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Article

Hypothyroidism Affects Uterine Function via the Modulation of Prostaglandin Signaling

by
Ilona Kowalczyk-Zieba
1,*,
Joanna Staszkiewicz-Chodor
1,
Dorota Boruszewska
1,
Krzysztof Lukaszuk
2,3,4,
Joanna Jaworska
1 and
Izabela Woclawek-Potocka
1
1
Department of Gamete and Embryo Biology, Institute of Animal Reproduction and Food Research, Polish Academy of Sciences, 10-747 Olsztyn, Poland
2
Department of Obstetrics and Gynecological Nursing, Faculty of Health Sciences, Medical University of Gdansk, 80-210 Gdansk, Poland
3
Department of Obstetrics and Gynecology, The Medical Center of Postgraduate Education, 02-091 Warsaw, Poland
4
INVICTA Fertility and Reproductive Center, 80-850 Gdansk, Poland
*
Author to whom correspondence should be addressed.
Animals 2021, 11(9), 2636; https://doi.org/10.3390/ani11092636
Submission received: 9 July 2021 / Revised: 27 August 2021 / Accepted: 2 September 2021 / Published: 8 September 2021
(This article belongs to the Section Animal Reproduction)
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Abstract

:

Simple Summary

A article proved that, in rats with PTU-induced hypothyroidism, the E2 level as well as the expression of the uterine-receptivity factors homeobox A10 and osteopontin was decreased. Additionally, we observed changes in the expression of PGE2, PGF2α, and PGI2 signaling pathway elements, and changes in the concentrations of those prostaglandins in uterine tissue. The results suggest that hypothyroidism may interfere with the prostaglandin signaling pathway, which may further result in a reduction in uterine receptivity.

Abstract

Thyroid hormones control the functions of almost all body systems. Reproductive dysfunctions, such as abnormal sexual development, infertility, or irregularities in the reproductive cycle, might be associated with thyroid disorders. Uterine receptivity is the period when the uterus is receptive to the implantation of an embryo. During the receptivity period (implantation window), a newly formed blastocyst is incorporated into the uterine epithelium. Prostaglandins are well-known primary mediators of pathological conditions such as inflammation and cancer but are also essential for the physiology of female reproduction. The aim of this study was to evaluate the possible relationship between hypothyroidism and changes in the prostaglandin signaling pathways in the uterus and in the process of uterine receptivity in a rat model. The results show that hypothyroidism impaired uterine receptivity by decreasing the level of E2 as well as decreasing the expression of the uterine-receptivity factors homeobox A10 and osteopontin. Moreover, hypothyroidism caused changes in the expression of elements of the prostaglandin E2, F2α, and I2 signaling pathways and changed the levels of those prostaglandins in the uterine tissue. The results suggest that the mechanisms by which hypothyroidism affects female reproductive abnormalities might involve the prostaglandin signaling pathway, resulting in a subsequent reduction in uterine receptivity.

1. Introduction

Thyroid hormones control the functions of almost all the body’s systems. They stimulate growth and development, affect metabolism, and are essential for the proper function of the central nervous system, cardiovascular system, and immune system, as well as influencing the reproductive system [1,2,3,4,5]. Thyroid hormones regulate the secretion of the main reproductive hormones—estradiol (E2) and progesterone (P4). These hormones are necessary for the maturation and development of the oocytes, prepare the endometrium for embryo implantation, and are important in the establishment and maintenance of early pregnancy. It has been shown that, in hypothyroidism, the levels of both E2 and P4 are decreased [5]. Reproductive dysfunction, including abnormal sexual development, infertility, or irregularities in the reproductive cycle, is associated with thyroid disorders [6,7]. It is known that induced hypothyroidism in rats causes a reduction in the absolute volume of the endometrium and a decrease in its muscle layer [7,8]. In humans, hypothyroidism can disrupt the menstrual cycle and ovulation [5,9]. It can also cause problems with fertilization and implantation, miscarriage, and late-pregnancy complications [10,11].
Uterine receptivity is the period when the uterus is receptive to an implanting embryo [12,13]. In rats, the receptivity period occurs between Days 4 and 5 of the estrous cycle [13,14], when the newly formed blastocysts incorporate into the uterine epithelium [13,15]. Estrogen and progesterone are hormones essential for implantation, which is mediated by an increase in the expression of the receptors for those hormones in the endometrium [13,16]. Several molecules are reported to be expressed in the endometrium exclusively during the uterine receptivity period and, therefore, could serve as markers of uterine receptivity [13,17]. Homeobox A10 (HOXA10) is expressed at high levels in adult human and mouse uteruses. Additionally, the significant increase in HOXA10 during the estrous cycle and at the time of implantation [18,19,20] suggests it plays an important role in cyclic endometrial development and uterine receptivity [20]. Other molecules considered as uterine-receptivity markers are osteopontin (OPN) and its receptor, β3 integrin (ITG3B). Both have been found to be coordinately expressed in the human endometrium across the menstrual cycle in fertile women. These glycoproteins are maximally expressed during the implantation window [21,22].
Prostaglandins (PGs) are biologically active lipids. They are well-known primary mediators of pathological conditions such as inflammation and cancer, but are also essential for the physiology of female reproduction [23]. PGs belong to the group of prostanoids that are generated from arachidonic acid (AA). This acid is converted to PGH2 with the participation of prostaglandin endoperoxide synthases (PTGSs). There are two main isoforms of prostaglandin endoperoxide synthases, PTGS1 and PTGS2 [24,25]. PGE2, PGF2α, and PGI2 are synthesized from PGH2 by PGE synthases (PTGES-1, PTGES-2, and PTGES-3), PGF synthase (PGFS), and PGI synthase (PGIS) [25,26]. Prostaglandins act by interacting with specific G-protein-coupled receptors [27,28,29]. PGE2 transduces signals through four types of receptors—PTGER1, 2, 3, and 4 (EP1, 2, 3, and 4)—while PGF2α acts through PTGFR (FP) [29,30,31]. PGI2 acts through PTGIR (IP) [25,32], but it can also act via the peroxisome-proliferator-activated receptors PPARα, PPARγ, and PPARδ, which are members of the nuclear-hormone-receptor superfamily [25,33].
PGE2 and PGF2α are very important factors in female reproduction. They are involved in blastocyst spacing, implantation, and decidualization, as well as in uterine contraction [29,31,34]. EP1, EP3, and FP affect smooth muscle contraction, while EP2 and EP4 affect the relaxation of smooth muscles [29,32,35]. The expression of EPs and FP in the human uterus varies during the menstrual cycle. EP1 dominates in the early-secretory phase, while EP2, EP3, and EP4 dominate in the mid-secretory phase, and FP, in the proliferative phase [29,36]. In pigs, the inhibition of the synthesis of PGs by blocking the activity of PTGS2 causes pregnancy loss [25,37]. An appropriate ratio between the luteoprotective PGE2 and the luteolytic PGF2α is very important for the successful establishment of pregnancy in pigs [25,38]. PGI2 is the most abundant prostanoid produced by the endometrium of mice and cattle. In mice, prostacyclin is critical for endometrial decidualization and embryo implantation. In rodents, cattle, and sheep, it has been demonstrated that signaling involving PGI2 and its receptor is an important component of the embryo–uterus interactions that are essential for successful implantation. PGI2 and PTGIR signaling are very important components of embryo–uterus interactions that are essential for successful implantation [25,39,40,41,42,43]. Furthermore, PGI2 increases embryonic cell proliferation and reduces apoptosis [25,44,45]. It also enhances the embryo hatching and live birth potential of mouse embryos [25,46,47].
The role of prostaglandins in embryo implantation is indisputably essential [48,49]. Poor endometrial receptivity during embryo implantation has been linked to reduced prostaglandin synthesis in the human endometrium [50]. On the other hand, it is also known that hypothyroidism can cause problems with fertilization and implantation, miscarriages, and late-pregnancy complications [10,11]. The aim of this study was to evaluate the possible relationship between PTU-induced hypothyroidism and changes in prostaglandin signaling pathways in the uterus and in the process of uterine receptivity in a rat model.

