Ovarian steroid hormones (mainly E2 and P4) regulate oviduct physiology. Serum-E2 acts on the oviduct epithelium from the basolateral cell compartment. Upon ovulation, the apical compartment of the oviduct epithelium is temporarily exposed to follicular fluid, which contains much higher levels of E2 than serum. The aim of this study was to evaluate the effects of human periovulatory follicular fluid levels of E2 on oviduct epithelial cells using two porcine in vitro models.
A cell line derived from the porcine oviductal epithelium (CCLV-RIE270) was characterized (lineage markers, proliferation characteristics and transformation status). Primary porcine oviduct epithelial cells (POEC) were cultured in air-liquid interface and differentiation was assessed histologically. Both cultures were exposed to E2 (10 ng/ml and 200 ng/ml). Proliferation of CCLV-RIE270 and POEC was determined by real-time impedance monitoring and immunohistochemical detection of Ki67. Furthermore, marker gene expression for DNA damage response (DDR) and inflammation was quantified.
CCLV-RIE270 was not transformed and exhibited properties of secretory oviduct epithelial cells. Periovulatory follicular fluid levels of E2 (200 ng/ml) upregulated the expression of inflammatory genes in CCLV-RIE270 but not in POEC (except for IL8). Expression of DDR genes was elevated in both models. A significant increase in cell proliferation could not be detected in response to E2.
CCLV-RIE270 and POEC are complementary models to evaluate the consequences of oviduct exposure to follicular fluid components. Single administration of periovulatory follicular fluid E2 levels trigger inflammatory and DNA damage responses, but not proliferation in oviduct epithelial cells.
Citation: Palma-Vera SE, Schoen J, Chen S (2017) Periovulatory follicular fluid levels of estradiol trigger inflammatory and DNA damage responses in oviduct epithelial cells. PLoS ONE 12(2): e0172192. https://doi.org/10.1371/journal.pone.0172192
Editor: Eric Asselin, Universite du Quebec a Trois-Rivieres, CANADA
Received: September 9, 2016; Accepted: February 1, 2017; Published: February 23, 2017
Copyright: © 2017 Palma-Vera et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: All relevant data are available at the following Figshare link (DOI): https://doi.org/10.6084/m9.figshare.4299725.
Funding: SEPV was supported by Dahlem Research School (FU Berlin), Germany. SC was supported by the Nature Science Funds from Hebei Ministry of Education (QN2014124), China.
Competing interests: The authors have declared that no competing interests exist.
Within the estrous cycle, changing serum levels of ovarian steroid hormones (mainly estradiol, E2, and progesterone, P4) regulate oviduct physiology in mammals [1–4], including transport and maturation of oocytes, sperm and early embryo development . During these cyclic changes, serum-E2 acts on the oviduct epithelium from the basolateral cell compartment. Upon ovulation, the luminal side (apical compartment) of the oviduct epithelium is temporarily exposed to follicular fluid, which induces an inflammatory-like process with macrophage infiltration and enhanced DNA damage .
Follicular fluid contains much higher levels of E2  than serum (up to 200 ng/ml). The impact of such high concentrations of apical E2 on the oviduct epithelium has not yet been elucidated. However, a recent study showed that already 10 nM E2 (~2.72 ng/ml) could upregulate transcription of the inflammatory chemokine IL8 in human oviductal epithelial cells in vitro .
In other cell types it was reported that E2 can have genotoxic and proliferative effects. Genotoxicity results from accumulation of ROS and depurinating adducts after oxidative metabolism of E2, whereas its proliferative properties result from the interaction of E2 with its nuclear and membrane-bound receptors [9,10]. Also, it was shown that E2 can either promote or inhibit inflammation, determined by the cell type and E2 concentrations among other factors .
Pig is an alternative model species for biomedical research, allowing sample collection at large scales for the establishment of complex in vitro models [12,13]. Recently, our group has established an air-liquid-interphase (ALI) model for culturing primary porcine oviduct epithelial cells (POEC) [14,15]. These cells become polarized, exhibit ciliated and secretory phenotypes and are able to respond to basolateral E2 and P4, thus, preserving the native features of the oviductal epithelium during the estrus cycle.
