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Hypermethylation and loss of retinoic acid receptor responder 1 expression in human choriocarcinoma

  • H. Huebner1,
  • R. Strick1,
  • D. L. Wachter2,
  • S. Kehl1,
  • P. L. Strissel1,
  • R. Schneider-Stock2,
  • A. Hartner3,
  • W. Rascher3,
  • L. C. Horn4,
  • M. W. Beckmann1,
  • M. Ruebner1 and
  • F. B. Fahlbusch3Email author
Contributed equally
Journal of Experimental & Clinical Cancer Research201736:165

https://doi.org/10.1186/s13046-017-0634-x

Received: 14 July 2017

Accepted: 13 November 2017

Published: 23 November 2017

Abstract

Background

Human placental development resembles tumorigenesis, due to the invasive and fusogenic potential of trophoblasts. However, these features are tightly controlled in trophoblasts. Disturbance of this spatial and temporal regulation is thought to contribute to the rare formation of choriocarcinomas. Promoter hypermethylation and loss of the tumor suppressor Retinoic acid receptor responder 1 (RARRES1) were shown to contribute to cancer progression. Our study investigated the epigenetic and transcriptional regulation of RARRES1 in healthy human placenta in comparison to choriocarcinoma cell lines and cases.

Methods

Three choriocarcinoma cell lines (Jeg-3, JAR and BeWo) were treated with three different retinoic acid derivates (Am580, Tazarotene and all-trans retinoic acid) and 5-aza-2′-deoxycytidine. We analyzed RARRES1 promoter methylation by pyrosequencing and performed realtime-PCR quantification to determine RARRES1 expression in placental tissue and trophoblastic cell lines. Additionally, RARRES1 was stained in healthy placentas and in biopsies of choriocarcinoma cases (n = 10) as well as the first trimester trophoblast cell line Swan71 by immunofluorescence and immunohistochemistry.

Results

In the choriocarcinoma cell lines, RARRES1 expression could not be induced by sole retinoic acid treatment. Stimulation with 5-aza-2′-deoxycytidine significantly induced RARRES1 expression, which then could be further increased with Am580, Tazarotene and all-trans retinoic acid. In comparison to healthy placenta, choriocarcinoma cell lines showed a hypermethylation of the RARRES1 promoter, which correlated with a reduced RARRES1 expression. In concordance, RARRES1 protein expression was lost in choriocarcinoma tissue. Additionally, in the trophoblastic cell line Swan71, we found a significant induction of RARRES1 expression with increased cell density, during mitosis and in syncytial knots.

Conclusions

Our findings showed that RARRES1 expression is absent in choriocarcinoma due to promoter methylation. Based on our analysis, we hypothesize that RARRES1 might exert tumor suppressive functions in multiple cellular processes (e.g. cell cycle regulation, adhesion, invasion and apoptosis).

Keywords

PlacentaRARRES1Retinoic acidChoriocarcinomaDNA methylationTIG1Epigenetic

Background

Human hemochorial placentation closely resembles processes otherwise seen in cancer. The capacity of trophoblasts to migrate and invade the maternal decidua, as well as their ability to form the syncytiotrophoblast (SCT) via cell-fusion, shares high similarities with tumor cells [1]. As a consequence, trophoblasts are often characterized to be of pseudo-malignant nature. Not surprisingly, expression patterns of tumor suppressor genes in cancer are similar to those found in placenta [2, 3]. Recently, retinoic acid receptor responder 1 (RARRES1), also known as Tazarotene-induced gene 1 (TIG1), was identified as an important tumor suppressor gene [4, 5]. It was initially described as a novel retinoic acid (RA) receptor (RARβ and γ) regulated gene in skin graft cultures [6]. RARRES1 is located on chromosome 3q25 and was reported to be one of the most commonly methylated loci in multiple cancers [79]. Epigenetic silencing of RARRES1 expression and its effect on tumor cell invasion, proliferation and survival further underscored its tumor suppressive properties [10]. In prostate cancer an association between RARRES1 hypermethylation and worse clinical outcome was reported [8].

Recently, we identified RARRES1 in the human placenta and determined its regulation by RA derivates. In the placenta, uncontrolled trophoblast growth result in malignant transformation as observed in choriocarcinomas [11].

Thus, in the light of previous reports regarding the role of epigenetic regulation of tumor suppressor genes in the human placenta [12, 13], we investigated the epigenetic and transcriptional regulation of the tumor suppressor RARRES1 in the human placenta, choriocarcinoma cell lines and biopsies, as well as its potential functional properties.