2. Materials and Methods

2.1. Animals

All the experimental procedures were approved by the Local Animal Care and Use Committee in Olsztyn, Poland (Agreement No. 40/2015/DTN).
Female Wistar rats aged 8–10 weeks were kept in the Animal Laboratory of the Institute of Animal Reproduction and Food Research of the Polish Academy of Sciences in Olsztyn. The rats were conventionally housed. They were divided into two groups: the control group (n = 20) and the experimental group with induced hypothyroidism (n = 20). The control group was fed ad libitum. Over the 90 days, the study group, besides the normal diet, also received 0.05% 6-propyl-2-thiouracil solution (PTU) (#46698-250MG, Sigma-Aldrich, Munich, Germany) by oral administration to induce hypothyroidism. The duration of the PTU treatment was selected based on a study by Jena and Bhanja [51]. Then, the animals were sacrificed. The blood serum and uterus were collected and immediately frozen. The tissues were stored at −80 °C until mRNA and protein extraction.

2.2. Confirmation of Hypothyroidism

To confirm hypothyroidism, the thyroid hormone index (T4, T3, and thyrotropin (TSH)) for the blood serum samples was obtained. Serum T3 (#EKU04275), T4 (#EKU04274), and TSH (#EKC39776) measurements were performed using ELISA kits according to the manufacturer’s instructions (Biomatik, ON, Canada).

2.3. mRNA Isolation and Real-Time PCR

mRNA was isolated using the Total RNA Mini Plus Kit (#036-100; A&A Biotechnology; Gdansk, Poland). The quality and quantity of the mRNA were measured using the NanoDrop 100 (Thermo Fisher Scientific; Waltham, MA, USA). Reverse transcription was performed using the Maxima First Strand cDNA Synthesis Kit for RT-qPCR (#K1642; Thermo Fisher Scientific; Waltham, MA, USA). Real-time PCR was performed with the ABI Prism 7900 (Applied Biosystems, Life Technologies, Waltham, MA, USA) sequence detection system using the Maxima SYBR Green/ROX qPCR Master Mix (#K0223; Thermo Fisher Scientific, Waltham, MA, USA). PCRs were performed in 384-well plates. The results for the mRNA transcription were normalized to β-actin (ACTB, internal control). The mRNA levels are shown in arbitrary units. The primers were designed using Primer3web version 4.0.0 (http://primer3.ut.ee; accessed on 23 April 2019), and their sequences are shown in Table 1. For the relative quantification of the mRNA levels, the Miner software was used (http://www.miner.ewindup.info; accessed on 23 April 2019).

2.4. Protein Isolation and Western Blotting

Total protein (n = 7) was isolated using the Radio Immuno Precipitation Assay Buffer (150 mM NaCl, 50 mM Tris, 0.1% SDS, 1% Triton × 100, 0.5% sodium deoxycholate, and 5 mM EDTA; pH = 7.2). The protein concentration was measured using the Micro BCA method. The levels of the proteins involved in prostaglandin signaling pathways—PTGS2, PTGES-2, PTGES-3, PTGER1, PTGER2, PTGER3, PTGER4, PGFS, PTGFR, PTGIS, and PTGIR—and the uterine-receptivity proteins HOXA10 and OPN were measured by Western blotting using the semi-dry method of transfer (Trans-Blot SD Cell, Bio-Rad; California, USA) onto polyvinylidene difluoride membranes (Immobilon-P Transfer Membrane; #IPVH00010, Millipore; Burlington, MA, USA). The primary antibodies used are shown in Table 2. β-actin antibody (#A2228-100UL, Sigma-Aldrich; Munich, Germany), diluted 1:4000, was used as the internal control for protein loading. The secondary antibodies used were goat anti-mouse IgG (whole molecule)–alkaline phosphatase (#A3562, Sigma-Aldrich; Munich, Germany), diluted 1:30,000, and goat anti-rabbit IgG–AP (#sc-2007, Santa Cruz, TX, USA), diluted 1:5000. The immune complexes were visualized using the alkaline phosphatase visualization procedure. The blots were scanned for densitometric analyses (Versa Doc Imagine System), and the specific bands were quantified using the Image Lab Software Version 5.2 (Bio-Rad Laboratories, CA, USA).

2.5. The Extraction of Prostaglandins and the Measurement of Their Concentrations in the Uterine Tissue

PGE2, PGF2α, and PGI2 were extracted from the uterine tissue using diethyl ether (#384210114, POCH, Gliwice, Poland). The concentrations of PGE2, PGF2α, and PGI2 were measured using the PGE2 high-sensitivity ELISA kit (#ADI-931-069; ENZO Life Sciences Inc., New York, NY, USA), the PGF2α high-sensitivity ELISA kit ((#ADI-931-069; ENZO Life Sciences Inc., New York, NY, USA), and the urinary prostacyclin ELISA kit (#ADI-901-025, ENZO Life Sciences Inc., New York, NY, USA), respectively.

2.6. Statistical Analyses

Statistical analyses were conducted using GraphPad Prism 7 (GraphPad Software, Inc., CA, USA). All the data are shown as the mean ± SEM, and differences were considered to be significantly different at a 95% confidence level (p < 0.05). Analyses were performed using Student’s t-tests.

3. Results

3.1. The Levels of Thyroid Hormones in the Blood Serum Samples

Figure 1 shows the T3, T4, and TSH levels in the blood serum samples in the control group and the experimental group with PTU-induced hypothyroidism. The levels of T3 and T4 were significantly decreased (p < 0.05), whereas the level of TSH was significantly increased (p < 0.05) in the blood serum samples from the experimental group in comparison to the control group.

