Expression of tissue factor and tissue factor pathway inhibitors during ovulation in rats: a relevance to the ovarian hyperstimulation syndrome
Reproductive Biology and Endocrinology volume 19, Article number: 52 (2021)
Blood coagulation has been associated with ovulation and female infertility. In this study, the expression of the tissue factor system was examined during ovulation in immature rats; the correlation between tissue factor and ovarian hyperstimulation syndrome (OHSS) was evaluated both in rats and human follicular fluids.
Ovaries were obtained at various times after human chorionic gonadotropin (hCG) injection to investigate the expression of tissue factor system. Expression levels of ovarian tissue factor, tissue factor pathway inhibitor (Tfpi)-1 and Tfpi-2 genes and proteins were determined by real-time quantitative polymerase chain reaction (qPCR), and Western blot and immunofluorescence analyses, respectively. Expression levels of tissue factor system were also investigated in ovaries of OHSS-induced rats and in follicular fluid of infertile women.
The expression of tissue factor in the preovulatory follicles was stimulated by hCG, reaching a maximum at 6 h. Tissue factor was expressed in the oocytes and the preovulatory follicles. Tfpi-2 mRNA levels were mainly increased by hCG in the granulosa cells whereas the mRNA levels of Tfpi-1 were decreased by hCG. Human CG-stimulated tissue factor expression was inhibited by the progesterone receptor antagonist. The increase in Tfpi-2 expression by hCG was decreased by the proliferator-activated receptor γ (PPARγ) antagonist. Decreased expression of the tissue factor was detected in OHSS-induced rats. Interestingly, the tissue factor concentrations in the follicular fluids of women undergoing in vitro fertilization were correlated with pregnancy but not with OHSS.
Collectively, the results indicate that tissue factor and Tfpi-2 expression is stimulated during the ovulatory process in rats; moreover, a correlation exists between the levels of tissue factor and OHSS in rats but not in humans.
Ovulatory follicles undergo inflammation-like changes in response to the luteinizing hormone (LH) surge . In rats, leukocyte infiltration in the periovulatory ovary  and extravasation of erythrocytes and fibrin clots in the follicular wall are observed during ovulation . Fibrinogen secretion by bovine granulosa cells plays a role in ovulation by increasing the proteolytic activity . Consistent with these observations, thrombin (a protease essential for fibrin formation) and its receptor are present in the periovulatory follicles in bovine [5, 6] and mouse  ovaries. In addition, the functional activity of thrombin and its receptor has been reported in human luteinized granulosa cells  and follicular fluid [8, 9]. These findings suggest the involvement of the blood coagulation system in the ovulatory process.
Tissue factor, a membrane-anchored glycoprotein, is the most important physiological regulator in thrombin generation and initiates the extrinsic pathway of coagulation via binding to factor VII . The catalytic activity of the tissue factor-factor VIIa complex is inhibited by tissue factor pathway inhibitors (TFPIs), TFPI-1 and TFPI-2, belonging to the Kunitz family of serine protease inhibitors . Tissue factor and TFPI-2 are detected in ovarian follicular fluid obtained from women undergoing in vitro fertilization . Recently, it has been reported that TFPI-2 expression is stimulated by an ovulatory dose of gonadotropins in rat and human ovaries . However, the detailed changes in the expression of the tissue factor system during the periovulatory period need to be assessed.
Factors regulating blood coagulation have been proven to be relevant to female infertility. Recurrent pregnancy loss is often related to increased levels of coagulant factors such as factor X and fibrinogen, and reduced levels of anticoagulant factors such as protein C . The presence of blood clots within the cumulus matrix is associated with reduced blastocyte formation during in vitro fertilization in humans . In addition, tissue factor acts as an important pro-inflammatory mediator in antiphospholipid antibody-induced pregnancy loss in mice . Circulating tissue factor is elevated in women with polycystic ovary syndrome [17, 18]. Interestingly, TFPI-1 levels in blood, but not in follicular fluid, are significantly different between patients with ovarian hyperstimulation syndrome (OHSS) and non-OHSS patients .
OHSS is the most serious complication that, occurs during ovulation induction for the in vitro fertilization procedure . The rat model of OHSS is established, demonstrating that vascular endothelial growth factor (VEGF) is a potential cause of the development of OHSS [21, 22]. Following treatment with human chorionic gonadotropins (hCG), an increase in VEGF concentration was observed in follicular fluid and serum in women undergoing in vitro fertilization . Clinical manifestations of OHSS include massive extravascular fluid accumulation and hemoconcentration due to capillary leakage . VEGF induces tissue factor expression in endothelial cells, increasing procoagulant properties of the vessel wall . High tissue factor and low TFPI-1 levels in plasma were reported in patients with severe OHSS [25, 26]; however, no relationship was observed between follicular fluids of patients with and without OHSS . Moreover, no report has yet elucidated the relationship between the tissue factor system and infertility factors, including OHSS in human follicular fluid.
