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Research Article

DNA Hypomethylation Contributes to Genomic Instability and Intestinal Cancer Initiation

Karyn L. Sheaffer, Ellen N. Elliott and Klaus H. Kaestner
DOI: 10.1158/1940-6207.CAPR-15-0349 Published July 2016

Abstract

Intestinal cancer is a heterogeneous disease driven by genetic mutations and epigenetic changes. Approximately 80% of sporadic colorectal cancers are initiated by mutation and inactivation of the adenomatous polyposis coli (APC) gene, which results in unrestrained intestinal epithelial growth and formation of adenomas. Aberrant DNA methylation promotes cancer progression by the inactivation of tumor suppressor genes via promoter methylation. In addition, global DNA hypomethylation is often seen before the formation of adenomas, suggesting that it contributes to neoplastic transformation. Previous studies employed mice with a hypomorphic mutation in DNA methyltransferase 1 (Dnmt1), which exhibited constitutive global DNA hypomethylation and decreased tumorigenesis in the ApcMin/+ mouse model of intestinal cancer. However, the consequences of intestinal epithelial-specific acute hypomethylation during ApcMin/+ tumor initiation have not been reported. Using temporally controlled intestinal epithelial-specific gene ablation, we show that total loss of Dnmt1 in the ApcMin/+ mouse model of intestinal cancer causes accelerated adenoma initiation. Deletion of Dnmt1 precipitates an acute response characterized by hypomethylation of repetitive elements and genomic instability, which surprisingly is followed by remethylation with time. Two months post-Dnmt1 ablation, mice display increased macroadenoma load, consistent with a role for Dnmt1 and DNA methylation in maintaining genomic stability. These data suggest that DNA hypomethylation plays a previously unappreciated role in intestinal adenoma initiation. Cancer Prev Res; 9(7); 534–46. ©2016 AACR.

See related article by Lee and Laird, p. 509

Introduction

Intestinal and colorectal cancers are multifactorial diseases with various inputs including diet, environment, genetic mutations, and epigenetic abnormalities. The disease first manifests as an overproliferation defect in the form of polyps that, if not removed, can progress to precancerous adenomas. Further transition to invasive and metastatic cancer is due to the accumulation of multiple genetic mutations and epigenetic changes that alter gene expression patterns, driving neoplastic transformation and growth (1). However, the extent to which epigenetic modifications, and specifically DNA methylation, contribute to the initiation and progression of intestinal cancer is unclear.

Neoplastic tissues frequently display global DNA hypomethylation, which can occur passively through loss of the maintenance methyltransferase, DNMT1, or actively by TET enzyme–mediated oxidation of methyl cytosine, followed by base excision repair (2–4). Alternatively, some tumors exhibit increased DNA methylation on specific tumor suppressor gene promoters, which requires the de novo DNA methyltransferases, DNMT3A and DNMT3B. Hypermethylation of tumor suppressor gene promoters causes decreased activity of the associated genes and promotes cancer cell growth in vitro (5). Comparison of human colon adenomas to control tissue revealed that although proximal promoter CpG islands are often hypermethylated in tumors, DNA hypomethylation is found genome-wide, including neighboring CpG island shores and repetitive elements (6, 7). Hypomethylated intergenic and intronic regions appear early in the transition from normal to neoplastic (8, 9), suggesting a more important role for DNA hypomethylation in cancer initiation than previously appreciated.

Previously, the role of Dnmt1 in intestinal tumorigenesis was studied in the ApcMin/+ mouse model. This paradigm mimics the hereditary human colon cancer syndrome Familial Adenomatous Polyposis (FAP), which is caused by germline mutations of the APC gene (10). LOH at the APC locus causes β-catenin stabilization and unrestricted Wnt activity, resulting in the formation of macroscopic adenomas by 3 months of age (11–13). LOH is also a common triggering mechanism for sporadic intestinal and colorectal tumor development (1), rendering the ApcMin/+ mouse a useful model for the study of intestinal cancer initiation.

Multiple hypomorphic Dnmt1 paradigms show complete block of macroscopic tumor formation (14–18). The authors concluded that Dnmt1 and DNA methylation are required for adenoma development in the ApcMin/+ model. These studies employed hypomorphic Dnmt1 mice, which express constitutively reduced Dnmt1 levels from earliest development onward in all tissues (15), including nonepithelial cells, such as myofibroblasts. Mesenchymally expressed genes have been shown to be strong modifiers of the ApcMin/+ tumor load (19) and could thus contribute to the observed phenotype in the Dnmt1-hypomorphic ApcMin/+ intestine. Furthermore, continuous DNA hypomethylation may mask acute affects during the neoplastic transformation, which occurs prior to reported observations of macroadenomas at 6 months of age. Because of these limitations, the precise mechanism of how DNA methylation acts within the intestinal epithelium during adenoma initiation remains to be determined.

To address this important knowledge gap, we employed a temporally controlled, intestinal epithelial-specific gene ablation model to delete Dnmt1 and decrease maintenance DNA methylation. Ablation of Dnmt1 causes an acute phenotype characterized by global DNA hypomethylation, genome instability, and apoptosis. The severe effects of Dnmt1 ablation result in a dramatic increase in adenoma initiation by accelerated LOH at the Apc locus. These results strongly support a role for DNA hypomethylation in chromosomal instability and tumor initiation.

Materials and Methods

Mice

Dnmt1loxP/loxP mice were provided by Rudolf Jaenisch (20), Villin-Cre-ERT2 mice were received from Sylvia Robine (21), and ApcMin/+ mice from the Jackson Laboratories (10, 12). For Dnmt1 deletion experiments, Cre recombination activity was induced by 3 daily intraperitoneal injections of 1.6 mg tamoxifen (Sigma) in an ethanol/sunflower oil mixture. In all experiments, littermate controls without the VillinCreERT2 transgene were also tamoxifen-treated. All procedures involving mice were conducted in accordance with approved Institutional Animal Care and Use Committee protocols.

Histology

Tissues were isolated and fixed using 4% paraformaldehyde in PBS and then embedded in paraffin. Antigen retrieval was performed using the 2100 Antigen-Retriever in Buffer A (Electron Microscopy Sciences) and standard immunostaining procedures were performed for Dnmt1 (Santa Cruz), E-cadherin (BD Transduction Laboratories), Sox9 (Millipore), Ki67 (BD Pharmingen), β-catenin (BD Transduction Laboratories), CycD1 (Biocare Medical), Epcam (Abcam), and γH2AX (Cell Signaling Technology). TUNEL staining was performed using TUNEL Label and Enzyme (Roche) and AlexaFluor 555-aha-dUTP (Life Technologies). Percentages of TUNEL+ nuclei were determined by counting the number of nuclei positive for TUNEL staining and dividing by the total number of nuclei in the image. The same method was performed to quantify the percentage of γH2AX+ cells. All microscopy was performed on a Nikon Eclipse 80i.

Laser capture microdissection

Tumor and nontumor epithelial cell DNA was collected using a Leica LMD7000 Laser Microdissection microscope and the Arcturus PicoPure DNA Isolation Kit (Applied Biosystems).

Targeted bisulfite sequencing

Mouse gDNA (100 ng) was bisulfite converted using the Epitect Bisulfite Kit (Qiagen). Template DNA was amplified using KAPA HIFI Uracel+ (KAPA) with primers directed to the LINE1 elements (22), the H19 imprinting control region, Olfm4 and Hes1 (23), Vdr, Hic1, Sfrp5, Mgmt, Dusp6, c-Fos, Msln, and S100a4. Primer sets and regions subsequently sequenced can be found in Supplementary Table S1. Sequencing libraries were prepared and analyzed using the BiSPCR2 strategy (LINE1, H19) or the standard protocol (Vdr, Hic1, Sfrp5, Mgmt, Dusp6, c-Fos, Msln, S100a4), described previously (23, 24).