3.2. Uterine Receptivity

Figure 2 shows the E2 and P4 levels in the blood serum samples in the control group and the experimental group with PTU-induced hypothyroidism. The level of E2 was significantly decreased (p < 0.05), whereas that of P4 was not changed (p > 0.05) in the blood serum samples from the experimental group in comparison to the control group.
Figure 3 shows mRNA and protein expression patterns of the uterine-receptivity factors osteopontin (OPN/OPN) and homeobox A10 (HOXA10/HOXA10). In both cases, the mRNA and protein expression levels were significantly lower in the group of rats with hypothyroidism than the control group (p < 0.05).

3.3. Prostaglandin Signaling in the Uterine Tissue

Figure 4 shows the mRNA and protein expression patterns of prostaglandin endoperoxide synthase 2 PTGS2/PTGS2 (COX-2). The mRNA level of PTGS2 was significantly higher in the group with hypothyroidism than the control group, while the protein level of PTGS2 was significantly lower in the group with hypothyroidism. Figure 5 shows the mRNA and protein expression patterns of PGE2 synthases. The mRNA and protein levels of PTGES-2/PTGES-2 were significantly higher in the experimental group with induced hypothyroidism than the control group (p < 0.05). There was significantly higher PTGES-3 mRNA expression in the group of animals with induced hypothyroidism (p < 0.05), while its protein expression was maintained at the same level in both groups. Figure 6 shows the mRNA and protein expression patterns of the PGE2 receptors. There was no significant difference in the mRNA expression of PTGER1 between the groups, whereas the expression of the PTGER1 protein was significantly lower in the experimental group with induced hypothyroidism than the control group (p < 0.05). The mRNA and protein expression levels of PTGER2/PTGER2 and PTGER3/PTGER3 show similar patterns. The expression levels were significantly lower in the group of animals with hypothyroidism than the control group of rats (p < 0.05). The mRNA and protein expression levels of PTGER4/PTGER4 were significantly higher in the experimental group in comparison to the control group of rats (p < 0.05). Figure 7 shows the mRNA and protein expression patterns of PGF2α synthase PGFS/PGFS and the receptor for PGF2α (PTGFR/PTGFR). The PGFS/PGFS expression pattern was similar for both mRNA and protein. It was significantly lower in the group of animals with hypothyroidism than the control group (p < 0.05). The mRNA and protein expression patterns of the PGF2α receptor PGFR/PGFR were opposite. The mRNA level was significantly higher, while the protein level was significantly lower, in the group of animals with hypothyroidism than the control group (p < 0.05). Figure 8 shows the mRNA and protein expression patterns of prostacyclin synthase PTGIS/PTGIS and the prostacyclin receptor PTGIR/PTGIR. The mRNA level of PTGIS was significantly higher in the group of rats with induced hypothyroidism than the control group of animals, while there was no difference in the protein level of PTGIS between the groups. In the case of the prostacyclin receptor, the mRNA level of PTGIR was significantly higher in the experimental group of animals than the control group, whereas the protein level of PTGIR was significantly lower in the group of rats with hypothyroidism than the control group (p < 0.05).

3.4. The Concentrations of Prostaglandins in the Uterine Tissue

Figure 9 shows the concentrations of PGs in the uterine tissue. The concentrations of PGE2, PGF2α, and PGI2 in the uterine tissue were significantly lower in the experimental group of animals with induced hypothyroidism than the control group of animals (p < 0.05).

