- Open Access
Regulated expression of matrix metalloproteinases, inflammatory mediators, and endometrial matrix remodeling by 17beta-estradiol in the immature rat uterus
Reproductive Biology and Endocrinology volume 7, Article number: 124 (2009)
Administration of a single physiological dose of 17beta-estradiol (E2:40 microg/kg) to the ovariectomized immature rat rapidly induces uterine growth and remodeling. The response is characterized by changes in endometrial stromal architecture during an inflammatory-like response that likely involves activated matrix-metalloproteinases (MMPs). While estrogen is known as an inducer of endometrial growth, its role in specific expression of MMP family members in vivo is poorly characterized. E2-induced changes in MMP-2, -3, -7, and -9 mRNA and protein expression were analyzed to survey regulation along an extended time course 0-72 hours post-treatment. Because E2 effects inflammatory-like changes that may alter MMP expression, we assessed changes in tissue levels of TNF-alpha and MCP-1, and we utilized dexamethasone (600 microg/kg) to better understand the role of inflammation on matrix remodeling.
Ovariectomized 21 day-old female Sprague-Dawley rats were administered E2 and uterine tissues were extracted and prepared for transmission electron microscopy (TEM), mRNA extraction and real-time RT-PCR, protein extraction and Western blot, or gelatin zymography. In inhibitor studies, pretreatment compounds were administered prior to E2 and tissues were harvested at 4 hours post-hormone challenge.
Using a novel TEM method to quantitatively assess changes in stromal collagen density, we show that E2-induced matrix remodeling is rapid in onset (< 1 hour) and leads to a 70% reduction in collagen density by 4 hours. Matrix remodeling is MMP-dependent, as pretreatment with batimastat ablates the hormone effect. MMP-3, -7, and -9 and inflammatory markers (TNF-alpha and MCP-1) are transiently upregulated with peak expression at 4 hours post-E2 treatment. MMP-2 expression is increased by E2 but highest expression and activity occur later in the response (48 hours). Dexamethasone inhibits E2-modulated changes in collagen density and expression of MMPs although these effects are variable. Dexamethasone upregulates MMP-3 mRNA but not protein levels, inhibiting E2-induced upregulation of MMP-7, and -9, and MCP-1 mRNA and protein but not inhibiting the hormone-induced increase in TNF-alpha mRNA.
The data demonstrate that E2-regulated endometrial remodeling is rapid in onset (<1 hour) and peak expression of MMPs and inflammatory mediators correlates temporally with the period of lowest stromal collagen density during uterine tissue hypertrophy.
The ovariectomized (OVX) immature rat has been used extensively to study hormone-specific regulatory processes in the mammalian uterus. In this model, administration of a single physiological dose of 17β-estradiol (E2; 40 μg/kg) induces a biphasic uterine growth response, characterized by rapid tissue hypertrophy followed by hyperplasia. The early hypertrophic growth phase peaks approximately 4 h after E2 administration and is characterized by extensive collagen matrix remodeling of the endometrial stroma . The controlled degradation and repair of the stromal extracellular matrix is a necessary component of a variety of normal reproductive processes, including endometrial cycling [2–4], implantation , and pregnancy , and involves regulated expression and activity of proteolytic enzymes including the matrix metalloproteinases (MMPs) by steroid hormones. Hormone-induced regulation of MMP expression is complex and appears to involve cell-type specific changes in expression of local paracrine mediators as well as direct and indirect effects on mRNA transcription via activated receptors.
Matrix metalloproteinases comprise a family of related enzymes, each of which can degrade at least one component of the extracellular matrix, consisting of numerous types of collagen, gelatin, elastin, fibronectin, and laminin, among others [reviewed in . In addition, MMPs have been shown to act on non-matrix substrates by modifying and/or activating other MMPs [8–10], growth factors , cytokines [12, 13], chemokines [14, 15], and other growth regulators that are matrix-bound or present on the cell surface [16, 17]. Expression is controlled at the level of transcription in response to proto-oncogenes and exogenous signals, including hormones [18, 19], cytokines [20, 21], and growth factors . At the post-translational level, MMPs in the extracellular space are regulated by endogenous inhibitors, including a group of tissue-derived inhibitors termed TIMPs (tissue inhibitors of metalloproteinases) [7, 23]. Furthermore, most MMPs are secreted as inactive proenzymes (proMMPs), also known as zymogens, requiring the cleavage of a specific propeptide domain for activation . Although the mechanisms governing proMMP activation are not completely understood, evidence suggests that inflammatory mediators function to regulate MMP activity in the extracellular space [4, 9, 20, 25].
Many studies have shown that administration of physiological dose level of estrogen to the immature or OVX rodent induces an acute inflammatory-like response, including the coordinated influx of blood-born macrophages, neutrophils, and eosinophils into the uterine endometrial stroma [26–31]. The pro-inflammatory and growth effects of E2 are antagonized by co-administration of anti-inflammatory agents, including the synthetic glucocorticoid dexamethasone [32–36] and the steroid hormone progesterone (P4) . Evidence suggests that the estrogen-mediated infiltration of inflammatory cells into the endometrial stroma may lead to activation of extracellular proMMPs, which have been shown to colocalize with leukocytes in the mouse  and human  endometrium. Proteinases released by inflammatory cells, including tryptase, chymase, leukocyte elastase, and MMPs, have been shown to activate proMMPs in culture [8, 9, 39, 40], while metabolites and oxidants generated by inflammatory cells may also regulate MMP activation [41–43]. These studies and others suggest an important role for inflammatory mediators in the activation of proMMPs in the endometrial extracellular matrix. In turn, activated MMPs have been shown to modulate inflammatory processes, including the activity and mobilization of chemokines and cytokines [44, 45] thereby regulating the further influx of inflammatory cells [11–16]. Therefore, MMPs and inflammatory mediators are components of a complex network governing uterine growth and remodeling, as well as other normal and disease processes.
