Metformin inhibits ovarian cancer via decreasing H3K27 trimethylation

Abstract

Metformin has been used for the treatment of type II diabetes mellitus for decades. Recently, used of metformin in the therapy of diverse human cancer types has received widespread attention, while the underlying mechanisms have been not fully elucidated. In the current study, 5-ethynyl-20-de-oxyuridine assay to detect cell proliferation, flow cytometry to detect apoptosis, scratch wound healing and Transwell migration assay to detect cell migration capacity. The current study reported that metformin inhibited cell proliferation and migration, and promoted apoptosis in ovarian cancer cells, particularly under normoglycemic conditions in vitro. Metformin treatment significantly promoted the phosphorylation of AMP-activated protein kinase (AMPK), and reduced histone H3 lysine 27 trimethylation (H3K27me3) and polycomb repressor complex 2 (PRC2) levels. Additionally, overexpression of EZH2 to increase H3K27me3 abrogated the effect of metformin on the cell proliferation, migration and apoptosis in SKOV3 and ES2 cells. Similar to metformin, another AMPK agonist, 2-deoxy-D-glucose, reduced the H3K27me3 level and PRC2 expression. In cells pretreated with Compound C, an AMPK inhibitor, metformin was not able to induce AMPK phosphorylation or reduce H3K27me3. Metformin-mediated AMPK activation and H3K27me3 inhibition were more robust in cells exposed to low glucose (5.5 mM) compared with those exposed to high glucose (25 mM). These findings implicate H3K27me3 repression mediated by AMPK phosphorylation in the antitumor effect of metformin in ovarian cancer, indicating that metformin alters epigenetic modifications by targeting PRC2 and supports the use of metformin in treatment of patients with epithelial ovarian cancer without diabetes.

Introduction

Ovarian cancer is the most lethal gynecologic malignancy and the fifth leading cause for cancer mortality among women in the United States (1). A reason for this high mortality is chemotherapeutic resistance, as recurrent and metastatic ovarian cancer usually exhibits resistant to platinum-based chemotherapy (2). Thus, there is an urgent need to identify novel drugs for use in ovarian cancer therapy.

Metformin (1,1-dimethylbiguanide), an oral biguanide first introduced in the 1950s, has been used as the first-line medication for the treatment of type II diabetes mellitus for decades. Recently metformin has gained renewed interest as a potential cancer chemotherapy adjuvant in adjuvant or neoadjuvant setting (3,4). Numerous studies have demonstrated antitumor effects of metformin in vitro and in vivo using models using different types of cancer cell lines, including breast, endometrial and ovarian cancer cell lines (5–7). Furthermore, clinical observational studies demonstrated that patients with ovarian cancer exposed to metformin had reduced disease recurrences and cancer-specific mortalities compared with unexposed women (8–10). A phase II clinical trial to assess whether the addition of metformin to standard chemotherapy improves survival in non-diabetic ovarian cancer patients is ongoing (NCT02122185; clinicaltrials.gov).

Although metformin has been used as an anti-diabetic agent for over half a century, its molecular mechanisms are still not fully understood. The most described mechanism of metformin is inhibition of mitochondrial respiratory chain complex I, leading to reduced ATP production and activation of AMP-activated protein kinase (AMPK), which in turn leads to increased glucose uptake by muscle, decreased glucose production in liver, and reduced blood glucose (11). In cancer cells, AMPK is considered a tumor-suppressing pathway, which inhibits the mammalian target of the rapamycin signaling, suppresses cell proliferation, and promotes apoptosis and cell-cycle arrest (12,13). AMPK-independent effects of metformin in cancer, such as the inhibition of protein kinase phosphorylation in breast and lung cancers, have been also reported (14). However, whether metformin inhibits ovarian cancer via the AMPK pathway and underlying downstream molecular mechanisms remains elusive.