Methods

Patient and tissue collection

Human term placentas (third trimester) were obtained from healthy patients (n = 74) after elective Caesarean section and processed within 1 h. The clinical data were summarized in Additional file 1: Table S1. After removal of the basal plate and chorionic membrane, a biopsy was obtained near the cord from every placenta. Placental tissues were snap frozen in liquid nitrogen and stored at −80 °C until further use. Formalin-fixed and paraffin-embedded (FFPE) sections were supplied by the Institute of Pathology, University Hospital Erlangen. Handling of patients and tissues was approved by the Ethics Committee at the University Erlangen-Nuremberg (No. 2180). A written informed consent was obtained from all participants. FFPE sections of 10 choriocarcinoma cases were provided by the Institute of Pathology of the University Hospital Leipzig. Five cases were intramolar and five pure choriocarcinomas.

Immunohistochemical (IHC) staining

Human FFPE placental sections were deparaffinized and rinsed in a series of descending ethanol concentrations. IHC stains were performed on tissue sections using the LSAB + HRP kit (Agilent, Hamburg, Germany) according to the manufacturer’s instructions. Anti-human RARRES1 (ab92884, Abcam, Cambridge, United Kingdom, 1:6000) antibody was used. Nuclei were counter-stained by hematoxylin.

Immunofluorescence (IF) staining

Human FFPE placental sections were deparaffinized and rehydrated as stated above. Slides were blocked using 1% bovine serum albumin in Tris-buffered saline (BSA/TBS) for 30 min at room temperature. Anti-human RARRES1 antibody was diluted in 1% BSA/TBS (1:400) and slides were incubated at 4 °C over-night. As secondary antibody Alexa Fluor 488 Donkey Anti-Mouse IgG (H + L) (Molecular Probes, Eugene, USA) was used at a dilution of 1:400 in 1% BSA/TBS and slides were incubated for 2 h at room temperature. Staining of the nuclei was performed using DAPI (Thermo Fischer, Darmstadt, Germany).

Villous cytotrophoblast isolation

Villous cytotrophoblasts (VT) from healthy placentas of 15 different individuals were isolated using the Trypsin-DNase-Dispase/Percoll method, as previously described [14]. Before DNA and RNA extraction the fractionated trophoblasts were cryopreserved in liquid nitrogen. By fluorescence activated cell sorting (FACSCalibur, BD Biosciences) we could determine a percentage of 86.6–90% of the fractionated cells being trophoblastic [14].

Cell culture

The choriocarcinoma cell lines BeWo, Jeg-3 and JAR were cultured under the following conditions: BeWo was grown in DMEM:F12 phenol-red free (high Glucose; Thermo Fischer, Darmstadt, Germany) supplemented with 10% fetal calf serum (FCS, Thermo Fischer, Darmstadt, Germany), 100 U/ml penicillin and 100 μg/ml streptomycin (1% P/S, Sigma-Aldrich, Taufkirchen, Germany). Jeg-3 cells were cultured in phenol-red free DMEM:F12 (Thermo Fischer, Darmstadt, Germany) supplemented with 10% FCS, 1% P/S and JAR cells in RPMI 1640 media (Thermo Fischer, Darmstadt, Germany) with 10% FCS, 10 mM Hepes (Sigma-Aldrich, Taufkirchen, Germany), 2 mM L-Glutamin (Sigma-Aldrich, Taufkirchen, Germany) and 0.1 mM non-essential amino acids (NEAA, Sigma Aldrich, Taufkirchen, Germany). The first trimester cell line Swan71 was a kind gift of Prof. G. Mor, Department of Obstetrics, Gynaecology and Reproductive Sciences, Reproductive Immunology Unit, Yale University School of Medicine, USA [15]. The cell line was grown in phenol red free DMEM:F12 with 10% FCS, 1%P/S and 0.1 mM NEAA.

For stimulation experiments cells were seeded at a density of 3x104/ml (Swan71, Jeg-3 and JAR) or 4x104/ml (BeWo) in a 12-well cell culture plate. Cell lines were cultivated in medium supplemented with 2.5% (Swan71) or 5% (Jeg-3, JAR, BeWo) charcoal treated fetal bovine serum (CTS, Thermo Fisher, Darmstadt, Germany) 24 h prior to and during stimulation. Cells were treated with 1.0 μM all-trans-retinoic acid (ATRA, Biomol, Hamburg, Germany), Tazarotene (TAZA, Sigma-Aldrich, Taufkirchen, Germany) or 200 nM Am580 (Tocris, Lille Cedex, France) for 24 to 72 h. In order to induce global DNA demethylation, the cell lines were additionally treated with 0.5 or 1.0 μM 2′-deoxy-5-azacytidine (AZA, Sigma-Aldrich, Taufkirchen, Germany) for 72 h.

For the analysis of RARRES1 expression in dependence of cell density, Swan71 and Jeg-3 cells were seeded at 0.75, 1.50, 3.0, 6.0, 12.0 and 18.0x104 cells/ml in 12-well dishes. After 48 h cells were harvested for RNA isolation (Additional file 2: Figure S1). Jeg-3 cells were additionally treated with AZA for 72 h before harvesting.