Tumor evaluation

Macroscopic tumors were counted immediately after tissue isolation using a stereoscope. Adenoma size was calculated by measuring the width of neoplastic lesions on hematoxylin and eosin (H&E)-stained small intestine sections using ImageJ. Histologic pathology was performed by the Comparative Pathology Core at the University of Pennsylvania School of Veterinary Medicine (Pennsylvania, PA) following the guidelines as described previously (25). LOH was determined as described previously (26).

Phosphorylated H3 cell-cycle quantification

ApcMin/+;Dnmt1loxP/loxP;Villin-Cre-ERT2 mutants and sibling ApcMin/+;Dnmt1loxP/loxP controls were injected with tamoxifen at 1 month of age. Small intestines were collected 1 week, 1 month, and 2 months following tamoxifen administration, in separate cohorts of mice. Following fixation, tissue sections were co-stained for phosphorylated histone H3 (PH3) to identify cells in M phase and β-catenin to identify regions of hyperproliferative neoplastic epithelium. We counted the number of PH3+ nuclei and divided it by the total number of nuclei in the respective region. This calculation was also performed for neoplastic intestinal epithelium at both 1 and 2 months post-tamoxifen time points, for controls and mutants.

qRT-PCR

Intestines isolated 1 week post-tamoxifen were gently scraped to remove villi and treated with EDTA to isolate crypt cells. Macroscopic tumors and adjacent normal tissue, from intestines isolated 2 months post-tamoxifen, were visualized and dissected using a stereoscope. RNA was extracted using the TRIzol RNA isolation protocol (Invitrogen), followed by RNA cleanup using the RNeasy Mini Kit (Qiagen). mRNA expression was measured using quantitative RT-PCR, as described previously (27). The SYBR green qPCR master mix (Agilent) was used in all qPCR reactions, and the fold change was calculated relative to the geometric mean of Tbp and β-actin, using the ΔCt method. The method of normalizing to the geometric mean of a set of reference genes has been described previously (28). Primer sequences can be found in Supplementary Table S1.

Results and Discussion

Deletion of Dnmt1 in the intestinal epithelium of adult ApcMin/+ mice induces acute global hypomethylation

To determine the role of Dnmt1 in intestinal adenoma initiation, we employed ApcMin/+;Dnmt1loxP/loxP;Villin-Cre-ERT2 mice to inducibly delete Dnmt1 throughout the intestinal epithelia. ApcMin/+;Dnmt1loxP/loxP;Villin-Cre-ERT2 mice and their ApcMin/+;Dnmt1loxP/loxP siblings (referred to as “mutants” and “controls,” respectively) were injected with tamoxifen at 4 weeks of age to induce Dnmt1 deletion (Supplementary Fig. S1). On the basis of our previous analysis of Dnmt1 ablation in the intestinal epithelium, we isolated the small intestine 1 week after tamoxifen treatment (23). To address the role of Dnmt1 in adenoma development, we analyzed a second cohort of mice in which we harvested the intestine and colon 2 months post-tamoxifen treatment, at 3 months of age. By 3 months of age, ApcMin/+ mice display macroscopic lesions (11, 12). Thus, 2 months post-tamoxifen allowed us to contrast adenoma development in Dnmt1 mutants with ApcMin/+;Dnmt1loxP/loxP controls. At 1 week and 2 months following tamoxifen treatment, Dnmt1 deletion was effective throughout the mutant epithelia of small intestine (Fig. 1A–D and G). Dnmt1 deletion was also maintained in mutant adenomas (Fig. 1E, F, and H). As ApcMin/+ mice exhibit tumors predominantly in the small intestine (12, 29), we focused our studies on adenoma development in the small intestinal epithelium. First, we analyzed the effects of Dnmt1 deletion in the non-neoplastic epithelium of ApcMin/+ mice.

Figure 1.
Figure 1.

Conditional ablation of Dnmt1 in the ApcMin/+ intestinal epithelium. A–F, Dnmt1 deletion is maintained 1 week (B) and 2 months (D) after tamoxifen treatment in the adult mouse small intestinal epithelium. Immunohistochemical staining of Dnmt1 protein is evident in the crypt epithelia located just above the submucosa (outlined in black) of control mice at both time points (A, C) but is absent in mutant mice (B, D). Neoplastic epithelia (outlined in red) display high levels of Dnmt1 protein in control animals (E). Deletion of Dnmt1 protein is maintained in the neoplastic epithelium (outlined in red) in mutant animals 2 months after tamoxifen treatment (F). G and H, qRT-PCR analysis comparing the relative gene expression levels of Dnmt1 in controls and mutants 1 week (G) and 2 months (H) after tamoxifen treatment (n = 3–5 per genotypes). Compared with controls, Dnmt1 mutants express significantly lower levels of Dnmt1, and deletion is maintained in macroscopic tumors isolated 2 months post-tamoxifen. Gene expression is calculated relative to the geometric mean of TBP and β-actin. All scale bars are 50 μm. *, P < 0.05; **, P < 0.01; Student t test.

To estimate global DNA methylation levels, we performed targeted bisulfite sequencing of the H19 imprinting control region (ICR) and the Long Interspersed Nucleotide Element 1 (LINE1). The process of imprinting is dependent on DNA methylation and refers to the methylation of alleles in a parental-specific manner to restrict gene expression to one allele (30). The H19 imprinting control region is methylated on the paternally inherited allele, thereby ensuring maternal allele expression (31). LINE1 retrotransposon loci comprise approximately 20% of the mouse and human genome, are maintained in a highly methylated state to inhibit transposase activity, and are a representative of genome-wide methylation levels (32–34). We employed laser capture microdissection (LCM) to collect crypts from mutant and control intestines 1 week following tamoxifen treatment. H19 methylation was maintained despite loss of Dnmt1 (Fig. 2A), implicating a role for Dnmt3a and Dnmt3b in maintaining genomic imprints, as suggested previously (35, 36). Strikingly, within 1 week following Dnmt1 deletion, we observed a 35% reduction in DNA methylation at the LINE1 loci in mutant crypts compared with the control crypt epithelium (Fig. 2B). Thus, Dnmt1 is required acutely to maintain DNA methylation levels on LINE1 elements but is not required for maintenance of imprinted loci in the rapidly proliferating intestinal epithelium.

Figure 2.
Figure 2.

DNA methylation dynamics following Dnmt1 deletion. Targeted bisulfite sequencing of the H19 imprinting control region and the LINE1 repetitive elements was performed to estimate maintenance methylation of Dnmt1-deficient intestinal crypt cells. Crypt epithelium was isolated by LCM from controls and mutants at 1 week (n = 3–4 per group), 1 month (n = 2 for controls, n = 4 for mutants), or 2 months (n = 4–7 per group) following tamoxifen treatment. (A, C, E) Targeted bisulfite sequencing of 6 CpGs in the H19 imprinting control region (Chr7: 149,766,621–149,766,690). At 1 week (A), 1 month (C), and 2 months (E) following tamoxifen administration, H19 methylation levels are comparable between Dnmt1 mutants and controls. B, D, F, targeted bisulfite sequencing of 9 CpGs in the LINE1 repetitive elements (NCBI Accession #D84391: 976–1,072). LINE1 methylation levels 1 week after tamoxifen injection are significantly reduced in crypts of mutant mice compared with controls (B). One month (D) and 2 months (F) after tamoxifen-induced ablation of Dnmt1, global DNA methylation levels have been restored to baseline. For all graphs, data are presented as average ± SEM. **, P < 0.01 by 2-tailed Student t test.