4. Discussion

Our present study provides a new understanding of the possible relationship between thyroid hormones and uterine receptivity, as well as prostaglandin signaling pathways in the rat uterus. To the best of our knowledge, this is the first report to investigate the effect of PTU-induced hypothyroidism on uterine receptivity and the uterine synthesis of prostaglandins in rats.
Hypothyroidism is a disease characterized by a defect in the production of thyroid hormones due to the insufficient stimulation by TSH of normal thyroid gland function. This condition is the consequence of an anatomic or functional disorder of the pituitary gland or the hypothalamus, resulting in variable alterations of TSH secretion [52]. Other causes include a congenital absence of the thyroid, radioiodine therapy for hyperthyroidism, surgical thyroidectomy, various drugs that affect thyroid function or cause thyroid inflammation, and a variety of other rarer causes [53]. Congenital hypothyroidism occurs in ~1/4000 infants [54]. The lifetime risk of overt hypothyroidism is around 5%, and this disease is usually preceded by subclinical hypothyroidism, which has an even higher prevalence (estimated to be up to 9%) [52].
It is known from the literature that thyroid hormones affect reproductive capacity and, in particular, play an important role during implantation and the early stages of embryo development. Successful implantation is the result of reciprocal interactions between the implantation-competent blastocyst and the receptive uterus [55]. Thus, thyroid hormones may also influence angiogenesis and immune function in the uterus during implantation. Angiogenesis is crucial for successful implantation, decidualization, and placentation. In the case of immune function, natural killer (NK) cells have emerged as crucial modulators of implantation and placental angiogenesis. It is known that NK cell concentrations are higher in patients with thyroid autoimmunity and recurrent spontaneous abortion or unexplained infertility. This suggests their involvement in the decrease in uterine receptivity and the increase in pregnancy loss. Thyroid hormones have been reported to significantly influence the concentrations of the female reproductive hormones estradiol (E2) and progesterone (P4) [5,11,56]. In the current study, we observed that the administration of PTU in the drinking water decreased the circulating E2 level compared to control. We did not observe any effect on the P4 level. Our results are partially consistent with the results of Kong et al. [5] and Tohei [57], who found that, in rats with hypothyroidism, the levels of both E2 and P4 were decreased. However, Hapon et al. [58] found significantly higher luteal P4 content on Day 21 of pregnancy in rats with hypothyroidism compared to control, suggesting that hypothyroidism impairs CL function during gestation, delaying the onset of parturition in the rat. As P4 and E2 are necessary for the maturation and development of oocytes, preparing the endometrium for embryo implantation, and are important in the establishment and maintenance of early pregnancy, changes in the physiological levels of these hormones caused by TH hormones may contribute to disorders of or disrupt the reproductive system. Furthermore, in our experiment, in the groups of animals with PTU-induced hypothyroidism, the levels of homeobox A10 (HOXA10/HOXA10) and osteopontin (OPN/OPN), which are considered to be uterine receptivity markers [13], were significantly lower in comparison to those in the control group. Hoxa10/HOXA10 has been found to be directly involved in embryogenesis and embryo implantation via the regulation of downstream genes. The cyclical endometrial expression of this factor, with a peak of expression occurring during the window of implantation, is observed in response to E2 and P4 [59]. Osteopontin, a member of the extracellular matrix (ECM) protein family, is involved in many physiological and pathological processes, including cell adhesion, cell proliferation and differentiation, angiogenesis, and tumor metastasis. Weintraub et al. [60] showed that OPN-deficient mice manifested a decreased pregnancy rate during mid-gestation and that the knockdown of OPN in mouse endometrial stromal cells restrained trophoblast invasion in vitro. Additionally, OPN was proved to be activated in mouse endometrial stromal cells (mESCs) and human endometrial stromal cells (hESCs) by E2 and P4 [61,62]. These results suggest that OPN plays an important role in regulating blastocyst implantation and decidualization. Our data confirm that, in hypothyroidism, uterine receptivity is reduced. A disturbed E2 level and decreased expression of HOXA10 and OPN may result in difficulties with the implantation of blastocysts and the maintenance of pregnancy.
Prostaglandin endoperoxide synthase 2 (PTGS2) is involved in inflammation and in essential reproductive processes, including ovulation, fertilization, implantation, and decidualization. PTGS2-deficient females are infertile, with abnormalities in ovulation, fertilization, implantation, and decidualization [63,64]. PTGS2 is the key enzyme involved in prostaglandin synthesis [65,66]. Gillio-Meina et al. [42] showed that the PTGS2 protein is gradually expressed in the rat endometrium in response to deciduogenic stimuli. In our study, we showed that the PTGS2 protein level was significantly lower in the group of rats with induced hypothyroidism in comparison to the control group of animals. Combining that information with the knowledge that induced hypothyroidism in rats caused a reduction in the absolute volume of the endometrium [7,8], it may be speculated that the decreased level of PTGS2 in the uterus in the group of rats with induced hypothyroidism was caused by the significantly reduced volume of endometrium.
PTGES-2 and PTGES-3 are responsible for the conversion of PGH2 to PGE2, while PGFS converts PGH2 to PGF2α. PGIS is responsible for the conversion of PGH2 to PGI2. These enzymes are involved in the reproductive processes [25,26]. Their expression at implantation sites in rats and other species has been reported [48,49]. In our study, we showed higher expression levels of PTGES-2 in the experimental group of animals, whereas the expression of PTGES-3 and PGIS was at the same level in the experimental and control groups. The expression of PGFS was significantly lower in the group of rats with hypothyroidism. This suggests that hypothyroidism may stimulate the synthesis of PTGES2 and inhibit the synthesis of PGFS but does not affect the synthesis of PTGES-3 or PGIS. In the present study, the mRNA and protein expression patterns of PGFR as well as PGIR were opposite. The mRNA level was significantly higher, while the protein level was significantly lower in the group of animals with hypothyroidism in comparison to the control group. This could be a result of post-translational changes in proteins. These changes regulate the functional activities of proteins in cells and their interactions with other cellular molecules. It is considered that this modification plays a key role in modulating protein function.
It has been reported that the prostaglandin receptors EP1, EP3, and FP promote uterine smooth muscle contraction, while EP2 and EP4 affect uterine smooth muscle relaxation [29,34,35]. Blesson et al. [29] also indicated that the expression levels of the receptors of PGs are regulated by steroid hormones. In the human endometrium, it has been found that the levels of PG receptors vary in a phase-specific manner. EP2, EP3, and EP4 dominate in the mid-secretory phase, while EP1 dominates in the early-secretory phase, and FP dominates in the proliferative phase. This suggests that the expression of those receptors may be regulated by E2 and P4 [29,36]. Our study showed that induced hypothyroidism caused lower expression levels of EP1, EP3, and FP and higher expression levels of EP2 and EP4. It suggests that hypothyroidism leads to the impairment of the uterus’ function and disturbances of the estrous cycle by inducing changes in the expression levels of PG receptors in the uterine tissue. Furthermore, EP2, EP3, and EP4 might participate in the regulation of stromal edema, endometrial blood flow, and blood vessel permeability [29,36]. This, in turn, indicates that hypothyroidism can cause abnormalities in the cyclic changes in the uterine blood supply via changes in the expression of those receptors in the rat uterus. It is known that, in rodents, PGI2′s signaling and the expression of its receptor (PTGIR) are very important components of embryo–uterus interactions and are essential for successful implantation [25,39,41,42]. In mice, PGI2 is also critical for endometrial decidualization and embryo implantation [25,39]. In addition, PGI2 increases embryonic cell proliferation and reduces apoptosis [25,44,45]. It also enhances embryo hatching and the live birth potential of mouse embryos [25,46,47]. In our study, we also demonstrated a lower level of PTGIR in the group of animals with induced hypothyroidism. This implies that hypothyroidism may cause changes in endometrial decidualization, leading to difficulties in embryo implantation and the maintenance of pregnancy.

5. Conclusions

In summary, this study is the first to characterize the influence of hypothyroidism on uterine receptivity and PG signaling in uterine tissue in a rat model. The results show that hypothyroidism impairs uterine receptivity by decreasing the level of E2 as well as the expression of the uterine-receptivity factors HOXA10 and OPN. Hypothyroidism also causes changes in the expression of elements of the PGE2, PGF2α, and PGI2 signaling pathways, and changes in the concentrations of those prostaglandins in uterine tissue. In general, it decreases the expression of those factors in the rat uterus. It is known that prostaglandins are strongly involved in uterine functions, such as decidualization and blastocyst implantation, and therefore, hypothyroidism causes abnormalities in the female reproductive system. Our results suggest that hypothyroidism may interfere with the prostaglandin signaling pathway, which may further result in a reduction in uterine receptivity. However, this hypothesis requires further investigation.

Author Contributions

I.W.-P. designed the study and revised the manuscript. I.K.-Z., J.S.-C. and D.B. participated in the collection of data. I.K.-Z. and J.S.-C. performed the experiments. I.K.-Z. and J.S.-C. analyzed the data and wrote the paper. I.K.-Z., J.J. and K.L. participated in the revision of the final version of the manuscript. All authors have read and agreed to the published version of the manuscript.

Funding

This paper was supported by the grant of the KNOW Scientific Consortium: “Healthy Animal-Safe Food” (a decision of the Ministry of Science and Higher Education No. 05–1/KNOW2/2015)”: “Healthy Animal-Safe Food”.

Institutional Review Board Statement

All the experimental procedures were approved by the Local Animal Care and Use Committee in Olsztyn, Poland (Agreement No. 40/2015/DTN).

Informed Consent Statement

Not applicable.

