Background
Cancer genomes accumulate mutations upon loss of genome stability. During carcinogenesis and progression of cancer, cells are challenged by various genotoxic insults, which pose threats to genomic stability [
1,
2]. Encounter of DNA lesions requires efficient DNA damage responses (DDR) to prevents loss and gain of genetic information. DNA lesions can be quickly monitored by ATM (Ataxia-Telangiectasia mutated) and ATR (A-T-related)-mediated cell cycle checkpoint [
3], followed by actions of repair factors such as RAD51, BRCA1 and 53BP1 to eliminate DNA breaks. For DNA double strand breaks (DSBs) that generated frequently during genomic replication, appropriate repair pathways including non-homologous end joining (NHEJ) and homologous recombination (HR) are activated in G1 and S/G2 phases, respectively [
4‐
6]. For HR, RAD51 is the essential recombinase, whose recruitment to DNA breaks is dependent on RPA-coated ssDNA (single-strand DNA) filaments and HR mediator factors (ie. BRCA2) [
7,
8].
Loss of DDR function via deleterious mutation impair genomic stability, and consequently lead to high-frequent point mutations and structural variation at chromosomal level, which eventually promote carcinogenesis [
9,
10]. For example, pathogenic mutations (ie.
BRCA1, BRCA2) that debilitates HR are frequently associated with increase of cancer predisposition, manifested in 17.1% of the familial and sporadic breast cancer patients [
11‐
13]. Similarly, ~ 50% cases of high-grade ovarian cancers carry
BRCA1 and
BRCA2 mutations, causing high-incidence of homologous recombination deficiency (HRD) [
14‐
16]. Although HR mutations, including those arisen from familiar and hereditary sources, affect all types of proliferating cells, risk of malignancies are mainly limited in tissues like breast, ovary and prostate [
17,
18]. Up to date, it remains mysterious why the epithelial compartments in these tissues are uniquely susceptible to carcinogenesis upon HR ablation.
Steroid hormones including estrogen, progestogen, androgen, and possibly their derivatives, are genotoxic to ovarian epithelial cells that expressing hormone receptors [
19]. Activation of hormone receptors (ie. ER) can induce DSBs and require Topoisomerase II (TOP2) to resolve decatenated DNA. It was reported that endogenous DNA lesion is transiently elevated in G1 phase of breast cancer cells upon increased concentration of estrogen [
20]. BRCA1 and endonuclease activity of MRE11 is obligated to remove TOP2 adducts-associated DSBs. Although this model points to the resolution of estrogen-induced TOP2 adducts, and can be expanded to ovarian epithelium whose microenvironment is periodically flushed with even higher concentration of estrogen [
21], it does not thoroughly explain the susceptibility of breast/ovarian epithelium to other HR mutations (ie.
BRCA2), which functions in S/G2 phase instead of G1. Moreover, the genomic footprints in
BRCA1-mutated breast cancer are distinct from those bearing
BRCA2 mutations, implying the involvement of different mutational processes/mechanisms [
22].
Here, we hypothesized that estrogen-induced genotoxicity contributes to the tissue susceptibility of ovarian epithelium to HRD. We characterized the DDR patterns using cell lines, clinically derived ovarian cancer tissues as well as mouse models. We show that arising of DNA breaks are independent of proliferation of OvCa cells, and thus irrelevant to erroneous genomic DNA replication. Instead, high-level estrogen contributes to the accumulation of DNA lesions in ER-positive OvCa, which act in both G1 and non-G1 phases of cell cycle. ER-induced genotoxicity requires functional HR. At last, estrogen-induced genotoxicity was rigorously reproduced in non-cancerous epithelial compartment of ovary and fallopian tubes. Altogether, we conclude that estrogen specifically challenge the genomic integrity in ovarian epithelium. This demands the functional HR to curb the carcinogenesis of ovarian cancer.