In the current study, we have developed a novel method to quantitatively analyze transmission electron micrographs to assess estrogen-induced endometrial collagen remodeling in the OVX immature rat model along a time course that includes both the hypertrophic and hyperplastic phases of uterine growth. Using matrix collagen density as a quantitative and reliable endpoint, we specifically determined that estrogen-induced stromal matrix remodeling is MMP-dependent. We further characterized hormone-regulated expression of MMP-3 (stromelysin-1), MMP-7 (matrilysin), MMP-2 (gelatinase A), and MMP-9 (gelatinase B), four metalloproteinases believed to function prominently in various reproductive processes [6, 38], as well as the inflammatory mediators TNF-α and MCP-1 along an extended post E2-treatment time course to assess changes in tissue protease and inflammatory potential through both the early hypertrophic and later hyperplastic growth phases. In addition, we have investigated the effect of the anti-inflammatory synthetic glucocorticoid dexamethasone on E2-induced stromal matrix remodeling and MMP and inflammatory mediator expression to better understand the role of inflammation in the tissue pathway linking estrogen receptor activation to changes in tissue ultrastructure necessary for uterine growth and remodeling.
Animal treatments and tissue preparations
All animal experiments were performed in compliance with NIH standards as specified in the Guide for Care and Use of Laboratory Animals (copyright 1996, National Academy of Sciences). Female Sprague-Dawley rats (Ace Animal Corp., Boyertown, PA) were ovariectomized at 21 days of age and allowed to recover for 3-5 days. For E2 time course experiments, animals were administered a single physiological dose of E2 (40 μg/kg in a 0.9% NaCl, 0.4% EtOH vehicle) by intraperitoneal (i.p.) injection at the indicated time intervals prior to tissue collection at necropsy. This in vivo dose level of E2 has been shown to induce changes in uterine wet weight, tissue architecture, and gene expression characteristic of estrogen receptor activation [1, 46–48]. For all other experiments, animals were i.p. administered a single 40 μg/kg bolus of E2 4 h prior to tissue harvest, while control animals received vehicle only in all studies. Batimastat was administered i.p. at a dose level (BB-9; 40 mg/kg in a 1× PBS, 0.1% Tween-20 vehicle) shown to be effective at inhibiting MMPs in vivo  4 h prior to E2 or saline control. Dexamethasone was administered i.p. at a dose level of 600 μg/kg in a 0.9% NaCl, 10% EtOH vehicle that has been previously used in rodent studies to assess in vivo steroid specific responses in the uterus [46–48]. Animals were treated twice with dexamethasone (600 μg/kg) at 20 and 4 h before E2 or saline control administration to elicit both early and late gene effects of the activated glucocorticoid receptor (GR) that may affect uterine responsiveness to E2 via genomic or nongenomic mechanisms. Batimastat was generously provided by GlaxoSmithKline, while other treatment compounds were obtained from Sigma-Aldrich (USA). Dose levels of all compounds were administered at injection volumes of 1 ml/100 g body weight. Inhibitor compounds were administered i.p., with control animals receiving the corresponding vehicle solution i.p. at the same treatment times as inhibitor injections.
For uterine tissue collection at necropsy, animals were euthanized by decapitation on the same day in accordance with the specific treatment time interval and the tissue was stripped of fat and mesentery, weighed, and the horns separated. One horn from each animal was flash frozen in liquid N2 and stored at -80°C for later RNA purification. For protein analyses, two isolated horns from different animals were pooled and fresh-processed for total protein extraction. For transmission electron microscopy analyses, tissues were immediately fixed in 2.5% glutaraldehyde in 0.1 M phosphate buffer.
Transmission electron microscopy (TEM)
Individual uteri were fixed in 2.5% glutaraldehyde in 0.1 M phosphate buffer, pH 7.4, and 2 mm-cross sections of each uterine horn were cut and incubated overnight at 4°C in 2.5% glutaraldehyde in 0.1 M phosphate buffer. Glutaraldehyde buffer was removed, and the samples were rinsed three times (15' each) in 0.1 M phosphate buffer. Samples were incubated in 1% osmium in 0.1 M phosphate buffer, rinsed, and dehydrated in a series of ethanol washes. Samples were incubated twice for 5' in propylene oxide and then transferred to a rotor for 1 h at room temperature in a 1:1 mixture of propylene oxide and epon [47% Embed 812, 31% DDSA (dodenyl succinic anhydride), 19% NMA (nadic methyl anhydride), 3% BDMA (benzyldimethylamine)], followed by an overnight incubation in 1:2 propylene oxide-epon, and finally 100% epon for 2-3 hrs. Individual uterine samples were embedded in 100% epon in silicon flat embedding molds, and capsules were polymerized in a 60°C oven for over 48 hrs. Ultrathin transverse sections (70 nm) were prepared using a diamond knife (Diatome) on a MT 6000-XL ultramicrotome, captured on 300-mesh copper grids, and stained with 2% uranyl acetate. All reagents and materials were obtained from Electron Microscopy Sciences (Hatfield, PA).