Epigenetic modifications, including DNA methylation of the CpG sites, and covalent modifications of the N-terminal tail of the core histones, have critical roles in tumor development and progression (15). Histone H3 lysine 27 trimethylation (H3K27me3) is recognized as an epigenetic marker in malignancies, because H3K27me3 reprograms epigenetic landscape and gene expression, which is associated with various pathways to drive tumorigenesis (16). In ovarian cancer, H3K27me3 contributes to the formation of the tumor microenvironment (17), the development of resistance to cisplatin and tumor progression (18). H3K27me3 is catalyzed by histone-lysine N-methyltransferase EZH2 that interacts with polycomb protein SUZ12 and polycomb protein EED as polycomb repressive complex 2 (PRC2) and mediates gene silencing through promoter methylation and chromatin remodeling (19). EZH2 depletion and H3K27me3 inhibition in ovarian cancer cells could inhibit tumor growth, migration, and invasion, and enhance sensitized tumor cells to cisplatin in vitro and in vivo (20,21). Notably, EZH2 and H3K27me3 have been reported to contribute to the development of renal injury and chronic inflammation in type 2 diabetes (22,23), demonstrating the role of H3K27me3 in energy stress.

In the present study, it was aimed to investigate whether metformin inhibits ovarian cancer through repressing H3K27me3. Given that metformin is predominantly used to treat patients with type II diabetes and high glucose concentration inhibits the activation of AMPK (24), the role of glucose concentration in the effects of metformin in ovarian cancer cells was also examined.

Materials and methods

Chemical, reagents and antibodies

The following chemicals were used in the current study. Metformin (1,1-dimethylbiguanide,) was purchased from Sigma-Aldrich (Merck KGaA, Darmstadt, Germany; cat. no. 150959). 2-Deoxy-D-glucose (2-DG; cat. no. S4701) and dorsomorphin 2HCl (Compound C) (cat. no. S7306) were purchased from Selleck Chemicals (Houston, TX, USA). Antibodies against phospho-AMPKα (p-AMPKα, Thr172; cat. no. 2535), AMPKα (cat. no. 2603), EZH2 (cat. no. 5246), SUZ12 (cat. no. 3737) were purchased from Cell Signaling Technology, Inc. (Danvers, MA, USA). Histone H3 (cat. no. 2348), H3K27me3 (cat. no. 2363), EED (cat. no. 5371) antibodies were purchased from ABclonal Biotech Co., Ltd. (Woburn, MA, USA). β-actin antibody (cat. no. 66009-1-Ig) was purchased from Proteintech, Inc. (Chicago, IL, USA). Horseradish peroxidase-conjugated (HRP) anti-mouse antibody (cat. no. 074-1806-1) and HRP anti-rabbit antibody (cat. no. 074-1506-1) were purchased from KPL, Inc. (Gaithersburg, MD, USA).

Cell lines and culture conditions

Human epithelial ovarian cancer cell lines SKOV3 (ovarian adenocarcinoma), ES2 (ovarian clear cell carcinoma), and A2780 (ovarian carcinoma) were purchased from China Center for Type Culture Collection (Wuhan University, Wuhan, China) and were cultured in Dulbecco's modified Eagle's medium (DMEM) (HyClone; GE Healthcare Life Sciences, Logan, UT, USA) containing 25 mM glucose (mimicking hyperglycemia) or 5.5 mM glucose (mimicking normoglycemia) supplemented with 10% fetal bovine serum (v/v; Hangzhou Sijiqing Biological Engineering Materials Co., Ltd., Hangzhou, China) at 37°C in 95% air and 5% CO₂.

For metformin treatment, ovarian cancer cells were seeded at a density of 4×10⁵ per well on 6-well plates and incubated for 24 h. Then they were treated with metformin of different concentrations (0, 2.5, 5 or 10 mM) for 24 h in triplicate. 2-DG, an AMPK activator, was used to induce AMPK phosphorylation in tumor cells, whereby cells were treated with 25 mM 2-DG for 24 h. To inhibit the metformin-mediated AMPK activation, cells were pretreated with 20 µM Compound C for 2 h followed by treatment with 5 mM metformin for 24 h.

Transduction in vitro

A recombinant lentivirus harboring EZH2 DNA (NM_004456; GeneChem Co., Ltd., Shanghai, China) was used to upregulate the EZH2 level in the SKOV3 and ES2 cells. An empty vector (Con307; GeneChem Co., Ltd.) was used as control. Stable transduction was conducted following the manufacturers' instructions. Transduction cells were selected with 25 µg/ml puromycin and monoclonal cells were used for subsequent experiments. The transfection efficiency was confirmed by western blot analysis.