In the present study, we aim to evaluate the effects of apical administration of human periovulatory follicular levels of E2. We employed two porcine cell models: a) an oviductal secretory cell line (CCLV-RIE270) and b) a polarized and in vivo-like POEC culture system that allows hormonal manipulation from both the basolateral and apical compartment [14–17]. We hypothesize that human periovulatory follicular levels of E2 (as they are found in the follicular fluid during ovulation) triggers DNA damage response (DDR), proliferation and inflammatory response simultaneously.
Materials and methods
Research material for this study derived from two sources: 1) porcine oviducts collected at a commercial slaughterhouse (Teterower Fleisch GmbH, Koppelbergstraße 2, 17166 Teterow, Germany) from pigs slaughtered for the purpose of meat production and 2) a porcine cell line (CCLV-RIE270) kindly provided by the cell line collection of the Friedrich-Loeffler-Institute, Germany. Thus, animals were not specifically killed for the purpose of this study and ethical approval was not required.
Phenol red free DMEM, accutase and GlutaMax were products of Gibco (Thermo Fisher Scientific, Dreieich, Germany). Reduced glutathione, collagenase 1A, bovine serum albumin (BSA), ascorbic acid, E2 and primers for qPCR were provided by Sigma-Aldrich (Neustadt, Germany). Other cell culture reagents and additives were purchased from Biochrom (division of Merck Millipore, Berlin, Germany) unless otherwise specified. Reagents used for RT-qPCR were obtained from Thermo Fisher Scientific (Dreieich, Germany).
Characterization of CCLV-RIE270 cells
The CCLV-RIE270 cells (1x106) were plated in T-25 cell culture flasks with 8 ml culture medium: DMEM (without phenol red) supplemented with 10% fetal bovine serum, 4 mM GlutaMax and 1 mM sodium pyruvate. Cells were passaged every 3 to 4 days at the ratio of 1:3 once cells reached 80% confluence.
We evaluated anchorage independent growth via soft agar colony formation by the CytoSelect™ 96-Well Cell Transformation Assay kit (Cell Biolabs, CA, USA) following the manufacturer’s instructions. A transformed human embryonal kidney cell line (HEK-293) was used as positive control, while a mouse fibroblast cell line (NIH-3T3) was taken as negative control. Briefly, Cells (5×103/well) were seeded in triplicate onto a 96-well plate. After 7 days incubation at 37°C and 5% CO2, cells were lysed and labeled with CyQuant GRdye. Fluorescence was determined with CytoFluor II Microplate Reader (Thermo Fisher Scientific, Dreieich, Germany) using a 485/530 nm filter set.
To check how cell growth and proliferation are affected by the seeding density, we performed impedance monitoring using the xCelligence system (Roche, Mannheim, Germany) following the manufacturer’s instructions. This system monitors cell proliferation in real-time by measuring electrical resistance across electrodes on the bottom of a 96-well tissue culture plate (E-Plate). Cells were seeded at the density of 5x103, 1x104, 2x104 and 4x104/well. For each seeding density, 5 replicates were included. Electrical impedance was monitored at intervals of 15 min. Cell impedance was represented as normalized cell index.
Detection of lineage markers.
Markers for secretory oviduct epithelial cells (OVGP1, PAX-8, ESR1) and epithelial markers (Cytokeratin, ß-Catenin) were evaluated by immunofluorescence (IF). Cells were grown on glass cover slips, fixed with histofix 4% (Carl Roth, Karlsruhe, Germany) overnight at 4°C, and unspecific binding sites were blocked with either 5% BSA plus 10% goat serum (Abcam, Cambridge, UK) or Roti-ImmunoBlock (1:50, Carl Roth, Karlsruhe, Germany) for 1 h at room temperature. Cells were incubated with the primary antibody overnight at 4°C. Primary antibodies and their respective dilutions (in blocking buffer) are listed in Table 1. Corresponding secondary antibodies were purchased from Thermo Fisher Scientific (Dreieich, Germany) and diluted in PBS + 1% BSA: goat anti rabbit Alexa 647 (1:200, A21245), donkey anti goat Alex 568 (1:40, A11057), and goat anti mouse Alexa 488 (1:40, A11017). Incubation time was 1 h at room temperature. Nuclei were counterstained either with TO-PRO-3 iodide (Mobitec, Berkheim, Germany) or SYBR Green I (Mobitec, Berkheim, Germany). Images were captured by the confocal laser scanning microscope LSM 800 equipped with ZEN software (Carl Zeiss, Oberkochen, Germany).
