G, Veerla S, Patschan O, Gudjonsson S, et al. DNA methylation analyses of urothelial carcinoma reveal distinct epigenetic subtypes and an association between gene copy number and methylation status. Epigenetics. 2012;7:858–67.

  45. 45.

    Tumeh PC, Harview CL, Yearley JH, Shintaku IP, Taylor EJM, Robert L, et al. PD-1 blockade induces responses by inhibiting adaptive immune resistance. Nature. 2014;515:568–71.

  46. 46.

    Herbst RS, Soria J-C, Kowanetz M, Fine GD, Hamid O, Gordon MS, et al. Predictive correlates of response to the anti-PD-L1 antibody MPDL3280A in cancer patients. Nature. 2014;515:563–7.

  47. 47.

    Gubin MM, Zhang X, Schuster H, Caron E, Ward JP, Noguchi T, et al. Checkpoint blockade cancer immunotherapy targets tumour-specific mutant antigens. Nature. 2014;515:577–81.

  48. 48.

    Snyder A, Makarov V, Merghoub T, Yuan J, Zaretsky JM, Desrichard A, et al. Genetic basis for clinical response to CTLA-4 blockade in melanoma. N Engl J Med. 2014;371:2189–99.

  49. 49.

    Troyanskaya O, Cantor M, Sherlock G, Brown P, Hastie T, Tibshirani R, et al. Missing value estimation methods for DNA microarrays. Bioinformatics. 2001;17:520–5.

  50. 50.

    Dedeurwaerder S, Defrance M, Calonne E, Denis H, Sotiriou C, Fuks F. Evaluation of the Infinium Methylation 450 K technology. Epigenomics. 2011;3:771–84.

  51. 51.

    Smyth GK. Linear models and empirical bayes methods for assessing differential expression in microarray experiments. Stat Appl Genet Mol Biol. 2004;3:Article3.

  52. 52.

    Ernst J, Kheradpour P, Mikkelsen TS, Shoresh N, Ward LD, Epstein CB, et al. Mapping and analysis of chromatin state dynamics in nine human cell types. Nature. 2011;473:43–9.

  53. 53.

    Cirenajwis H, Ekedahl H, Lauss M, Harbst K, Carneiro A, Enoksson J, et al. Molecular stratification of metastatic melanoma using gene expression profiling - prediction of survival outcome and benefit from molecular targeted therapy. Oncotarget. 2015;6:12297–309.

  54. 54.

    Lauss M, Visne I, Kriegner A, Ringnér M, Jönsson G, Höglund M. Monitoring of technical variation in quantitative high-throughput datasets. Cancer Inform. 2013;12:193–201.

Download references

Acknowledgements

The study has been supported by the Swedish Cancer Society, The Swedish Research Council, BioCARE, Berta Kamprad Foundation, The Gunnar Nilsson Cancer Foundation, The Gustav Vth Jubilee Foundation, and Governmental Support for Medical Research (ALF).

Author information

Affiliations

  1. Department of Oncology and Pathology, Clinical Sciences, Lund University Hospital, Lund University, Lund, 221 85, Sweden

    • Martin Lauss
    • , Markus Ringnér
    • , Anna Karlsson
    • , Katja Harbst
    • , Johan Staaf
    •  & Göran Jönsson

  2. Section of Oncology, Department of Clinical Science, University of Bergen, Bergen, Norway

    • Christian Busch
    • , Jürgen Geisler
    •  & Per Eystein Lønning

  3. Department of Clinical Oncology, Haukeland University Hospital, Bergen, Norway

    • Christian Busch
    • , Jürgen Geisler
    •  & Per Eystein Lønning

  4. Present Address: Department of Clinical Molecular Biology and Laboratory Sciences, Akershus University Hospital, Lørenskog, Norway

    • Jürgen Geisler

  5. Institute of Clinical Medicine, University of Oslo, Oslo, Norway

    • Per Eystein Lønning

Authors

  1. Search for Martin Lauss in:

  2. Search for Markus Ringnér in:

  3. Search for Anna Karlsson in:

  4. Search for Katja Harbst in:

  5. Search for Christian Busch in:

  6. Search for Jürgen Geisler in:

  7. Search for Per Eystein Lønning in:

  8. Search for Johan Staaf in:

  9. Search for Göran Jönsson in:

Corresponding author

Correspondence to Göran Jönsson.