Proliferation assay

5-Ethynyl-20-deoxyuridine (EdU) DNA cell proliferation kits were purchased from Guangzhou RiboBio Co., Ltd. (Guangzhou, China). Cell proliferation activity was evaluated according to the manufacturer's instructions. Briefly, ovarian cancer cells were seeded in triplicate at a density of 5×10³ cells/well in 96-well plates. After24 h, cells were washed with PBS twice and fixed with 4% formaldehyde at room temperature for 30 min. Subsequently, the cells were treated with 0.5% Triton X-100 for 10 min at room temperature for permeabilization, followed by incubation with EdU at room temperature for 1 h. Finally, the cells were counter-stained with 5 µg/ml Hoechst 33342 at room temperature for 30 min. The proportion of EdU-incorporated cells was defined as the proliferation rate. The assay was performed in three biological replicates.

Analysis of cell apoptosis via flow cytometry

The effects of metformin on ovarian cancer cell apoptosis were assessed by flow cytometry using Annexin V-fluorescein isothiocyanate (FITC)/propidium iodide (PI) staining kit (BD Pharmingen; BD Biosciences, San Jose, CA, USA). As cells transduced with lenti-virus carried green fluorescence, their apoptosis rates were assessed by using Annexin V-phycoerythrin (PE)/7-aminoactinomycin D (7-AAD) staining kit (BD Pharmingen; BD Biosciences). After 24 h of exposure to metformin, cells were washed twice with ice-cold PBS, re-suspended in 500 µl binding buffer, and stained with 5 µl FITC-conjugated 5 µl Annexin V or 5 µl Annexin V-PE conjugated and 7 µl 7-AAD, following gentle mixing, cells were incubated at room temperature shielded from light for 15 min. Following washing with binding buffer, flow cytometry analysis was performed using a flow cytometry sorting system (MoFlo XDP) with Summit 6.2 software (both from Beckman Coulter, Inc., Brea, CA, USA). Each assay was run at least three times.

Scratch wound healing assay

Cells were seeded into 6-well plates at a destiny of 6×10⁵ cells/well. Following incubation overnight, a scratch wound was introduced on the cell mono-layer using a 100 µl pipette tip. PBS was used to wash away the floating cells and then cultured in serum-free growth media. The migration of cells into the wound area was observed at 0 h and 24 h. For quantification, the wound gap was imaged using a light microscope (Olympus Corporation, Tokyo, Japan), then measured using Image-Pro Plus 6.0 (Media Cybernetics, Inc., Rockville, MD, USA) and the mean recovery gaps were to normalized 0 h. Each assay was performed at least three times.

Transwell migration assay

Transwell chambers (6.5-mm diameter; 24-well) were used for migration assays (Costar; Corning Incorporated, Corning, NY, USA). SKOV3 (5×10⁴ cells/ml), ES2 (5×10⁴ cells/ml), A2780 (8×10⁴ cells/ml) in 100 µl serum-free DMEM were seeded in each Transwell insert. The lower chamber was contained 650 µl DMEM medium supplemented with 20% fetal bovine serum. After incubation at 37°C for 24 h, non-migrated cells on the upper membrane surface were wiped with a cotton swab. Cells that had migrated to the lower surfaces of each filter were fixed with 4% paraformaldehyde for 30 min and stained with 0.1% crystal violet at room temperature for 1 h. Then, cells were counted in five randomly selected visual fields under a light microscope (Olympus Corporation). Each assay was performed at least three times.

Reverse transcription-quantitative polymerase chain reaction (RT-qPCR)

Total RNA was isolated and extracted using TRIzol^® reagent (Thermo Fisher Scientific, Inc., Waltham, MA, USA) according to the manufacturer's instructions, and 1 µg total RNA in a final volume of 20 µl was used for RT with PrimeScript RT Master Mix Kit (Takara Bio, Inc., Otsu, Japan). Reverse transcription reaction was performed under the following conditions: 37°C for 15 min, 85°C for 5 sec, 4°C for 5 min. PCR reaction system included 10 µl Eva Green Mix, 1 µl cDNA, 10 µM forward primer, 10 µM reverse primer, with ddH₂O up to 20 µl. The mRNA was quantitated using a TaqMan One Step Gold RT-PCR kit (Applied Biosystems; Thermo Fisher Scientific, Inc.). qPCR was performed under the following conditions: 40 cycles at 95°C for 5 sec and 60°C for 30 sec (EZH2, SUZ12 and β-actin); 40 cycles at 95°C for 5 sec and 52°C for 30 sec (EED). Primer sequences are shown in Table I. The relative expression levels of EZH2, SUZ12 and EED to β-actin were calculated using the 2^−ΔΔCq method (25). All reactions were in triplicate and at least three biological replicated were assessed.