To determine whether global hypomethylation of repetitive elements was sustained over time, we isolated crypt epithelium from mutants and controls 1 and 2 months following tamoxifen treatment. Surprisingly, we found no differences in methylation levels in all conditions tested, demonstrating that DNA methylation had been fully restored after temporary loss following Dnmt1 ablation (Fig. 2C–F). These results were unexpected, as Dnmt1 deletion was maintained at 2 months after tamoxifen administration (Fig. 1C–F). Recovery of DNA methylation was likely driven by the de novo DNA methyltransferases Dnmt3a and 3b, which are also expressed in the intestinal epithelium (23).

Dnmt1 mutants display increased tumor initiation

One and 2 months following tamoxifen injection, the small intestine was examined for neoplastic transformation. Surprisingly, H&E staining revealed a dramatic increase in the number of neoplastic lesions throughout the mutant small intestine at 2 months, but not 1 month, post-tamoxifen (Fig. 3A–D). Indeed, mutants displayed more than 6-fold more macroscopic adenomas than controls at 2 months following tamoxifen injection (Fig. 3E; n = 17–20 per group). In addition, mutant small intestinal tumors were on average twice as large as those of controls at 2 months post-tamoxifen injection (Fig. 3F; n = 5–8 per group). Furthermore, we observed 58% incidence of neoplastic transformation in colons of mutant mice (n = 12) compared with 14% in controls (n = 7; Supplementary Fig. S2).

Figure 3.
Figure 3.

Deletion of Dnmt1 in adult ApcMin/+ mice accelerates adenoma initiation. A–D, H&E staining of control and mutant intestinal epithelium 1 month (A and B) and 2 months (C and D) after tamoxifen injection. H&E staining shows disruption of normal intestinal epithelial morphology in the small intestine of tamoxifen-treated mutants compared with control mice (B vs. A, D vs. C). Scale bars are 50 μm. C, intestinal epithelial-specific Dnmt1 deletion causes increased incidence of macroscopic tumors. Total number of macroscopic tumors was counted throughout the entire small intestine of mutant and control mice, 1 month (n = 5–7 per group) and 2 months (n = 17–20 per group) following tamoxifen treatment. E, Dnmt1 deletion results in increased size of neoplastic lesions in the small intestine 2 months after tamoxifen treatment. Neoplastic lesions were measured in control and mutant mice at 1 month (n = 2 for controls, n = 3 for mutants) and 2 months (n = 5 for controls, n = 8 for mutants) following tamoxifen injection. For all graphs, data are presented as average ± SEM. ***, P < 0.001 by one-way ANOVA.

Previously, it had been reported that partial loss of Dnmt1 produces a block in the progression of adenomas in the ApcMin/+mouse paradigm (14–18), which is in sharp contrast to our findings of an increased number of macroscopic lesions in the ApcMin/+;Dnmt1loxP/loxP;VillinCreERT2 deletion model. To confirm that these lesions are bona fide adenomas, we consulted with a pathologist to perform histopathologic assessment on the intestines of mutant and control mice, 1 and 2 months following tamoxifen treatment at 4 weeks of age. Using criteria described by Biovin and colleagues (25), we found 15-fold more lesions that had progressed to adenomas in mutant mice compared with ApcMin/+controls (Supplementary Fig. S3B) at 2 months post-tamoxifen injection. At 1 month post-tamoxifen, all lesions observed in both controls and Dnmt1 mutants displayed similar histopathology and were characterized as gastrointestinal intraepithelial neoplasias (Supplementary Fig. S3A).

DNA hypomethylation is observed at specific genes in tumors

DNA methylation is important for maintaining appropriate intestinal stem cell gene expression, and loss of Dnmt1 in the intestinal epithelium results in increased crypt cell proliferation (23). Previously, we observed that 1 week following deletion of Dnmt1, DNA methylation was decreased at enhancers associated with genes critical for intestinal stem cell proliferation, Hes1 and Olfm4 (23). Thus, altered DNA methylation could be responsible for the dramatic increase in lesions observed in our mutant animals. We employed LCM to collect crypt epithelia and neoplastic tumors from mutant and control intestines 2 months following tamoxifen treatment. We employed targeted bisulfite sequencing of the H19 ICR and LINE1 loci to determine whether global methylation levels were changed in tumors compared with epithelia in mice 2 months following tamoxifen injection. Interestingly, DNA methylation of the H19 ICR and LINE1 loci were unchanged in all conditions (Fig. 4A and B). Control mice displayed increased methylation at Hes1 and Olfm4 in tumors compared with adjacent epithelia (Fig. 4C). Mutant mice exhibited little change in methylation when comparing control and mutant epithelia (Fig. 4C). However, mutant tumors are significantly hypomethylated at the Hes1 enhancer compared with control tumors (Fig. 4C). Furthermore, mutant tumors are significantly hypomethylated at both Hes1 and Olfm4 loci compared with adjacent non-neoplastic epithelia (4C, dashed lines). These data are intriguing because Hes1 expression is increased in stem cell–like cells in colon cancer (37), and our results suggest that DNA methylation may play a role in activating Hes1 expression in tumors.

Figure 4.
Figure 4.

Dnmt1-mutant tumors show increased hypomethylation at potential oncogenes. Targeted bisulfite sequencing was performed to estimate maintenance methylation of Dnmt1-deficient tumors, relative to controls tumors and to adjacent non-neoplastic crypt epithelium. Tumors and crypt epithelium were isolated by LCM from controls and mutants 2 months following tamoxifen treatment. A and B, analysis of 9 CpGs in the LINE1 repetitive elements (NCBI Accession #D84391: 976–1,072) revealed no alterations in methylation of the repetitive transposable elements (A). Analysis of 6 CpGs in the H19 imprinting control region (Chr7: 149,766,621–149,766,690) showed that H19 methylation levels are comparable between Dnmt1 mutants and controls, in both tumor and nontumor epithelium. C, potential enhancer regions of genes involved in intestinal stem cell identity and proliferation, Olfm4 and Hes1 were analyzed for methylation changes in all conditions. Regional averages of 7 CpGs in the Olfm4 enhancer (chr14: 80,399,983–80,400,271) and 6 CpGs in the Hes1 enhancer (chr16: 30,055,572–30,055,738) are shown. The Hes1 enhancer shows increased methylation in control tumors compared with adjacent tissue, which is abolished by Dnmt1 deletion. D, genes with cancer-specific promoter hypermethylation, Vdr, Hic1, Sfrp5, Mgmt were analyzed for methylation changes in all conditions. Regional averages of 8 CpGs in the Vdr promoter (chr15: 97,731,208–97,731,590), 16 CpGs in Hic1 promoter (chr11: 74,983,743–74,983,918), 16 CpGs in the Sfrp5 promoter (chr19: 42,276,328–42,276,453), and 19 CpGs in Mgmt promoter (chr7: 144,086,076–144,086,345) are shown. Only Vdr and Mgmt displayed significant hypermethylation in control tumors compared with adjacent tissue. Loss of Dnmt1 caused significant loss of hypermethylation at both loci, suggesting that hypermethylation of these genes is not required for tumor progression. E, genes with cancer-specific promoter hypomethylation, Dusp6, c-Fos, Msln, S100a4, were analyzed for methylation changes in all conditions. Regional averages of 8 CpGs in the Dusp6 promoter (chr10: 98,728,738–98,729,028), 14 CpGs in the c-Fos promoter (chr12: 86,817,243–86,817,533), 6 CpGs in the Msln promoter (chr17: 25,891,502–25,891,643), and 3 CpGs in the S100a4 promoter (chr3: 90,407,319–90,407,489) are shown. Only Dusp6 and c-Fos displayed significant hypomethylation in control tumors compared with adjacent tissue. Dnmt1 deletion caused even more drastic loss of methylation at both promoters, suggesting that loss of Dnmt1 may be driving activation of potential oncogenes during tumor growth.