A minimum of 3 blocks with tissue from different areas along the length of each uterine horn were chosen at random from a total pool of 5-6 blocks and were used to prepare ultrathin sections to provide a comprehensive survey of whole organ ultrastructure representatively. A minimum of 6 transverse sections were prepared per tissue block and viewed using a Hitachi 7600 microscope fitted with an AMT digital camera. Visual analyses and micrograph surveys were restricted to the endometrial stromal compartment at a minimum of 3 random sites within the endometrium of each section so as to avoid bias. At each random site within the endometrial stromal matrix compartment, 3-6 digital photomicrographs at 12,000× magnification were taken. For quantitative analysis of collagen density, the full area of photomicrographs was digitally fitted with an 8 × 8 square grid containing a total of 64 cross-points, and each cross-point was evaluated to determine the structure that it overlaid. Image J software (NIH) was used to quantify the total number of crossbars landing on collagen fibrils (positive hits), and the values were expressed as a ratio to the total number of crossbars to determine a percent matrix density volume for each photomicrograph. Stromal areas with a high percentage of collagen fibrils cut in transverse were selected to best ensure that quantitative crossbar analysis was not significantly affected by dramatic differences in collagen fiber orientation. A total of 36-75 micrographs were analyzed per time point or treatment condition. Values for all micrographs for each animal were averaged, and statistical differences between averages of each time point or treatment group were analyzed using one-way ANOVA. Error bars on graphs represent standard error, and a standard P value of ≤ 0.05 was considered significant.
RNA isolation and quantitative real-time PCR
For TaqMan® quantitative real-time PCR analyses of mRNA levels, total RNA was prepared individually from the uterus of each rat. Each uterus was disrupted for 2-3 minutes in 0.75 mL QIAzol lysis reagent (Qiagen, Valencia, CA) using a 5 mm bead in a TissueLyser (Qiagen-Retsch). The homogenate was subjected to a 0.2 mL chloroform extraction and centrifugation at 4°C for 15 min at 20,000 × g, and 0.35 mL aqueous phase was collected for RNA purification using an RNeasy kit (Qiagen) according to the manufacturer's protocol. Residual genomic DNA was removed by on-column RNase-free DNase treatment during RNA purification, and the RNA concentration was adjusted to 0.05 mg/mL. Messenger RNA levels were analyzed using quantitative real-time PCR on an ABI Prism 7900 Sequence Detection System and TaqMan® gene expression assays (Applied Biosystems, Foster City, CA) for MMP-2 (Rn01538174_m1), MMP-3 (Rn00591740_m1), MMP-7 (Rn00563467_m1), MMP-9 (Rn00579162_m1), TNF-α (Rn01753871_m1), MCP-1 (Rn01456716_g1) and eukaryotic 18s rRNA (Hs99999901_s1). To compare mRNA expression levels among samples, mRNA for each gene of interest was normalized to the expression of a housekeeping gene, 18s rRNA, and differences in gene expression were calculated as a fold change to the mean of the vehicle group.
Protein extraction, SDS-PAGE, and immunoblotting
Detailed methods for protein extraction, SDS-PAGE, and immunoblotting have been described previously . In brief, 2-3 uterine tissues were pooled and homogenized in 50 mM Tris pH 7.5, 150 mM NaCl, 1 mM CaCl2, 0.05% Brij 35, 1 mM PMSF, and 10 μg/ml leupeptin using a polytron homogenizer (Brinkman Instruments, Westbury, NY). Homogenates were centrifuged at 15,000 × g for 30 minutes at 4°C and the supernatants removed and protein quantified. Extracted total protein (20 μg) samples were loaded into the wells of a pre-cast gel (4-20% Tris-HCl; BioRad, Hercules, CA) and resolved by electrophoresis in a Mini-Protein II module (BioRad) according to the manufacturer's protocol. Resolved proteins were transferred to an Immobilon-P membrane (Millipore, Billerica, MA), which was blocked (5% BSA in 1× Tris-buffered saline + 0.1% Tween-20 + 2% normal goat serum) and then incubated in a 1:2000 dilution of affinity-purified polyclonal rabbit anti-MMP-2 IgG (Novus Biologicals, Littleton, CO; #NB200-193), anti-human MMP-7 IgG (Lifespan Bioscience, Seattle, WA; #LS-B1237), anti-MMP-3 IgG (Abcam, Cambridge, MA; #ab53015), anti-MMP-9 IgG (Abcam #ab7299), anti-TNF-α IgG (Cedarlane, Burlington, NC; #CL9572AP), anti-MCP-1 IgG (Millipore, Billerica, MA; #AB1834P) or monoclonal mouse anti-β actin IgG (Abcam #ab6276) overnight in blocking solution at 4°C with gentle agitation. Membranes were washed and incubated in a 1:10,000 dilution of secondary HRP-conjugated goat α-rabbit IgG or α-mouse IgG (Jackson Immunologicals, West Grove, PA) in blocking solution and then washed and transferred to a solution of SuperSignal Substrate reagents (Pierce/Thermo Scientific, Rockford, IL) for enhanced chemiluminescent signal detection, imaged, and analyzed using the FluorChem SA system (Alpha Innotech, San Leandro, CA) and AlphaEase FC software. Band intensities were measured as integrated density volumes (IDV) and expressed as % of control lane values for comparisons between treatment groups. Specificity of bands identified using primary antibodies was confirmed by exposing sample blots to either 2% normal goat serum alone, secondary goat HRP-conjugated antibody in the absence of primary antibody, or normal rabbit IgG (Jackson Immunologicals) only prior to secondary antibody incubation.
