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The Journal of Clinical Investigation logoLink to The Journal of Clinical Investigation
. 2018 Jun 18;128(7):3186–3197. doi: 10.1172/JCI98931

HIF2α in the uterine stroma permits embryo invasion and luminal epithelium detachment

Leona Matsumoto 1, Yasushi Hirota 1,2,✉, Tomoko Saito-Fujita 1, Norihiko Takeda 3, Tomoki Tanaka 1, Takehiro Hiraoka 1, Shun Akaeda 1, Hidetoshi Fujita 4, Ryoko Shimizu-Hirota 5, Shota Igaue 1, Mitsunori Matsuo 1, Hirofumi Haraguchi 1, Mayuko Saito-Kanatani 1, Tomoyuki Fujii 1, Yutaka Osuga 1
PMCID: PMC6025968  PMID: 29911998

Abstract

Although it has been reported that hypoxia inducible factor 2 α (Hif2a), a major transcriptional factor inducible by low oxygen tension, is expressed in the mouse uterus during embryo implantation, its role in pregnancy outcomes remains unclear. This study aimed to clarify functions of uterine HIF using transgenic mouse models. Mice with deletion of Hif2a in the whole uterus (Hif2a-uKO mice) showed infertility due to implantation failure. Supplementation with progesterone (P4) and leukemia inhibitory factor (LIF) restored decidual growth arrest and aberrant position of implantation sites in Hif2a-uKO mice, respectively, but did not rescue pregnancy failure. Histological analyses in Hif2a-uKO mice revealed persistence of the intact luminal epithelium, which blocked direct contact between stroma and embryo, inactivation of PI3K-AKT pathway (embryonic survival signal), and failed embryo invasion. Mice with stromal deletion of Hif2a (Hif2a-sKO mice) showed infertility with impaired embryo invasion and those with epithelial deletion of Hif2a (Hif2a-eKO mice) showed normal fertility, suggesting the importance of stromal HIF2α in embryo invasion. This was reflected in reduced expression of membrane type 2 metalloproteinase (MT2-MMP), lysyl oxidase (LOX), VEGF, and adrenomedullin (ADM) in Hif2a-uKO stroma at the attachment site, suggesting that stromal HIF2α regulates these mediators to support blastocyst invasion. These findings provide new insight that stromal HIF2α allows trophoblast invasion through detachment of the luminal epithelium and activation of an embryonic survival signal.

Keywords: Development, Reproductive Biology

Keywords: Embryonic development, Obstetrics/gynecology, hypoxia

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Introduction

Infertility is a worldwide issue estimated to affect up to 30% of couples in both developed and developing countries (1). Infertile patients undergoing in vitro fertilization and embryo transfer (IVF-ET) are on the rise, and many of them experience recurrent implantation failure, which is a major problem in IVF-ET programs. The process of embryo implantation spanning blastocyst apposition and attachment with the uterine epithelium, along with invasion of blastocyst trophectoderm into the endometrium, is executed by molecular interactions between the embryo and uterus (2–5). Among others, progesterone (P4) signaling, heparin-binding EGF-like growth factor (HB-EGF), and leukemia inhibitory factor–STAT3 (LIF-STAT3) signaling were reported as key molecular mediators of embryo apposition and attachment (6–11). However, other key molecules and pathways in these processes remain elusive.

Hypoxia inducible factor (HIF) is a major transcription factor that responds to low oxygen tension and induces the expression of hypoxia-related genes such as VEGF and erythropoietin (12). Through the induction of these genes, HIF is involved in various physiological responses such as metabolism, cell death, and angiogenesis (13). HIF is composed of 2 subunits, α and β (14). The HIFα subunit has 3 isotypes, HIF1α, HIF2α, and HIF3α, whereas the HIFβ subunit has 2 types, ARNT1 and ARNT2 (14). A previous study showed that the expression of Hif1a is primarily in the uterine luminal epithelium during the peri-implantation period, and the expression of Hif2a is mainly in the stroma at the same time, whereas Hif3a is undetectable in the uterus (15). Notably, Hif2a is strongly expressed in the uterine stroma after embryo attachment (15). Based on expression patterns, we speculated that HIFα has functional roles in embryo implantation. Hif1a and Hif2a homozygous null embryos die during gestation (16, 17), impeding functional analysis of HIF in the reproductive system. To overcome this difficulty, we generated mice with uterine tissue–specific deletion of Hif1a and Hif2a using Pgr-Cre and Ltf-Cre drivers as previously described (18–21), and examined critical pregnancy events. Mice with Hif2a deletion in the entire uterus (Hif2a-uKO mice) were infertile, whereas mice with uterine deletion of Hif1a (Hif1a-uKO mice) showed subfertility, indicating the importance of uterine HIFα in fertility. The luminal epithelial barrier surrounding the embryo disappears just before embryo invasion in the littermate controls, whereas it persists and prevents embryo invasion in Hif2a-uKO mice, suggesting impairment of this invasion process as a cause of infertility in Hif2a-uKO mice. Importantly, detachment of luminal epithelium from stroma, which permits direct contact between stroma and embryo, and activation of PI3K-AKT pathway as an embryonic survival signal are not observed in Hif2a-uKO mice (unlike the littermate controls), providing evidence for a role of HIF2α in embryo invasion. Our findings offer insights that uterine HIF2α is critical for embryo invasion through activation of an embryo survival signal and detachment of the luminal epithelium.

Results

Mice with uterine deletion of Hif2a show infertility and those with uterine deletion of Hif1a show subfertility.