Additional information

Competing interests

The authors declare that they have no competing interests.

Authors’ contribution

ML and GJ conceived and designed the study. ML and GJ drafted the manuscript with the help of MR and JS. AK and KH performed methylation analysis. CB, JG and PEL interpreted data and provided tumor samples. All authors read and approved the manuscript.

Additional files

Additional file 1: Figure S1.

Robustness of methylation subtypes. Principal component analysis to monitor data bias due to technical variables in the Bergen (A) and TCGA (B) cohorts, respectively. The entire set of 473,864 CpGs was used for principal component analysis. The heatmaps indicate the association of a sample annotation to each of the principal components. The strength of association is specified by the log10 p-value of the linear model with the respective principal component as dependent variable and sample annotation as regressor. DNAconc = DNA concentration. Technical variables of TCGA data are termed as defined by the TCGA consortium. TCGA = The Cancer Genome Atlas Consortium. Abbreviations as in Figure 1 of the main manuscript. (C) Sample overlap when using different CpG sets for group discovery in Bergen and TCGA data, respectively. For group discovery we used CpGs with variant methylation between melanoma and melanocytes. CpGs were required to be either methylated or de-methylated in at least 10 tumors for our final subtypes. The CpG set for 10 tumors contained 9,886 melanoma-methylated and 5,236 melanoma-demethylated CpGs. The heatmap displays the overlap of the resulting three consensus clusters at various tumor cutoffs. (D) Heatmap of TCGA sample co-occurrence between unsupervised consensus clusters and methylation subtypes obtained from (supervised) nearest centroid classification. Figure S2. Promoter island consensus clusters. The group discovery CpG set was reduced to CpGs located within 1500 bp upstream of transcription start sites and within a CpG island. In total this analysis includes 947 CpGs, of which 930 are hypermethylated, and 17 are hypomethylated in tumors as compared to melanocytes. Two-group consensus solutions were favorable to three-group solutions in Bergen and TCGA data, respectively. Figure S3. Signature expression across methylation subtypes in TCGA data. (A) ESTIMATE scores and tumor purity. P-value from Kruskal-Wallis test. (B) Mean expression values of gene modules and GO-term ‘cell cycle’. P-value from anova. TCGA tumor data. Figure S4. Aberrant methylation in melanoma compared to colon, lung and breast cancer. (A) Venn diagrams of aberrant methylation on the CpG and gene level. (B) Aberrant methylation in ES-cell chromatin context. Chromatin categories as in ENCODE project. (C) Aberrant methylation in melanocyte chromatin context. Chromatin categories as in Epigenome Roadmap project. Figure S5. Driver gene mutations and methylation subtypes in the TCGA cohort. (A) Number of non-silent mutations per sample across methylation subtypes. (B) Non-silent and hotspot mutations of reported melanoma driver genes across subtypes. Figure S6. Expression of MAPK and PI(3)K pathway genes across methylation subtypes. (A) Expression of MAPK and PI(3)K pathway. fdr = false discovery rate for p-values from anova using Benjamini-Hochberg adjustment. (B) Cross-table of gene expression and methylation subtypes. (PDF 865 kb)

Additional file 2: Table S1.

Centroids of methylation subgroups. (XLS 1550 kb)

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Keywords

  • Melanoma
  • DNA methylation
  • Gene expression
  • Melanocytes
  • Molecular subtypes
  • Polycomb

BMC Medical Genomics

ISSN: 1755-8794

Contact us