Extracted total protein (20 μg) samples were mixed 1:1 with zymography sample buffer (Bio-Rad) and incubated at room temperature for 10 min. Samples were loaded into the wells of a pre-cast gel (10% gelatin, BioRad) and resolved by electrophoresis in a Mini-Protein II module (BioRad) under non-reducing conditions. Active human MMP-2 (Calbiochem/EMD Biosciences, Gibbstown, NJ; #PF023) was loaded in one lane of the gel as a control. After electrophoretic separation, the gel was washed twice for 30 minutes each in 1× renaturation buffer (Bio-Rad) at room temperature (RT) with gentle agitation and then incubated in 1× development buffer (Bio-Rad) for 30 minutes at RT. Fresh development buffer was added and the gel incubated at 37°C for 18-24 hours. Developed gels were stained with Coomassie Brilliant Blue R-250 (0.5% in 30% methanol, 10% acetic acid) for 30 minutes at RT. The gel was destained in 30% methanol, 10% acetic acid until clear bands representing proteolytic areas were visualized. Gels were visualized with the FluorChem SA system (Alpha Innotech) and analyzed using AlphaEase FC software. Band intensities were measured as integrated density volumes (IDV) and expressed as % of control lane values for comparisons between treatment groups.
Data is represented as the average ± standard error of the mean (SE). Data were analyzed initially via one-way ANOVA followed by Tukey's Honestly Significant post-comparison test to assess differences between treatment groups. P values ≤ 0.05 were considered significantly different.
E2induces rapid remodeling of uterine stromal matrix ultrastructure
To better characterize previously described E2-induced changes in uterine stromal collagen matrix remodeling , we developed a novel method to quantitatively assess changes in collagen fibril density using a grid overlay analysis of TEM photomicrographs (as described in Methods). This method establishes matrix density as a quantifiable endpoint for studies aimed at assessing changes in activity of matrix processing enzymes, including the MMPs, induced by bioactive compounds and inhibitors in a very precise and direct manner. We assessed collagen matrix density using micrographs prepared from uterine sections along the entire length of the uterine horn to best represent whole tissue architecture changes and over an extended time course after administration of a single physiological dose of E2 (40 μ/kg) to study stromal collagen architecture throughout both the early hypertrophic and latter hyperplastic phases of uterine growth. Qualitative assessment of micrographs indicates that a dense irregular organization of collagen fibers is clearly observed within saline-treated tissues (0 h), but this organization rapidly disappears such that a significant difference is evident within 45 minutes of hormone administration. Matrix density reaches a low point by 4 h when only a few isolated fibrils within the stromal compartment remain (Figure 1). Quantitative analysis of collagen matrix density supports a significant decrease (~30% less than 0 h-saline levels) within 45 minutes post-E2 treatment and a continual decline over time, reaching its lowest value (~70% less than 0 hr) at 4 h and remaining low through the 24 h treatment interval (Figure 2).
Stromal matrix remodeling is dependent upon activity of MMPs
Upon establishing a quantitative method to assess changes in stromal matrix density, we assessed effects of a broad-range hydroxamate inhibitor of MMPs, batimastat (40 mg/kg), on E2-induced matrix remodeling in OVX animals (Figure 3) to better characterize the role of activated MMPs in hormone-stimulated collagen reorganization. Matrix density was analyzed in saline- or batimastat-pretreated animals 4 h after E2 administration, the time point at which collagen density was observed to be at its lowest after hormone treatment (Figures 1 and 2). Transmission electron microscopy assessment (Figure 3) shows that batimastat alone has no effect on the stromal collagen network (Sal-Sal vs. Bat-Sal), but overall collagen density in batimastat-pretreated E2-induced animals (Bat-E2) is significantly higher (~4-fold) compared to those receiving saline pretreatment and E2 treatment (Sal-E2), clearly indicating that E2-induced uterine matrix remodeling is, at least in part, dependent upon activated MMPs.
E2induces transient upregulation of uterine MMP mRNA and protein
While effects of ovarian hormones on uterine MMP expression have been studied under a variety of conditions in the rodent and human, we chose to fully characterize temporal changes in expression of MMP-2, MMP-3, MMP-7, and MMP-9 induced specifically by E2 in the immature OVX rat and to examine any correlation in enzyme levels with the time course of collagen matrix remodeling. The enzymes surveyed include those known to be expressed by uterine epithelial (MMP-7) as well as stromal (MMP-2, MMP-3 and MMP-9) cells . In addition, collagen substrates for MMP-2 (I, III, IV, V, VII, X, XI), MMP-3 (II, III, IV, V, VII, IX, X), MMP-7 (I, IV, X), and MMP-9 (IV, V, VII, XIV) have been characterized in vitro . Levels of mRNA and protein for these MMPs were assessed following saline treatment (0 h) and at 5 intervals (4-72 h) post-E2 administration. While mRNA transcripts for all MMPs analyzed (Figure 4A) are detected in the uterus in saline control tissues (0 h), significant increases in transcript levels are induced within 4 h by E2 treatment for MMP-3, MMP-7, and MMP-9. Of these enzymes, the fold induction (~150-fold) for MMP-7 is clearly the most robust (Figure 4). In contrast, levels of MMP-2 mRNA do not increase until later in the time course, with peak fold induction (~7 fold) occurring at 48 h post-hormone administration, thereby placing it on a different time line of regulation compared to MMP-3, MMP-7, and MMP-9. Upregulation of mRNA for all enzymes is transient, as transcript levels decline significantly and return to control values by 72 h.