To explore the role of uterine HIF in pregnancy, we generated females with deletion of Hif1a and Hif2a in the entire uterus (Hif1a-uKO and Hif2a-uKO, respectively) by crossing Hif1a- or Hif2a-loxP mice with Pgr-Cre mice. We first confirmed that HIF1α and HIF2α mRNA levels were significantly reduced in the uterus of Hif1a-uKO and Hif2a-uKO mice, respectively (Figure 1, A and B and Supplemental Figure 1; supplemental material available online with this article; https://doi.org/10.1172/JCI98931DS1). Hif1a-uKO mice, Hif2a-uKO mice, and their littermate controls (Hif1a control, Hif2a control) were mated with WT fertile male mice. We found that approximately 50% of the plug-positive Hif1a-uKO mice did not deliver any pups and the number of pups with Hif1a-uKO dams was significantly reduced (Figure 1, C and D). Surprisingly, we found that Hif2a-uKO mice were infertile (Figure 1, C and D), suggesting that uterine Hifa, especially Hif2a, is critical for successful pregnancy. Based on these results, we focused on the role of Hif2a in the uterus in the subsequent analyses by using Hif2a-uKO mice.

Figure 1. Hif2a-uKO mice show infertility, and Hif1a-uKO mice show subfertility.

Figure 1

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(A and B) Hif2a mRNA levels were reduced in the uterine luminal epithelium and stroma of Hif2a-uKO mice, respectively (n = 4). (C and D) Hif1a-uKO mice were subfertile, and Hif2a-uKO mice were infertile. Hif1a-uKO mice, Hif2a-uKO mice, and their littermate controls (Hif1a control, Hif2a control) were mated with WT fertile male mice. (A, B, D) Mean ± SEM, Student’s t test. (C) Fisher’s exact probability test. In all panels, *P < 0.05.

Hif2a-uKO mice showing normal ovulation and preimplantation embryo development undergo impaired embryo implantation.

We examined ovulation and fertilization in Hif2a-uKO mice by flushing eggs and/or embryos on day 2 of pregnancy (day 1 = vaginal plug), and found both processes to be normal (Figure 2, A–C). We also confirmed normal development of preimplantation embryos and their timely transport from the oviduct into uterine lumens of Hif2a-uKO mice by recording the number of blastocysts retrieved through flushing the uteri on day 4 of pregnancy (Figure 2, D and E). Successful implantation is the result of reciprocal interactions between the blastocyst and the receptive uterus. Stromal edema on day 4 morning leads to uterine luminal closure, placing the blastocyst in close apposition with the luminal epithelium. We previously reported that proliferation-to-differentiation switching, cessation of epithelial proliferation, and acceleration of stromal proliferation in the uterus on day 4 morning are hallmarks of uterine receptivity in embryo implantation (7). Immunostaining of Ki67, a cell proliferation marker, revealed that uteri of Hif2a-uKO mice had normal proliferation-to-differentiation switching, comparable to the controls (Supplemental Figure 2, A–C). Embryo apposition is followed by intimate adherence of the blastocyst trophectoderm to the luminal epithelium (attachment reaction), marking the first discernible sign of implantation from midnight of day 4 to day 5 morning. The attachment reaction coincides with increased stromal vascular permeability at the site of the blastocyst and can be demarcated by distinct blue bands along the uterus after intravenous injection of Chicago blue dye solution (8). We found that the number of distinct implantation sites in Hif2a-uKO mice was comparable to Hif2a controls on day 5 morning (Figure 2, F and G). With the implantation process in progress, stromal cells surrounding the implanting embryo undergo decidualization. The luminal epithelium surrounding the implantation sites disappears on day 5 evening, and embryo invasion into the stroma starts from day 5 night to day 6 morning. Decidual growth peaks on day 8 of pregnancy. To determine whether this process is normal in Hif2a-uKO mice, we counted the number of implantation sites in Hif2a-uKO mice and the controls on days 6 and 8 of pregnancy. The number of implantation sites remained comparable between the 2 groups on day 6 (Figure 2, H and I), but normal implantation sites with decidualization completely disappeared in Hif2a-uKO mice on day 8 (Figure 2, J and K). By H&E staining, we confirmed that embryos were completely degraded and decidualization was impaired in Hif2a-uKO mice on day 8 of pregnancy (Figure 2L), suggesting decidual growth arrest and implantation failure in Hif2a-uKO mice.

Figure 2. Hif2a-uKO mice show implantation failure.

Figure 2

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(A–E) Ovulation, fertilization, and development of preimplantation embryos were normal in Hif2a-uKO mice. A and D, P > 0.05, mean ± SEM, Student’s t test; B, P > 0.05, Fisher’s exact probability test; C and E, scale bar, 200 μm. (F and G) Attachment reaction occurred normally in Hif2a-uKO mice at 1000 hours on day 5. P > 0.05, mean ± SEM, Student’s t test. Arrow and arrowhead indicate implantation site and ovary, respectively. (H and I) Decidualization was observed in Hif2a-uKO mice at 1000 hours on day 6. P > 0.05, mean ± SEM, Student’s t test. (J–L) Embryo implantation and decidualization were completely disturbed in Hif2a-uKO mice at 1000 hours on day 8. In K, *P < 0.05, mean ± SEM, Student’s t test. In L, arrowhead indicates an embryo; arrow, a destroyed embryo with blood cell infiltration; dec, decidua.

P4 administration rescues decidualization in Hif2a-uKO mice but does not rescue pregnancy failure.