Methods
Cell culture
Cancer cell lines were grown in Dulbecco’s DMEM supplemented with 10% calf serum plus 100 U/ml Penicillin and 100 mg/ml streptomycin. SKOV-3 (HTB-77) and A549 (CCL-185™) were purchased from ATCC. HO8910 (3111C0001CCC000280) and HO8910-PM (3111C0001CCC000281) were purchased from National Infrastructural of Cell Line Resources, Beijing. OVCAR-8TR and L02 lines were gifted by collaborating laboratory. Cell lines were authenticated upon purchase and regularly tested for mycoplasma contamination.
Biopsies, cryosections and ex vivo culture of ovarian tissue
Ovarian tissues diagnosed with OvCa were used in this study along with one ‘healthy’” ovary without detectable malignancy. Freshly excised tissue blocks were embedded in OCT, followed by snap frozen in liquid nitrogen and stored in -80 °C. Deep frozen tissue blocks were sectioned at 8 μm using microtome (LEICA, CM3050 S). For ex vivo culture of OvCa biopsies, freshly excised tissues were subjected to mincing and enzymatic digestion (Collagenase A, Roche, 10,103,578,001; Trypsin, GIBCO, 25200–056) for 2 h with occasional vortex. Isolated single cells were dispersed in RPMI-1640/10% FBS and grown in media supplemented with 10 mg/ml Matrigel (BD, 356234). After 48 h, experiments were performed when 70% of cells were attached.
In vivo experiments
Eight reproductively mature female mice (C57/B6, 6 weeks old) were divided into two groups: group A, no estrogen treatment; group B, intraperitoneal injection with estrogen (Selleck, S1709, 1 mg/kg) for 6 h. Dissected liver, ovary and fallopian tube were instantly frozen in liquid nitrogen and cryosectioned for indirect immunofluorescent staining. All animals were housed in standard SPF condition throughout the experiments. Animals were sacrificed with minimal pain by neck broken protocol following approved CO2 euthanasia procedure.
Immunostaining and fluorescence microscopy
Cryopreserved sections or cells grown on coverslip were fix with 4% paraformaldehyde (PFA) and permeabilize with 0.3%TritonX-100, followed by blocking in PBS with 3%BSA, 3% donkey serum and 0.2% Triton X-100. Primary antibodies were diluted with antibody buffer (3% Triton/10% BSA in PBS) and incubated overnight: phoshpo-BRCA1 (Bethyl, A300-001A, 1:1000), phosphor-RPA32 (NOVUS, NB100–544,1:3000), RAD51 (Proteintech, 14,961–1-AP, 1:500), Cyclin A2 (Huabio, ET-1612-26,1:500), anti-53BP1 (Bethyl, A300-272A,1:1000), anti-γH2AX (Millipore, 05–636,1:500), anti-BRCA2 (Invitrogen, MA5–32986, 1:500). Fluorescent images were acquired using OLYMPAS (BX51) and images were processed analysed using Image-Pro Plus software.
Chemical treatments
Cells were treated with hormones at the following concentrations: tamoxifen (Sigma, T5648), 50 nM; estrogen (17β-estradiol, Wako), 50 nM. Intraperitoneal injection of estradiol (Selleck, S1709, 1 mg/Kg) was applied to animals. Time of treatment are described for each experiment.
RNA interference and RT-PCR
Lipofectamine 3000 transfection kit (Invitrogen, 3,000,015) was used for siRNA transfection for cells grown to 70% confluency. Cells were collected 48 h after transfection for indicated experiments. Individual siRNA duplexes used were: BRCA1 (target sequence: UCUGCUGUAUUGGAACAAAUU); BRCA2 (target sequence: AAC AACAAUUACGAACCAAACUU). Knockdown efficiencies of these genes are shown in Supplementary Figure
2. To quantify gene expression levels, total cellular RNA was extracted by using TRIzol® Reagent (Invitrogen) and cDNA was synthesized using Eastep RT Master Mix Kit (Promega). RT-PCR products were visualized by agarose gel electrophoresis. mRNA levels were normalized using GAPDH or actin RNA as internal control.
Statistical analysis
The Student’s t-test was performed on all data analysis. Each experiment had at least three independent biological replicates. Unless otherwise specified, data are showed as mean ± s.e.m. p < 0.05 was considered to be statistically significant. Excel and GraphPad Prism was used to create the graphs and calculate the p value.