Western blot analyses (Figure 4B) were completed to determine if uterine MMP protein changes in correlation with the mRNA induction profiles for each enzyme. MMP-2, MMP-3, and MMP-9 are detected in saline tissues and increase after E2 treatment in accord with peak changes in mRNA for each gene. Levels of the latent (~72 kDa) form of MMP-2 increase significantly within 4 h, but peak changes in latent and active (~64 kDa) protein do not occur until ~24-48 h post-E2 treatment (Figure 4B), which correlates temporally with the peak in mRNA content (Figure 4A). Tissue levels of MMP-3 (~62 kDa) and MMP-9 (~90 kDa) increase within 4 h of E2 treatment (Figure 4B) in conjunction with changes in mRNA (Figure 4A). While levels of MMP-9 decline over time, reaching control values within 24 h, MMP-3 protein remains elevated through 72 h, although the mRNA for this enzyme reaches control levels within 24 h after hormone administration (Figure 4A). This indicates that MMP-3 protein is temporally stabilized and levels do not decline to those observed prior to E2 stimulation. Latent MMP-7 (~29 kDa) is not detectable in control tissues (0 h), but levels of the enzyme increase significantly by 4 h post-E2 treatment, then decline over time to return to control values by 48 h (Figure 4B) in correlation to the temporal pattern of mRNA expression (Figure 4A). Upregulation of MMP-3, MMP-7, and MMP-9 protein expression 4 h post-E2 indicates that these enzymes are in fact elevated rapidly by hormone treatment with peak increases in protein content occurring at the time point when stromal collagen matrix is lowest (Figures 1 and 2).
E2-induced changes in activity of the gelatinase enzymes were assessed via gelatin zymography (Figure 5) to confirm overall protein expression levels observed via Western blot. The major bands representing gelatin-degrading activity were identified as active MMP-9 (~90 kDa) and latent and active MMP-2 (~72 kDa and 64 kDa, respectively). Overall activity of MMP-2 was greater than that of MMP-9 based upon band intensities. Levels of active MMP-2 decrease slightly within 4-12 h of hormone treatment (Figure 5). However, both latent and active forms of MMP-2 increase by 48 h post-E2 treatment, with peak activity correlating temporally with the highest level of total protein observed via Western blot (Figure 4). Activity of MMP-9 increases significantly at 4 h post E2-treatment (Figure 5) also corresponding to the time point when total protein levels are highest (Figure 4). Activity of MMP-3 and MMP-7 was assessed via casein gel zymography, however sensitivity of the assay was not sufficient to permit quantitative analysis (data not shown).
E2induces transient upregulation of the pro-inflammatory cytokine TNF-α and the β-chemokine MCP-1
E2-induced changes in expression of the pro-inflammatory cytokine, TNF-α, and the β-chemokine MCP-1, were assessed over the biphasic growth response to better characterize the tissue inflammatory response and to compare changes temporally with matrix processing and MMP expression. Levels of TNF-α mRNA and protein transiently increase with a peak in expression occurring 4 h after hormone treatment (Figure 6A). TNF-α mRNA increases nearly 25 fold at 4 h and remains elevated through 12 h post-E2 treatment before declining to control values by 48 h. Western blot analysis (Figure 6B) identified the homotrimeric form of the protein (~51 kDa) as well as lower MW forms. Analysis of the receptor-ligand homotrimeric form shows slight elevation of protein early (1-2 h) with maximum levels occurring at 4 and 12 h post E2 administration (Figure 6B), correlating temporally to the major time points of mRNA elevation. This pattern clearly indicates a potent overall enhancement of tissue levels of TNF-α expression, most notably during the early hypertrophic period of uterine growth following hormone treatment. MCP-1 mRNA expression is also significantly upregulated (~80 fold) 4 h post-E2 treatment. While mRNA levels return to control values within 24 h, MCP-1 protein increases by 4 h but remains elevated through 48 h before returning to control tissue levels 72 h post-treatment (Figure 6B). Western blot analysis detects a higher MW form of MCP-1 (~20 kDa) which may represent an intact bioactive form of the chemokine, as well as a lower MW form (~16 kDa) which may represent a proteolytic and receptor-inactive product (Figure 6B). Blot analysis indicates that levels of the higher MW MCP-1 product peak at 4 h whereas the lower MW product peaks at ~24 h post treatment. E2 treatment thus rapidly increases levels of two potent pro-inflammatory chemicals, TNF-α and MCP-1, and the induction correlates temporally with the hypertrophic phase of tissue growth, which is characterized by tissue edema and stromal matrix remodeling.