Data Availability Statement

The data that support the findings of this study are available on request from the corresponding author, I.K.-Z.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Jannini, E.A.; Ulisse, S.; D’Armiento, M. Thyroid hormone and male gonadal function. Endocr. Rev. 1995, 16, 443–459. [Google Scholar] [PubMed]
  2. Metz, L.D.; Seidler, F.J.; McCook, E.C.; Slotkin, T.A. Cardiac alpha-adrenergic receptor expression is regulated by thyroid hormone during a critical developmental period. J. Mol. Cell Cardiol. 1996, 28, 1033–1044. [Google Scholar] [CrossRef]
  3. Krassas, G.E. Thyroid disease and female reproduction. Fertil. Steril. 2000, 74, 1063–1070. [Google Scholar] [CrossRef]
  4. Choksi, N.Y.; Jahnke, G.D.; St Hilaire, C.; Shelby, M. Role of thyroid hormones in human and laboratory animal reproductive health. Birth. Defects Res. B Dev. Reprod. Toxicol. 2003, 68, 479–491. [Google Scholar] [CrossRef]
  5. Kong, L.; Wei, Q.; Fedail, J.S.; Shi, F.; Nagaoka, K.; Watanabe, G. Effects of thyroid hormones on the antioxidative status in the uterus of young adult rats. J. Reprod. Dev. 2015, 61, 219–227. [Google Scholar] [CrossRef] [Green Version]
  6. Thomas, R.; Reid, R.L. Thyroid disease and reproductive dysfunction. J. Obstet. Gynaecol. 1987, 70, 789–798. [Google Scholar]
  7. Parija, S.C.; Raviprakash, V.; Telang, A.G.; Varshney, V.P.; Mishra, S.K. Influence of hypothyroid state on 45Ca2+ influx and sensitivity of rat uterus to nifedipine and diltiazem. Eur. J. Pharmacol. 2001, 421, 207–213. [Google Scholar]
  8. Inuwa, I.; Williams, M.A. Morphometric study on the uterine horn and thyroid gland in hypothyroid, and thyroxine-treated hypothyroid rats. J. Anat. 1996, 188, 383–393. [Google Scholar]
  9. Doufas, A.G.; Mastorakos, G. The hypothalamic-pituitary-thyroid axis and the female reproductive system. Ann. N. Y. Acad. Sci. 2000, 900, 65–76. [Google Scholar] [CrossRef] [PubMed]
  10. Reh, A.; Chaudhry, S.; Mendelsohn, F.; Im, S.; Rolnitzky, L.; Amarosa, A.; Levitz, M.; Srinivasa, S.; Krey, L.; Berkeley, A.S.; et al. Effect of autoimmune thyroid disease in older euthyroid infertile woman during the first 35 days of an IVF cycle. Fertil. Steril. 2011, 95, 1178–1181. [Google Scholar] [CrossRef] [Green Version]
  11. Dittrich, R.; Beckmann, M.W.; Oppelt, P.G.; Hoffmann, I.; Lotz, L.; Kuwert, T.; Mueller, A. Thyroid hormone receptors and reproduction. J. Reprod. Immunol. 2011, 90, 58–66. [Google Scholar] [CrossRef]
  12. Turnbull, L.W.; Lesny, P.; Killick, S.R. Assessment of uterine receptivity prior to embryo transfer: A review of currently available imaging modalities. Hum. Reprod. Update. 1995, 1, 505–514. [Google Scholar] [CrossRef]
  13. Shahzad, H.; Giribabu, N.; Karim, K.; Kassim, N.; Muniandy, S.; Kumar, K.E.; Salleh, N. Quercetin interferes with the fluid volume and receptivity development of the uterus in rats during the peri-implantation period. Reprod. Toxicol. 2017, 71, 42–54. [Google Scholar] [CrossRef]
  14. Yoshinaga, K. Uterine receptivity for blastocyst implantation. Ann. N. Y. Acad. Sci. 1988, 541, 423–443. [Google Scholar] [CrossRef]
  15. Murphy, C.R. Uterine receptivity and the plasma membrane transformation. Cell Res. 2004, 14, 259–267. [Google Scholar] [CrossRef]
  16. Okada, A.; Ohta, Y.; Inoue, S.; Hiroi, H.; Muramatsu, M.; Iguchi, T. Expression of estrogen, progesterone and androgen receptors in the oviduct of developing, cyclic and preimplantation rats. J. Mol. Endocrinol. 2003, 30, 301–315. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  17. Psychoyos, A. Uterine receptivity for nidation. Ann. N. Y. Acad. Sci. 1986, 476, 36–42. [Google Scholar] [CrossRef] [PubMed]
  18. Satokata, I.; Benson, G.; Maas, R. Sexually dimorphic sterility phenotypes in Hoxa-10 deficient mice. Nature 1995, 374, 460–463. [Google Scholar] [CrossRef] [PubMed]
  19. Taylor, H.S.; Avici, A.; Olive, D.; Igarashi, P. HOXA10 is expressed in response to sex steroids at the time of implantation in the human endometrium. J. Clin. Investig. 1998, 101, 1379–1384. [Google Scholar] [CrossRef] [Green Version]
  20. Bagot, C.N.; Kliman, H.J.; Taylor, H.S. Maternal HOXA10 is required for pinopod formation in the development of mouse uterine receptivity to embryo implantation. Dev. Dyn. 2001, 222, 538–544. [Google Scholar] [CrossRef]
  21. Apparao, K.B.; Murray, M.J.; Fritz, M.A.; Meyer, W.R.; Chamberes, A.F.; Truong, P.R.; Lessey, B.A. Osteopontin and its receptor alphavbeta(3) integrin are coexpressed in the human endometrium during menstrual cycle but regulated differentially. J. Clin. Endocrinol. Metab. 2001, 86, 4991–5000. [Google Scholar]
  22. Casals, G.; Ordi, J.; Creus, M.; Fa’bregues, F.; Carmona, F.; Casamitjana, R.; Balasch, J. Osteopontin and avb3 integrin as markers of endometrial receptivity: The effect of different hormone therapies. Reprod. Biomed. Online 2010, 21, 349–359. [Google Scholar] [CrossRef]
  23. Loftin, C.D.; Tiano, H.F.; Langenbach, R. Phenotypes of the COX-deficient mice indicte physiological and pathological roles for COX-1 and COX-2. Prostaglandins Lipid Mediat. 2002, 68, 177–185. [Google Scholar] [CrossRef]
  24. Smith, W.L.; DeWitt, D.L. Prostaglandin endoperoxide synthases- 1 and -2. Adv. Immunol. 1996, 62, 167–215. [Google Scholar]
  25. Morawska, E.; Kaczmarek, M.M.; Blitek, A. Regulation of prostacyclin synthase expression and prostacyclin content in the pig endometrium. Theriogenology 2012, 78, 2071–2086. [Google Scholar] [CrossRef]
  26. Helliwell, R.J.; Adams, L.F.; Mitchell, M.D. Prostaglandin synthases: Recent developments and a novel hypothesis. Prostaglandins Leukot Essent. Fatt. Acids 2004, 70, 101–113. [Google Scholar] [CrossRef] [PubMed]
  27. Liu, J.; Akahoshi, T.; Jiang, S.; Namai, R.; Kitasato, H.; Endo, H.; Kameya, T.; Kondo, H. Induction of neutrophil death resembling neither apoptosis nor necrosis by ONO-AE-248, a selective agonist for PGE2 receptor subtype 3. J. Leukoc. Biol. 2000, 68, 187–193. [Google Scholar] [PubMed]