After collection at the slaughterhouse, oviduct tissues were immediately transported on ice to the laboratory. Surrounding tissue was trimmed and oviducts were washed in PBS. Oviduct epithelial cells were isolated as previously described . Briefly, oviducts were filled with collagenase and squeezed to detach epithelial clusters. Cell clusters were further singled out by accutase and either seeded immediately or stored in liquid nitrogen for later use.
Cells were seeded on 12-well hanging inserts (PET membrane, 0.4 μm pore size, Merck Millipore, Darmstadt, Germany) at a concentration of 4.5×105/400 μl of growth medium. Inserts were placed into 12-well plates containing 1.5 ml of growth medium consisting of two parts of phenol red free Ham’s F12 (with 10% fetal bovine serum), one part of 3T3 conditioned medium (produced as described previously ), 100 U/ml penicillin, 100 μg/ml streptomycin, 50 μg/ml gentamicin, 1 μg/ml amphotericin B, 10 μg/ml reduced glutathione and 10 μg/ml ascorbic acid. Cells were incubated in a humid chamber at 37°C with 5% CO2. After 3 days, the medium inside the insert was removed, allowing cells to remain in an ALI. Medium changes were performed twice a week and cultures were treated with E2 after 3 weeks of culture.
Characterization of POEC.
After 3 weeks of cultivation, membranes were cut out of the inserts, sequentially fixed with Bouin´s solution and histofix 4%, dehydrated in a graded ethanol series, and then vertically embedded in paraplast (Leica, Wetzlar, Germany) as described previously . Sections of 4 μm were prepared for hematoxylin-eosin staining or immunohistochemical (IHC) detection.
The presence of ciliary marker Acetylated Tubulin was detected by IF. To illustrate the cilia structure from an aerial view, the membrane was removed from the insert, fixed in 4% histofix, and processed directly for staining without embedding in paraplast. Protocol for IF was performed as described in the paragraph “Detection of lineage markers”.
E2 stimulation experiments
Two different concentrations of E2 (10 ng/ml and 200 ng/ml) were employed for stimulation, as E2 levels reported for human follicular fluid around the time point of ovulation vary widely in the literature [18,19]. CCLV-RIE270 (passage 32, 5 replicates) was stimulated with E2 in a total volume of 8 ml of medium for 20 min, 3 h and 24 h in T-25 flasks.
After 3 weeks ALI culture, POEC from 5 different animals were apically exposed to E2 in a total volume of 400 μl for 3 h and 24 h. The amount of E2 per surface unit (cm2) was taken into account, in order to expose CCLV-RIE270 and POEC to comparable amounts of E2. As controls, only vehicle (ethanol) was applied to cultures.
After E2 stimulation, proliferation of CCLV-RIE270 was measured by real-time impedance monitoring using the xCelligence system. Cells were seeded onto the E-Plate at a density of 5x103/well. After 48 h of culture, cells were treated with E2 (10 ng/ml, 200 ng/ml and ethanol as negative control) for 24 h (5 replicates). Thereafter, medium was refreshed, and cell growth was further monitored up to 200 h.
Furthermore, proliferation of CCLV-RIE270 and POEC stimulated with E2 for 24 h was assessed by IHC detection of Ki67. CCLV-RIE270 grown on glass cover slips (n = 5 replicates per group) were treated with E2 (10 or 200ng/ml) or solvent for 24h when they reached ~50% confluence and fixed in ice-cold methanol. Cells were washed, blocked and subjected to incubation with anti-Ki67 antibody at 4°C overnight. Antigen detection was visualized by the EnVision Dual Link System-HRP kit (Dako, Hamburg, Germany) and counterstained with hemalum. Cover slips were mounted on glass slides and at least 13 consecutive microscopic pictures were taken (magnification x400). Images were acquired with an Axio Imager A1 upright microscope equipped with AxioVison Rel.4.8 software (Carl Zeiss, Oberkochen, Germany). The total number of nuclei and Ki67 positive cells were counted using Image J software. POEC membranes were embedded in paraplast as described above, sections of approx. 4 μm were subjected to heat-induced antigen retrieval in citrate buffer (10 mM, pH 6.0, 3 min), followed by incubation with anti-Ki67 antibody at 4°C overnight. Staining and acquisition of micrographs (at least 5 pictures per sample) was performed as described above. The total number of nuclei and Ki67 positive cells over the membrane length were counted for all samples (n = 5 animals).