Therefore, the present study was aimed to investigate the time- and cell-specific expression of tissue factor, TFPI-1 and TFPI-2 by gonadotropin treatment during the ovulatory process in rats. Moreover, as angiogenic factors play a role in the pathogenesis of OHSS , the relationship between the tissue factor system and OHSS was tested in the experimental model of OHSS in rats and in infertile patients undergoing in vitro fertilization.
Materials and methods
Hormones and reagents
Equine chorionic gonadotropin (eCG/PMSG), human chorionic gonadotropin (hCG), and chemical inhibitors including indomethacin, nordihydroguaiaretic acid, GW9662 were purchased from Sigma (St. Louis, MO, USA). RU486 was purchased from Enzo Life Sciences, Inc. (Farmingdale, NY, USA).
Animals for superovulation induction and administration of ovulation-inhibiting agents
Immature female Sprague-Dawley rats were purchased from Korea Basic Science Institute (Gwangju, Korea) and Samtako BioKorea (Seoul, Korea). They were housed in groups in a room with controlled temperature and photoperiod (10-h dark/14-h light; lights on from 0600 to 2000 h). The animals had ad libitum access to food and water. Immature rats (26 days old; body weight, 60–65 g) were s.c. injected with 10 IU of eCG to induce multiple follicle growth. Two days later, some eCG-primed rats were i.p. injected with 10 IU hCG to induce superovulation. All animals were maintained and treated in accordance with the National Institutes of Health Guide for the Care and Use of Laboratory Animals, as approved by the Institutional Animal Care and Use Committee at Chonnam National University.
Five eCG-primed rats for each treatment group were i.p. injected 30 min before hCG administration with ovulation-inhibiting agents including progesterone receptor antagonist (RU486, 10 mg/kg body weight), cyclooxygenase inhibitor (indomethacin, 10 mg/kg body weight), lipoxygenase inhibitor (nordihydroguaiaretic acid, 3 mg/kg body weight), or proliferator-activated receptor γ (PPARγ) antagonist (GW9662, 2 mg/kg body weight) . Six hours after hCG injection, the rats were euthanized using CO2 administration method and ovaries, upon removal of oviduct and fat pad, were collected for RNA isolation.
Preparation of the rat model of ovarian hyperstimulation syndrome (OHSS)
To prepare the OHSS rat model, immature rats (22 days old) were s.c. injected with 10 IU eCG at 0900 for four consecutive days to promote follicular development; this was followed by an i.p. injection of 30 IU hCG on the 5th day (on the 26th day of life) to induce OHSS (Fig. 1). As the control, rats were injected with 0.9% saline instead of hCG on the 5th day. Manifestation of OHSS includes the increased ovarian weight, VEGF expression and vascular permeability 48 h after hCG administration . Subsequently, the rats were euthanized 48 h after hCG administration (on the 28th day of life); then, the ovaries were collected for RNA isolation. Ovaries were also collected from rats that were stimulated for superovulation in a routine manner 0 h and 48 h after hCG administration.
Collection of ovaries and isolation of granulosa and theca cells of preovulatory follicles
Ovaries were collected from immature rats at different time points (0, 3, 6, 9 and 12 h) after eCG/hCG administration for RNA and protein detection of tissue factor, TFPI-1 and TFPI-2. For the isolation of the granulosa and theca cells of preovulatory follicles, the ovaries were incubated in DMEM/Ham’s F-12 medium (Gibco, Grand Island, NY, USA) containing 0.5 M sucrose and 10 mM EGTA at 37°С for 30 min. The ovaries were then washed thrice with phosphate buffered saline (PBS), and flattened to a single layer to easily identify the preovulatory follicles using fine forceps under a dissection microscope. The granulosa and theca cells were isolated from the preovulatory follicles using a 21-gauge needle for the measurement of mRNA levels.
RNA isolation and real-time PCR analysis
To detect mRNA levels of tissue factor, TFPI-1 and TFPI-2 in ovaries and preovulatory follicles after hCG treatment (0, 3, 6, 9 and 12 h), total RNA was extracted using TRIzol reagent (Molecular Research Center, Inc., Cincinnati, OH, USA), according to the manufacturer’s instructions. Ten or twenty micrograms of total RNA was reverse-transcribed using the RevertAid M-MuLV reverse transcriptase kit (Fermentas, St. Leon-Rot, Germany) to evaluate gene expression. Real-time PCR was then performed on a Rotor-Gene Q 5plex (QIAGEN, Hilden, Germany), located at Korea Basic Science Institute (Gwangju, Korea), using the QuantiTect SYBR Green PCR Kit (QIAGEN) at 95°С for 20 s, 60°С for 20 s, and 72°С for 30 s. Specific primers were designed using the PRIMER3 software (Table 1). The average Ct value in triplicate for each gene was divided by the linear Ct value of β-actin to obtain relative abundance of the transcripts. β-Actin was used as an internal control for all measurements.