Aberrant DNA methylation drives intestinal cancer cell growth in multiple paradigms (14–18) and could be responsible for the dramatic increase in lesion growth observed in our mutant animals. Hypermethylation of tumor suppressor genes allows unrestrained growth and is a hallmark of the colorectal cancer CpG island methylator phenotype (CIMP; ref. 38). We tested promoter methylation of four genes that have been previously shown to be hypermethylated in adenomas, Vdr, Hic1, Sfrp5, and Mgmt (39–43). To our surprise, only Vdr and Mgmt showed increased methylation in adenomas, relative to nontumor epithelia (Fig. 4D). Dnmt1 deficiency reduced methylation in mutant tumors compared with control tumors in an inconsistent manner (Fig. 4D), suggesting that hypermethylation at these loci is not required for tumor growth. DNA hypomethylation has also been reported at several potential oncogenes including Dusp6, c-Fos, Msln, and S100a4 (43–46). Although none of these gene promoters show significant loss of methylation in tumors compared with the respective normal epithelia, we observed significantly decreased methylation at Dusp6 and c-Fos in Dnmt1 mutant relative to control adenomas (Fig. 4E). c-Fos is a potent driver of colon cancer cell growth (47), and its expression is regulated by DNA hypomethylation in several cancer types (48, 49). These data suggest that hypomethylation at oncogenes may be driving tumor growth in Dnmt1-deficient ApcMin/+ mutant animals.

Dnmt1-null tumors are initiated by LOH and Wnt activation

We further investigated tumor initiation to determine whether the observed changes in DNA methylation were a causative factor of neoplastic transformation. Adenoma formation in the ApcMin/+ mouse model is driven by LOH at the Apc locus, which causes nuclear accumulation of β-catenin and activation of Wnt signaling (13). LOH is observed in virtually all ApcMin/+ intestinal tumors (26, 50). To characterize adenoma initiation by LOH in detail, we employed LCM to isolate neoplastic and normal intestinal epithelial cells from mutant mice and their control siblings, 2 months following tamoxifen treatment. Since the number of macroscopic lesions found in controls at 1-month post-tamoxifen is very small (Fig. 3E, Supplementary Fig. S3), we focused on the 2-month time point for LOH analysis. DNA was isolated from these samples (∼1,000 cells per sample), and the status of the Apc alleles was examined as described previously (26). Mutant tumors displayed LOH at a rate similar to that of control tumors (Fig. 5A), demonstrating that Dnmt1-mutant ApcMin/+ mice initiate tumors by the same mechanism.

Figure 5.
Figure 5.

Dnmt1-deficient ApcMin/+ intestinal tumors display increased Wnt signaling. A, control and mutant mice were tamoxifen-treated at 4 weeks of age, and intestines were harvested 2 months later. Intestinal tumors from control and mutant mice were isolated by LCM for PCR testing of LOH at the Apc locus. Results of PCR testing demonstrate that mutant tumors display LOH at a rate similar to that of controls. B–J, control and mutant mice were tamoxifen-treated at 4 weeks of age, and intestines were harvested 1 or 2 months later for immunostaining analysis of Wnt signaling targets. B–D, nuclear β-catenin, as visualized by immunohistochemical staining, is increased in Dnmt1-mutant intestine 2 months after tamoxifen treatment (D), compared with tamoxifen-treated, age-matched control small intestine (B). One month following Dnmt1 ablation, mutant small intestine displays nuclear β-catenin levels similar to that observed in the 2-month controls (C compared with B, respectively). E–G, expression of the Wnt signaling target cyclin D1 (CycD1) is increased in Dnmt1-deficient tumors (G) relative to age-matched control tumors (E). At 1-month post-Dnmt1 ablation, CycD1 staining appears slightly increased compared with the 2-month controls (F vs. E, respectively). CycD1 (red), DAPI (blue). H–J, Sox9 immunofluorescent staining shows increased Sox9 levels in Dnmt1-deficient tumors (J) compared with control tumors (H) 2 months following tamoxifen treatment. At 1 month after Dnmt1 ablation, increased Sox9 expression is visible by immunostaining (I compared with control, H). Sox9 (red), DAPI (blue). All scale bars are 50 μm.

Several lines of evidence confirm that the numerous adenomas that develop in the Dnmt1-deficient ApcMin/+ mice are the result of Wnt pathway activation. Mutant adenomas at both 1 and 2 months following tamoxifen treatment exhibited increased nuclear β-catenin protein (Fig. 5B–D) relative to 2-month controls. Multiple Wnt signaling targets, such as CyclinD1 (Fig. 5E–G) and Sox9 (Fig. 5H–J), were also strongly activated. These data demonstrate that total loss of Dnmt1 in the mature small intestinal epithelium promotes neoplastic progression, most likely through a mechanism that enhances LOH at the ApcMin/+ locus.

Dnmt1-mutant mice display acute increases in proliferation and apoptosis

Because of the dramatic difference in lesion size and hypomethylation at potential oncogenes observed in the inducible Dnmt1-mutant intestine, we investigated whether Dnmt1 deficiency had a direct impact on cell proliferation in ApcMin/+ adenomas or the non-neoplastic crypt epithelium. We determined percentages of control and mutant epithelial cells in M phase by staining for pH3, at 1 week, 1 month, and 2 months post-tamoxifen treatment. One week post-tamoxifen (Fig. 6A–C), the percentage of pH3+ nuclei was significantly increased in the Dnmt1-deficient epithelium relative to control (n = 4 per group). Interestingly, at 1 month (Fig. 6D–F) and 2 months (Fig. 6G–I) following tamoxifen injection, the proliferation rate was equivalent in Dnmt1-positive or -negative tumors and in the adjacent crypt epithelium.

Figure 6.
Figure 6.

Loss of Dnmt1 in the ApcMin/+ intestine causes an acute increase in crypt cell proliferation. Percentage of cells in mitosis was determined by immunostaining and counting of pH3+ nuclei in the small intestine 1 week, 1 month, and 2 months following tamoxifen treatment. The percentage of pH3+ cells was calculated as the number of pH3+ nuclei divided by the total number of epithelial nuclei. A–C, one week following tamoxifen injection, mutants displayed a significantly increased percentage of pH3+ cells (C, n = 4 per genotype). Representative images of pH3 immunostaining are shown for controls (A) and Dnmt1 mutants (B). D–F, one month after tamoxifen treatment, mutants (E) and controls (D) displayed comparable percentages of pH3+ cells, in both tumors and noncancerous epithelia (F). Twenty-four tumors across 5 mice were counted for Dnmt1 mutants; 4 tumors across 4 mice were counted for controls. Approximately 1,500 noncancerous cells were counted from the same biologic replicates to calculate pH3 frequency in nontumor tissue. G–I, two months after tamoxifen treatment, mutants (H) and controls (G) displayed comparable percentages of pH3+ cells, in both tumors and noncancerous epithelia (I). Twenty-four tumors across 7 mice were counted for Dnmt1 mutants; 8 tumors across 3 mice were counted for controls. Nontumor epithelia quantified as in (D-F). E-cadherin (green) outlines the intestinal epithelium. All scale bars are 50 μm. For all graphs, data are presented as average ± SEM. **, P < 0.01 by Student t test (C). One-way ANOVA was performed for (F, I), and the results were not significant.

We also examined the small intestine at all three time points for signs of cell death using terminal deoxynucleotidyl transferase–mediated dUTP nick end labeling (TUNEL), which detects DNA fragmentation in apoptotic cells. We quantified the percent of epithelial cells that were TUNEL+, similar to the pH3 staining quantification. Mutants 1 week after tamoxifen treatment displayed a significantly higher proportion of TUNEL+ cells compared with controls (Fig. 7A–C). Both control and mutant adenomas exhibited only rare epithelial cells positive for TUNEL, and we found no differences in cell death between mutant and control neoplastic and non-neoplastic epithelia, at 1 month (Fig. 7D–F) or 2 months (Fig. 7G–I) following tamoxifen administration. However, many subepithelial cells were TUNEL-positive (Fig. 7D, E, G, and H). These data demonstrate that loss of Dnmt1 in the adult intestinal epithelium in vivo has acute temporary effects on intestinal proliferation and apoptosis but no effect on ApcMin/+ adenoma proliferation or cell death. Overall, our results suggest that the increase in adenoma number and size found in the Dnmt1-mutant mice is driven by accelerated tumor initiation through LOH.