Genomic DNA extraction of tissues and cultivated cell lines

Genomic DNA was isolated from cultivated cell lines or 50–100 mg placental tissues as previously described in detail [16]. DNA was dissolved in 0.01% DEPC water.

Bisulfite treatment and PCR amplification

Bisulfite treatment of 0.5–2.0 μg genomic DNA of placental tissues and trophoblast-like cell lines was performed using the EpiTect Bisulfite Kit (Qiagen, Hilden, Germany) according to the manufacturer’s instructions. Converted DNA (100 ng) was amplified using a thermal cycler (Thermo Fischer, Darmstadt, Germany) and the HRM-Mastermix (Qiagen, Hilden, Germany). Bisulfite treated DNA was used in a 25 μl reaction volume with 10 μM of both the forward and the reverse primer (Additional file 3: Table S2). PCR conditions were 95 °C for 15 min, 50 cycles of denaturation (30s at 95 °C), annealing (30s at 50 °C for the CpG region 1 and 55 °C for region 2) and extension (30s at 72 °C), followed by a final extension period of 7 min at 72 °C. Successful conversion and amplification were controlled using capillary electrophoresis (QIAxcel, Qiagen, Hilden, Germany).

Pyrosequencing

Pyrosequencing (PyroMark Q24, Qiagen, Hilden, Germany) was performed according to the manufacturer’s instructions using PyroMark Gold Q24-reagents (Qiagen, Hilden, Germany). PCR and sequencing primer were designed using the PSW Assay design software 1.0.6 (Biotage, Sweden) as well as the online program MethPrimer [17]. 75 pmol of the respective CpG region specific sequencing primer was used (Additional file 3: Table S2). Each CpG region of interest was split into two sections and analyzed separately to obtain reproducible results. The second section was sequenced using serial pyrosequencing according to Tost et al. (2006) [18]. The methylation pattern was quantified by the PyroMark Q24-CpQ-Assay (Qiagen, Hilden, Germany). Correct sequencing was monitored using the EpiTect-PCR-Control-DNA set including methylated, unmethylated and unconverted control DNA. Data were analyzed by the PyroMark Q24 software.

RNA extraction and cDNA synthesis

RNA was isolated from third trimester placental tissues as well as cultivated cell lines using peqGOLD TriFast (PEQLAB, Erlangen, Germany), as previously described [16]. Isolated RNA was treated with DNase I (Roche, Mannheim, Germany) to avoid DNA contamination during expression analysis. The High-Capacity-cDNA-Reverse-Transcription kit (Thermo Fischer, Darmstadt, Germany) was used to generate cDNA in a thermal cycler (ABI2720) for 2 h at 37 °C.

Quantitative Realtime PCR (qRT-PCR)

Quantification of RARRES1 mRNA expression in placental tissues and cell lines was achieved by qRT-PCR analysis as previously described [14]. In short, 10 nM forward and reverse primers and 40 ng cDNA were used to analyze the amplification of RARRES1 via SYBR-green based technology (SYBR Select Master Mix, Thermo Fischer, Darmstadt, Germany). The expression was normalized using 18SrRNA and GAPDH as reference genes. Due to lack of differences, 18SrRNA data are presented only. Primer sequences are listed in Additional file 3: Table S2.

Statistical analysis

All data are presented as mean ± standard error of the mean (SEM), which was calculated using Microsoft Excel 2010 (Microsoft Corporation, Redmond, Washington, USA). Differences between the subgroups were analyzed using the Mann-Whitney U-test (SPSS, IBM Inc., Nuremberg, Germany). Significances were adjusted using post hoc Bonferroni testing. P-values of less than 0.05 were considered as statistically significant.

Results

RARRES1 promoter hypermethylation and reduced gene expression in choriocarcinoma cell lines

The RARRES1 gene is localized on Chromosome 3q25.32 (Fig. 1a). To investigate the methylation pattern of the RARRES1 promoter in placental tissues and cell lines, we performed pyrosequencing of two different CpG regions within the promoter. We chose an ATG-proximate (CpG region 1) and distal region (CpG region 2) of the size of about 100 bp each. These selected CpG regions are part of a CpG island, which was reported to be hypermethylated in prostate cancer and to contain several putative retinoic response elements [19]. CpG region 1 is 115 bp long and starts 166 bp upstream of the ATG codon. This region includes 10 CpG positions. The CpG region 2 lies about 900 bp further upstream, containing seven CpGs (Fig. 1a, black pins). Pyrosequencing of the RARRES1 promoter revealed a hypomethylation of CpG region 1 (0–20% methylation) compared to region 2 (60–90% methylation) for placental tissues, isolated trophoblasts and the Swan71 cells (Fig. 1b). All analyzed choriocarcinoma cell lines had a strong hypermethylation (50–100%) pattern of both promoter sections (Fig. 1b).
Fig. 1