Western blot analyses
The ovarian lysates (30 μg) were resolved by 10% SDS-PAGE and transferred to nitrocellulose membranes (Amersham Bioscience, Arlington Heights, IL, USA), as previously described . Briefly, the transferred membrane was blocked using 5% skim milk before immunoblotting using anti-tissue factor polyclonal antibodies (American Diagnostica, Inc., Stamford, CT, USA; 1:500 dilution) and horseradish peroxidase-conjugated secondary IgGs (1:1000 final dilution). Gapdh (Santa Cruz Biotechnology, Santa Cruz, CA, USA) was used as the loading control. Signals were visualized via enhanced chemiluminescence (Amersham Biosciences).
The localization of the tissue factor protein was determined by immunofluorescence as previously described . Briefly, paraffin sections of ovary (5 μm thick) were incubated with 10% normal horse serum in PBS for 30 min to block non-specific binding of the antibody. The ovarian sections were probed with primary anti-tissue factor antibodies (American Diagnostica, Inc., 1:500 dilution) overnight and, then, washed thrice with PBS, followed by incubation with AlexaFluor 633 fluorescence antibodies (Invitrogen, Carlsbad, CA, USA; 1:500 dilution) for 1 h. After washing thrice with PBS, the sections were mounted on slides and the nuclei were stained with 4′, 6-diamidino-2-phenylindole (DAPI) in ProLong Gold Antifade reagent (Invitrogen). Digital images were captured using a TCS SP5 AOBS laser-scanning confocal microscope (Leica Microsystems, Heidelberg, Germany), located at the Korea Basic Science Institute Gwangju center.
Collection of follicular fluid from women undergoing in vitro fertilization (IVF) and measurement of tissue factor concentrations via enzyme-linked immunosorbent assay (ELISA)
Follicular fluid was collected from 80 patients undergoing ovarian stimulation for IVF. Characteristics of patients based on the cause of infertility were presented in Supplemental Table 1. Forty-nine patients with infertility due to male (n = 22) or tubal factors (n = 27) served as controls. The male infertility patients were described as total motile count of < 10 million sperms/ml or normal morphology in < 4% of the sperm by strict criteria. Five women showed mild signs of OHSS after hCG administration during the IVF procedure. The causes of infertility among five OHSS patients include unknown factor (n = 3), oocyte donor and tubal factor. The inclusion criteria were age 21–42 years and normal uterine cavity on hysteroscopy. Patients who presented allergy to gonadotropins or other medications used in the treatment, or abusive use of any medications during the treatment were excluded. Our research was approved by the Institutional Review Board of Creation & Love Women’s Hospital (CLWH-IRB-2009-001).
Only clear follicular fluid, without blood or flushing medium contamination, was processed. After oocyte transfer, the follicular fluid (≈10 mL) aspirated from each patient was centrifuged for 10 min at 500×g. Supernatants of the follicular fluid samples were stored at − 80°С until the tissue factor concentrations were determined using an ELISA kit (EIAab Science Co., Wuhan, China). All the procedures were carried out according to the manufacturer’s instructions. Concentrations of tissue factor were detected in follicular fluids obtained from women with different infertility factors.
Statistical analyses were performed using the statistical software GraphPad Prism 5 (GraphPad Software, Inc. La Jolla, CA, USA). Data obtained from rat ovaries were presented as the means ± SEM. One way ANOVA, followed by Dunnett’s test, was used for comparisons among multiple groups. Comparisons between any two points were evaluated using Student’s two-tailed t-test. The levels of tissue factor in human follicular fluid were presented as the mean ± SD or median (range). Correlation analysis was performed using Spearman’s rho test. Pregnant and non-pregnant women were compared using the Kruskal-Wallis test or Mann–Whitney’s U-test. Fisher’s F-test was used to assess the relationship between two variables for parametric data. P < 0.05 was considered significant.
Ovarian expression of tissue factor and Tfpi during ovulation in vivo
To examine gonadotropin regulation, the total RNA extracted from the preovulatory follicles of ovaries at different time points after hCG treatment was analyzed using real–time RT-PCR. As shown in Fig. 2a, the levels of tissue factor mRNA reached a maximum at 6 h (56.9-fold vs. that at 0 h; P < 0.05) and slightly decreased at 12 h in the granulosa cells. The expression of tissue factor in the theca cells increased gradually until 12 h (7.9-fold vs. that at 0 h). Western blot analysis revealed that the tissue factor protein had a molecular weight of 47 kDa, probably indicating that the tissue factor protein lacked the cytoplasmic domain, identical to the full-length protein at the initiation of thrombin generation (Fig. 2b). The levels of tissue factor protein increased transiently, reaching a maximum at 9 h after hCG treatment (5.3-fold vs. that at 0 h; P < 0.05). Immunofluorescence analysis demonstrated that the tissue factor protein was found in both the granulosa and theca cells at 12 h after hCG treatment (Fig. 2c). Interestingly, hCG treatment for 12 h increased tissue factor expression in the cumulus cells (Fig. 2c, asterisk) as well as in oocytes (Fig. 2c, arrowhead). No specific signal was detected in ovarian sections that were treated with goat control antibodies (anti-IgG; data not shown).