Gene expression analysis
Gene expression of CCLV-RIE270 and POEC was assessed by RT-qPCR. Primer sequences, product sizes and transcript identifiers are shown in Table 2. Annealing temperature was 60°C for all primers.
Cultures were washed with PBS before RNA was extracted with a commercial kit following the manufacturer’s instructions (NucleoSpin RNA, Macherey-Nagel, Dueren, Germany). RNA quantity and purity were measured by NanoDrop ND-1000 (Peqlab Biotechnology, Erlangen, Germany), whereas RNA quality was measured by Agilent 2100 Bioanalyzer (Agilent Technologies, Waldbronn, Germany). All samples used in this study exhibited an RNA integrity number higher than 9.
RNA (1μg) was treated with DNase I (1 U, 30 min at 37°C), linearized at 65°C for 5 min and annealed to a mixture (1:1 v/v) of oligo dT and random hexamers (2.5 μM each). Then, RNA was converted into cDNA by adding dNTPs (0.5 mM) and RevertAid reverse transcriptase (200 U, 25°C for 10 min, 42°C for 60 min and 70°C for 10 min) in a total volume of 20 μL. Quantitative PCR was performed in duplicates using LightCycler 96 system (Roche, Mannheim, Germany). For this, cDNA was amplified in a final volume of 12 μl containing 0.5 μM forward primer, 0.5 μM reverse primer, 1X FastStrat Essential DNA Green Master (Roche, Mannheim, Germany). PCR amplification was performed as follows: initial denaturation at 95°C for 10 min, 45 cycles of 95°C for 20 s, 60°C for 20 s, and 72°C for 10 s.
Expression levels of mRNAs were determined in duplicate and relative gene expression was calculated by applying the 2-ΔΔCT method , corrected for PCR efficiency. Reference genes for normalization were determined using the GeNorm algorithm, part of the R package “NormqPCR” .
Data from POEC was tested for normality (Shapiro Wilk test). Normal data was analyzed by repeated-measures analysis of variance (ANOVA), followed by pairwise paired t-test with Bonferroni correction. Data that did not follow a normal distribution was compared using Friedman rank sum test, followed by pairwise paired Wilcoxon rank sum test with Bonferroni correction. For each experiment, 5 animals were used. All analyses were performed using the R statistical software.
Data from CCLV-RIE270 was tested for normality (Shapiro Wilk test). Normal data was analyzed by one way ANOVA, followed by pairwise t-test with Bonferroni correction. Data that did not follow a normal distribution was compared using Kruskal-Wallis rank sum test, followed by pairwise Wilcoxon rank sum test with Bonferroni correction. For each experiment, 5 biological replicates were used. All analyses were performed using the R statistical software.
Characterization of CCLV-RIE270 and POEC
CCLV-RIE270 exhibited typical epithelial arrangement: polygonal shape and growth in discrete islands (Fig 1A). Cells did not show proliferation in soft agar and were thus not transformed (Fig 1B). The proliferative pattern of CCLV-RIE270 was evaluated by impedance measurement. Four seeding densities (5x103, 1x104, 2x104 and 4x104/well) were tested (Fig 1C). Generally, when seeded at 1-2x104cells/well, 80% confluence was reached within 3–5 days. For the purpose of defining the most suitable seeding number to evaluate the effect of E2 on proliferation, an optimal growth curve would reach its plateau (confluence) towards the endpoint of the experiment (approx. 200 h), leaving room to evaluate the effects of E2 stimulation starting after 48 h. According to this criterion, the lowest seeding amount (5x103cells/well) was chosen for E2 stimulation.
A: Phase-contrast micrograph, magnification x100; B: Anchorage independent growth: comparison among CCLV-RIE270, NIH-3T3 and HEK-293 cell lines. RFUs, relative fluorescence units; n = 3 replicates. C: Proliferation curves of CCLV-RIE270 seeded at different densities as measured by real-time impedance monitoring (xCelligence), shaded regions indicate standard deviations (n = 5 replicates).