RARRES1 methylation and expression pattern. a Gene locus of RARRES1 on chromosome 3. The ideogram shows the RARRES1 locus on 3q25.32. The genetic region is drawn schematically with the coding regions as black squares. Two CpG regions within the promoter were selected for further analysis. CpGs are marked with black pins. Red arrows symbolize the sequencing primers for the pyrosequencing reaction. b Heat-map for the promoter methylation pattern. DNA of 3rd trimester placentas (P; from n = 74 individuals), 3rd trimester trophoblasts (Tr; from n = 15 individuals), the trophoblast-like cell line Swan71 (n = 1) and the choriocarcinoma cell lines Jeg-3, JAR and BeWo (n = 1 each) were analyzed using pyrosequencing. The methylation intensity was illustrated by heat map coloring as indicated by the scale below, where green represents the unmethylated state (0%) and black the completely methylated state (100%). c Gene-expression analysis of RARRES1 in placental tissues (from n = 10 individuals), primary trophoblasts (from n = 5 individuals) as well as Swan71 cells and the choriocarcinoma cell lines (n = 9). Gene expression is indicated as relative to RARRES1 expression of 3rd trimester placentas (P). d QRT-PCR analysis of AZA-treated cell lines relative to control (n = 9). Significance is marked by asterisks (* p < 0.05, ** p < 0.005). Data represent mean ± SEM

To investigate the influence of promoter methylation on gene expression we analyzed RARRES1 expression by qRT-PCR (Fig. 1c). RARRES1 mRNA expression was highest in primary isolated trophoblasts (12-fold compared to placental tissue), followed by the expression in Swan71 cells (5-fold) and total placental tissue (P). Corresponding to their methylation pattern, all choriocarcinoma cell lines showed a significantly lower RARRES1 expression compared to placental tissue (p < 0.005), primary trophoblasts and the Swan71 cell line (Fig. 1c). To verify the correlation between increased CpG region 1 methylation and decreased RARRES1 gene expression, we treated the cell lines with 0.5 μM (BeWo, JAR, n = 9) or 1.0 μM (Jeg-3, Swan71, n = 9) AZA for a time period of 72 h (Fig. 1d). Pyrosequencing of DNA from AZA treated cells revealed a significant decrease of CpG region 1 methylation in Jeg-3 and JAR cell lines (Additional file 4: Figure S2). RARRES1 expression was significantly increased by AZA treatment in all choriocarcinoma cell lines (100- to 1200-fold, p < 0.005, Fig. 1d). In the Swan71 cell line RARRES1 gene expression was about 2.5-fold higher following AZA-treatment when compared to untreated control (Fig. 1d).

Induction of RARRES1 expression by retinoic acid stimulation

RARRES1 gene expression is known to be upregulated by RAR-specific RAs in different tissues (Fig. 2a) [6]. Thus we investigated the effect of different RA derivates (Am580, TAZA and ATRA) stimulation on RARRES1 gene expression in the choriocarcinoma cell lines and the first trimester cell line Swan71. ATRA is a RA which binds to all RARs (α, β and γ), whereas Am580 specifically binds to RARα [20]. TAZA is a RARβ and γ specific agonist [6]. Interestingly, a significant induction of RARRES1 expression could only be achieved in the Swan71 cell line by Am580 (20-fold after 48 h), TAZA (17-fold after 72 h) and ATRA (35-fold after 48 h), with ATRA as the strongest agonist (Fig. 2c). On the other hand stimulation of the choriocarcinoma cell lines did not result in a significant increase of RARRES1 expression (Fig. 2c). Furthermore, we stimulated primary trophoblasts with Am580, TAZA and ATRA for 48 h. We observed a significant induction of RARRES1 expression of approximately 3.0-fold compared to untreated cells (Fig. 2d). We hypothesized that the lack of RA-responsiveness in choriocarcinoma cell lines might be due to the high methylation pattern of the RARRES1 promoter (Fig. 1b and Fig. 2b). For verification, we additionally treated the choriocarcinoma cell lines with AZA for 72 h prior and during stimulation with RAR-specific RAs. Demethylation by AZA treatment allowed significant induction of RARRES1 gene expression by RA stimulation compared to solitary AZA exposure (Fig. 2e). In Jeg-3 cells RARRES1 expression was increased by 5-fold with Am580, TAZA and ATRA treatment. RARRES1 expression of Jeg-3 cells after AZA and ATRA treatment was as high as RARRES1 expression in untreated Swan71 cells. Increased RARRES1 expression could also be observed for JAR and BeWo (1.4 to 1.8-fold and 1.2 to 1.8-fold, respectively; Fig. 2e). Treatment with AZA did not alter the RA response of Swan71 cells.
Fig. 2