Gonadotropin regulation of tissue factor pathway inhibitor (Tfpi) expression was also examined using real-time RT-PCR analysis. The levels of ovarian Tfpi-2 mRNA were stimulated, reaching a maximum at 6 h after hCG treatment (68.7-fold increases vs. 0 h) whereas the levels of Tfpi-1 mRNA gradually decreased until 12 h after hCG treatment (Fig. 3a). The Tfpi-1 gene was expressed in both the granulosa and theca cells, with a gradual decrease in expression after hCG treatment (Fig. 3b, left panel). However, although the granulosa cell expression of Tfpi-2 showed a transient stimulation at 6 h (18.8-fold vs. 0 h), the levels of Tfpi-2 in the thecal cells were greatly increased, reaching a maximum at 6 h after hCG treatment (236.8-fold vs. 0 h; P < 0.05) (Fig. 3b, right panel).
Regulation of tissue factor and Tfpi expression by ovulation-inhibiting agents in vivo
To study the effect of ovulation-inhibiting agents on the expression of hCG-regulated tissue factor, Tfpi-1, and Tfpi-2, progesterone receptor antagonist (RU486), cyclooxygenase inhibitor (indomethacin), lipoxygenase inhibitor (nordihydroguaiaretic acid, NDGA), or PPARγ antagonist (GW9662) was administered 30 min before hCG stimulation in eCG-primed immature rats. Quantitative analysis using real-time PCR revealed that, at 6 h, the hCG-induced mRNA levels of tissue factor were inhibited by RU486 (68.1% inhibition; P < 0.05) but not the other agents (Fig. 4). The mRNA levels Tfpi-1 were not affected by any inhibitor. Interestingly, injection with GW9662 significantly inhibited the hCG-induced Tfpi-2 mRNA levels (96% inhibition vs. hCG at 6 h).
Ovarian expression of tissue factor and Tfpi in the OHSS model in rats
Blood clotting is related to OHSS . Changes in the expression of tissue factor and TFPIs were therefore examined in a hormone-induced OHSS model in rats . To validate the induction of OHSS in rats, the indexes for the occurrence of OHSS were examined. Ovarian weight was increased after hCG administration for 48 h in ovulation-induced rats (Fig. 5a). Ovarian weight was markedly increased in OHSS-induced rats upon administration of 30 IU of hCG for 48 h compared with that in rats treated with saline for 48 h. The ovarian levels of vascular endothelial growth factor (Vegf) were increased in ovulation- and OHSS-induced rats treated with hCG and saline, respectively, for 48 h (Fig. 5b). The levels of Vegf mRNA were higher (P < 0.05) in OHSS-induced rats administered with hCG than in those administered with saline. The vascular permeability was also higher in OHSS-induced rats administered with hCG than in those administered with saline indicating the elevation of capillary permeability (Supplemental Fig. S1). These results indicated the successful induction of OHSS in rats.
Although the ovarian expression of tissue factor was not changed by hCG in the ovulation model, the mRNA levels of ovarian tissue factor were significantly lower in OHSS-induced rats injected with hCG than in those injected with saline (Fig. 6a), suggesting that tissue factor can be a potential biomarker of OHSS in humans. The levels of ovarian Tfpi-1 and Tfpi-2 remained unaltered upon hCG administration in ovulation- or OHSS-induced rats (Fig. 6b and c).
Detection of tissue factor in follicular fluid samples obtained from women undergoing in vitro fertilization (IVF)
As tissue factor expression was stimulated during ovulation and decreased in the OHSS rat model, the possibility of using tissue factor as a biomarker of female infertility was investigated by determining the amount of tissue factor in the follicular fluids of women undergoing IVF. No correlation was found between the tissue factor level and age of the women (Fig. 7a). Interestingly, the tissue factor levels in follicular fluids collected at oocyte retrieval were correlated with pregnant outcome. Infertile patients who became pregnant had a significant lower levels of tissue factor in follicular fluids at oocyte retrieval (447.6 ± 78.25 pg/mL) than those who did not become pregnant (547.2 ± 50.95 pg/mL) (Fig. 7b, P = 0.0301). Tissue factor levels were not different between OHSS (531.4 ± 59.38 pg/mL) and non-OHSS group (515.0 ± 45.49 pg/mL) (Fig. 7c). The correlation between tissue factor levels and the causes of infertility was also examined. Tissue factor levels were not different between control group (500.1 ± 52.59 pg/mL) and PCOS (580.0 ± 135.60 pg/mL) or endometriosis group (506.6 ± 114.40 pg/mL) (Fig. 7d).