  28. Jabbour, H.N.; Sales, K.J. Prostaglandin receptor signaling and function in human endometrial pathology. Trends Endocrinol. Metab. 2004, 15, 398–404. [Google Scholar] [CrossRef] [PubMed]
  29. Blesson, C.S.; Büttner, E.; Masironi, B.; Sahlin, L. Prostaglandin receptors EP and FP are regulated by estradiol and progesterone in the uterus of ovariectomized rats. Reprod. Biol. Endocrinol. 2012, 10, 3. [Google Scholar] [CrossRef] [Green Version]
  30. Narumiya, S.; Sugimoto, Y.; Ushikubi, F. Prostanoid receptors: Structures, properties, and functions. Physiol. Rev. 1999, 79, 1193–1226. [Google Scholar] [CrossRef] [PubMed]
  31. Makino, S.; Zaragoza, D.B.; Mitchell, B.F.; Robertson, S.; Olson, D.M. Prostaglandin F2alpha and its receptor as activators of human decidua. Semin. Reprod. Med. 2007, 25, 60–68. [Google Scholar] [CrossRef]
  32. Narumiya, S.; FitzGerald, G.A. Genetic and pharmacological analysis of prostanoid receptor function. J. Clin. Investig. 2001, 108, 25–30. [Google Scholar] [CrossRef]
  33. Kota, B.P.; Huang, T.H.; Roufogalis, B.D. An overview on biological mechanisms of PPARs. Pharmacol. Res. 2005, 51, 85–94. [Google Scholar] [CrossRef]
  34. Yang, Z.M.; Das, S.K.; Wang, J.; Sugimoto, Y.; Ichikawa, A.; Dey, S.K. Potential sites of prostaglandin action in the periimplantation mouse uterus: Differentia expression and regulation of prostaglandin receptor genes. Biol. Reprod. 1997, 56, 368–379. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  35. Grigsby, P.L.; Sooranna, S.R.; Adu-Amankwa, B.; Pitzer, B.; Brockman, D.E.; Johnson, M.R.; Myatt, L. Regional expression of prostaglandin E2 and F2alpha receptors in hyman myometrium, amnion and choriodecidua with advancing gestation and labor. Biol. Reprod. 2006, 75, 297–305. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  36. Catalano, R.D.; Wilson, M.R.; Boddy, S.C.; Jabbour, H.N. Comprehensive expression analysis of prostanoid enzymes and receptors in the human endometrium across the menstrual cycle. Mol. Hum. Reprod. 2011, 17, 182–192. [Google Scholar] [CrossRef] [PubMed]
  37. Kraeling, R.R.; Rampacek, G.B.; Fiorello, N.A. Inhibition of pregnancy with indomethacin in mature gilts and prepubertal gilts induced to ovulate. Biol. Reprod. 1985, 32, 105–110. [Google Scholar] [CrossRef] [Green Version]
  38. Davis, D.L.; Blair, R.M. Studies of uterine secretion and products of primary cultures of endometrial cells in pigs. J. Reprod. Fertil. Supply 1993, 48, 143–155. [Google Scholar] [CrossRef]
  39. Lim, H.; Gupta, R.A.; Ma, W.G.; Parija, B.C.; Moller, D.E.; Morrow, J.D.; Dubois, R.D.; Trzaskos, J.M.; Dey, S.K. Cyclo-oxygenase-2-derived prostacyclin mediates embryo implantation in the mouse via PPARdelta. Genes. Dev. 1999, 13, 1561–1574. [Google Scholar] [CrossRef]
  40. Cammas, L.; Reinaud, P.; Bordas, N.; Dubois, O.; Germain, G.; Charpigny, G. Developmental regulation of prostacyclin synthase and prostacyclin receptors in the ovine uterus and conceptus during the peri-implantation period. Reproduction 2006, 131, 917–927. [Google Scholar] [CrossRef] [Green Version]
  41. Kengni, J.H.; St-Louis, I.; Parent, S.; Leblanc, V.; Shooner, C.; Asselin, E. Regulation of prostaglandin D synthase and prostacyclin synthase in endometrium of cyclic, pregnant and pseudopregnant rats and their regulation by sex steroids. J. Endocrinol. 2007, 195, 301–311. [Google Scholar] [CrossRef] [Green Version]
  42. Gillio-Meina, C.; Phang, S.H.; Mather, J.P.; Knight, T.G. Expression patterns and role of prostaglandin-endoperoxide synthases, prostaglandin E synthases, prostacyclin synthases, prostacyclin synthase, prostacyclin receptor, peroxisome proliferator-activated receptor delta and retinoid x receptor alpha in rat endometrium during artificially-induced decidualization. Reproduction 2009, 137, 537–552. [Google Scholar] [PubMed] [Green Version]
  43. Ulbrich, S.E.; Schulke, K.; Groebner, A.E.; Reichenbach, H.D.; Angioni, C.; Geisslinger, G.; Meyer, H.H.D. Quantitative characterization of prostaglandins in the uterus of early pregnant cattle. Reproduction 2009, 138, 371–382. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  44. Pakrasi, P.L.; Jain, A.K. Evaluation of cyclooxygenase 2 derived endogenous prostacyclin in mouse preimplantation embryo development in vitro. Life Sci. 2007, 80, 1503–1507. [Google Scholar] [CrossRef] [PubMed]
  45. Pakrasi, P.; Jain, A.K. Cyclooxygenase-2-derived endogenous prostacyclin reduces apoptosis and enhances embryo viability in mouse. Prostaglandins Leukot. Essent. Fatty Acids 2008, 79, 27–33. [Google Scholar] [CrossRef] [PubMed]
  46. Huang, J.C.; Wun, W.S.; Goldsby, J.S.; Wun, I.C.; Falconi, S.M.; Wu, K.K. Prostacyclin enhances embryo hatching but not sperm motility. Hum. Reprod. 2003, 18, 2582–2589. [Google Scholar] [CrossRef] [Green Version]
  47. Huang, J.C.; Goldsby, J.S.; Wun, W.S. Prostacyclin enhances the implantation and life birth potentials of mouse embryos. Hum. Reprod. 2004, 19, 1856–1860. [Google Scholar] [CrossRef] [Green Version]
  48. Salleh, N. Diverse roles of prostaglandins in blastocyst implantation. Sci. World J. 2014, 2014, 1–11. [Google Scholar] [CrossRef] [Green Version]
  49. Shahnazi, M.; Niuri, M.; Mohaddes, G.; Latifi, Z.; Fattahi, A.; Mohammadi, M. Prostaglandin E pathway in uterine tissue during window of preimplantation in female mice mated with intact and seminal vesicle-excited male. Reprod. Sci. 2017, 1, 1–9. [Google Scholar]
  50. Wacławik, A. Novel insights into the mechanism of pregnancy establishment: Regulation of prostaglandin synthesis and signaling in pig. Reproduction 2011, 142, 389–399. [Google Scholar] [CrossRef] [Green Version]
  51. Jena, S.; Bhanja, S. Hypothyroidism alters antioxidant defence system in rat brainstem during postnatal development and adulthood. Neurol. Sci. 2014, 35, 1269–1274. [Google Scholar] [CrossRef] [PubMed]