Retinoic acid induced RARRES1 expression. a Scheme of Retinoic acid (RA) binding to Retinoic acid receptor (RAR and RXR) dimers. b Transcriptional activation of RARRES1 expression is blocked by promoter methylation (Meth). c Swan71, Jeg-3, JAR and BeWo cells were treated with Am580, TAZA and ATRA for 24 to 72 h. d Primary trophoblasts (from n = 4 individuals) were treated with Am580, TAZA and ATRA for 48 h. Significance in (c) and (d) was calculated relative to untreated control cells (Ctrl.). e Cells were stimulated with Am580, TAZA and ATRA after AZA-treatment. Significance was determined in comparison to solely AZA-treated cells. Expressions of (c-e) are relative to Ctrl. Significance is marked by asterisks (* p < 0.05, ** p < 0.005). Data represent mean ± SEM

Loss of RARRES1 expression in choriocarcinoma tissue

As shown earlier (Fig. 1d and Fig. 2c), hypermethylation of the RARRES1 promoter was observed in choriocarcinoma cell lines and correlated with reduced gene expression and loss of transcriptional activation of RARRES1. In the light of these results we analyzed the RARRES1 expression in choriocarcinoma tissue (n = 10). Immunohistochemical and immunofluorescence staining of choriocarcinoma sections (intramolare a-e and pure f-j) revealed a loss of RARRES1 protein in malignant cancer cells (Fig. 3, white arrow heads). In contrast, cells of the molar trophoblast showed a strong RARRES1 positivity (Fig. 3c; black arrow head). Fig. 3 shows two choriocarcinoma cases (a-e and f-j) that were representative for the other eight analyzed tissues (data not shown).
Fig. 3

RARRES1 expression in choriocarcinoma sections. Sections of choriocarcinomas ((a-e) intramolare choriocarcinoma and (f-j) pure choriocarcinoma; n = 2 representative patients) were stained with anti-RARRES1 antibody by immunohistochemistry (a-c and f-h) or immunofluorescence (d, e, i and j). RARRES1 positive staining is indicated in brown (a-c and f-h) or green (d, e, i and j), nuclei are blue. RARRES1 positive cells are marked by black arrow heads; white arrow heads show RARRES1 negative cells; (c, e, h and j) are magnifications of the sections in (b, d, g and i) marked by squares, respectively. The bar equals 100 μm

Correlation of RARRES1 expression with cell density

As RARRES1 is downregulated in choriocarcinoma and significantly higher expressed in primary trophoblasts, we hypothesized that RARRES1 might be of importance for normal trophoblastic development. By immunofluorescence staining of placental sections, we observed a prominent RARRES1 expression especially in VTs attached to the SCT (Fig. 4a and b ; white arrow heads). Additionally, extravillous trophoblasts (EVTs) were RARRES1 positive (Fig. 4a , c ). In order to analyze whether cell-cell connectivity influences RARRES1 expression, we plated Swan71 and Jeg-3 cells in different cell densities, ranging from 0.75 to 18.0x104 cells /ml (Additional file 2: Figure S1), and analyzed RARRES1 gene expression normalized to 18SrRNA (Fig. 4b and c ). We observed a significant increase of RARRES1 expression with increasing Swan71 cell number per well (n = 6, Fig. 4c , a ). High cell-cell contact rates, as observed in cell numbers above 6x104/ml, were related with a significantly (p < 0.005) higher RARRES1 expression (8.5-fold higher at 18.0x104/ml compared to 0.75x104/ml). In Jeg-3 cells the RARRES1 expression did not change with increasing cell density (Fig. 4c , b ). We hypothesized that this effect might be related to RARRES1 promoter hypermethylation. Thus, we additionally treated Jeg-3 cells with AZA and analyzed RARRES1 gene expression in dependence of cell density. After AZA treatment we detected a significant increase of RARRES1 expression (p < 0.05, 4.5-fold at 18.0x104 cells /ml) with rising cell numbers (Fig. 4c, b). In order to analyze the potential role of RARRES1 in cell connectivity we further applied real-time Electric Cell-substrate Impedance Sensing (ECIS) to RARRES1 overexpressing and Mock transfected Jeg-3 cells (Additional file 5). We observed a trend of increased impedance of confluent Jeg-3 cells overexpressing RARRES1 compared to Mock control (Additional file 6: Figure S3). Furthermore, RARRES1 or Mock transfected cells showed no difference in proliferation or migration (Additional file 5 and Additional file 6: Figure S3).
Fig. 4