Immunofluorescence demonstrated that CCLV-RIE270 express lineage markers for oviductal secretory cells (OVGP1, PAX-8 and ESR1) as well as epithelial markers (Cytokeratin, ß-Catenin), validating the secretory origin of CCLV-RIE270 (Fig 2).
Epithelial markers (β-Catenin, Cytokeratin) and lineage markers (OVGP1, ESR1 and PAX-8) detected by immunofluorescence. Scale bar = 40 μm.
POEC exhibited epithelial polarity and both ciliated and secretory phenotypes after 3 weeks of culture (Fig 3A). Presence of ciliated cells was visualized by the ciliary marker Acetylated Tubulin (Fig 3B).
Effect of E2 on proliferation in oviduct epithelial cells
After defining the appropriate seeding density (5x103/well), proliferation of CCLV-RIE270 in response to E2 was evaluated by impedance monitoring. Visual inspection of Fig 4A suggests a dose dependent shift in the growth curve of CCLV-RIE270. However, the differences between the groups do not reach statistical significance.
A: After 2 days propagation, CCLV-RIE270 cells were treated with E2 (10 ng/ml, 200 ng/ml) or vehicle (ethanol) for 24 h and then further cultured up to 200 h. Cell growth was monitored in real-time using the xCelligence system, shaded regions indicate standard deviations (n = 5 replicates); B: Percentage of Ki67 positive CCLV-RIE270 cells after 24 h E2 stimulation, n = 5 animals; C: representative images for Ki67 staining in POEC. Scale bar = 20 μm. NC, negative control; D: Percentage of Ki67 positive POEC after 24 h E2 stimulation, n = 5 animals.
We also determined the percentage of positive Ki67 foci to assess proliferation of CCLV-RIE270 (Fig 4B) and POEC (Fig 4D). There were no significant differences observed between the groups neither in CCLV-RIE270 nor in POEC. However, in the 200 ng E2/ml group, regions with several successive Ki67 positive cells were frequently observed in POEC (Fig 4C).
E2 regulates expression of genes related to inflammation and DDR
Gene expression assessed in this study represented three main aspects of cell response: specific response to E2 (ESR1, PGR), inflammation (PTGS2, CAT, IL8, IL6 and C3) and DDR (CDKN1A, DDB2, GADD45G, TP53 and BAX). Stimulation with E2 (10 ng/ml and 200 ng/ml) significantly increased the expression of ESR1 after 24 h in both CCLV-RIE270 and POEC (Fig 5A). PGR was significantly upregulated in the differentiated POEC in vitro model only (24 h, 200 ng/ml E2) (Fig 5A). E2 upregulated the expression of PTGS2 in CCLV-RIE270 in a time and dose dependent manner (Fig 5B). After 24 h, PTGS2 expression was back to control levels in all groups. Also, CAT, IL8 and IL6 expression was increased by E2 stimulation in CCLV-RIE270, while C3 was only moderately affected. POEC only showed slight induction of IL8 transcription after 24 h of E2 exposure (Fig 5B). In the POEC model none of the E2 concentrations influenced PTGS2, IL6 or C3 transcription levels at any time point (Fig 5B). Both E2 doses caused an increase in mRNA of CDKN1A and DDB2 after 24 h of E2 exposure in CCLV-RIE270 (Fig 6). In POEC, only expression of DDB2 was slightly elevated after 24h. GADD45G expression was upregulated after 20 min in CCLV-RIE270 and after 3 h in POEC, whereas TP53 was not affected in any of the culture models (Fig 6). Finally, the expression of the apoptotic gene BAX was slightly increased in response to E2 after 20 min and after 24 h (200 ng/ml) in CCLV-RIE270, whereas in POEC its transcription was not affected (Fig 6).
A: Expression of steroid receptors (ESR1 and PGR). B: Expression of inflammation-related marker genes. Data is shown as fold changes relative to the control group and normalized with the reference genes SDHA and ACTB. Asterisks indicate statistical significance (p ≤ 0.05). N = 5 replicates. NC, negative control.