Figure 7.
Figure 7.

Loss of Dnmt1 results in a short-term increase in intestinal epithelial apoptosis but is not altered 1 or 2 months following Dnmt1 deletion. TUNEL staining (red) was performed to detect apoptotic cells, with E-cadherin (green) to outline the epithelium. The percentage of apoptotic cells was determined by counting of the TUNEL-positive (TUNEL+) nuclei in the small intestine 1 week, 1 month, and 2 months following tamoxifen treatment. The percentage of TUNEL+ cells was calculated as the number of TUNEL+ nuclei divided by the total number of epithelial nuclei. A–C, one week following tamoxifen treatment, Dnmt1 mutants have significantly higher rates of apoptosis than controls (B vs. A; quantitation in C). N = 4 per group. ***, P < 0.001 by Student t-test. D–F, one month after tamoxifen injection, both tumor and nontumor epithelia contain TUNEL-positive cells, which is unchanged in mutant mice (D vs. E, quantitation in F). n = 3 biologic replicates per group, with 8 tumors counted from controls and 14 tumors counted from mutants. G–I, two months after tamoxifen injection, both tumor and nontumor epithelia contain TUNEL-positive cells at low frequency in control mice, which is unchanged in mutant mice (H vs. G, quantitation in I). n = 3–5 biological replicates per group; two tumors were counted from controls, and 10 tumors were counted from mutants. All scale bars are 50 μm. For all graphs, data are presented as average ± SEM. One-way ANOVA test was performed in (F, I), and results were not significant.

Dnmt1-deficient ApcMin/+ intestinal epithelia exhibit increased genomic instability

Next, we considered the molecular mechanisms behind the accelerated LOH we observed in the Dnmt1-deficient intestinal epithelium. We hypothesized that the established role of Dnmt1 in the preservation of genomic stability might contribute to the phenotype. DNA methylation has been linked to mismatch repair (MMR) deficiency and genomic instability in multiple contexts, in both cell lines and disease. In the HCT116 colorectal cancer cell line, ablation of catalytically active DNMT1 causes cell-cycle arrest and apoptosis due to increased chromosomal instability (51, 52). In mouse embryonic stem cells, loss of Dnmt1 also causes global hypomethylation and increased mutation rates (53).

To determine levels of DNA damage in mutant and control mice, we performed γH2AX staining, which visualizes DNA double-strand breaks as a marker of chromosomal instability. One week following tamoxifen administration, we discovered a dramatic increase in the fraction of γH2AX+ epithelial cells in Dnmt1-mutant versus controls, which contained no γH2AX+ epithelial cells (Fig. 8A–C). One month post-tamoxifen injection, mutants and controls displayed a similar number of γH2AX+ nuclei (Fig. 8D–F). There was a significant difference between neoplastic and non-neoplastic epithelium in control mice, and a similar statistically relevant change was observed in mutants (Fig. 8F). Two months following tamoxifen treatment, nontumor epithelia in both the control and mutant mice showed very little γH2AX (Fig. 8G–I). Although we found many more epithelial cells within Dnmt1-deficient tumors to be γH2AX+ compared with control tumors (Fig. 8I), these data were not statistically significant. These results demonstrate that increased genomic instability occurs as a result of Dnmt1 deletion in the ApcMin/+ model and that genomic instability occurs prior to tumor development. We propose that this temporary decrease in genomic stability, combined with elevated proliferation and apoptosis levels, contributes to accelerated LOH and enhanced tumorigenesis in the inducible ApcMin/+;Dnmt1loxP/loxP;Villin-Cre-ERT2 mice.

Figure 8.
Figure 8.

The Dnmt1-deficient ApcMin/+ intestine displays increased chromosomal instability. Mice were tamoxifen-treated at 4 weeks of age, and intestines were harvested 1 week, 1 month, or 2 months later for immunofluorescent staining analysis. γH2AX (red) was used to visualize DNA double-strand breaks as a marker of genome instability, and E-cadherin (green) was used to outline the epithelium. The percentage of γH2AX-positive (γH2AX+) cells was calculated as the number of γH2AX+ nuclei divided by the total number of epithelial nuclei. A–C, One week following tamoxifen treatment, the number of γH2AX+ nuclei is increased in mutant compared with control small intestines (B compared with A, quantification in C). n = 4 biological replicates per group. ***, P < 0.001 by Student t test. D–F, one month post-tamoxifen injection, both mutant and control non-neoplastic epithelia display low levels of DNA damage, which is significantly increased in tumors of both groups (F). n = 3 biological replicates per group; 2 tumors were counted for controls, 8 tumors were counted for mutants. G–I, two months following tamoxifen treatment, increased levels of γH2AX+ foci continue to be seen in mutant tumors compared with mutant non-neoplastic epithelium (I). There is no significant difference between control and mutant γH2AX+ levels (G vs. H, quantification in I). n = 3–4 biological replicates per group; 3 tumors were counted from controls, and 12 tumors were counted from mutants. All scale bars are 50 μm. For F and I, *, P < 0.05; **, P < 0.01; ***, P < 0.001, one-way ANOVA.

Discussion

The results presented above have major implications for the fields of DNA methylation and intestinal cancer biology. We show that loss of the DNA methyltransferase Dnmt1 in the ApcMin/+ cancer model results in acute hypomethylation and DNA damage but does not affect tumor cell proliferation or apoptosis. We posit that decreased genomic stability accelerates LOH at the Apc locus, resulting in increased tumor initiation and larger tumors over time. Our work adds to the body of evidence that implicates a crucial role for Dnmt1 and DNA methylation in maintaining genome stability.

Importantly, our study demonstrates increased intestinal adenoma formation after deletion of Dnmt1. Our experimental paradigm results in intestine-specific, temporal loss of Dnmt1 and acute hypomethylation, followed by recovery of global genome DNA methylation, in contrast to prior work, which had employed germline hypomorphic Dnmt1 alleles (14–18). These previous studies thus differed both in the timing of Dnmt1 deletion and in the lack of tissue specificity and described a constitutive hypomethylation phenotype which may be a contributing factor to our disparate results. Our Dnmt1-deficient tumors 2 months after tamoxifen administration exhibit significant hypomethylation of several potential oncogenes, yet display minimal DNA methylation changes genome-wide. We cannot rule out that the genome remethylation occurring from 1 week to 1 month post-tamoxifen contributes to accelerated tumorigenesis in our conditional Dnmt1 ablation intestinal cancer model. However, the significantly enhanced genomic instability, proliferation, and apoptosis observed immediately following Dnmt1 ablation, combined with the increased adenoma formation at 1 and 2 months post-tamoxifen, strongly suggest a role for Dnmt1 in maintaining genomic stability and preventing intestinal cancer initiation.

Interestingly, our model results in acute global hypomethylation at LINE1 repetitive elements. DNA methylation is associated with the silencing of LINE1 transcription (54), and LINE1 hypomethylation is highly variable in colorectal carcinomas (55). It has been hypothesized that LINE1 retrotransposition events can interrupt critical genes, such as APC, and drive tumorigenesis (54). In particular contexts, such as APC heterozygosity, changes in genome stability are critical drivers of cancer initiation. Our data support the general theory that DNA hypomethylation causes increased DNA damage, and LINE1 hypomethylation may also be contributing to our observed phenotype.