Table I.

Primer sequences used for reverse transcription-quantitative polymerase chain reaction.

Primer	Forward (5′-3′)	Reverse (5′-3′)
EZH2	TTGTTGGCGGAAGCGTGTAAAATC	TCCCTAGTCCCGCGCAATGAGC
SUZ12	GCATTGCCCTTGGTGTACTC	TGGTCCGTTGCGACTAAAA
EED	ATGCTGTCAGTATTGAGAGTGGC	GAGGCTGTTCACACATTTGAAAG
β-actin	GCCAACACAGTGCTGTCTGG	GCTCAGGAGGAGCAATGATCTTG

EZH2, histone-lysine N-methyltransferase EZH2; SUZ12, polycomb protein SUZ12; EED, polycomb protein EED.

Western blot analysis

Ovarian cancer cells were homogenized in cold NP40 buffer (Beyotime Institute of Biotechnology), protease inhibitor cocktail (Complete™, EDTA-free) and phosphatase inhibitor cocktail (PhosStop) (both from Roche Applied Science, Penzberg, Germany) and sonicated on ice, and the lysates were centrifuged at 13,684 x g for 10 min at 4°C. Protein was quantified using a bicinchoninic acid assay (Beyotime Institute of Biotechnology). The protein samples were boiled in protein sample buffer for 8 min. Then, 30 µg protein per well was resolved on 10% SDS-polyacrylamide gels and transferred onto polyvinylidene fluoride membranes (GE Healthcare Life Sciences, Little Chalfont, UK). The membranes were probed with H3K27me3 antibody (1:1,000), H3 antibody (1:5,000), EZH2 antibody (1:2,000), SUZ12 antibody (1:1,000), EED antibody (1:2,000), AMPKα antibody (1:1,000), p-AMPKα antibody (1:1,000), and β-actin antibody (1:5,000) for 24 h in 4°C following blocking with 5% skim milk in Tris-buffered saline and Tween-20 (TBST). Following washing in TBST the membrane was incubated with HRP anti-mouse antibody (1:5,000) or HRP anti-rabbit antibody (1:5,000) at room temperature for 1 h. Protein bands were measured via Novex ECL HRP chemiluminescent substrate reagent (Thermo Fisher Scientific, Inc.) and scanned using Image Lab Software in Molecular Imager^® ChemiDoc™ XRS⁺ (Bio-Rad Laboratories, Inc., Hercules, CA, USA) and normalized to internal control β-actin. All the experiments were repeated at least three times.

Statistical analysis

Data are presented as the mean ± standard deviation. One-way analysis of variance with Tukey's post hoc tests were used for multiple comparisons between groups. P<0.05 was considered to indicate a statistically significant difference.

Results

Metformin inhibits ovarian cancer growth and migration in vitro

To examine the effect of metformin on the aggressive progression of ovarian cancer, SKOV3, A2780 and ES2 cells cultured in hyperglycemic medium or normoglycemic medium were treated with 10 mM metformin for 24 h, and cell proliferation, apoptosis and migration ability were then determined. Untreated cells served as control. EdU assays demonstrated that the cell proliferation was significantly reduced by metformin under both hyperglycemic and normoglycemic conditions. Compared with the control cells, the proliferation rates in SKOV3, A2780 and ES2 cells were decreased by 6.55, 38.72 and 33.96% following metformin treatment in hyperglycemic medium, respectively. In normoglycemic medium, the proliferation rates in SKOV3, A2780 and ES2 were decreased by 9.1, 33.37 and 34.7%, respectively. Intriguingly, the cell proliferation rates in the normoglycemic cells were significantly lower than those in the hyperglycemic cells exposure to metformin (Fig. 1).

Figure 1.

Metformin inhibits the proliferation of ovarian cancer cells. EdU assays demonstrate that metformin reduces proliferation of (A) SKOV3, (B) A2780 and (C) ES2 cells. Representative fluorescence microscopy images of EdU incorporation and Hoechst 33342 staining of nuclei (magnification, ×100). The proliferation rates of SKOV3, A2780, and ES2 cells were calculated. Data are presented as the mean ± standard deviation. ^*P<0.05; ^**P<0.01; ^***P<0.001. Met, metformin; Glu, glucose; EdU, 5-ethynyl-20-deoxyuridine; NC, negative control.