  52. Persani, L. Clinical review: Central hypothyroidism: Pathogenic, diagnostic, and therapeutic challenges. J. Clin. Endocrinol. Metab. 2012, 97, 3068–3078. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  53. Biondi, B.; Cooper, D.S. Thyroid hormone therapy for hypothyroidism. Endocrine 2019, 66, 18–26. [Google Scholar] [CrossRef]
  54. Gruters, A.; Krude, H. Detection and treatment of congenital hypothyroidism. Nat. Rev. Endocrinol. 2012, 18, 104–113. [Google Scholar] [CrossRef] [PubMed]
  55. Colicchia M Campagnolo, L.; Baldini, E.; Ulisse, S.; Valensise, H.; Moretti, C. Molecular basis of thyrotropin and thyroid hormone action during implantation and early development. Hum. Reprod. Update. 2014, 20, 884–904. [Google Scholar] [CrossRef]
  56. Krassas, G.E.; Poppe, K.; Glinoer, D. Thyroid function and human reproductive health. Endocr. Rev. 2010, 31, 702–755. [Google Scholar] [CrossRef] [Green Version]
  57. Tohei, A. Studies on the functional relationship between thyroid, adrenal and gonadal hormones. J. Reprod. Dev. 2004, 50, 9–20. [Google Scholar] [CrossRef] [Green Version]
  58. Hapon, M.B.; Motta, A.B.; Ezquer, M.; Bonafede, M.; Jahn, A.G. Hypothyroidism prolongs corpus luteum function in the pregnant rat. Reproduction 2007, 133, 197–205. [Google Scholar] [CrossRef] [Green Version]
  59. Zanatta, A.; Rocha, A.M.; Carvalho, F.M.; Pereira, R.M.; Taylor, H.S.; Motta, E.L.; Baracat, E.C.; Serafini, P.C. The role of the Hoxa10/HOXA10 gene in the etiology of endometriosis and its related infertility: A review. J. Assist. Reprod. Genet. 2010, 27, 701–710. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  60. Weintraub, A.S.; Lin, X.; Itskovich, V.V.; Aguinaldo, J.G.; Chaplin, W.F.; Denhardt, D.T.; Fayad, Z.A. Prenatal detection of embryo resorption in osteopontin-deficient mice using serial noninvasive magnetic resonance microscopy. Pediatr. Res. 2004, 55, 419–424. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  61. Von Wolff, M.; Bohlmann, M.K.; Fiedler, C.; Ursel, S.; Strowitzki, T. Osteopontin is up-regulated in human decidual stromal cells. Fertil. Steril. 2004, 81, 741–748. [Google Scholar] [CrossRef]
  62. Qi, Q.R.; Xie, Q.Z.; Liu, X.L.; Zhou, Y. Osteopontin is expressed in the mouse uterus during early pregnancy and promotes mouse blastocyst attachment and invasion in vitro. PLoS ONE 2014, 9, e104955. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  63. Lim, H.; Paria, B.C.; Das, S.K.; Dinchuk JE Langenbach, R.; Trzaskos, J.M.; Dey, S.K. Multiple female reproductive failures in cyclooxygenase 2-deficient mice. Cell 1997, 91, 197–208. [Google Scholar] [CrossRef] [Green Version]
  64. St-Louis, I.; Singh, M.; Brasseur, K.; Leblanc, V.; Parent, S.; Asselin, E. Expression of COX-1 and COX-2 in the endometrium of cyclic, pregnant and in a model of pseudopregnant rats and their regulation by sex steroids. Reprod. Biol. Endocrinol. 2010, 24, 103. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  65. Chandrasekhaaran, N.V.; Dai, H.; Roos, K.L.T.; Evanson, N.K.; Tomsik, J.; Elton, T.S.; Simmons, D.L. COX-3, a cyclooxygenase-1 variant inhibited by acetaminophen and other analgesic/ antipyretic drugs: Cloning, structure and expression. Proc. Natl. Acad. Sci. USA 2002, 90, 13926–13931. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  66. Duffy, D.M. Novel contraceptive targets to inhibit ovulation: The prostaglandin E2 pathway. Hum. Reprod. Update. 2015, 21, 652–670. [Google Scholar] [CrossRef] [Green Version]
Animals 11 02636 g001 550
Figure 1. The levels of T3, T4, and TSH in blood serum samples (ng/mL). The data are presented as the mean ± SEM. Asterisks indicate significant differences ((* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
Figure 1. The levels of T3, T4, and TSH in blood serum samples (ng/mL). The data are presented as the mean ± SEM. Asterisks indicate significant differences ((* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
Animals 11 02636 g001
Animals 11 02636 g002 550
Figure 2. The levels of (A) E2 (pg/mL) and (B) P4 (ng/mL) in blood serum samples. The data are presented as the mean ± SEM. Asterisks indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
Figure 2. The levels of (A) E2 (pg/mL) and (B) P4 (ng/mL) in blood serum samples. The data are presented as the mean ± SEM. Asterisks indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
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Animals 11 02636 g003 550
Figure 3. The effects of hypothyroidism on the mRNA and protein abundance of uterine-receptivity factors in the uterine tissue of rats: (A,C): OPN/OPN; (B,D): HOXA10/HOXA10. The values are presented as arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
Figure 3. The effects of hypothyroidism on the mRNA and protein abundance of uterine-receptivity factors in the uterine tissue of rats: (A,C): OPN/OPN; (B,D): HOXA10/HOXA10. The values are presented as arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
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Animals 11 02636 g004 550
Figure 4. The effect of hypothyroidism on the mRNA (A) and protein (B) abundance of prostaglandin-endoperoxide synthase 2 in the uterine tissue of rats. The values are presented in arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
Figure 4. The effect of hypothyroidism on the mRNA (A) and protein (B) abundance of prostaglandin-endoperoxide synthase 2 in the uterine tissue of rats. The values are presented in arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
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Animals 11 02636 g005 550
Figure 5. The effects of hypothyroidism on the mRNA and protein abundance of PGE2 synthase 2 in the uterine tissue of rats: (A,C): PTGES-2/PTGES-2; (B,D): PTGES-3/PTGES-3. The values are presented in arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