Dexamethasone pretreatment inhibits E2-induced uterine growth and changes in uterine tissue ultrastructure
Because peak changes in matrix density and cytokine expression correlate temporally with the hypertrophic phase of E2-induced uterine growth, it was of interest to assess the effects of the anti-inflammatory synthetic glucocorticoid, dexamethasone (600 μg/kg) on this inflammatory-like response. Dexamethasone pretreatment alone induces a decrease in uterine wet weight and significantly inhibits the typical increase in uterine wet weight effected by E2 (Figure 7) in a manner consistent with previously published reports . With respect to stromal matrix density, dexamethasone alone produces both a qualitative and quantitative change in matrix structure (Figure 8); there is a noticeable and statistically significant increase in stromal matrix density as compared to saline control animals (Dex-Sal vs. Sal-Sal). This indicates that dexamethasone modulates stromal matrix remodeling so as to generate a more densely organized collagen architecture in the immature uterus. In addition, dexamethasone pretreatment inhibits E2-induced matrix remodeling; stromal collagen density is much higher (~4-fold) in dexamethasone-pretreated (Dex-E2) animals as compared to saline-pretreated E2-challenged animals (Sal-E2). Quantitative analysis of collagen density indicates that collagen levels are equivalent in the Dex-E2 as compared to control animals (Sal-Sal). It should be noted that the magnitude of inhibition of collagen matrix remodeling induced by E2 is smaller in dexamethasone pretreated animals (Figure 8 bottom, Dex-E2 vs. Sal-E2) indicating that it is not fully efficacious at inhibiting the E2 response.
Dexamethasone pretreatment modifies E2-induced changes in uterine MMP expression
In light of the inhibitory effect on E2-induced stromal matrix remodeling (Figure 8), MMP mRNA and protein levels were analyzed in animals pre-treated with dexamethasone. Dexamethasone treatment increases expression of MMP-3 mRNA, when compared to levels in control animals (Figure 9A; Dex-Sal vs. Sal-Sal). In addition, dexamethasone does not inhibit the E2-induced increase in MMP-3 mRNA (Figure 9A; Dex-E2 vs. Sal-E2). Levels of mRNA in Dex-E2 animals are not significantly different from those in Dex-Sal controls, indicating that dexamethasone induction of mRNA expression for MMP-3 is not modified in the presence of E2. Transcript levels for MMP-7 and MMP-9 are unaffected by pretreatment (Figure 9A, Dex-Sal vs. Sal-Sal), although dexamethasone pretreatment does significantly inhibit the E2-induced upregulation of mRNA for these two enzymes (Dex-E2 vs. Sal-E2). Dexamethasone does not induce a change in MMP-2 mRNA (Figure 9A); however, effects on the E2-induced upregulation of MMP-2 mRNA were not assessed since only the 4 h post-hormone treatment time point was studied, and transcript levels for this enzyme do not significantly increase until 48 h post-E2 administration (Figure 4A).
Western blot analyses of MMP protein levels support the effects of dexamethasone on mRNA expression. Pretreatment inhibits E2-induced upregulation of protein expression for MMP-3, MMP-7, and MMP-9 (Figure 9B; Dex-E2 vs. Sal-E2). Interestingly, levels of MMP-3 protein do not increase in response to dexamethasone pretreatment despite evidence of an elevation of tissue mRNA (Figure 9A). Gelatin zymography shows that dexamethasone pretreatment did not affect activity of MMP-2 or MMP-9 (Figure 10), although dexamethasone pretreatment does decrease the E2-induced upregulation of MMP-9 total protein levels (Figure 9B). Because full activity of MMPs may not be recovered as a result of refolding of the enzymes after electrophoresis in gel zymography , it is unclear whether dexamethasone affects levels of active MMP-9 in vivo.
Dexamethasone pretreatment affects E2-induction of uterine MCP-1 and TNF-α expression
Dexamethasone potently inhibits the E2-induced upregulation of MCP-1 mRNA and protein observed at 4 h post-hormone treatment (Figure 11). However, pretreatment does not affect E2-induced upregulation of TNF-α mRNA (Figure 11A), though it does decrease protein content (Figure 11B).
An examination of tissue responses in the E2-treated OVX rat provides an opportunity to study selective effects of the hormone that can be defined in the temporal context of the hypertrophic and hyperplastic growth responses. In this model, E2 induces uterine growth that is characterized by changes in endometrial tissue architecture and gene expression. We used TEM analysis to more specifically assess changes in stromal collagen matrix quantitatively. A significant decrease in matrix density is observed as early as 45 minutes and reaches its lowest value, with an approximate 70% reduction of the original collagen network, at 4 hours post-hormone treatment, coinciding with the peak time point of uterine hypertrophy. This indicates that activation of matrix-processing enzymes is extremely rapid and implies regulation of inherent proteases through an estrogen receptor (ER)-mediated pathway.
Pretreatment with the broad-range MMP inhibitor batimastat effectively ablates E2-induced changes in stromal ultrastructure supporting a critical role for these enzymes in tissue remodeling. These results differ from those by Kaitu'u and colleagues , who reported that batimastat reduced MMP activity but did not alter endometrial breakdown or repair as assessed through light microscopy in a mouse decidualization model. The contrasting results may reflect a difference in matrix processing during E2-specific induction of tissue growth in the immature uterus as compared to tissue regression following progesterone withdrawal in a decidualization model. In addition, analysis of fine matrix structure and density using quantitative TEM provides a more sensitive measure of changes in collagen organization indicative of tissue remodeling as compared to qualitative assessment of tissue appearance via light microscopy .