Ovulation resembles the tissue remodeling process of blood coagulation. In this study, we report that tissue factor, an initiator of the extrinsic coagulation pathway, is induced during ovulation in rats. We also report that tissue factor expression is correlated with OHSS in rats and humans, which is characterized by an excessive response to ovulation-inducing hormones as well as massive hemoconcentration . The expression of TFPI-1 was decreased by hCG, suggesting the potentiation of the tissue factor activity. Furthermore, the hCG-mediated stimulation of tissue factor expression in the granulosa cells of the preovulatory follicles required progesterone receptor activation. As the progesterone receptor is the key transcription factor inducing follicular rupture , the tissue factor gene, as a downstream gene for the progesterone receptor, may be involved in follicular rupture via formation of a fibrin clot after the release of fertilizable oocyte . In contrast to TFPI-1, TFPI-2 expression was stimulated during ovulation. The increased expression of TFPI-2 mediated by hCG, observed in human and rat preovulatory follicles, may play a role in the tissue remodeling process that occurs during follicular rupture .
It is likely that tissue factor produced by the granulosa cells is the major coagulation factor during follicular rupture. The ovulatory surge of LH progressively triggers an elevation in ovarian blood flow and vascular permeability followed by ovarian hyperemia, edema, and extravasation of blood in preovulatory follicles, ultimately resulting in the rupture of the follicular wall . Tissue factor was produced 9–12 h after LH/hCG administration, indicating that tissue damage during follicular rupture may trigger the expression of tissue factor. Follicular rupture occurs about 12 h after the LH surge in rodents. Tissue factor may play a role in repairing the damaged follicular wall via formation of a fibrin clot after the release of the oocyte into the oviduct. The present observation, in which the tissue factor gene is a downstream gene for the progesterone receptor, supports the hypothesis that tissue factor may be the major ovarian coagulation factor during periovulatory tissue remodeling. Studies on the targeted deletion of the progesterone receptor gene in mice indicate that the progesterone receptor is specifically and absolutely required for the rupture of the preovulatory follicle and oocyte release . Tissue factor was also expressed in the cumulus cells and oocytes. The fact that the presence of blood clots in the human cumulus-oocyte complex was associated with reduced oocyte quality and blastocyst formation  indicates that tissue factor expressed in the cumulus cells and oocytes may be required for post-fertilization development.
Tissue factor may stimulate angiogenesis in the corpus luteum by inducing VEGF expression. The development of the corpus luteum is accompanied by rapid angiogenesis with the comparable rates of vascular formation in the growing tumors . VEGF is the most remarkable regulator of angiogenesis in the corpus luteum [32, 33]. Of note, tissue factor, apart from its essential role in the coagulation process, exerts a role in angiogenesis in the tumor , possibly via release of VEGF . Because the corpus luteum secrets progesterone to maintain intrauterine pregnancy , the present observation of correlation between levels of tissue factor and pregnancy may reflect a role of tissue factor in the function of corpus luteum by stimulating angiogenesis via VEGF.
Tissue factor could be used as a marker for OHSS. Several mediators involved in ovulation have been proposed as factors leading to OHSS such as estrogens, histamine, prostaglandins, cytokines  and the renin-angiotensin . Vascular endothelial growth factor (VEGF) has also been implicated as a prime causative factor of OHSS progression. Levels of VEGF in serum and follicular fluid may predict the occurrence, severity, and progression of OHSS [23, 38]. In our study, an increase in the ovarian expression of Vegf was observed in the OHSS-induced rats. Using this OHSS model, a decrease in the ovarian expression of tissue factor was observed in OHSS-induced rats, suggesting that tissue factor may be one of the indicators for the occurrence of OHSS. Changes in the hemostatic system have been reported to be responsible for an increased thrombotic risk in patients with OHSS .
Although the tissue factor levels were correlated with OHSS in rats, we could not observe the correlation between tissue factor levels in follicular fluid and OHSS patients undergoing in vitro fertilization (IVF). However, an increase in tissue factor levels in the plasma has been reported in patients with severe OHSS . These different outcomes may be attributed to the difference in samples, follicular fluid vs. plasma. The concentration of the tissue factor protein in human follicular fluid has been estimated to be 3.7-fold higher than that in the plasma . In mammalian ovarian follicular fluid, only the tissue factor-dependent extrinsic pathway is present ; most tissue factors in follicular fluid must be generated locally by the granulosa cells of preovulatory follicles . Additionally, it must be noted that the samples of human follicular fluid were obtained from women undergoing massive hCG stimulation during IVF. Therefore, depending on the measurement of tissue factor levels in plasma or follicular fluid, different outcomes between OHSS and non-OHSS patients might be produced. Decreased TFPI-1 levels have been reported in the plasma, but not the follicular fluid, of patients with OHSS . Further studies are needed to confirm the possible use of tissue factor as a biomarker for OHSS using a large number of samples.