FITC/PI flow cytometry assays demonstrated that the apoptosis rates in SKOV3 and ES2 cells were significantly increased following metformin treatment under normoglycemia, but not under hyperglycemia. Furthermore, all three ovarian cancer cell lines undergoing metformin treatment in normoglycemic condition exhibited a higher apoptosis rate compared with those treated with metformin in hyperglycemic condition (Fig. 2). Scratch wound healing assays and Transwell migration assays revealed that the migration capacity of ovarian cancer cells under hyperglycemic and normoglycemic conditions were inhibited by metformin, with more intensive inhibition under normoglycemic condition (Figs. 3 and 4). As 10 mM metformin increases apoptosis under hypoglycaemia, it may impact the migration results. To exclude the influence of increased apoptosis on H3K27me3 and migration, ovarian cancer cells were exposed to a low metformin concentration (2.5 mM) under normoglycemic condition. As shown in Fig. 5A and B, 2.5 mM metformin did not enhance the cell apoptosis, while the migration and H3K27me3 level were decreased (Figs. 5C and 6A). These results suggest that metformin inhibits cell proliferation and migration, and promotes apoptosis, and that reduction of glucose concentration enhances the sensitivity of ovarian cancer cells to metformin.

Figure 2.

Metformin promotes the apoptosis of ovarian cancer cells. Percentage of apoptotic (A) SKOV3, (B) A2780 and (C) ES2 cells were detected by flow cytometry analysis using Annexin V-fluorescein isothiocyanate/PI staining. Apoptotic cells includes Annexin V(-)/PI(+), Annexin V(+)/PI(−) and Annexin V(+)/PI(+) cells. Data are presented the mean ± standard deviation. ^*P<0.05; ^**P<0.01. PI, propidium iodide; Met, metformin; Glu, glucose; NC, negative control.

Figure 3.

Metformin inhibits migration of ovarian cancer cells. Migration of (A) SKOV3, (B) A2780 and (C) ES2 cells were measured by scratch wound healing assay. Representative bright-field images (magnification, ×100) and quantification of recovered distance at 24 h after 10 mM metformin treatment. Data are presented the mean ± standard deviation. ^*P<0.05; ^**P<0.01; ^***P<0.001. Met, metformin; Glu, glucose; NC, negative control.

Figure 4.

Metformin inhibits migration of ovarian cancer cells. Migration of (A) SKOV3, (B) A2780 and (C) ES2 cells were measured by Transwell migration assay. Representative bright-field images of the cell migration (magnification, ×100) and quantification of migrated cells at 24 h after 10 mM metformin treatment are shown. Data are presented the mean ± standard deviation. ^*P<0.05; ^**P<0.01;^***P<0.001. Met, metformin; Glu, glucose; NC, negative control.

Figure 5.

Metformin (2.5 mM) has no significant effect on apoptosis of ovarian cancer cells, however migration is inhibited. Percentage of apoptotic (A) SKOV3 and (B) ES2 cells were detected by flow cytometry analysis using Annexin V-fluorescein isothiocyanate/PI staining. Apoptotic cells include Annexin V(−)/PI(+), Annexin V(+)/PI(−) and Annexin V(+)/PI(+) cells. Migration of (C) SKOV3 and (D) ES2 were measured by scratch wound healing assay. Representative bright-field images (magnification, ×100) and quantification of recovered distance at 24 h after 2.5 mM metformin treatment. Data are presented the mean ± standard deviation. ^*P<0.05. PI, propidium iodide; Met, metformin; Glu, glucose; NC, negative control.

Figure 6.

Metformin decreases H3K27me3 and expression of polycomb repressor complex 2 in ovarian cancer cells. The protein expression of (A) H3K27me3 and (B) EZH2, SUZ12 and EED in A2780, SKOV3 and ES2 cells were assayed by western blot analysis. Met, metformin; Glu, glucose; H3K27me3, histone H3 lysine 27 trimethylated; H3, histone H3; EZH2, histone-lysine N-methyltransferase EZH2; SUZ12, polycomb protein SUZ12; EED, polycomb protein EED.