It has been reported that murine decidua-derived factors serve as luteotrophins to prolong the life span of the corpus luteum and maintain luteal P4 production (22–24). Prolactin-related factors Prl3c1 and Prlr are hallmarks of decidual health and contribute to activation of the corpus luteum and ovarian secretion of P4 in rodents (25–31). In Hif2a-uKO mice, the expression of Prl3c1 and Prlr was significantly reduced (Figure 3, A–C), suggesting that unhealthy decidual condition compromises luteotrophy in Hif2a-uKO mice. As expected, serum P4 levels are significantly reduced in Hif2a-uKO mice on days 6 and 8 of pregnancy when decidualization prominently occurs (Figure 3D). In contrast, serum estradiol-17β (E2) levels on days 4, 5, 6, and 8 of pregnancy were comparable between controls and Hif2a-uKO mice (Figure 3E). To clarify whether the decreased levels of P4 were involved in decidual growth arrest of Hif2a-uKO mice, we examined the effect of luteal support in Hif2a-uKO mice by daily subcutaneous injection of P4 from day 2 of pregnancy (2 mg/mouse/day). P4 administration successfully restored the number and weight of implantation sites in Hif2a-uKO mice on day 8 of pregnancy (Figure 3, F and G, and Supplemental Figure 3). The expression of decidualization marker BMP2 (32, 33) was comparable between Hif2a-uKO mice with P4 treatment and the control mice (Supplemental Figure 4), suggesting that P4 supplementation rescues decidualization failure in Hif2a-uKO mice. However, H&E staining demonstrated that P4 supplementation did not recover embryo survival in Hif2a-uKO mice on day 8 of pregnancy (Figure 3H). These findings indicate that P4 reduction is not the cause of pregnancy failure in Hif2a-uKO mice. In fact, Hif2a-uKO mice with daily P4 injection showed reduced weight of implantation sites on day 12 (Figure 3, I and J) and never delivered pups (Figure 3K).

Figure 3. P4 administration does not recover implantation failure but rescues decidualization in Hif2a-uKO mice.

Figure 3

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(A–C) Decidual prolactin-related factors Prl3c1 and Prlr, hallmarks of decidual health and luteotrophin, were reduced in Hif2a-uKO mice during decidualization. In A and C, n ≥ 4, *P < 0.05, mean ± SEM, Student’s t test. In B, scale bar, 200 μm; arrowhead, an embryo; arrow, a destroyed embryo with blood cell infiltration; dec, decidua. (D and E) Serum P4 levels were reduced in Hif2a-uKO mice compared with the controls on days 6 and 8 of pregnancy, whereas serum E2 levels were comparable between them. *P < 0.05, mean ± SEM, Student’s t test. (F and G) Daily injection of P4 from day 2 of pregnancy (2 mg/mouse/day) restored decidualization in Hif2a-uKO mice on day 8 of pregnancy. P > 0.05, mean ± SEM, Student’s t test. Arrow and arrowhead indicate implantation site and ovary, respectively. (H) P4 supplementation did not recover embryo survival in Hif2a-uKO mice on day 8 of pregnancy. No embryo was observed at the implantation site of Hif2a-uKO mice with P4 treatment. Scale bar, 200 μm; dec, decidua. (I–K) Hif2a-uKO mice with daily P4 injection showed the reduced weight of implantation sites on day 12, and did not deliver any pups in parturition. *P < 0.05, mean ± SEM, Student’s t test.

Pregnancy failure in Hif2a-uKO mice is due to insufficiency of uterine factors.

P4 is a major ovarian factor essential for pregnancy, but the ovary produces other factors to support pregnancy. To evaluate the contribution of ovarian factors (including P4) to the implantation phenotype in Hif2a-uKO mice, we performed transplantation of WT ovaries into Hif2a-uKO mice or littermate controls by ovariectomy to normalize ovarian functions (Figure 4A) and evaluated the implantation phenotype of these mice. Normal implantation sites were observed in control mice with transplantation of WT ovaries on day 8 of pregnancy, while normal implantation sites were never observed in Hif2a-uKO mice that received WT ovaries (Figure 4, B and C). P4 supplementation did not recover implantation failure but did rescue decidualization in Hif2a-uKO mice with ovarian transplantation (Figure 4, B and C). These experiments using mice with ovarian transplantation did not rescue the similar phenotypes observed in those without ovarian transplantation, indicating that implantation failure in Hif2a-uKO mice is not derived from ovarian factors but from a uterine factor. Importantly, ovarian Hif2a mRNA levels were comparable between Hif2a-uKO mice and their controls (Figure 4D).

Figure 4. Implantation failure in Hif2a-uKO mice is not triggered by ovarian factors but by uterine factors.

Figure 4

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(A) A scheme of transplantation of WT ovaries into Hif2a-uKO mice or the littermate controls with ovariectomy. (B and C) Ovarian transplantation of WT ovaries in Hif2a-uKO mice did not rescue the phenotype of implantation failure observed in those without ovarian transplantation. In B, scale bar, 500 μm; arrowhead, an embryo; arrow, a destroyed embryo with blood cell infiltration; dec, decidua. In C, P > 0.05, mean ± SEM, Student’s t test. (D) Ovarian Hif2a mRNA levels were comparable between Hif2a-uKO mice and their controls. P > 0.05, n = 5, mean ± SEM, Student’s t test.

Uterine HIF2α confers appropriate homing of the implanting embryo in the crypt.