The DNA demethylating agents azacytidine and decitabine have been tested as anticancer therapeutics in colorectal cancer to abrogate DNA hypermethylation and the silencing of tumor suppressor genes (56, 57). Decitabine and azacytidine are most commonly used to treat acute myeloid leukemia (AML) and myelodysplastic syndromes, with variable success rates (58–60). Our results indicate that DNA demethylation actually contributes to cancer formation, and warrant caution in treating patients with gastrointestinal cancer with a potential tumor-enhancing drug.

In conclusion, we show that deletion of Dnmt1 in the adult intestinal epithelium of ApcMin/+ mice causes accelerated formation of adenomas. Loss of Dnmt1 results in acute hypomethylation and genomic instability, accompanied by increased proliferation and apoptosis. Although Dnmt1-deficient adenomas eventually recover global DNA methylation, they continue to display hypomethylation at several potential oncogenes, highlighting an unappreciated role for DNA hypomethylation in intestinal tumor development. These results support a fundamental role for DNA methylation in preserving genomic integrity during intestinal tumor formation.

Disclosure of Potential Conflicts of Interest

No potential conflicts of interest were disclosed.

Authors' Contributions

Conception and design: K.L. Sheaffer, K.H. Kaestner

Development of methodology: K.L. Sheaffer

Acquisition of data (provided animals, acquired and managed patients, provided facilities, etc.): K.L. Sheaffer, E.N. Elliott

Analysis and interpretation of data (e.g., statistical analysis, biostatistics, computational analysis): K.L. Sheaffer, E.N. Elliott

Writing, review, and/or revision of the manuscript: K.L. Sheaffer, E.N. Elliott, K.H. Kaestner

Administrative, technical, or material support (i.e., reporting or organizing data, constructing databases): K.L. Sheaffer

Study supervision: K.L. Sheaffer, K.H. Kaestner

Grant Support

This work was supported by NIH grant R37-DK053839 (to K.H. Kaestner).

The costs of publication of this article were defrayed in part by the payment of page charges. This article must therefore be hereby marked advertisement in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.

Acknowledgments

The authors thank Haleigh Zillges, Joe Grubb, Jonathan Schug, and Elizabeth Buza for technical assistance. A special thank you to services provided by the University of Pennsylvania Functional Genomics Core (P30-DK19525). They also thank the University of Pennsylvania Department of Dermatology, especially Dr. John Seykora and Dr. Stephen Prouty, for Leica LCM training and equipment access. They acknowledge the support of Dr. Adam Bedenbaugh and the Morphology Core of the Penn Center for the Study of Digestive and Liver Diseases (P30-DK050306).

Footnotes

  • Note: Supplementary data for this article are available at Cancer Prevention Research Online (http://cancerprevres.aacrjournals.org/).

  • Received September 21, 2015.
  • Revision received January 26, 2016.
  • Accepted February 8, 2016.