The lower levels of tissue factor in the follicular fluid collected at oocyte retrieval was observed in infertile women who became pregnant compared with those who did not become pregnant, suggesting the possible use of tissue factor as a pregnancy index. Pregnancy itself leads to a hypercoagulable state secondary to increased concentrations of coagulant factors . Indeed, the expression of coagulation factors, including antithrombin and fibrinogen, is significantly decreased in the chorionic villi of patients with recurrent spontaneous abortion . It is thus likely that coagulation factors play a role in maintaining a normal pregnancy. Tissue factor expression in neutrophils contributes to pregnancy loss induced by antiphospholipid antibodies in mice . However, concentrations of tissue factor or TFPI-1 in the plasma of patients with OHSS are not correlated with the outcomes of pregnancy . The present hypothesis of the predictive role of tissue factor as a pregnancy index should be assessed by ad hoc studies.
In contrast to the expression of tissue factor, TFPI-1 expression decreased continuously after LH/hCG administration, providing an environment for higher activity of tissue factor. The presence of TFPI-1 has been reported in human granulosa cells and preovulatory follicular fluid . In contrast, TFPI-2 expression was markedly increased upon LH/hCG administration. Unlike TFPI-1, which inhibits the activity of tissue factor, the true function of TFPI-2 has not yet been clearly elucidated. TFPI-2 is involved in blood coagulation due to its ability to inhibit the formation of the tissue factor-factor VIIa complex [40, 41]. TFPI-2 also plays a role in remodeling the extracellular matrix by virtue of being a serine protease inhibitor . TFPI-2 inhibits the protease activity of plasmin  and metalloproteinases . Indeed, it has been demonstrated that TFPI-2 regulates ovulatory proteolysis by manipulating the activity of plasmin during the periovulatory period . Therefore, TFPI-2 could have a role in modulating the remodeling of the extracellular matrix rather than modulating blood coagulation during the periovulatory period. As the PPARγ plays a role in tissue remodeling during ovulation , our finding that TFPI-2 expression was suppressed by a PPARγ antagonist supports this hypothesis.
In summary, we have shown that tissue factor and TFPI-2 are induced in preovulatory follicles during the ovulatory process in rat ovaries and provide compelling evidence that tissue factor system can regulate the ovulatory process via progesterone receptor and PPARγ pathways. In addition, the levels of tissue factor are higher in ovaries of OHSS-induced rats supporting the hypothesis that tissue factor can be used as a biomarker for OHSS. The concentration of tissue factor in the follicular fluids was correlated with pregnancy of patients, but not with OHSS, undergoing IVF. Further investigation is needed on a large number of patients with infertility to determine the possible role of tissue factor as a marker for OHSS and pregnancy.
Availability of data and materials
Equine chorionic gonadotropin
ELISA, enzyme-linked immunosorbent assay; human chorionic gonadotropin
in vitro fertilization
ovarian hyperstimulation syndrome
real-time quantitative polymerase chain reaction
tissue factor pathway inhibitor
vascular endothelial growth factor
Espey LL. Ovulation as an inflammatory reaction--a hypothesis. Biol Reprod. 1980;22(1):73–106.
Oakley OR, Kim H, El-Amouri I, Lin PC, Cho J, Bani-Ahmad M, Ko C. Periovulatory leukocyte infiltration in the rat ovary. Endocrinology. 2010;151(9):4551–9.
Park JI, Jeon HJ, Jung NK, Jang YJ, Kim JS, Seo YW, Jeong M, Chae HZ, Chun SY. Periovulatory expression of hydrogen peroxide-induced sulfiredoxin and peroxiredoxin 2 in the rat ovary. Gonadotropin regulation and potential modification. Endocrinology. 2012;153(11):5512–21.
Parrott JA, Whaley PD, Skinner MK. Extrahepatic expression of fibrinogen by granulosa cells. Potential role in ovulation. Endocrinology. 1993;133(4):1645–9.
Cheng Y, Kawamura K, Deguchi M, Takae S, Mulders SM, Hsueh AJ. Intraovarian thrombin and activated protein C signaling system regulates steroidogenesis during the periovulatory period. Mol Endocrinol. 2012;26(2):331–40.
Roach LE, Petrik JJ, Plante L, LaMarre J, Gentry PA. Thrombin generation and presence of thrombin receptor in ovarian follicles. Biol Reprod. 2002;66(5):1350–8.
Hirota Y, Tachibana O, Uchiyama N, Hayashi Y, Nakada M, Kita D, Watanabe T, Higashi R, Hamada J. Gonadotropin-releasing hormone (GnRH) and its receptor in human meningiomas. Clin Neurol Neurosurg. 2009;111(2):127–33.
Gentry PA, Plante L, Schroeder MO, LaMarre J, Young JE, Dodds WG. Human ovarian follicular fluid has functional systems for the generation and modulation of thrombin. Fertil Steril. 2000;73(4):848–54.
Kim YS, Kim MS, Lee SH, Choi BC, Lim JM, Cha KY, Baek KH. Proteomic analysis of recurrent spontaneous abortion: identification of an inadequately expressed set of proteins in human follicular fluid. Proteomics. 2006;6(11):3445–54.