Follicular fluid reaches the distal oviduct epithelium shortly after ovulation and induces an inflammatory-like and DNA damage response. E2 concentrations peak before ovulation in the follicular fluid, reaching much higher levels than in serum . To better understand the role of E2 in the response of the oviduct epithelium to follicular fluid, we evaluated the consequences of follicular fluid E2 on two porcine oviductal epithelial cell models. We hypothesized that apical application of periovulatory follicular levels of E2 would simultaneously trigger inflammatory and DNA damage responses, as well as proliferation.
The exposure of oviduct epithelial cells to follicular fluid concentrations of E2 promoted transcription of IL6, IL8 and PTGS2, indicative of an inflammatory-like response. This is in line with results produced by exposing bovine  or human  oviductal epithelial cells in vitro to human follicular fluid. Eddie et al  reported an upregulation of IL8 in response to a lower concentration of E2 (10 nM) in oviduct epithelial cells. Similarly, superovulation in mouse promoted the recruitment of pro-inflammatory macrophages in the oviduct . Taken together, this suggests that E2 is at least one of the contributors to the ovulation-related inflammatory response. A possible mechanism for this E2 effect is the production of intracellular ROS, which can induce PTGS2, cytokine and chemokine synthesis . Catalase is an antioxidant enzyme, which fights free radicals, and its level relates to the stage of cellular oxidative stress . After E2 stimulation, expression of catalase was up-regulated in oviductal epithelial cells, reflecting an increased oxidative status. Thus, we hypothesize that at periovulatory follicular levels, E2 could promote an inflammation-like reaction by increasing the levels of ROS in oviduct epithelial cells.
The proliferative role of E2 has been reported in other cell types [9,10], however, after determination of impedance and Ki67 expression, 24 h after applying E2 at follicular fluid levels, no significant induction of proliferation was induced in our oviduct epithelial cell models. This is in line with a previous in vitro study in human fallopian tube cells, where exposure to E2 for 7 days did not induce proliferation .
Upregulation of CDKN1A, DDB2 and GADD45G indicated that DDR was triggered by high-level E2 stimulation. After DNA damage, transcription of CDKN1A, DDB2 and GADD45G is induced by activation of p53, a transcription factor encoded by TP53 [26,27]. Transcription of TP53 was not significantly affected by the E2 treatment, but the upregulation of its downstream effectors indicates that the follicular fluid E2 induces DDR in oviduct epithelial cells.
Discrepancies in gene expression were found between the two models. There are two key distinctions that might explain why the pronounced inflammatory and DNA damage responses to E2 seen in CCLV-RIE270 were not recapitulated by POEC. First, secretory oviduct epithelial cells are more prone to genotoxic stress than ciliated cells . Thus, if the same genotoxic stimulus is applied, milder responses will be triggered in cultures having both ciliated and secretory cell populations (e.g. POEC), in contrast to cultures consisting of pure secretory cells (e.g. CCLV-RIE270). Second, there are structural differences between CCLV-RIE270 and POEC. For instance, the surface of exposure to E2 is larger in CCLV-RIE270 (non-polarized, flat cells) than in POEC (polarized, columnar shaped cells). Other differences include specific cell to cell contacts and membrane properties.
Considering that spontaneous serous ovarian cancer is linked to increased number of lifetime ovulations in humans , and that it is likely to arise from the oviductal tube epithelium , the long term cumulative effects of follicular fluid components on oviduct epithelial cells deserve special attention. Moreover, porcine models for the study of human diseases hold great potential [12,13], which is why we consider POEC and CCLV-RIE270 as suitable in vitro models to understand the early origins of serous ovarian cancer in the oviduct. On the one hand, POEC can be maintained in vitro in a highly differentiated state [14–16] without passaging for at least 3 months , offering the possibility to evaluate the effects of follicular fluid components repeatedly over several weeks on a mixture of secretory and ciliated cells. On the other hand, CCLV-RIE270 is immortalized, easy to use, and provides a pure secretory cell population, preserving their original phenotype, as shown by expression of specific marker proteins (especially OVGP1, a functional marker for oviductal secretory cells) and by the absence of anchorage independent growth.
We conclude that CCLV-RIE270 and POEC can be used as complementary in vitro systems to evaluate the consequences of oviductal exposure to follicular fluid components. Using these two models we were able to demonstrate that single administration of E2 at periovulatory follicular fluid levels simultaneously activates DDR and inflammation, but not proliferation in oviduct epithelial cells in vitro.