Figure 5. The effects of hypothyroidism on the mRNA and protein abundance of PGE2 synthase 2 in the uterine tissue of rats: (A,C): PTGES-2/PTGES-2; (B,D): PTGES-3/PTGES-3. The values are presented in arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
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Animals 11 02636 g006 550
Figure 6. The effects of hypothyroidism on the mRNA and protein abundance of PGE2 receptors in the uterine tissue of rats: (A,E): PTGER1/PTGER1; (B,F): PTGER2/PTGER2; (C,G): PTGER3/PTGER3; (D,H): PTGER4/PTGER. The values are presented in arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
Figure 6. The effects of hypothyroidism on the mRNA and protein abundance of PGE2 receptors in the uterine tissue of rats: (A,E): PTGER1/PTGER1; (B,F): PTGER2/PTGER2; (C,G): PTGER3/PTGER3; (D,H): PTGER4/PTGER. The values are presented in arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
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Figure 7. The effects of hypothyroidism on the mRNA and protein abundance of PGF2α synthase and its receptor in the uterine tissue of rats: (A,C): PGFS/PGFS; (B,D): PTGFR/PTGFR. The values are presented in arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
Figure 7. The effects of hypothyroidism on the mRNA and protein abundance of PGF2α synthase and its receptor in the uterine tissue of rats: (A,C): PGFS/PGFS; (B,D): PTGFR/PTGFR. The values are presented in arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
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Figure 8. The effects of hypothyroidism on the mRNA and protein abundance of PGI2 synthase and its receptor in the uterine tissue of rats: (A,C): PGIS/PGIS; (B,D): PTGIR/PTGIR. The values are presented as arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
Figure 8. The effects of hypothyroidism on the mRNA and protein abundance of PGI2 synthase and its receptor in the uterine tissue of rats: (A,C): PGIS/PGIS; (B,D): PTGIR/PTGIR. The values are presented as arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
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Animals 11 02636 g009 550
Figure 9. The effect of hypothyroidism on the concentrations (pg/mL) of PGs in uterine tissue of rats: (A): PGE2; (B): PGF2α; (C): PGI2. The values are presented in arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
Figure 9. The effect of hypothyroidism on the concentrations (pg/mL) of PGs in uterine tissue of rats: (A): PGE2; (B): PGF2α; (C): PGI2. The values are presented in arbitrary units and expressed as the mean ± SEM. Stars indicate significant differences (* p ≤ 0.05, ** p ≤ 0.01, *** p ≤ 0.001, **** p ≤ 0.0001), as determined by Student’s t-test.
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Table
Table 1. Primers used for real-time PCR.
Table 1. Primers used for real-time PCR.
Gene SymbolGeneBank Accession No.Forward Primer
Reverse Primer		Primer Size (bp)
PTGS2NM_0172325′-AAAGGCCTCCATTGACCAGA-3′
5′-TCGATGTCATGGTAGAGGGC-3′		20
20
PTGES2NM_001107832.15′-AAAGGAAGCCAGGACGGAGGA-3′
5′-CCTCGGCAGGTGTTCGGT-3′		21
18
PTGES3M_001130989.15′-GCTGCCGGAGAGGAGTCG-3′
5′-AGGCTGCATGGTGAACGGG-3′		18
19
PTGER1M_001278475.15′-GCTCCCTGCCTTTCACAATCT-3′
5′-TCTCAGGACTGGTGGTCTAAGGA-3′		21
23
PTGER2NM_031088.15′-GAAAGGACTTCTATGGCGGAGG-3′
5′-AAGCAAAGATTGTGAAAGGCAGG-3′		22
24
PTGER3NM_012704.15′-CGCAGATGGGAAAGGAGAAGGA-3′
5′-AGGTTGTTCATCATCTGGCAGAACT-3′		22
25
PTGER4NM_032076.35′-CATTCCCGCTCGTGGTGCGA-3′
5′TCTGCTGATGGTCTTTCACCACAC-3′		19
23
PGFSNM_138510.15′-GGTATCTCTGAAGCCAGGGGA-3′
5′-TTGGACACCCCGATGGACTTG-3′		21
21
PTGFRNM_013115.15′-CCCTTTCTGGTGACGATGGC-3′
5′-TCCGTAGCAGAATGTAGACCCA-3′		20
22
PTGISNM_031557.25′-GGGCCTCCTGACTTCCTGTTG-3′
5′-AGCTTTTCCTGCTCTCGGTGT-3′		21
21
PTGIRNM_001077644.15′-TCCCTGCCTCTCACGATCAG-3′
5′-AAAACGGAAGGCGTGGAGGT-3′		20
20
OPNAB001382.15′-TGAAAGTGGCTGAGTTTGGC-3′
5′-TCGTCGTCATCATCGTCCAT-3′		20
20
HOXA10NM_001129878.15′-CATTCAGGCCCCATCTCAGA-3′
5′-TTCAGCCCCTCATAGCCAAA-3′		20
20
ACTBKJ696744.15′-CCACACCCGCCACCAGTTCG-3′
5′-CTAGGGCGGCCCACGATGGA-3′		20
20
Table
Table 2. Antibodies used for Western blotting.
Table 2. Antibodies used for Western blotting.
ProteinCatalog N°HostDilutionPredicted Molecular Weight (kDa)
PTGS-2Santa Cruz, sc-7951Rabbit1:10085
PTGES-2Cayman, 160145Rabbit1:20033
PTGES-3Abcam, ab92503Rabbit1:10,00019
PTGER1Abcam, ab183073Rabbit1:300042
PTGER2Abcam, ab16151Mouse1:20053
PTGER3Abcam, ab16152Mouse1:10043
PTGER4Santa Cruz, sc-20677Rabbit1:10053
PGFSAbcam, ab84327Rabbit1:50036
PTGFRCayman, 101802Rabbit1:20064
PTGISAbcam, ab23668Rabbit1:25057
PTGIRCayman, 10005518Rabbit1:20067
OPNAbcam ab8448Rabbit1:100066
HOXA10Abcam ab23392Rabbit1:100042
ACTBSigmaAldrich A2228Mouse1:400042
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Kowalczyk-Zieba, I.; Staszkiewicz-Chodor, J.; Boruszewska, D.; Lukaszuk, K.; Jaworska, J.; Woclawek-Potocka, I. Hypothyroidism Affects Uterine Function via the Modulation of Prostaglandin Signaling. Animals 2021, 11, 2636. https://doi.org/10.3390/ani11092636

AMA Style

Kowalczyk-Zieba I, Staszkiewicz-Chodor J, Boruszewska D, Lukaszuk K, Jaworska J, Woclawek-Potocka I. Hypothyroidism Affects Uterine Function via the Modulation of Prostaglandin Signaling. Animals. 2021; 11(9):2636. https://doi.org/10.3390/ani11092636

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Kowalczyk-Zieba, Ilona, Joanna Staszkiewicz-Chodor, Dorota Boruszewska, Krzysztof Lukaszuk, Joanna Jaworska, and Izabela Woclawek-Potocka. 2021. "Hypothyroidism Affects Uterine Function via the Modulation of Prostaglandin Signaling" Animals 11, no. 9: 2636. https://doi.org/10.3390/ani11092636

APA Style

Kowalczyk-Zieba, I., Staszkiewicz-Chodor, J., Boruszewska, D., Lukaszuk, K., Jaworska, J., & Woclawek-Potocka, I. (2021). Hypothyroidism Affects Uterine Function via the Modulation of Prostaglandin Signaling. Animals, 11(9), 2636. https://doi.org/10.3390/ani11092636

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