Cimmino G, Cirillo P. Tissue factor: newer concepts in thrombosis and its role beyond thrombosis and hemostasis. Cardiovasc Diagn Ther. 2018;8(5):581–93.
Price GC, Thompson SA, Kam PC. Tissue factor and tissue factor pathway inhibitor. Anaesthesia. 2004;59(2004):483–92.
Bungay SD, Gentry PA, Gentry RD. Modelling thrombin generation in human ovarian follicular fluid. Bull Math Biol. 2006;68(8):2283–302.
Puttabyatappa M, Al-Alem LF, Zakerkish F, Rosewell KL, Brannstrom M, Curry TE Jr. Induction of tissue factor pathway inhibitor 2 by hCG regulates Periovulatory gene expression and plasmin activity. Endocrinology. 2017;158(1):109–20.
Kwak-Kim J, Yang KM, Gilman-Sachs A. Recurrent pregnancy loss: a disease of inflammation and coagulation. J Obstet Gynaecol Res. 2009;35(4):609–22.
Ebner T, Moser M, Shebl O, Sommergruber M, Yaman C, Tews G. Blood clots in the cumulus-oocyte complex predict poor oocyte quality and post-fertilization development. Reprod BioMed Online. 2008;16(6):801–7.
Girardi G, Mackman N. Tissue factor in antiphospholipid antibody-induced pregnancy loss: a pro-inflammatory molecule. Lupus. 2008;17(10):931–6.
Carvalho LML, Ferreira CN, Candido AL, Reis FM, Soter MO, Sales MF, Silva IFO, Nunes FFC, Gomes KB. Metformin reduces total microparticles and microparticles-expressing tissue factor in women with polycystic ovary syndrome. Arch Gynecol Obstet. 2017;296(4):617–21.
Gonzalez F, Kirwan JP, Rote NS, Minium J. Elevated circulating levels of tissue factor in polycystic ovary syndrome. Clin Appl Thromb Hemost. 2013;19(3):66–72.
Thyzel E, Siegling S, Tinneberg HR, Gotting C, Kleesiek K. Age dependent assessment of TFPI levels in follicular fluid of women undergoing IVF. Clin Chim Acta. 2005;361(1–2):176–81.
Delvigne A, Rozenberg S. Epidemiology and prevention of ovarian hyperstimulation syndrome (OHSS). A review. Hum Reprod Update. 2002;8(6):559–77.
Ishikawa K, Ohba T, Tanaka N, Iqbal M, Okamura Y, Okamura H. Organ-specific production control of vascular endothelial growth factor in ovarian hyperstimulation syndrome-model rats. Endocr J. 2003;50(5):515–25.
Ohba T, Ujioka T, Ishikawa K, Tanaka N, Okamura H. Ovarian hyperstimulation syndrome-model rats; the manifestation and clinical implication. Mol Cell Endocrinol. 2003;202(1–2):47–52.
Gao F, Vasquez SX, Su F, Roberts S, Shah N, Grijalva V, Imaizumi S, Chattopadhyay A, Ganapathy E, Meriwether D, Johnston B, Anantharamaiah GM, Navab M, Fogelman AM, Reddy ST, Farias-Eisner R. L-5F, an apolipoprotein A-I mimetic, inhibits tumor angiogenesis by suppressing VEGF/basic FGF signaling pathways. Integr Biol (Camb). 2011;3(4):479–89.
Shen BQ, Lee DY, Cortopassi KM, Damico LA, Zioncheck TF. Vascular endothelial growth factor KDR receptor signaling potentiates tumor necrosis factor-induced tissue factor expression in endothelial cells. J Biol Chem. 2001;276(7):5281–6.
Balasch J, Reverter JC, Fabregues F, Tassies D, Ordinas A, Vanrell JA. Increased induced monocyte tissue factor expression by plasma from patients with severe ovarian hyperstimulation syndrome. Fertil Steril. 1996;66(4):608–13.
Rogolino A, Coccia ME, Fedi S, Gori AM, Cellai AP, Scarselli GF, Prisco D, Abbate R. Hypercoagulability, high tissue factor and low tissue factor pathway inhibitor levels in severe ovarian hyperstimulation syndrome: possible association with clinical outcome. Blood Coagul Fibrinolysis. 2003;14(3):277–82.
Elchalal U, Schenker JG. The pathophysiology of ovarian hyperstimulation syndrome--views and ideas. Hum Reprod. 1997;12(6):1129–37.
Robker RL, Hennebold JD, Russell DL. Coordination of ovulation and oocyte maturation: a good egg at the right time. Endocrinology. 2018;159(9):3209–18.
Lydon JP, DeMayo FJ, Funk CR, Mani SK, Hughes AR, Montgomery CA Jr, Shyamala G, Conneely OM, O'Malley BW. Mice lacking progesterone receptor exhibit pleiotropic reproductive abnormalities. Genes Dev. 1995;9(18):2266–78.