Metformin inhibits H3K27me3 in ovarian cancer cells

To investigate whether H3K27me3 has a role in the mechanism of metformin, the alterations in H3K27me3 level and the expression of three main components of the PRC2 (i.e. EZH2, SUZ12 and EED) following metformin treatment were assessed. Ovarian cancer cells were treated with various concentrations of metformin (0, 2.5, 5 and 10 mM) in medium containing 5.5 or 25 mM glucose for 24 h. Western blot analysis demonstrated that metformin suppressed H3K27me3 level in ovarian cancer cells in a dose-dependent manner, particularly in medium with lower glucose concentration (Fig. 6A). The protein and mRNA expression of EZH2, SUZ12 and EED were decreased to varying extents following exposure to metformin under normoglycemic condition in all three cell lines, while the suppression was rather modest in the cells under hyperglycemic conditions (Figs. 6B and 7). Under hyperglycemic conditions, the protein level of SUZ12 was reduced in SKOV3 (Fig. 6B), but there was no significant inhibition in mRNA levels (Fig. 7), which may be due to post-transcriptional modifications.

Figure 7.

Metformin decreases PRC2 of ovarian cancer cells. mRNA expression of EZH2, SUZ12 and EED in (A) SKOV3, (B) A2780 and (C) ES2 cells determined by reverse transcription-quantitative polymerase chain reaction analysis. Data are presented the mean ± standard deviation. ^*P<0.05; ^**P<0.01; ^***P<0.001. Met, metformin; Glu, glucose; EZH2, histone-lysine N-methyltransferase EZH2; SUZ12, polycomb protein SUZ12; EED, polycomb protein EED.

Metformin inhibits ovarian cancer through decreased-H3K27me3

To demonstrate the role of H3K27me3 in the metformin-mediated antitumor effect, H3K27me3 level was upregulated in SKOV3 and ES2 cells using an EZH2 DNA lentivirus (Fig. 8A), and cell proliferation (Fig. 8B–D), migration abilities (Fig. 9) and apoptosis (Fig. 10) were assessed. Ovarian cancer cells were treated with 10 mM metformin in medium containing 5.5 mM glucose under normoglycemic condition for 24 h. Cells transfected with empty lentivirus served as the negative control. Upregulation of H3K27me3 enhanced the proliferation and migration of ovarian cancer cells (Figs. 8 and 9). Compared with the cells transfected with empty lentivirus, metformin did not significantly affect the cell proliferation, apoptosis or migration of SKOV3 and ES2 cells transfected with EZH2 lentivirus (Figs. 8–10). These results indicate that decreased H3K27me3 is essential for the antitumor effect of metformin in ovarian cancer cells.

Figure 8.

Overexpression of EZH2suppresses the inhibitory effect of metformin on proliferation of ovarian cancer cells. (A) EZH2 DNA lentivirus upregulated EZH2 andH3K27me3 protein expression. The protein expression of EZH2 and the level of H3K27me3 in SKOV3 and ES2 cells were assayed by western blot analysis. (B) EdU assays evaluated the proliferation of ovarian cancer cells. Representative fluorescence microscopy images of EdU incorporation and Hoechst 33342 staining of nuclei (magnification, ×100). The proliferation rates of (C) SKOV3 and (D) ES2 cells. Data are presented the mean ± standard deviation. ^*P<0.05; ^***P<0.001. EZH2, histone-lysine N-methyltransferase EZH2; H3K27me3, histone H3 lysine 27 trimethylated; H3, histone H3; NC, negative control; Met, metformin; EdU, 5-ethynyl-20-deoxyuridine.

Figure 9.

Overexpression of EZH2 suppresses the inhibitory effect of metformin on migration of ovarian cancer cells. Migration of (A) SKOV3 and (B) ES2 cells were measured by Transwell migration assay (crystal violet staining), and (C) a scratch wound healing assay was performed using SKOV3 cells. Representative bright-field images of the cell migration (magnification, ×100) and quantification of migrated cells or recovered distance at 24 h after 10 mM metformin treatment are shown. Data are presented the mean ± standard deviation. ^*P<0.05; ^**P<0.01. NC, negative control; Met, metformin; EZH2, histone-lysine N-methyltransferase EZH2.

Figure 10.

Overexpression of EZH2 suppresses the effect of metformin on apoptosis of ovarian cancer cells. Percentage of apoptotic (A) SKOV3 and (B) ES2 cells were detected by flow cytometry analysis using Annexin V-PE/7-AAD staining. Apoptotic cells include Annexin V(−)/7-AAD(+), Annexin V(+)/7-AAD(−) and Annexin V(+)/7-AAD(+) cells. Data are presented the mean ± standard deviation. ^*P<0.05. PE, phycoerythrin; 7-AAD, 7-aminoactinomycin D; NC, negative control; Met, metformin; EZH2, histone-lysine N-methyltransferase EZH2.