References

  1. 1.↵
    1. Fearon ER
    . Molecular genetics of colorectal cancer. Annu Rev Pathol 2011;6:479–507.
    OpenUrlCrossRefPubMed
  2. 2.↵
    1. Smith ZD,
    2. Meissner A
    . DNA methylation: roles in mammalian development. Nat Rev Genet 2013;14:204–20.
    OpenUrlCrossRefPubMed
  3. 3.↵
    1. Tahiliani M,
    2. Koh KP,
    3. Shen Y,
    4. Pastor WA,
    5. Bandukwala H,
    6. Brudno Y,
    7. et al.
    Conversion of 5-methylcytosine to 5-hydroxymethylcytosine in mammalian DNA by MLL partner TET1. Science 2009;324:930–5.
    OpenUrlAbstract/FREE Full Text
  4. 4.↵
    1. Cortellino S,
    2. Xu J,
    3. Sannai M,
    4. Moore R,
    5. Caretti E,
    6. Cigliano A,
    7. et al.
    Thymine DNA glycosylase is essential for active DNA demethylation by linked deamination-base excision repair. Cell 2011;146:67–79.
    OpenUrlCrossRefPubMed
  5. 5.↵
    1. Rhee I,
    2. Bachman KE,
    3. Park BH,
    4. Jair KW,
    5. Yen RW,
    6. Schuebel KE,
    7. et al.
    DNMT1 and DNMT3b cooperate to silence genes in human cancer cells. Nature 2002;416:552–6.
    OpenUrlCrossRefPubMed
  6. 6.↵
    1. Berman BP,
    2. Weisenberger DJ,
    3. Aman JF,
    4. Hinoue T,
    5. Ramjan Z,
    6. Liu Y,
    7. et al.
    Regions of focal DNA hypermethylation and long-range hypomethylation in colorectal cancer coincide with nuclear lamina-associated domains. Nat Genet 2012;44:40–6.
    OpenUrlCrossRefPubMed
  7. 7.↵
    1. Luo Y,
    2. Wong CJ,
    3. Kaz AM,
    4. Dzieciatkowski S,
    5. Carter KT,
    6. Morris SM,
    7. et al.
    Differences in DNA methylation signatures reveal multiple pathways of progression from adenoma to colorectal cancer. Gastroenterology 2014;147:418–29.
    OpenUrlCrossRefPubMed
  8. 8.↵
    1. Goelz SE,
    2. Vogelstein B,
    3. Hamilton SR,
    4. Feinberg AP
    . Hypomethylation of DNA from benign and malignant human colon neoplasms. Science 1985;228:187–90.
    OpenUrlAbstract/FREE Full Text
  9. 9.↵
    1. Feinberg AP,
    2. Gehrke CW,
    3. Kuo KC,
    4. Ehrlich M
    . Reduced genomic 5-methylcytosine content in human colonic neoplasia. Cancer Res 1988;48:1159–61.
    OpenUrlAbstract/FREE Full Text
  10. 10.↵
    1. Su LK,
    2. Kinzler KW,
    3. Vogelstein B,
    4. Preisinger AC,
    5. Moser AR,
    6. Luongo C,
    7. et al.
    Multiple intestinal neoplasia caused by a mutation in the murine homolog of the APC gene. Science 1992;256:668–70.
    OpenUrlAbstract/FREE Full Text
  11. 11.↵
    1. Cheung AF,
    2. Carter AM,
    3. Kostova KK,
    4. Woodruff JF,
    5. Crowley D,
    6. Bronson RT,
    7. et al.
    Complete deletion of Apc results in severe polyposis in mice. Oncogene 2010;29:1857–64.
    OpenUrlCrossRefPubMed
  12. 12.↵
    1. Moser AR,
    2. Pitot HC,
    3. Dove WF
    . A dominant mutation that predisposes to multiple intestinal neoplasia in the mouse. Science 1990;247:322–4.
    OpenUrlAbstract/FREE Full Text
  13. 13.↵
    1. Sansom OJ,
    2. Reed KR,
    3. Hayes AJ,
    4. Ireland H,
    5. Brinkmann H,
    6. Newton IP,
    7. et al.
    Loss of Apc in vivo immediately perturbs Wnt signaling, differentiation, and migration. Genes Dev 2004;18:1385–90.
    OpenUrlAbstract/FREE Full Text
  14. 14.↵
    1. Yamada Y,
    2. Jackson-Grusby L,
    3. Linhart H,
    4. Meissner A,
    5. Eden A,
    6. Lin H,
    7. et al.
    Opposing effects of DNA hypomethylation on intestinal and liver carcinogenesis. Proc Natl Acad Sci U S A 2005;102:13580–5.
    OpenUrlAbstract/FREE Full Text
  15. 15.↵
    1. Laird PW,
    2. Jackson-Grusby L,
    3. Fazeli A,
    4. Dickinson SL,
    5. Jung WE,
    6. Li E,
    7. et al.
    Suppression of intestinal neoplasia by DNA hypomethylation. Cell 1995;81:197–205.
    OpenUrlCrossRefPubMed
  16. 16.↵
    1. Eads CA,
    2. Nickel AE,
    3. Laird PW
    . Complete genetic suppression of polyp formation and reduction of CpG-island hypermethylation in Apc(Min/+) Dnmt1-hypomorphic Mice. Cancer Res 2002;62:1296–9.
    OpenUrlAbstract/FREE Full Text
  17. 17.↵
    1. Cormier RT,
    2. Dove WF
    . Dnmt1N/+ reduces the net growth rate and multiplicity of intestinal adenomas in C57BL/6-multiple intestinal neoplasia (Min)/+ mice independently of p53 but demonstrates strong synergy with the modifier of Min 1(AKR) resistance allele. Cancer Res 2000;60:3965–70.
    OpenUrlAbstract/FREE Full Text
  18. 18.↵
    1. Trasler J,
    2. Deng L,
    3. Melnyk S,
    4. Pogribny I,
    5. Hiou-Tim F,
    6. Sibani S,
    7. et al.
    Impact of Dnmt1 deficiency, with and without low folate diets, on tumor numbers and DNA methylation in Min mice. Carcinogenesis 2003;24:39–45.
    OpenUrlAbstract/FREE Full Text
  19. 19.↵
    1. Perreault N,
    2. Sackett SD,
    3. Katz JP,
    4. Furth EE,
    5. Kaestner KH
    . Foxl1 is a mesenchymal Modifier of Min in carcinogenesis of stomach and colon. Genes Dev 2005;19:311–5.
    OpenUrlAbstract/FREE Full Text
  20. 20.↵
    1. Jackson-Grusby L,
    2. Beard C,
    3. Possemato R,
    4. Tudor M,
    5. Fambrough D,
    6. Csankovszki G,
    7. et al.
    Loss of genomic methylation causes p53-dependent apoptosis and epigenetic deregulation. Nat Genet 2001;27:31–9.
    OpenUrlCrossRefPubMed
  21. 21.↵
    1. el Marjou F,
    2. Janssen KP,
    3. Chang BH,
    4. Li M,
    5. Hindie V,
    6. Chan L,
    7. et al.
    Tissue-specific and inducible Cre-mediated recombination in the gut epithelium. Genesis 2004;39:186–93.
    OpenUrlCrossRefPubMed
  22. 22.↵
    1. Lane N,
    2. Dean W,
    3. Erhardt S,
    4. Hajkova P,
    5. Surani A,
    6. Walter J,
    7. et al.
    Resistance of IAPs to methylation reprogramming may provide a mechanism for epigenetic inheritance in the mouse. Genesis 2003;35:88–93.
    OpenUrlCrossRefPubMed
  23. 23.↵
    1. Sheaffer KL,
    2. Kim R,
    3. Aoki R,
    4. Elliott EN,
    5. Schug J,
    6. Burger L,
    7. et al.
    DNA methylation is required for the control of stem cell differentiation in the small intestine. Genes Dev 2014;28:652–64.
    OpenUrlAbstract/FREE Full Text
  24. 24.↵
    1. Bernstein DL,
    2. Kameswaran V,
    3. Le Lay JE,
    4. Sheaffer KL,
    5. Kaestner KH
    . The BisPCR(2) method for targeted bisulfite sequencing. Epigenetics Chromatin 2015;8:27.
    OpenUrlCrossRefPubMed
  25. 25.↵
    1. Boivin GP,
    2. Washington K,
    3. Yang K,
    4. Ward JM,
    5. Pretlow TP,
    6. Russell R,
    7. et al.
    Pathology of mouse models of intestinal cancer: consensus report and recommendations. Gastroenterology 2003;124:762–77.
    OpenUrlCrossRefPubMed
  26. 26.↵
    1. Luongo C,
    2. Moser AR,
    3. Gledhill S,
    4. Dove WF
    . Loss of Apc+ in intestinal adenomas from Min mice. Cancer Res 1994;54:5947–52.
    OpenUrlAbstract/FREE Full Text
  27. 27.↵
    1. Gupta RK,
    2. Gao N,
    3. Gorski RK,
    4. White P,
    5. Hardy OT,
    6. Rafiq K,
    7. et al.
    Expansion of adult beta-cell mass in response to increased metabolic demand is dependent on HNF-4alpha. Genes Dev 2007;21:756–69.
    OpenUrlAbstract/FREE Full Text
  28. 28.↵
    1. Vandesompele J,
    2. De Preter K,
    3. Pattyn F,
    4. Poppe B,
    5. Van Roy N,
    6. De Paepe A,
    7. et al.
    Accurate normalization of real-time quantitative RT-PCR data by geometric averaging of multiple internal control genes. Genome Biol 2002;3:RESEARCH0034.
    OpenUrlCrossRefPubMed
  29. 29.↵
    1. Moser AR,
    2. Dove WF,
    3. Roth KA,
    4. Gordon JI
    . The Min (multiple intestinal neoplasia) mutation: its effect on gut epithelial cell differentiation and interaction with a modifier system. J Cell Biol 1992;116:1517–26.
    OpenUrlAbstract/FREE Full Text
  30. 30.↵
    1. Plasschaert RN,
    2. Bartolomei MS
    . Genomic imprinting in development, growth, behavior and stem cells. Development 2014;141:1805–13.
    OpenUrlAbstract/FREE Full Text
  31. 31.↵
    1. Tremblay KD,
    2. Saam JR,
    3. Ingram RS,
    4. Tilghman SM,
    5. Bartolomei MS