Parr EL. Absence of neutral proteinase activity in rat ovarian follicle walls at ovulation. Biol Reprod. 1974;11(5):509–12.
Robker RL, Akison LK, Russell DL. Control of oocyte release by progesterone receptor-regulated gene expression. Nucl Recept Signal. 2009;7:e012.
Lu E, Li C, Wang J, Zhang C. Inflammation and angiogenesis in the corpus luteum. J Obstet Gynaecol Res. 2019;45(10):1967–74.
Berisha B, Schams D, Rodler D, Pfaffl MW. Angiogenesis in the ovary - the Most important regulatory event for follicle and corpus luteum development and function in cow - an overview. Anat Histol Embryol. 2016;45(2):124–30.
Bluff JE, Brown NJ, Reed MW, Staton CA. Tissue factor, angiogenesis and tumour progression. Breast Cancer Res. 2008;10(2):204.
Zhang Y, Deng Y, Luther T, Müller M, Ziegler R, Waldherr R, Stern DM, Nawroth PP. Tissue factor controls the balance of angiogenic and antiangiogenic properties of tumor cells in mice. J Clin Invest. 1994;94(3):1320–7.
Miura R, Haneda S, Matsui M. Ovulation of the preovulatory follicle originating from the first-wave dominant follicle leads to formation of an active corpus luteum. J Reprod Dev. 2015;61(4):317–23.
Kwik M, Maxwell E. Pathophysiology, treatment and prevention of ovarian hyperstimulation syndrome. Curr Opin Obstet Gynecol. 2016;28(4):236–41.
Naredi N, Talwar P, Sandeep K. VEGF antagonist for the prevention of ovarian hyperstimulation syndrome: current status. Med J Armed Forces India. 2014;70(1):58–63.
Shimada H, Kasakura S, Shiotani M, Nakamura K, Ikeuchi M, Hoshino T, Komatsu T, Ihara Y, Sohma M, Maeda Y, Matsuura R, Nakamura S, Hine C, Ohkura N, Kato H. Hypocoagulable state of human preovulatory ovarian follicular fluid: role of sulfated proteoglycan and tissue factor pathway inhibitor in the fluid. Biol Reprod. 2001;64(6):1739–45.
Petersen LC, Sprecher CA, Foster DC, Blumberg H, Hamamoto T, Kisiel W. Inhibitory properties of a novel human Kunitz-type protease inhibitor homologous to tissue factor pathway inhibitor. Biochemistry. 1996;35(1):266–72.
Iino M, Foster DC, Kisiel W. Quantification and characterization of human endothelial cell-derived tissue factor pathway inhibitor-2. Arterioscler Thromb Vasc Biol. 1998;18(1):40–6.
Chand HS, Foster DC, Kisiel W. Structure, function and biology of tissue factor pathway inhibitor-2. Thromb Haemost. 2005;94(6):1122–30.
Rao CN, Cook B, Liu Y, Chilukuri K, Stack MS, Foster DC, Kisiel W, Woodley DT. HT-1080 fibrosarcoma cell matrix degradation and invasion are inhibited by the matrix-associated serine protease inhibitor TFPI-2/33 kDa MSPI. Int J Cancer. 1998;76(5):749–56.
Herman MP, Sukhova GK, Kisiel W, Foster D, Kehry MR, Libby P, Schonbeck U. Tissue factor pathway inhibitor-2 is a novel inhibitor of matrix metalloproteinases with implications for atherosclerosis. J Clin Invest. 2001;107(9):1117–26.
Komar CM. Peroxisome proliferator-activated receptors (PPARs) and ovarian function--implications for regulating steroidogenesis, differentiation, and tissue remodeling. Reprod Biol Endocrinol. 2005;3:41.
This study was supported by a grant from the Basic Science Research Program through the National Research Foundation of Korea (NRF), funded by the Ministry of Education, Science, and Technology, Republic of Korea (Grant 2010–0023342 to M.-K.C.), and the National Research Foundation (NRF) of Korea grant funded by the Korea government (NRF-2015R1A2A2A01006519 to S.Y.C.).
Ethics approval and consent to participate
This study was approved by the Institutional Animal Care and Use Committee at Chonnam National University. Informed consent was obtained from each patient at Center for Recurrent Miscarriage and Infertility. Creation and Love Women’s Hospital, Gwangju 61917, Republic of Korea.
Consent for publication
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Cite this article
Jang, Y.J., Kim, H.K., Choi, B.C. et al. Expression of tissue factor and tissue factor pathway inhibitors during ovulation in rats: a relevance to the ovarian hyperstimulation syndrome. Reprod Biol Endocrinol 19, 52 (2021). https://doi.org/10.1186/s12958-021-00708-1
- Tissue factor
- Tissue factor pathway inhibitor
- Ovarian hyperstimulation syndrome