While a number of MMPs are known to be expressed in cell-type as well as cycle-specific patterns in the uterus [2, 5, 50], E2-specific regulation in an OVX rodent model has been studied in vivo for only a few . Using this model we show that expression of MMP-3, MMP-7, and MMP-9 is upregulated at both RNA and protein level early within the E2-induced growth response correlating with the time point where stromal collagen matrix density reaches its lowest point (4 h). While substrates for these enzymes include fibrillar, fibril-associated, and network forming collagens , in vivo substrates are unknown. Therefore, although expression correlates with maximum matrix remodeling temporally, we cannot conclude that these particular proteases are directly causative. As an epithelial cell expressed protease, MMP-7 is likely not critically involved in stromal matrix processing directly, whereas MMP-3 and MMP-9 are known to be expressed by stromal cells or infiltrating leukocytes . Expression of MMP-2 increases most significantly later in the growth response (48 h) suggesting a complex level of regulation that may involve E2-triggered production of signal compounds which, in turn, enhance MMP-2 production. Interestingly, tissue levels of MMP-3 protein also remain elevated late in the growth response (24-72 h), indicating extended in-tissue stabilization of this enzyme. The overall elevation of MMP-2 and MMP-3 content late, as compared to MMP-7 and MMP-9 protein which peak early in the growth response, implies alternate temporal functions for tissue MMPs that may include activation of matrix processing during both tissue growth and regression phases. While providing important insight into the E2-triggered response at the whole tissue level, our analysis of changes in MMP mRNA and protein content does not define stromal-specific changes in enzyme content and activity. Future studies to analyze MMP activity via in situ zymography and mRNA expression using laser capture microdissection and subsequent gene profiling would provide a more precise window into the stromal tissue response.
While we observed transient upregulation of MMP-2 and MMP-9 mRNA and protein expression in response to E2 in the OVX immature rat uterus, Zhang and colleagues  did not observe an effect of E2 on MMP-2 mRNA levels in the OVX adult mouse through 24 h post-hormone treatment, though they did observe a decrease in MMP-9 mRNA, but not protein activity, 4-8 h post-treatment. Since we observe peak changes in MMP-2 mRNA expression at 48 h after E2 administration, it is unclear if a similar response would be evident in an OVX adult model as that time point was not assessed . In contrast, our analysis of MMP-9 mRNA protein via both Western blot and zymography clearly shows upregulation by 4 h post-E2 administration. Data inconsistencies may reflect differences in rodent model (mouse vs. rat) or in tissue responsiveness between the immature (first time hormone exposure) as opposed to an adult (hormone-primed) uterus.
A variety of inflammatory mediators [8, 9, 40, 52, 53] have been shown to regulate expression and activity of MMPs, and, E2 is known to induce an acute inflammatory-like response within the uterus . We show that E2 induces potent and rapid upregulation of TNF-α, with peak increases in mRNA and protein occurring at the time point where MMP expression and stromal matrix processing are upregulated (4 h). It is difficult to understand the exact role of TNF-α expression in E2-induced uterine matrix remodeling or in MMP gene transcription as this bioactive compound is expressed in tissues and held in an inactive state through cell surface or extracellular matrix-binding interactions. Although ADAM-17 (TACE) is the best characterized TNF-α sheddase, MMP-2, MMP-3, MMP-7, and MMP-9 have been shown to release TNF-α from the cell surface in a similar mechanism [13, 45]. Protease-mediated shedding of TNF-α may induce signal pathway activation that precedes an overall upregulation of mRNA and protein expression for this inflammatory mediator, thus analysis of expression alone is not a full indicator of TNF-α activity in vivo. A study of E2-induced changes in activity of the TNF-α pathway, including activation of NF-κB, will be important for a better understanding of the role of this inflammatory agent as a critical regulator of MMP expression in the estrogen response pathway.
Expression of the β-chemokine MCP-1 (CCL2), a potent chemoattractant for macrophages, T cells, basophils, and mast cells is also potently upregulated at 4 h. Enhanced production of MCP-1 is known to occur during the proliferative phase of the cycling uterus and, expression is stimulated by TNF-α [55–57]. The timing of highest tissue levels of MCP-1 at 4 h correlates with the peak in expression of TNF-α, suggesting that it may be a key signal component for inducing leukocyte influx by creating in-tissue gradients of chemokines, like MCP-1, which are triggered early during the hypertrophic phase of uterine growth. MCP-1 is also a substrate for a variety of MMPs, including MMP-3 , and protease-mediated processing has been shown to inhibit bioactivity of β-chemokines, thereby regulating the timing and intensity of leukocyte influx once an inflammatory response is underway [14, 44, 45, 58].
Correlations between E2-regulated uterine growth, inflammation, and MMP expression and activation in the immature OVX uterus led us to investigate the effects of dexamethasone, the synthetic glucocorticoid and anti-inflammatory agent. We show that dexamethasone modifies stromal matrix collagen density and, pretreatment with dexamethasone effectively inhibits E2-induced collagen remodeling. These data suggest that the regulation of collagen density is under the influence of activated glucocorticoid-receptor (GR) and, implicates the MMP system because dexamethasone is known to inhibit MMP expression . Dexamethasone effects on MMP expression however, are complex. Of the MMPs that are upregulated 4 h post-E2 treatment, dexamethasone pretreatment inhibits both MMP-7 and MMP-9 mRNA and protein expression but does not inhibit the E2-induced increase in MMP-3 mRNA or protein.