We thank Lisa Speck, Caterina Poeppel, Christine Meyer and Petra Reckling, FBN Dummerstorf, Germany, for their excellent technical support. We are grateful to Ralf Poehland, FBN Dummerstorf, for supporting imaging procedures. We appreciate Matthias Lenk, cell line collection of the Friedrich-Loeffler-Institute, Germany, for kindly providing the CCLV-RIE270 cell line.
- Conceptualization: SC JS.
- Formal analysis: SEPV JS SC.
- Investigation: SC SEPV.
- Project administration: SC JS.
- Supervision: SC.
- Visualization: SEPV.
- Writing – original draft: SEPV.
- Writing – review & editing: SC JS.
- 1. Abe H, Hoshi H. Regional and cyclic variations in the ultrastructural features of secretory cells in the oviductal epithelium of the Chinese Meishan pig. Reprod Domest Anim. 2007 Jun;42(3):292–8. pmid:17506808
- 2. Steinhauer N, Boos A, Gunzel-Apel AR. Morphological changes and proliferative activity in the oviductal epithelium during hormonally defined stages of the oestrous cycle in the bitch. Reprod Domest Anim. 2004 Apr;39(2):110–9. pmid:15065993
- 3. Aguilar JJ, Cuervo-Arango J, Mouguelar H, Losinno L. Histological Characteristics of the Equine Oviductal Mucosa at Different Reproductive Stages. J Equine Vet Sci. 2012 Feb;32(2):99–105.
- 4. Abe H, Oikawa T. Observations by scanning electron microscopy of oviductal epithelial cells from cows at follicular and luteal phases. Anat Rec. 1993 Mar;235(3):399–410. pmid:8430910
- 5. Menezo Y, Guerin P. The mammalian oviduct: biochemistry and physiology. Eur J Obstet Gynecol Reprod Biol. 1997 May;73(1):99–104. pmid:9175697
- 6. King SM, Hilliard TS, Wu LY, Jaffe RC, Fazleabas AT, Burdette JE. The impact of ovulation on fallopian tube epithelial cells: evaluating three hypotheses connecting ovulation and serous ovarian cancer. Endocr Relat Cancer. 2011;18(5):627–42. pmid:21813729
- 7. de los Santos MJ, Garcia-Laez V, Beltran D, Labarta E, Zuzuarregui JL, Alama P, et al. The follicular hormonal profile in low-responder patients undergoing unstimulated cycles: Is it hypoandrogenic? Hum Reprod. 2013 Jan;28(1):224–9. pmid:23019297
- 8. Eddie SL, Quartuccio SM, Zhu J, Shepherd JA., Kothari R, Kim JJ, et al. Three-dimensional modeling of the human fallopian tube fimbriae. Gynecol Oncol. 2015;136(2):348–54. pmid:25527363
- 9. Yager JD. Mechanisms of estrogen carcinogenesis: The role of E2/E1–quinone metabolites suggests new approaches to preventive intervention–A review. Steroids. 2015;99:56–60. pmid:25159108
- 10. Cavalieri E, Rogan E. The Molecular Etiology and Prevention of Estrogen-Initiated Cancers. Mol Aspects Med. 2014 Apr 30;0:1–55.
- 11. Straub RH. The Complex Role of Estrogens in Inflammation. Endocr Rev. 2006 Dec 1;28(5):521–74.