To examine the detailed mechanism of implantation failure in Hif2a-uKO mice, we evaluated blastocyst attachment on day 5 morning. By histological analysis of Hif2a-deficient uteri, we found that the positioning of the embryo attachment at the bottom of the endometrial crypt was impaired in Hif2a-uKO mice (Figure 5A and Supplemental Figure 5). COX2, a marker of embryo attachment reaction (34), was similarly expressed in the implantation sites of both Hif2a-uKO and control mice (Figure 5, B and C). The expression of LIF, a key regulator of embryo attachment (9, 10, 35), was significantly decreased in Hif2a-deficient uteri on day 5 morning (Figure 5D). In accordance with LIF reduction, activation of STAT3, a downstream signaling effector of LIF (11), was eliminated in the implantation sites of Hif2a-uKO uteri, as evident from phosphorylated STAT3 immunostaining (Figure 5E). To evaluate whether the decrease of LIF in Hif2a-deficient uteri leads to implantation failure, we injected recombinant LIF (20 μg/mouse on day 4) intraperitoneally in Hif2a-uKO mice in addition to P4 injection. Although LIF administration markedly normalized the positioning of embryo attachment to the crypt (Figure 5F and Supplemental Figure 5), it did not rescue pregnancy failure in Hif2a-uKO mice (Figure 5G). Since LIF is transcriptionally regulated by HIF (36, 37), uterine HIF2α may determine the positioning of the embryo through LIF induction.

Figure 5. Uterine HIF2α places the implanting embryo in the bottom of the endometrial crypt through induction of LIF.

Figure 5

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(A) The positioning of embryo attachment at the bottom of the endometrial crypt was impaired in Hif2a-uKO mice at 1000 hours on day 5. Scale bar, 100 μm; arrowhead, an embryo; s, stroma; le, luminal epithelium. (B and C) COX2, a marker of embryo attachment reaction, was similarly expressed in the implantation sites of both Hif2a-uKO and control mice. P > 0.05, n ≥ 5, mean ± SEM, Student’s t test. (D) The expression of LIF, a key regulator of embryo attachment, was decreased at the implantation site of Hif2a-uKO mice on day 5 morning. *P < 0.05, n ≥ 5, mean ± SEM, Student’s t test. (E) Activation of STAT3, a downstream signaling of LIF, was eliminated in the implantation site of Hif2a-uKO mice, as demonstrated by phosphorylated STAT3 immunostaining. (F) Intraperitoneal injection of recombinant LIF (20 μg/mouse on day 4) into Hif2a-uKO mice in addition to P4 injection normalized the position of embryo attachment to the bottom of the endometrial crypt on day 5 morning. (G) LIF administration could not rescue implantation failure in Hif2a-uKO mice on day 6 morning (arrow, a destroyed embryo with blood cell infiltration).

Persistent preservation of the intact luminal epithelium surrounding the embryo is associated with failed embryo invasion in Hif2a-uKO mice.

We next used histological analysis to evaluate the process of embryo invasion from day 5 to day 6 in Hif2a-uKO mice. We found that alignment of the luminal epithelium disappeared at the implantation site and that trophoblast invasion starts in control mice at 2100 hours on day 5 (Figure 6A). In contrast, alignment of luminal epithelium was intact at the implantation site and trophoblast invasion did not occur in Hif2a-uKO mice at the same time (Figure 6A). On day 6 morning, blood cell infiltration without the normal embryo structure was observed at the implantation site of Hif2a-uKO mice, whereas the stromal area with trophoblast invasion expanded in the controls (Figure 6A). At 1700 hours on day 5 just before initiation of embryo invasion, epithelial expression of E-cadherin, a tight junction regulator as well as a marker of epithelium, was eliminated. Epithelial alignment collapsed at the implantation sites of the controls, whereas both E-cadherin expression and epithelial alignment persisted in Hif2a-uKO mice (Figure 6B), suggesting that intact alignment of luminal epithelium is associated with failed embryo invasion.

Figure 6. Intact alignment of luminal epithelium surrounding the embryo is associated with failed embryo invasion in Hif2a-uKO mice.

Figure 6

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(A) Alignment of luminal epithelium disappeared at the implantation site, and trophoblast invasion started in the control mice at 2100 hours on day 5. In contrast, alignment of luminal epithelium was intact at the implantation site, and trophoblast invasion did not occur in Hif2a-uKO mice at the same time. On day 6 morning, destroyed embryo with blood cell infiltration was observed at the implantation site of Hif2a-uKO mice, while the stromal area with trophoblast invasion expanded in the controls. Scale bar, 200 μm; arrowhead, an embryo; s, stroma; le, luminal epithelium; arrow, a destroyed embryo with blood cell infiltration. (B) Expression of E-cadherin, a tight junction regulator as well as a marker of epithelium, was eliminated and epithelial alignment was collapsed at implantation sites of the controls, while both E-cadherin expression and epithelial alignment were persistent in Hif2a-uKO mice on day 5 evening.

Direct contact between embryo and uterine stroma is involved in embryonic cell survival and invasion.

Although the disappearance of the luminal epithelium attached to the embryo occurred in control mice on day 5 evening, apoptosis of the luminal epithelium was not observed at that time (Figure 7A), suggesting that apoptosis is not a key mechanism for the elimination of the luminal epithelium around the embryo. In contrast, apoptosis was observed in the trophoblast attached to the intact luminal epithelium in Hif2a-uKO mice, indicating programmed death in embryos that fail to initiate direct contact with endometrial stroma. We next hypothesized that epithelial mesenchymal transition (EMT) could be involved in the disappearance of the luminal epithelium around the embryo; we investigated this process using R26GRR/Ltf-Cre mice, which can be used for tracing cells with uterine epithelium origin. However, epithelium-derived cells were not observed in the uterine stroma surrounding the invading embryo (Supplemental Figure 6), suggesting that EMT does not play a key role in the elimination of the luminal epithelium around the embryo.

Figure 7. Direct contact between embryo and uterine stroma is involved in embryonic cell survival and invasion.