Discussion
Genomic surveillance system is a critical anti-cancer barrier considering its function in preventing genomic mutations. Risk for ovarian cancer is remarkably increased in cases losing the DDR genes like BRCA1, BRCA2 and ARID1A/1B. It is a long-term mystery how germline BRCA mutations predominantly affect female reproductive tissues. In this study, we present evidence that elevation of DNA lesions, corresponding to the ubiquitous activation of BRCA1, is not tightly associated with active genomic replication in OvCa. Our data strongly support the genotoxicity of estrogen can insult genomes of OvCa cells in both G1 and S phase cells, which is highly dependent on the expression of nuclear receptors (ie. ER). Moreover, DNA damage induced upon steroid hormone exposure obligate the function of HR genes as ablation of BRCA1 and BRCA2 significantly abrogate the counteraction against estrogen-induced genotoxicity in a subset of OvCa cells.
Although this study mainly involves in vitro work, our data can large reflect the physiological situation of ovarian and fallopian epithelium. Above all, it is difficult to determine the ‘physiological concentration’ of estrogen, due to the natural variation at different menstrual stages, as well as for different tissues (ie. some labs estimated the estrogen concentration in ovary is 100 times higher than other tissues [
30]). The in vitro concentration of estrogen corresponding to physiological dosage is estimated for 1 nM [
31], and DNA damage could be induced upon exposure to estrogen at this dosage [
32]. In this study, we applied higher concentrations of estrogen (50 nM) to visualize DNA damage in OVCAR-8TR cells for the purpose of accelerating the toxic effect of E2 and obtaining quantifiable DNA lesions.
In the light of our in vitro and in vivo data, we conclude that genomic integrity of epithelial compartments in ovarian and fallopian tube is more liable to be challenged by estrogen, relative to non-female reproductive tissues. Considering the expressing level of nuclear receptor and high concentrations of steroids in milieu of ovarian epithelium, the genotoxicity of estrogen would generate strong mutagenic effects in ovarian epithelium. Particularly, given the requirement of HR for eliminating estrogen-induced DNA damage, pathogenic mutations in BRCA1, BRCA2 and ARID1A/1B would dramatically exacerbate the mutagenic potential of periodical hormone challenge.
The observation of prevalent induction of DNA breaks and BRCA1 activation/phosphorylation regardless of proliferation status and cell cycle phases indicates a form of replication-independent genotoxicity. This phenomenon is reproduced in OvCa cell lines, primary cancer culture, as well as non-cancerous murine ovarian and fallopian epithelium. Combining the potential of genotoxicity upon estrogen exposure, we conclude that both normal ovarian epithelium and OvCa cells can rigorously respond to high-concentration of estrogen in a ER dependent manner. The genomic insult by steroid hormone is significant, considering the long-term and monthly attack and relatively high dosage of damage (5–15 DSBs per cell in cell culture and normal epithelium), which is equivalent to 0.5–1 Gy of ionizing radiation.
Although we failed to monitor BRCA1 phosphorylation in estrogen-treated murine ovarian epithelium, possibly due to antibody specificity, our data implicate that BRCA1 participates in preventing damage accumulation in both replicating and non-replicating cells in cancer tissue (Fig.
3a). It is likely that BRCA1 cooperates with MRE11 to dispose Top2 adducts in G1 phase, but functions with BRCA2 and RAD51 in S/G2 phase to facilitate HR in removing breaks caused by replication-transcription collisions. Thus, the role of
BRCA1 upon estrogen challenges exceed the HR mechanism, which is also supported by different mutational processes revealed by distinct patterns of genomic imprints born by
BRCA1 and
BRCA2-mutated cancers [
22]. Nevertheless, we conclude that multiple functions of
BRCA1 in counteracting estrogen-induced genotoxicity reflect its central role in obviating the genomic instability of ovarian epithelium and thus disease progression of OvCa.
Open AccessThis article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit
http://creativecommons.org/licenses/by/4.0/. The Creative Commons Public Domain Dedication waiver (
http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated in a credit line to the data.
Publisher’s Note
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.