Correlation of cell density and RARRES1 expression. a RARRES1 expression was analyzed in human third trimester placental sections by immunofluorescence staining. RARRES1 positivity is indicated by green. Nuclei are blue. a (a-b) represent the villous, c the extravillous part. b is a magnification of the square in a. White arrow heads indicate RARRES1 positive VTs, which are in cell-cell contact with the SCT. The bars equal 100 μm. b Scheme of the experimental procedure. Swan71 cells were seeded at different cell densities and RNA was isolated after 48 h. By qRT-PCR we compared the expression pattern of different genes in dependence of low to high cell densities normalized to 18SrRNA. c qRT-PCR analysis of RARRES1 (a and b), RARα, β, γ and RXRα (c) as well as E-Cadherin, N-Cadherin and TJP1 (d) expression in Swan71 (a, c and d) and Jeg-3 (b) cells. Gene expression was normalized to 18 s rRNA expression and set relative to the expression level observed at 0.75x104 cells per ml. Significance is marked by asterisks (* p < 0.05, ** p < 0.005) and calculated relative to the expression at a cell density of 0.75*104/ml. Data represent mean ± SEM

In order to investigate whether other genes involved in RA signaling were additionally upregulated with increasing cell density, we analyzed gene expression of the transcription factors RARα, β, γ and RXRα (Fig. 4c, c). We detected a significant increase of RARβ, γ and RXRα expression (Fig. 4c, c, p < 0.05), with RARβ exhibiting the most prominent increase (6.1-fold). Additionally, we analyzed the expression pattern of the epithelial and mesenchymal marker genes E- and N-Cadherin and the tight junction protein 1 (TJP1) (Fig. 4c, d). E-Cadherin increased significantly with rising cell density, while N-Cadherin expression increased up to 2.0-fold at a density of 3.0x104/ml but declined at densities over 6.0x104 cells/ml (Fig. 4c, d). Similarly, we observed a small increase of TJP1 expression at 3.0x104 cells/ml, which decreased with rising cell numbers (Fig. 4c, d). We further analyzed gene expression of RARβ, E-Cadherin, N-Cadherin and TJP1 in Jeg-3 and JAR cells with siRNA-induced knock-down of RARRES1 and RARRES1 overexpression using a pDest-26 plasmid. We did not detect any differences regarding the gene expression compared to mock controls (data not shown).

High RARRES1 expression in apoptotic and proliferative cells

In order to characterize specific RARRES1 expression in human placental tissue and trophoblastic cell lines, we performed immunohistochemical and immunofluorescence staining (Fig. 5a and b ). We especially detected high RARRES1 expression within syncytial knots (Fig. 5a , a and b). We further observed high RARRES1 expression in silenced cells with fragmented nuclei by immunofluorescence staining of Swan71 (Fig. 5a, c). Additionally, dividing cells showed a strong RARRES1 expression in placental tissue (Fig. 5b, a and b) as well as in Swan71 cells (Fig. 5b, c-h). RARRES1 expression was especially high during the meta-, ana- and telophase of proliferating Swan71 cells (Fig. 5b, c-h).
Fig. 5

RARRES1 expression in placental tissue and Swan71 cells. a RARRES1 localization in syncytial knots and apoptotic cells was analyzed by immunohistochemistry of placental sections (a and b) and immunofluorescence of fixed Swan71 cells (c and d). RARRES1 positivity is indicated by brown (a and b) or red (c) staining. Nuclei are blue (a-d). b RARRES1 expression in dividing cells was analyzed by immunohistochemistry (a and b) of placental sections and immunofluorescence staining of Swan71 cells (c-h). Black arrow heads mark a VT during mitosis (b). Swan71 cells showed strong RARRES1 positivity during meta- (c and d), ana- (e and f) and telophase (g and h) of mitosis. The bars equal 100 μm

Discussion

Taking the role of RARRES1 as a tumor suppressor with a high methylation pattern in a variety of cancer types into consideration, we predicted that the RARRES1 expression matched promoter methylation in placental tissues and cell lines [9, 2123]. DNA from 3rd trimester placental tissues showed a low methylation pattern of CpG region 1 compared to a significantly higher overall methylation of CpG region 2. Consequently, we assumed CpG region 2 of the RARRES1 promotor might be less relevant for RA-induced transcriptional activation compared to CpG region 1. In all observed choriocarcinoma cell lines both analyzed CpG regions were hypermethylated, which was accompanied by a significant decrease of RARRES1 mRNA expression.

One limitation of the provided results is that AZA treatment of primary trophoblasts could not be performed due to the lack of proliferative capacity of third trimester trophoblasts. Trophoblasts of the third trimester undergo a terminal differentiation leading to an irreversible exit from the cell cycle and thus, AZA treatment of primary trophoblasts would not originate in the incorporation of 5′-AZA-2-dC into the DNA [24]. However, treatment of choriocarcinoma cell lines with AZA abolished the effect of high methylation resulting in an increased RARRES1 gene expression. Nevertheless, we cannot rule out that increase of RARRES1 expression was due to secondary side-effects, e.g. AZA-induced increase of transcription factors. It is well known that genes involved in RA-signaling are commonly methylated in cancer and that their expression can be induced by AZA treatment [19, 25]. For example, methylation of RARRES1 correlates with RARβ promoter methylation in prostate cancer and treatment of colon and breast carcinoma cells with AZA induced a demethylation of the RARβ promoter region and a restoration of RARβ expression [19, 26, 27].