Figure 7

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(A) Apoptosis of luminal epithelium was not apparently observed on day 5 evening, when the disappearance of luminal epithelium attached to the embryo occurred in the control mice. In contrast, apoptosis was observed in the trophoblast attached to intact luminal epithelium in Hif2a-uKO mice. Scale bar, 200 μm, arrowhead, an embryo. (B) Transmission electron microscopic analyses of embryo-uterine interface at 1900 hours on day 5 demonstrated the newly-formed gaps between the stroma and the luminal epithelium (arrowhead) and the invading trophoblast into these gaps in the control mice, but not in Hif2a-uKO mice. Scale bar, 1 μm; s, stroma; tro, trophoblast; le, luminal epithelium. (C and D) Expression of MT2-MMP and LOX at the stroma of implantation sites collected by laser capture microdissection was downregulated in Hif2a-uKO mice compared with the controls *P < 0.05, n = 4, mean ± SEM, Student’s t test.

Transmission electron microscopic analyses of embryo-uterine interface at 1900 hours on day 5 showed newly formed gaps between the stroma and the luminal epithelium and the invading trophoblast within these gaps in the control mice, but not in Hif2a-uKO mice (Figure 7B), suggesting a role for uterine HIF2α in the detachment of the luminal epithelium from uterine stroma along with trophoblast invasion by direct contact with the stroma. Of note, this epithelial detachment was similarly observed in ICR mice on a different genetic background (Supplemental Figure 7), indicating that loss of the epithelial barrier is a common critical phenomenon during implantation.

In terms of the detachment of luminal epithelium from stroma, mRNA expression of membrane type 2 metalloproteinase (MT2-MMP) and lysyl oxidase (LOX) at the stroma of implantation sites collected by laser capture microdissection (LCM) was downregulated in Hif2a-uKO mice compared with the controls (Figure 7, C and D). We also confirmed the downregulation of these genes by in situ hybridization (Supplemental Figures 8 and 9). MT2-MMP and LOX are known transcription targets of HIF (38, 39). MT2-MMP, located on the cellular membrane, activates MMP2 outside the cell wall (40, 41) and breaks extracellular matrices composed of basement membrane together with the secreted MMP2, thereby serving as a regulator of basement membrane remodeling (42, 43). MT2-MMP also cleaves E-cadherin at the epithelial junction and regulates epithelial cell remodeling (44). LOX, secreted by the stroma, remodels the extracellular matrix by facilitating covalent cross-linking (45) and promotes cancer metastasis and invasion (45, 46). LOX and MT2-MMP in the stroma may cooperatively promote basement membrane remodeling and weaken the stroma-to-epithelium contact by changing the distribution of E-cadherin and the conformation of extracellular matrices between luminal epithelium and stroma. Our findings indicate that stromal Hif2a induces MMPs and LOX, which release the luminal epithelium from the stroma and promote trophoblast invasion.

Stromal Hif2a is critical for embryo invasion and activation of the PI3K-AKT pathway in the implanting embryo.

To clarify the importance of stromal HIF2α in embryo invasion, we generated mice with uterine stromal deletion of Hif2a (Hif2a-sKO mice, Hif2a-loxP/Amhr2-Cre). We confirmed that Hif2a mRNA levels were significantly reduced in the stroma of Hif2a-sKO mice (Supplemental Figure 10, A and B). As expected, the similar infertility phenotype with both impaired embryo invasion and persistent presence of luminal epithelium was observed in Hif2a-sKO mice (Figure 8, A–C), suggesting that stromal Hif2a controls embryo invasion. Moreover, we also generated mice with uterine epithelial deletion of Hif2a (Hif2a-eKO mice, Hif2a-loxP/Ltf-Cre) to evaluate the function of Hif2a in the luminal epithelium. Hif2a mRNA levels were significantly reduced in the luminal epithelium of Hif2a-eKO mice (Supplemental Figure 10, C and D). However, Hif2a-eKO mice demonstrated normal fertility (Figure 8D), emphasizing the significance of stromal HIF2α. Taken together, these findings indicate that stromal HIF2α detaches the luminal epithelium surrounding the embryo and activates an embryonic survival signal, which finally enables blastocyst invasion into the stroma.

Figure 8. Stromal Hif2a is critical for embryo invasion and PI3K-AKT pathway is activated in the implanting embryos.

Figure 8

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(A–C) Infertility phenotype with both impaired embryo invasion and persistent presence of luminal epithelium was observed in Hif2a-sKO mice. In A and B, *P < 0.05, mean ± SEM, Student’s t test. In C, scale bar, 200 μm; arrowhead, an embryo; s, stroma; arrow, a destroyed embryo with blood cell infiltration. (D) Hif2a-eKO mice demonstrated normal fertility. P > 0.05, mean ± SEM, Student’s t test. (E) Intensity of phosphorylated AKT staining was strong in the control trophoblast compared with Hif2a-uKO one. (F and G) Expression of VEGF and ADM at the stroma of implantation sites collected by laser capture microdissection was decreased in Hif2a-uKO mice. *P < 0.05, mean ± SEM, Student’s t test.