    . A paternal-specific methylation imprint marks the alleles of the mouse H19 gene. Nat Genet 1995;9:407–13.
    OpenUrlCrossRefPubMed
  32. 32.↵
    1. Yang AS,
    2. Estécio MR,
    3. Doshi K,
    4. Kondo Y,
    5. Tajara EH,
    6. Issa JP
    . A simple method for estimating global DNA methylation using bisulfite PCR of repetitive DNA elements. Nucleic Acids Res 2004;32:e38.
    OpenUrlAbstract/FREE Full Text
  33. 33.↵
    1. Kuramochi-Miyagawa S,
    2. Watanabe T,
    3. Gotoh K,
    4. Totoki Y,
    5. Toyoda A,
    6. Ikawa M,
    7. et al.
    DNA methylation of retrotransposon genes is regulated by Piwi family members MILI and MIWI2 in murine fetal testes. Genes Dev 2008;22:908–17.
    OpenUrlAbstract/FREE Full Text
  34. 34.↵
    1. Gregory TR
    . Synergy between sequence and size in large-scale genomics. Nat Rev Genet 2005;6:699–708.
    OpenUrlCrossRefPubMed
  35. 35.↵
    1. Riggs AD,
    2. Xiong Z
    . Methylation and epigenetic fidelity. Proc Natl Acad Sci U S A 2004;101:4–5.
    OpenUrlFREE Full Text
  36. 36.↵
    1. Chen T,
    2. Ueda Y,
    3. Dodge JE,
    4. Wang Z,
    5. Li E
    . Establishment and maintenance of genomic methylation patterns in mouse embryonic stem cells by Dnmt3a and Dnmt3b. Mol Cell Biol 2003;23:5594–605.
    OpenUrlAbstract/FREE Full Text
  37. 37.↵
    1. Gao F,
    2. Zhang Y,
    3. Wang S,
    4. Liu Y,
    5. Zheng L,
    6. Yang J,
    7. et al.
    Hes1 is involved in the self-renewal and tumourigenicity of stem-like cancer cells in colon cancer. Sci Rep 2014;4:3963.
    OpenUrlPubMed
  38. 38.↵
    1. Issa JP
    . CpG island methylator phenotype in cancer. Nat Rev Cancer 2004;4:988–93.
    OpenUrlCrossRefPubMed
  39. 39.↵
    1. Marik R,
    2. Fackler M,
    3. Gabrielson E,
    4. Zeiger MA,
    5. Sukumar S,
    6. Stearns V,
    7. et al.
    DNA methylation-related vitamin D receptor insensitivity in breast cancer. Cancer Biol Ther 2010;10:44–53.
    OpenUrlCrossRefPubMed
  40. 40.↵
    1. Abouzeid HE,
    2. Kassem AM,
    3. Abdel Wahab AH,
    4. El-mezayen HA,
    5. Sharad H,
    6. Abdel Rahman S
    . Promoter hypermethylation of RASSF1A, MGMT, and HIC-1 genes in benign and malignant colorectal tumors. Tumour Biol 2011;32:845–52.
    OpenUrlCrossRefPubMed
  41. 41.↵
    1. Suzuki H,
    2. Watkins DN,
    3. Jair KW,
    4. Schuebel KE,
    5. Markowitz SD,
    6. Chen WD,
    7. et al.
    Epigenetic inactivation of SFRP genes allows constitutive WNT signaling in colorectal cancer. Nat Genet 2004;36:417–22.
    OpenUrlCrossRefPubMed
  42. 42.↵
    1. Qi J,
    2. Zhu YQ,
    3. Luo J,
    4. Tao WH
    . Hypermethylation and expression regulation of secreted frizzled-related protein genes in colorectal tumor. World J Gastroenterol 2006;12:7113–7.
    OpenUrlCrossRefPubMed
  43. 43.↵
    1. Grimm C,
    2. Chavez L,
    3. Vilardell M,
    4. Farrall AL,
    5. Tierling S,
    6. Böhm JW,
    7. et al.
    DNA-methylome analysis of mouse intestinal adenoma identifies a tumour-specific signature that is partly conserved in human colon cancer. PLoS Genet 2013;9:e1003250.
    OpenUrlCrossRefPubMed
  44. 44.↵
    1. Rosty C,
    2. Ueki T,
    3. Argani P,
    4. Jansen M,
    5. Yeo CJ,
    6. Cameron JL,
    7. et al.
    Overexpression of S100A4 in pancreatic ductal adenocarcinomas is associated with poor differentiation and DNA hypomethylation. Am J Pathol 2002;160:45–50.
    OpenUrlCrossRefPubMed
  45. 45.↵
    1. Choi EK,
    2. Uyeno S,
    3. Nishida N,
    4. Okumoto T,
    5. Fujimura S,
    6. Aoki Y,
    7. et al.
    Alterations of c-fos gene methylation in the processes of aging and tumorigenesis in human liver. Mutat Res 1996;354:123–8.
    OpenUrlCrossRefPubMed
  46. 46.↵
    1. Sato N,
    2. Maitra A,
    3. Fukushima N,
    4. van Heek NT,
    5. Matsubayashi H,
    6. Iacobuzio-Donahue CA,
    7. et al.
    Frequent hypomethylation of multiple genes overexpressed in pancreatic ductal adenocarcinoma. Cancer Res 2003;63:4158–66.
    OpenUrlAbstract/FREE Full Text
  47. 47.↵
    1. Pandey MK,
    2. Liu G,
    3. Cooper TK,
    4. Mulder KM
    . Knockdown of c-Fos suppresses the growth of human colon carcinoma cells in athymic mice. Int J Cancer 2012;130:213–22.
    OpenUrlCrossRefPubMed
  48. 48.↵
    1. Shukla V,
    2. Coumoul X,
    3. Lahusen T,
    4. Wang RH,
    5. Xu X,
    6. Vassilopoulos A,
    7. et al.
    BRCA1 affects global DNA methylation through regulation of DNMT1. Cell Res 2010;20:1201–15.
    OpenUrlCrossRefPubMed
  49. 49.↵
    1. Dizik M,
    2. Christman JK,
    3. Wainfan E
    . Alterations in expression and methylation of specific genes in livers of rats fed a cancer promoting methyl-deficient diet. Carcinogenesis 1991;12:1307–12.
    OpenUrlAbstract/FREE Full Text
  50. 50.↵
    1. Levy DB,
    2. Smith KJ,
    3. Beazer-Barclay Y,
    4. Hamilton SR,
    5. Vogelstein B,
    6. Kinzler KW
    . Inactivation of both APC alleles in human and mouse tumors. Cancer Res 1994;54:5953–8.
    OpenUrlAbstract/FREE Full Text
  51. 51.↵
    1. Chen T,
    2. Hevi S,
    3. Gay F,
    4. Tsujimoto N,
    5. He T,
    6. Zhang B,
    7. et al.
    Complete inactivation of DNMT1 leads to mitotic catastrophe in human cancer cells. Nat Genet 2007;39:391–6.
    OpenUrlCrossRefPubMed
  52. 52.↵
    1. Spada F,
    2. Haemmer A,
    3. Kuch D,
    4. Rothbauer U,
    5. Schermelleh L,
    6. Kremmer E,
    7. et al.
    DNMT1 but not its interaction with the replication machinery is required for maintenance of DNA methylation in human cells. J Cell Biol 2007;176:565–71.
    OpenUrlAbstract/FREE Full Text
  53. 53.↵
    1. Chen RZ,
    2. Pettersson U,
    3. Beard C,
    4. Jackson-Grusby L,
    5. Jaenisch R
    . DNA hypomethylation leads to elevated mutation rates. Nature 1998;395:89–93.
    OpenUrlCrossRefPubMed
  54. 54.↵
    1. Miousse IR,
    2. Koturbash I
    . The fine LINE: methylation drawing the cancer landscape. Biomed Res Int 2015;2015:131547.
    OpenUrlPubMed
  55. 55.↵
    1. Estécio MR,
    2. Gharibyan V,
    3. Shen L,
    4. Ibrahim AE,
    5. Doshi K,
    6. He R,
    7. et al.
    LINE-1 hypomethylation in cancer is highly variable and inversely correlated with microsatellite instability. PLoS One 2007;2:e399.
    OpenUrlCrossRefPubMed
  56. 56.↵
    1. Braiteh F,
    2. Soriano AO,
    3. Garcia-Manero G,
    4. Hong D,
    5. Johnson MM,
    6. Silva LeP,
    7. et al.
    Phase I study of epigenetic modulation with 5-azacytidine and valproic acid in patients with advanced cancers. Clin Cancer Res 2008;14:6296–301.
    OpenUrlAbstract/FREE Full Text
  57. 57.↵
    1. Goel A,
    2. Boland CR
    . Epigenetics of colorectal cancer. Gastroenterology 2012;143:1442–60.e1.
    OpenUrlCrossRefPubMed
  58. 58.↵
    1. Kadia TM,
    2. Jabbour E,
    3. Kantarjian H
    . Failure of hypomethylating agent-based therapy in myelodysplastic syndromes. Semin Oncol 2011;38:682–92.
    OpenUrlCrossRefPubMed
  59. 59.↵
    1. Nebbioso A,
    2. Carafa V,
    3. Benedetti R,
    4. Altucci L
    . Trials with ‘epigenetic’ drugs: an update. Mol Oncol 2012;6:657–82.
    OpenUrlCrossRefPubMed
  60. 60.↵
    1. Fenaux P,
    2. Mufti GJ,
    3. Hellstrom-Lindberg E,
    4. Santini V,
    5. Finelli C,
    6. Giagounidis A,
    7. et al.
    Efficacy of azacitidine compared with that of conventional care regimens in the treatment of higher-risk myelodysplastic syndromes: a randomised, open-label, phase III study. Lancet Oncol 2009;10:223–32.
    OpenUrlCrossRefPubMed
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Cancer Prevention Research: 9 (7)
July 2016
Volume 9, Issue 7

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DNA Hypomethylation Contributes to Genomic Instability and Intestinal Cancer Initiation
Karyn L. Sheaffer, Ellen N. Elliott and Klaus H. Kaestner
Cancer Prev Res July 1 2016 (9) (7) 534-546; DOI: 10.1158/1940-6207.CAPR-15-0349
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