- 12. Bendixen E, Danielsen M, Larsen K, Bendixen C. Advances in porcine genomics and proteomics—a toolbox for developing the pig as a model organism for molecular biomedical research. Brief Funct Genomics. 2010;9(3):208–19. pmid:20495211
- 13. Flisikowska T, Kind A, Schnieke A. The new pig on the block: modelling cancer in pigs. Transgenic Res. 2013;22(4):673–80. pmid:23748932
- 14. Miessen K, Sharbati S, Einspanier R, Schoen J. Modelling the porcine oviduct epithelium: a polarized in vitro system suitable for long-term cultivation. Theriogenology. 2011 Sep;76(5):900–10. pmid:21719086
- 15. Chen S, Einspanier R, Schoen J. Long-term culture of primary porcine oviduct epithelial cells: validation of a comprehensive in vitro model for reproductive science. Theriogenology. 2013 Nov;80(8):862–9. pmid:23973051
- 16. Chen S, Einspanier R, Schoen J. In vitro mimicking of estrous cycle stages in porcine oviduct epithelium cells: estradiol and progesterone regulate differentiation, gene expression, and cellular function. Biol Reprod. 2013 Sep;89(3):54. pmid:23904510
- 17. Chen S, Einspanier R, Schoen J. Transepithelial electrical resistance (TEER): a functional parameter to monitor the quality of oviduct epithelial cells cultured on filter supports. Histochem Cell Biol. 2015 Nov;144(5):509–15. pmid:26223877
- 18. Wunder DM, Mueller MD, Birkhäuser MH, Bersinger NA. Steroids and protein markers in the follicular fluid as indicators of oocyte quality in patients with and without endometriosis. J Assist Reprod Genet. 2005 Jun 14;22(6):257–64. pmid:16021855
- 19. Wen X, Li D, Tozer AJ, Docherty SM, Iles RK. Estradiol, progesterone, testosterone profiles in human follicular fluid and cultured granulosa cells from luteinized pre-ovulatory follicles. Reprod Biol Endocrinol. 2010 Oct 11;8:117. pmid:20937107
- 20. Livak KJ, Schmittgen TD. Analysis of relative gene expression data using real-time quantitative PCR and the 2(-Delta Delta C(T)) Method. Methods. 2001 Dec;25(4):402–8. pmid:11846609
- 21. Perkins JR, Dawes JM, McMahon SB, Bennett DLH, Orengo C, Kohl M. ReadqPCR and NormqPCR: R packages for the reading, quality checking and normalisation of RT-qPCR quantification cycle (Cq) data. BMC Genomics. 2012;13(1):1–8.
- 22. Lau A., Kollara A, St John E, Tone AA, Virtanen C, Greenblatt EM, et al. Altered expression of inflammation-associated genes in oviductal cells following follicular fluid exposure: Implications for ovarian carcinogenesis. Exp Biol Med. 2014;239(1):24–32.
- 23. Bahar-Shany K, Brand H, Sapoznik S, Jacob-Hirsch J, Yung Y, Korach J, et al. Exposure of fallopian tube epithelium to follicular fluid mimics carcinogenic changes in precursor lesions of serous papillary carcinoma. Gynecol Oncol. 2014;132(2):322–7. pmid:24355484
- 24. Hussain SP, Harris CC. Inflammation and cancer: an ancient link with novel potentials. Int J cancer. 2007 Dec;121(11):2373–80. pmid:17893866
- 25. Chelikani P, Fita I, Loewen PC. Diversity of structures and properties among catalases. Cell Mol Life Sci. 2004 Jan;61(2):192–208. pmid:14745498
- 26. Meng X, Dong Y, Sun Z. Mechanism of p53 downstream effectors p21 and Gadd45 in DNA damage surveillance. Sci China Ser C, Life Sci. 1999 Aug;42(4):427–34.
- 27. Hwang BJ, Ford JM, Hanawalt PC, Chu G. Expression of the p48 xeroderma pigmentosum gene is p53-dependent and is involved in global genomic repair. Proc Natl Acad Sci U S A. 1999 Jan;96(2):424–8. pmid:9892649
- 28. Levanon K, Ng V, Piao HY, Zhang Y, Chang MC, Roh MH, et al. Primary ex vivo cultures of human fallopian tube epithelium as a model for serous ovarian carcinogenesis. Oncogene. 2010;29(8):1103–13. pmid:19935705
- 29. Nik NN, Vang R, Shih I-M, Kurman RJ. Origin and pathogenesis of pelvic (ovarian, tubal, and primary peritoneal) serous carcinoma. Annu Rev Pathol. 2014;9:27–45. pmid:23937438
- 30. Chen S, Einspanier R, Schoen J. Characterizing the differentiation process of oviductal epithelial cells in air-liquid interface (ALI) culture. In: 48th Annual Conference Physiology and Pathology of Reproduction and simultaneously 40th Joint Congress of Veterinary and Human Medicine. Zürich: Reproduction In Domestic Animals; 2015. p. 12.