In accordance with invasion capacity of the embryo, intensity of phosphorylated AKT staining was stronger in the control trophoblast compared with the Hif2a-uKO trophoblast (Figure 8E). FOXO1 is a transcriptional factor regulated by the PI3K-AKT pathway (47). FOXO1 is phosphorylated by activated AKT and is translocated from the nucleus to the cytosol (47). Nuclear accumulation of FOXO1 was observed in the embryos attached to uteri of Hif2a-uKO mice, although it was stained inside the cytosol in the invaded embryo of control mice (Supplemental Figure 11). These findings indicate that direct contact between the embryo and uterine stroma is required for activation of the PI3K-AKT–FOXO1 pathway as an embryonic survival signal to avoid programmed embryonic death. VEGF, adrenomedullin (ADM), and LOX, which can activate the PI3K-AKT pathway and are regulated by HIF (48–50), are expressed in the uterine stroma and involved in the process of embryo implantation (15, 51–54). We found that mRNA expression of VEGF and ADM as well as LOX at the stroma of implantation sites collected by LCM technique was significantly decreased in Hif2a-uKO mice (Figure 7D and Figure 8, F and G), suggesting that HIF2α-regulated stromal VEGF, ADM, and LOX activate the trophoblast cell survival pathway in normal conditions.

Discussion

In the present study, we found that mice with deletion of uterine Hif2a showed infertility because of pregnancy failure. Deficiency of uterine Hif2a downregulated the expression of decidual luteotrophin, which supports decidual growth through ovarian P4 production, but P4 administration did not recover implantation failure and rescued only decidualization. Mice with uterine deficiency of Hif2a displaced the implanting embryo in the aberrant position because of decreased LIF expression, but LIF supplementation normalized only the position of embryo attachment and did not recover implantation. These findings indicate that uterine HIF2α contributes to successful implantation regardless of decidualization and the position of embryo attachment. More importantly, TEM revealed that the luminal epithelium attached to the embryo spontaneously detached from the stroma and that the embryo can directly contact the uterine stroma in control mice. Persistent alignment of the luminal epithelium surrounding the embryo with the inactivated embryonic survival signal blocked embryo invasion into the uterine stroma in Hif2a-uKO mice (Figure 9). Direct contact between the embryo and the uterine stroma might be involved in embryonic cell survival and invasion in Hif2a-uKO mice (Figure 9).

Figure 9. Potential pathways that contribute to embryo implantation through HIF.

Figure 9

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(A) Stromal HIF releases luminal epithelium from stroma through LOX and MT2-MMP, which permits direct contact between stroma and trophoblast. (B) Stromal HIF activates PI3K-AKT pathway as a trophoblast survival signal pathway through the induction of LOX, VEGF, and ADM, which promotes embryo invasion.

Since the surface of the endometrium is distant from uterine blood vessels, it is possible that oxygen concentration in the luminal epithelium and the stroma near embryos is relatively low compared with the inner endometrium and the myometrium (55). Therefore, it is estimated that the luminal epithelium before implantation is in a hypoxic state and that angiogenesis prominently occurs after implantation. After angiogenesis in implantation sites, oxygen concentration dynamically rises in the uterus. Previous studies have investigated the role of hypoxia in placental formation (56). On the other hand, few studies have focused on the role of hypoxia in the uterus during implantation. Hif1a and Hif2a were shown to be strongly expressed in the mouse uterus during embryo implantation in a previous report (15), and HIFα is functionally critical for successful embryo implantation in our study. Physiological uterine hypoxia during implantation may contribute to embryo implantation through HIF, although factors other than hypoxia, such as embryonic stimuli, may be associated with the induction of HIF.

P4 signaling in the uterus is essential throughout pregnancy, and decidual luteotrophin activates the corpus luteum to maintain luteal function. Luteotrophin is one example of molecular interactions from the uterus to the ovary in rodents. In humans, chorionic gonadotrophin supports luteal function instead of decidual factors, suggesting that maintenance of luteal function by positive feedback of implantation-derived factors may be common machinery for successful pregnancy in mammals. The current study showed that luteal support cannot rescue implantation failure in mice with uterine deletion of Hif2a. These data are in accordance with the clinical fact that many patients do not become pregnant through IVF-ET treatment, even after sufficient luteal support. Dysregulation of HIF may be involved in recurrent implantation failure in humans.

Decreased LIF expression and aberrant position of the implantation site were observed in Hif2a-uKO mice during embryo attachment. Since a previous report has demonstrated that HIF2α, not HIF1α, transcriptionally induces LIF expression in human colon cancer cell lines (37), it is possible that uterine HIF2α induces LIF via transcriptional regulation in mice. In mouse embryonic stem cells, hypoxia-induced HIF1α directly suppresses expression of the LIF receptor through transcriptional regulation and inactivates LIF-STAT3 signaling (36). These findings indicate that HIF1α and HIF2α regulate LIF-STAT3 signaling in different and complex detail. As for the uterus, HIF2α may dominantly activate LIF-STAT3 signaling.

Disappearance of the luminal epithelium might be an important process in embryo invasion. In addition to apoptosis, entosis and phagocytosis of the luminal epithelium by the trophoblast after attachment have been reported (57, 58). In control mice, apoptotic cells in the luminal epithelium at the implantation site are rarely observed; therefore, apoptosis as the cause behind the disappearance of the luminal epithelium can be ruled out. Similarly, entosis of the luminal epithelium was not observed in either Hif2a-uKO or the control mice. Our observation demonstrated that EMT from the luminal epithelium to the stroma did not occur during implantation in mice. We discovered intermittent gaps between the luminal epithelium and the stroma that lead to the detachment of the luminal epithelium, which might be a critical process for embryo invasion; these processes are impaired in Hif2a-uKO mice.

In concurrence with the detachment of the luminal epithelium from the stroma just before embryo invasion, the trophoblast enters the gap. Previous literature suggested the possibility that uterine stromal cells actively disrupt the epithelial basement membrane (59). The stroma produces several soluble factors, such as VEGF and ADM, to activate the PI3K-AKT–FOXO1 pathway as an embryonic survival signal and to promote trophoblast invasion into the stroma. MT2-MMP activates MMP2, breaks the extracellular matrix of basement membrane, and regulates epithelial E-cadherin distribution (40–42, 44). LOX debilitates the extracellular matrix of the basement membrane (45, 46). Therefore, LOX and MT2-MMP may cooperatively support remodeling of the basement membrane between the uterine stroma and the luminal epithelium. Since it remains unclear how the luminal epithelium detaches from the stroma and how embryonic activation occurs following invasion, further investigation is needed.