Metformin inhibits H3K27me3 through AMPK pathway

Given that metformin is an AMPK activator, whether metformin suppresses PRC2 through the AMPK pathway was investigated. AMPKα and p-AMPKα levels were assessed in cancer cells treated with 0, 2.5, 5 and 10 mM metformin. As shown in Fig. 11A, metformin induced phosphorylation of AMPKα at Thr-172 in a dose-dependent manner, the ratio of p-AMPKα/AMPKα was dramatically increased in the ovarian cancer cells cultured in normoglycemic medium, while the increase was slight in the cells in hyperglycemic medium. These results confirmed that metformin induced the activation of AMPK in ovarian cancer cells. Another AMPK activator, 2-DG, and an AMPK inhibitor, Compound C, were used to evaluate the effects of AMPK activation on H3K27me3 and PRC2. Similar to metformin, 2-DG increased the p-AMPK/AMPK ratio, and repressed the expression of H3K27me3, EZH2, SUZ12 and EED (Fig. 11B). In the cells pretreated with Compound C, metformin was not able to induce AMPK phosphorylation or inhibitEZH2, SUZ12, EED or H3K27me3 (Fig. 11C), suggesting AMPK activation is required for metformin-induced PRC2 inhibition.

Figure 11.

Metformin inhibits H3K27me3 through the AMPK pathway. (A) Metformin activates AMPK of ovarian cancer cells in normoglycemic condition. (B) 2-DG activates AMPK and suppresses H3K27me3, PRC2 of ovarian cancer cells in normoglycemic condition. (C) Compound C inhibits the effect of metformin on PRC2 and H3K27me3 when ovarian cancer cells were cultured in normoglycemic condition. The protein expression of p-AMPKα, AMPKα, H3K27me3, EZH2, SUZ12 and EED in A2780, SKOV3 and ES2 cells were assayed by western blot analysis. The expression was normalized to β-actin. Met, metformin; Glu, glucose; p-AMPKα, phospho-AMPKα; AMPKα, AMP-activated protein kinase; 2-DG, 2-deoxy-D-glucose; EZH2, histone-lysine N-methyltransferase EZH2;SUZ12, polycomb protein SUZ12; EED, polycomb protein EED; 2-DG, dorsomorphin 2HCl; H3K27me3, histone H3 lysine 27 trimethylation.

Discussion

Multiple meta-analyses have now reported that metformin may reduce the incidence of overall cancer by 10–40%, with lower risks of cancer-specific mortality (26–29). In patients with ovarian cancer, as revealed by a case-control study, metformin intake is significantly associated with improved 5-year survival (73 vs. 44%, P=0.002) (10). In mouse models, metformin inhibited the growth of ovarian cancer xenografts (5). The present study produced in vitro evidence supporting the anti-tumor effects of metformin in ovarian cancer and reported that H3K27me3 was abrogated by metformin through AMPK activation, which sheds new light on the underlying mechanism of metformin as an antitumor drug.

Metformin promoted cell apoptosis and repressed cell proliferation and migration in all three epithelial ovarian cancer cell lines used in the study (A2780, ES2 and SKOV3). Similar results have been reported in other epithelial ovarian cancer cell lines, including PA-1, OVCAR-3 and HO8910-PM (30,31). It is well established that tumor cells can be starved by the metformin-mediated ATP depletion that confers susceptibility to cell death. In addition to regulating energy homeostasis, metformin was previously reported to alter folate metabolism, disturbing nucleotide synthesis and inhibiting cell proliferation (32). It is notable that the antitumor effects of metformin were more robust in the low glucose medium, which provides preliminary evidence supporting the use of metformin for the treatment of ovarian cancer in non-diabetic patients. In line with the findings of the current study, low glucose was previously reported to enhance the cytotoxicity of metformin in breast cancer and thyroid cancer cells (33,34). Zhuang et al (35) reported that lowering glucose potentiated metformin mediated ATP depletion and cell death by reducing metformin-stimulated glycolysis in ovarian and breast cancer cells, which may partially explain the influences of glucose on metformin actions. Consistently, in the current study, AMPK was more strongly activated by metformin in low glucose medium, compared with high glucose medium.