Regardless of secondary side-effects, we hypothesize that RARRES1 expression and functional activity might be lost in choriocarcinomas, supporting the concept that placental RARRES1 might act in a suppressive manner and in cases of choriocarcinoma as a tumor suppressor. This is in line with our observation that RARRES1 protein expression in the intramolar choriocarcinoma tissue is limited to cells of the molar trophoblast. In comparison to the choriocarcinoma cell lines BeWo, JAR and Jeg-3, the first-trimester trophoblast-like cell line Swan71 showed a hypomethylation pattern at CpG region 1, while CpG region 2 was hypermethylated as well. Unlike Jeg-3, JAR and BeWo, this cell line does not originate from choriocarcinoma tissue. Swan71 is a telomerase immortalized cell line that is used as a model for first trimester trophoblasts [15]. In Swan71 cells the methylation of the entire RARRES1 promoter was similar to the methylation pattern observed in placental tissues and isolated trophoblasts of the third trimester.

Peng et al. [9] previously analyzed RARRES1 promoter methylation (up to 600 bp upstream of the ATG codon) in primary breast tumors along with matched adjacent benign tissues. In these patients, the methylation pattern of CpG region 1 (~200 bp upstream of the ATG codon) of the benign tissues was comparable to the pattern we observed in healthy placental tissue. Their data showed a low-to-high methylation pattern with increasing distance to the start codon of RARRES1. Even though Peng et al. solely investigated methylation up to 600 bp upstream from the ATG, this increase of methylation resembles the higher methylation pattern at CpG region 2 (>1000 bp upstream) observed by us. As CpG region 1 was hypomethylated in our placental tissues and subsequently open for transcriptional regulation, we hypothesized that the promoter area around CpG region 1 could be responsible for maintenance of RARRES1 gene expression and that hypomethylation of this region might be essential for transcriptional regulation of RARRES1 in trophoblasts.

With regard to functional aspects of RARRES1 expression, earlier publications showed that RARRES1 is associated with a regulatory role in cancer invasiveness and tumorigenicity [5, 10]. For example, it is capable of suppressing the invasion and colony-forming ability of prostate cancer cells [10]. Here, we detected a high RARRES1 expression in VTs and EVTs and a loss of RARRES1 in malignant choriocarcinoma cells. Thus, we hypothesized that RARRES1 might influence trophoblast function during gestational development, possibly negatively regulating trophoblast invasion and/or fusion ability. Furthermore, our preliminary results in RARRES1 transfected Jeg-3 cells might indicate a potential role in cell connectivity.

Overall, RARRES1 is known to influence many cellular processes. It is able to interact with the transmembrane protein 192 (TMEM192) and thus induces the expression of autophagy related proteins [28]. Additionally, it was shown that RARRES1 affects the expression of valosine-containing protein (VCP), which induces the degradation of free polypeptides and thus is essential for autophagy, too [23, 29]. During human placental development autophagy is associated with the formation of syncytial knots and a reduced trophoblast invasion [30, 31]. This is in line with RARRES1 expression in syncytial knots and apoptotic cells seen by us. Consequently, we hypothesized that loss of RARRES1 in choriocarcinoma cells might induce an increased invasiveness and hinder autophagy as seen during malignant transformation [32]. On the other hand, RARRES1 is capable of inducing EB1 protein expression, which is essentially involved in the regulation of spindle dynamics and the spindle assembly checkpoint machinery [23, 33]. Furthermore, loss of both RARRES1 and EB1 protein expression is thought to be associated with the presence of cancer [33]. In Swan71 cells RARRES1 is strongly expressed during cell division (ana-, meta- and telophase). Thus, it might be of importance for cell cycle regulation in human trophoblasts and loss of protein expression might be associated with cell cycle deregulation in term of malignant transformation.