Dynamic molecular changes following embryo attachment are very complicated, and uterine HIF plays various roles in pregnancy. This study revealed that uterine HIF2α is involved in a series of implantation processes, embryo attachment, decidualization, and especially, embryo invasion. The mechanism of embryo invasion has been scarcely reported, and we believe our results provide new evidence that stromal HIF2α controls embryo invasion. The association between human implantation failure and HIF function needs to be clarified in future studies.

Methods

Mice.

WT mice (C57BL/6J and ICR, Japan SLC), Hif1a-floxed mice (16, 60), Hif2a-floxed mice (60, 61) (Jackson Laboratories), Ltf-Cre mice (21), Amhr2-Cre mice (19), Pgr-Cre mice (18), and Rosa26 Cre-reporter knock-in mice (R26GRR mice) (62) were used in this study. R26GRR mice were provide by Ken-ichi Yagami (University of Tsukuba, Tsukuba, Japan) and RIKEN BRC (Tsukuba, Japan). Ltf-Cre mice were provided by Sudhansu K. Dey (Cincinnati Children’s Hospital Medical Center, Cincinnati, OH, USA). Amhr2-Cre mice were provided by Richard Behringer (The University of Texas MD Anderson Cancer Center, Houston, TX, USA). Pgr-Cre mice were provided by Francesco J. DeMayo (National Institute of Environmental Health Sciences, Research Triangle Park, NC, USA). Ltf, Amhr2, and Pgr are expressed in the luminal epithelium, the stroma/myometrium, and all the layers of uterus, respectively. Therefore, Ltf-Cre, Amhr2-Cre, and Pgr-Cre mice have the specific expression of Cre recombinase in the uterine epithelium, the stroma, and whole uterus, respectively (63). Mice with deletion of Hif1a or Hif2a in whole uterus (Hif1a-uKO mice and Hif2a-uKO mice, respectively) were generated by crossing Pgr-Cre with Hif1a- or Hif2a-floxed mice. Mice with deletion of Hif2a in the uterine epithelium or in the stroma (Hif2a-eKO mice and Hif2a-sKO mice, respectively) were generated by crossing Hif2a-floxed mice with Ltf-Cre or Amhr2-Cre mice. Cre-negative homozygous littermates for the conditional alleles were used as controls. R26GRR mice exhibit green emission before Cre-mediated recombination and red emission after the recombination. For epithelial cell lineage tracing in the uterus, we generated R26GRR/Ltf-Cre mice, which have red fluorescence in the uterine epithelium-derived cells (63).

Analysis of pregnancy events.

For evaluation of pregnancy phenotypes, 2- to 5-month-old female mice of each line were mated with fertile males, and day 1 of pregnancy was defined as the day when we recognized vaginal plug. Ovulation, fertilization, preimplantation embryo development, and implantation were assessed as described (64). To treat Hif2a-uKO mice with exogenous P4 and recombinant LIF protein, daily subcutaneous injections of P4 (2 mg/mouse/day) from day 2 of pregnancy and intraperitoneal injection of recombinant LIF (20 μg/mouse) at 0900 hours on day 4 of pregnancy were performed, respectively. Recombinant LIF was produced using LIF expression vector as previously described (65, 66). The LIF expression vector was provided by Eiichi Hondo (Nagoya University, Japan).

Ovarian transplantation.

Ovarian transplantation was performed as described (67). Female mice were anesthetized, the ovarian fat pad with the ovary was exteriorized, the bursa opened, and ovaries removed. The excised ovaries were held briefly in M2 medium and grafted back into the bursal cavity of recipient mice. More than 3 weeks after transplantation, the mice with ovary transplantation were mated with fertile WT males.

H&E staining and immunostaining.

Frozen sections (12 μm), or formalin-fixed paraffin-embedded sections (6 μm) were subjected to H&E staining and immunohistochemistry. For immunostaining, antibodies against Ki67 (SP6, Thermo Fisher Scientific), and phosphorylated STAT3 (pSTAT3; EP2147Y, Abcam), COX2 (AA570-598, Cayman Chemical), E-cadherin (24E10, Cell Signaling Technology), phosphorylated AKT (pAKT; D9E, Cell Signaling Technology), and FOXO1 (C29H4, Cell Signaling Technology) were used.

Fluorescence assay.

Frozen sections (12 μm) were subjected to immunofluorescence. Alexa Fluor 488–conjugated anti-rat immunoglobulin G and Alexa Fluor 555–conjugated anti-rabbit immunoglobulin G were used for protein detection, and nuclear staining was performed with 4, 6-diamidino-2-phenylindole using a fluorescence microscope (DM5000B and HyD, Leica Microsystems GmbH).

Measurement of serum P4 and E2 levels.

Blood samples from mice were collected on the indicated days of pregnancy. Serum was separated by centrifugation (850g for 15 minutes) and stored at –80°C until analysis. Serum P4 levels were measured by Progesterone EIA kit (Cayman Chemical), and E2 levels were measured by Estradiol ELISA kit (CalBiotech).

In situ hybridization.

Sense or antisense DIG-labeled cRNA probes for Prl3c1, MT2-MMP, and LOX were generated using appropriate polymerases from respective cDNAs as previously described (68). Specific RNA probes were prepared by DIG Labeling Kit (Roche Diagnostics GmbH) and paraffin sections (6 μm) were incubated with the probes and colored using NBT/BCIP solution (Roche Diagnostics GmbH) counterstained by methyl green solution (Wako Pure Chemical Industries).