The clarification of the molecular mechanisms under the antitumor effect of metformin will be of important clinical relevance regarding predicting the response to metformin therapy and selecting appropriate patients for the treatment. In the present study, metformin treatment resulted in decreased-H3K27me3 accompanied by repressed EZH2, SUZ12 and EED expression in ovarian cancer cells. The inhibition of EZH2 transcription by metformin has been previously observed in breast cancer and pancreatic cancer cells, which may be associated with re-expression of the microRNAs (miRs) targeting EZH2, including miR-26a and miR-101 (36,37). In prostate cancer cells, metformin reduced the level of histone-lysine N-methyltransferase SUV39H1, a histone methyltransferase of H3 Lys9, and inhibited SUV39H1-mediated cell migration (38). These findings suggest that reduced specific histone methylation marks may mediate the antitumor effects of metformin. Further research may be warranted to investigate the presence of these histone marks on gene promoters and the consequent alterations in gene transcription in tumor cells.

AMPK is an important metabolic sensor that regulates energy homeostasis; activated AMPK induces energy sparing pathways to maintain ATP levels in response to hypoxia, fuel deprivation and low glucose level (39). As expected, in the present study, metformin-stimulated AMPK activation was dependent on the content of glucose in the environment. Notably, the metformin-induced PRC2 inhibition was rescued by pretreatment with an AMPK inhibitor (Compound C), suggesting that AMPK activation was required for the inhibitory effect of metformin on H3K27me3. Recently, Demoinet et al (40) demonstrated that AMPK is a pivotal molecular link to couple the chromatin environment and consequent adaptive changes in gene expression, and resolution of epigenetic modifications in Caenorhabditis elegans. Furthermore, AMPK inactivation was reported to be associated with enrichment of H3K27me3 in gut epithelial cells (41). All these findings suggest cross-talking between energy stress and the methylation of histones in tumor cells.

In addition, the findings of the current study demonstrated that the decrease in H3K27me3 is required for the anti-tumor effect mediated by metformin in ovarian cancer cells. H3K27me3 contributes to CpG methylation in gene promoter regions and chromatin configuration, which in turn reduces the accessibility of transcription factors and the transcriptional activity of nearby genes, resulting in transcriptional repression. H3K27me3 has been reported to regulate the expression of genes involved in ovarian cancer cell proliferation, apoptosis and metastasis, such asp57, Harakiri, Aplasia Ras homolog member I and tissue inhibitor of metalloproteinase 2 (20,42–44). Notably, Zhao et al (45) demonstrated that enhancing H3K27me3 occupancy at the E3 ubiquitin-protein ligase NEDD4-likepromoter increased transforming growth factor-β signal transduction in ovarian cancer cells, which has a critical role in tumor progression (46). These downstream mechanisms of H3K27me3 may partially explain the antitumor effects of metformin.

Taken together, the findings suggest that the antitumor effect of metformin in ovarian cancer cells may be partially attributed to the metformin-mediated AMPK activation and the consequent reduction of H3K27me3, particularly under normoglycemia condition. Several small molecular inhibitors of EZH2 are being assessed in clinical trials to treat patients with malignancies. For example, CPI-1205 and Tazemetostat are current being used in patients with B-cell lymphoma and synovial sarcoma in phase I clinical trials (NCT02395601 and NCT02601937; clinicaltrials.gov), respectively. However, it usually takes >10 years to take a novel drug from the laboratory to clinical use. By contrast, repurposing of metformin as an antitumor agent is a shortcut, as above all, its biological safety has been well documented. The findings of the current study indicate that metformin maybe an epigenetic regulator targeting PRC2 and support the use of metformin in treatment of patients with epithelial ovarian cancer without diabetes.

Funding

This study was supported by the National Science Foundation of China (grant nos. 81672573, 81472443 and 81372807).

Availability of data and materials

The data sets generated during the current study are available from the corresponding author on reasonable request.

Authors' contributions

ZW, JG and JC contributed to the conception and design; GT, YZ and TL contributed to acquisition of data; GT, ZH and LY contributed to analysis and interpretation of data for the work; all authors drafted the work and revised it critically for important intellectual content; all authors approved the final manuscript to be published; all authors agree to be accountable for all aspects of the work in ensuring that questions related to the accuracy or integrity of any part of the work are appropriately investigated and resolved.

Ethics approval and consent to participate

Not applicable.

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.