Another hallmark of cancer progression and especially metastasis is the epithelial to mesenchymal transition (EMT). In breast cancer cells RARRES1 was reported to interfere with beta-Catenin and AGBL2 function [34, 35]. Both proteins are involved in EMT of cancer cells or EVTs [3538]. Expression of RARRES1 during the differentiation of EVTs to giant cells might thus be important to limit myometrial trophoblast invasiveness. On the other hand, loss of RARRES1 expression in choriocarcinoma cells might be essential for cancer cell invasion into the surrounding tissue. Additionally, we observed an induction of RARRES1 and RARβ expression at high cell densities of Swan71 cells. RARβ is important for the transcriptional regulation of RARRES1 expression and thus might be an essential inductor of high cell-density related RARRES1 expression. In the light of high RARRES1 expression in the SCT-neighboring VTs, we predict that RARRES1 might also be involved in the regulation of cell-cell or cell-matrix contacts. As a tumor suppressor it might induce contact inhibition either through transmembrane connections or cell cycle regulation, and thus influence trophoblast behavior. Through its interaction with AGBL2, RARRES1 can inhibit the detyrosination of α-Tubulin [39]. α-Tubulin detyrosination is an important hallmark of EMT [40]. An increase of detyrosinated α-Tubulin induces the formation of microtentacles, which promote the penetration of endothelial cell layers and thus are directly linked to cancer invasiveness and metastasis [41]. Additionally, beta-Catenin is essential for cell adhesion and increases during cancer cell EMT [42]. Loss of RARRES1 expression stimulates the nuclear localization of beta-Catenin, which leads to the dissociation of E-Cadherin/beta-Catenin/alpha-Catenin complexes [34]. This process is important for the induction of cancer cell EMT and might explain the loss of RARRES1 expression in choriocarcinoma cases. In addition to increased RARRES1 expression with high cell densities, we also observed rising E-Cadherin expression. This underscores the possible connection between RARRES1 and the E-Cadherin/beta-Catenin/alpha-Catenin complex. Thus, the ability of RARRES1 to reduce invasiveness and tumorigenicity might be due to its properties as a molecule regulating cell-adhesion [19]. RARRES1-triggered enhanced cell-cell contact of cancer cells might mediate contact inhibition of cell proliferation as well as decreased invasiveness and a reduced migratory capability [43]. Future studies should consider the in-depth investigation of RARRES1/E-Cadherin signaling and its potential regulatory role for cell-cell contact.

Conclusion

Our data demonstrated that RARRES1 expression is lost in choriocarcinoma cases due to promotor hypermethylation. RARRES1 protein expression analysis by immunohistochemistry allowed the discrimination of intramolar and pure choriocarcinoma cases. We further hypothesized that RARRES1 might be a negative regulator of EMT through induction of contact inhibition.

Abbreviations

ATRA: 

All-trans retinoic acid

EMT: 

Epithelial-mesenchymal transition

EVT: 

Extravillous trophoblast

FFPE: 

Formalin fixed paraffin embedded

IF: 

Immunofluorescence

IHC: 

Immunohistochemistry

P: 

Placental tissue

qRT-PCR: 

Quantitative Realtime-PCR

RAR: 

Retinoic acid receptor

RARRES1: 

Retinoic acid receptor responder 1

SCT: 

Syncytiotrophoblast

SEM: 

Standard error of the mean

TAZA: 

Tazarotene

Tr: 

Primary trophoblasts

VT: 

Villous trophoblast

Declarations

Acknowledgements

The authors wish to thank all patients who participated in this study. The authors thank Dr. P. Klinger and I. Mons (Experimental Tumor Pathology, Institute of Pathology, University Clinic Erlangen, Germany) for expert technical assistance with the pyrosequencing..

Funding

This work was supported by Erlangener Leistungsbezogene Anschubfinanzierung und Nachwuchsfoerderung (ELAN) fond (13–06–14-1 to F.B. Fahlbusch and M. Ruebner) and Dr. Robert Pfleger Stiftung (Bamberg, Germany; to F.B. Fahlbusch and M. Ruebner).

Availability of data and materials

The datasets used and analyzed during the current study are available from the corresponding author on reasonable request.

Authors’ contributions

The present work was performed by HH in partial fulfillment of the requirements for obtaining the degree „Dr. rer nat” at the Friedrich-Alexander-University Erlangen-Nuremberg (FAU), Germany. HH performed and analyzed the experiments. RS, MR and FBF contributed to the conception and design of the work. RS and PLS contributed to the interpretation of the data achieved during cell cultural experiments. RSS contributed to design of the pyrosequencing procedure and analysis of DNA-methylation data. DLW and LCH analyzed and interpreted the chorioncarcinoma stainings. SK and MWB contributed to the acquisition of patients to participate in the study. All authors revised the manuscript critically and approved the version to be published.

Ethics approval and consent to participate

Handling of patients and tissues was approved by the Ethics Committee at the University Erlangen-Nuremberg (No. 2180). A written informed consent was obtained from all participants.

Consent for publication

Not applicable

Competing interests

The authors declare that they have no competing interests.

Publisher’s Note

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

Authors’ Affiliations

(1)
Department of Gynaecology and Obstetrics, University Hospital Erlangen, Friedrich-Alexander University Erlangen-Nuremberg, Comprehensive Cancer Center Erlangen-EMN, Erlangen, Germany
(2)
Institute of Pathology, University Hospital Erlangen, Friedrich-Alexander University Erlangen-Nuremberg, Comprehensive Cancer Center Erlangen-EMN, Erlangen, Germany
(3)
Department of Pediatrics and Adolescent Medicine, University Hospital Erlangen, Friedrich-Alexander University Erlangen-Nuremberg, Erlangen, Germany
(4)
Division Molecular Pathology, Institute of Pathology, University of Leipzig, Leipzig, Germany

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Copyright

© The Author(s). 2017

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