Laser capture microdissection.

LCM was performed as previously described (7). Frozen sections (20 μm) were mounted on polyethylene naphthalate slides (Leica Microsystems), fixed in cold acetone, stained in 0.05% toluidine blue, and dehydrated in ethanol. The target regions in the sections were microdissected with a LMD7000 system (Leica Microsystems). The luminal epithelium and stroma close to a crypt at the antimesometrial pole were dissected out from the uteri by LCM.

RT-quantitative PCR (qPCR).

For conventional RNA analyses, total RNA extraction from frozen whole tissues was performed as previously described (7). As for LCM samples, the extracted RNA was amplified using an Ovation PicoSL WTA system V2 (NuGEN Technology), and qPCR was performed as previously described (7). A housekeeping gene (β-actin [Actb]) was used as an internal standard for normalizing the relative mRNA expression. Sequences of qPCR primers are listed in Supplemental Table 1.

TUNEL assay.

In situ detection of apoptosis was performed using the In Situ Cell Death Detection Kit (Roche) following the manufacturer’s instructions. The signal was detected using a confocal laser scanning microscope (LSM700, Carl Zeiss Microscopy GmbH).

Transmission electron microscopy.

Uterine tissues were fixed with a buffered mix of 2.5% glutaraldehyde and 1.6% paraformaldehyde in phosphate buffer (0.1 M, pH 7.4) for 17 hours, and postfixed with 0.1 M cacodylate buffer and 1% osmium tetroxide for 30 minutes, dehydrated, replaced with propylene oxide, embedded in epoxy resin, and hardened at 60°C for 24 hours. The tissues were sectioned using a diamond knife at a thickness of 60–70 nm, mounted onto single slot copper grids with a support film, stained with lead citrate and uranyl acetate, and imaged at 80 kV in a transmission electron microscope (JEM-1011, JEOL).

Statistics.

Statistical analyses were performed using a 2-tailed Student’s t test and Fisher’s exact probability test. A value of P < 0.05 was considered statistically significant.

Study approval.

All mice used in this investigation were housed in the University of Tokyo Animal Care Facility according to the institutional guidelines for the use of laboratory animals. All the animal experiments in the present study were reviewed and approved by the animal experiment committee of the University of Tokyo (Tokyo, Japan).

Author contributions

YH and TSF designed the study. LM, YH, TSF, TT, SA, TH, and SI performed experiments and collected the data. NT, HF, RSH, MM, HH, MSK, and TF provided technical assistance for the experiments. LM, YH, and TSF analyzed the data. YH, TSF, NT, RSH, and YO discussed and interpreted the results. YH and TSF wrote the manuscript. RSH critically reviewed the manuscript. YH supervised the study.

Supplementary Material

Supplemental data
jci-128-98931-s404.pdf (995.2KB, pdf)

Acknowledgments

We thank Ken-ichi Yagami (University of Tsukuba) and RIKEN BRC through the National Bio-Resource Project of the MEXT, Japan, for providing R26GRR mice, Sudhansu K. Dey (Cincinnati Children’s Hospital Medical Center) for providing Ltf-Cre mice and reviewing the manuscript critically, Richard Behringer (The University of Texas MD Anderson Cancer Center) for providing Amhr2-Cre mice, Francesco J. DeMayo (National Institute of Environmental Health Sciences) for providing Pgr-Cre mice, Eiichi Hondo (Nagoya University) for providing the LIF expression vector, and Katie A. Gerhardt (Cincinnati Children’s Hospital Medical Center) for efficient editing of the manuscript. This work was supported by grants from the Japan Agency for Medical Research and Development (AMED) PRIME (JP18gm5910010), the Japan Society for the Promotion of Science, KAKENHI (16H04679, 16K15701, 16K15700, 16H05469, 15K10660, 15H04979, 17K16833, 17H06640, 15K15596, 16K10668), and the Takeda Science Foundation.

Version 1. 06/18/2018

Electronic publication

Version 2. 06/26/2018

Labeling errors corrected in Figure 1, C and D

Version 3. 07/02/2018

Print issue publication

Footnotes

Conflict of interest: The authors have declared that no conflict of interest exists.

Reference information: J Clin Invest. 2018;128(7):3186–3197.https://doi.org/10.1172/JCI98931.

Contributor Information

Leona Matsumoto, Email: leona-0525@goo.jp.

Yasushi Hirota, Email: yhirota-tky@umin.ac.jp.

Tomoko Saito-Fujita, Email: tomoafrica072573@gmail.com.

Norihiko Takeda, Email: ntakeda-tky@umin.ac.jp.

Tomoki Tanaka, Email: tomokitanakatomoki@gmail.com.

Takehiro Hiraoka, Email: t_hiraoka1985@yahoo.co.jp.

Shun Akaeda, Email: shakaeda@gmail.com.

Hidetoshi Fujita, Email: fujitam@tokyo-med.ac.jp.

Ryoko Shimizu-Hirota, Email: rsh_keio@yahoo.co.jp.

Shota Igaue, Email: shoutaigaue8848@gmail.com.

Mitsunori Matsuo, Email: machio1128@hotmail.co.jp.

Hirofumi Haraguchi, Email: haraguchi-tky@umin.ac.jp.

Mayuko Saito-Kanatani, Email: mayuko3110@gmail.com.

Tomoyuki Fujii, Email: fujiit-tky@umin.org.

Yutaka Osuga, Email: yutakaos-tky@umin.ac.jp.

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