In addition to effects on the MMP system, dexamethasone is also known to block the pro-inflammatory effects of E2 in the uterus . Glucocorticoids have been shown to suppress expression of chemoattractant chemokines, such as MCP-1 , and possibly, through inhibition of MMP expression, may decrease sheddase activity and ECM processing important for liberation of inherent bioactive agents, including TNF-α, that activate signal pathways to enhance inflammatory processes. Our data clearly show that dexamethasone has no effect on TNF-α or MCP-1 mRNA or protein expression. However, dexamethasone pretreatment potently inhibits E2-induced upregulation of MCP-1 mRNA and protein expression and decreases levels of TNF-α protein observed at 4 h post-treatment, thereby supporting its effects as a suppressor of both inflammatory signaling as well as matrix remodeling.
Collectively our data show that E2-induced endometrial matrix remodeling, production of MMPs, and inflammatory mediators correlate temporally with the early phase of uterine growth which is hypertrophic and inflammatory-like in nature. Dexamethasone as an anti-inflammatory agent inhibits these processes however, because activated GR can directly modify expression of MMPs and inflammatory agents such as MCP-1, further investigation is necessary to determine the role of inflammation itself on matrix remodeling. One model of the E2 response would be that hormone-triggered rapid activation of inherent proteases leads to matrix processing that liberates bound inflammatory mediators like TNF-α, thereby producing inflammation and leukocyte influx. Alternatively, rapid E2-induced inflammation triggered by ER signal pathways and production of paracrine regulators like prostaglandins would drive influx of leukocytes which, in turn, activate inherent proteases to effect changes in stromal matrix architecture necessary for tissue expansion as growth proceeds. Evidence indicates that infiltrating leukocytes contribute to tissue protease density [8, 9, 61–63] and neutrophilic depletion clearly inhibits endometrial repair in the mouse . Further studies must focus upon the timing of E2-induced changes in expression and activity of inflammatory mediators and leukocyte influx in relation to matrix processing to more clearly delineate the E2 response pathway. In addition, the use of other kinds of anti-inflammatory agents such as COX inhibitors, that would specifically inhibit production of prostaglandins, will also provide a better understanding of the role of inflammatory reactions per se on matrix processing.
This study using the OVX immature rat model contributes to a better understanding of specific regulation of MMP expression and endometrial tissue remodeling induced by E2 and the counter-regulatory effects of dexamethasone. We have established a novel assay system for measuring stromal collagen matrix density as a reliable and specific endpoint for assessment of matrix remodeling. The data demonstrate that E2-regulated endometrial remodeling is rapid in onset (<1 hour) and peak changes in expression of MMP-3, -7, and -9 and the inflammatory mediators TNF-α and MCP-1, correlate temporally with the period of lowest stromal collagen density during uterine tissue hypertrophy (4 h). Our survey of changes in expression of MMPs and inflammatory mediators provides the groundwork for further studies of molecular triggers that link ER activation with inflammatory-like responses and matrix processing in the uterus.
Pastore GN, diCola LP, Dollahon NR, Gardner RM: The effect of estradiol on collagen structure and organization in the immature rat uterus. Proceedings of the Society for Experimental Biology and Medicine. 1989, 191: 69-77.
Goffin F, Munaut C, Frankenne F, Perrier D'Hauterive S, Beliard A, Fridman V, Nervo P, Colige A, Foidart JM: Expression pattern of metalloproteinases and tissue inhibitors of matrix-metalloproteinases in cycling human endometrium. Biol Reprod. 2003, 69: 976-984. 10.1095/biolreprod.103.015933.
Rodgers WH, Matrisian LM, Giudice LC, Dsupin B, Cannon P, Svitek C, Gorstein F, Osteen KG: Patterns of matrix metalloproteinase expression in cycling endometrium imply differential functions and regulation by steroid hormones. Journal of Clinical Investigation. 1994, 94: 946-953. 10.1172/JCI117461.
Salamonsen LA, Woolley DE: Menstruation: induction by matrix metalloproteinases and inflammatory cells. J Reprod Immunol. 1999, 44: 1-27. 10.1016/S0165-0378(99)00002-9.
Feng J, Woessner JF, Zhu C: Matrilysin activity in the rat uterus during the oestrous cycle and implantation. Journal of Reproduction and Fertility. 1998, 114: 347-350.
Wolf K, Sandner P, Kurtz A, Moll W: Messenger ribonucleic acid levels of collagenase (MMP-13) and matrilysin (MMP-7) in virgin, pregnant, and postpartum uterus and cervix of rat. Endocrinology. 1996, 137: 5429-5434. 10.1210/en.137.12.5429.
Hahn-Dantona E, Ramos-DeSimone N, Sipley J, Nagase H, French DL, Quigley JP: Activation of proMMP-9 by a plasmin/MMP-3 cascade in a tumor cell model. Regulation by tissue inhibitors of metalloproteinases. Ann N Y Acad Sci. 1999, 878: 372-387. 10.1111/j.1749-6632.1999.tb07696.x.
Imai K, Yokohama Y, Nakanishi I, Ohuchi E, Fujii Y, Nakai N, Okada Y: Matrix metalloproteinase 7 (matrilysin) from human rectal carcinoma cells. Journal of Biological Chemistry. 1995, 270: 6691-6697. 10.1074/jbc.270.12.6691.
Lees M, Taylor DJ, Woolley DE: Mast cell proteinases activate precursor forms of collagenase and stromelysin, but not of gelatinases A and B. European Journal of Biochemistry. 1994, 223: 171-177. 10.1111/j.1432-1033.1994.tb18980.x.
Ramos-DeSimone N, Hahn-Dantona E, Sipley J, Nagase H, French DL, Quigley JP: Activation of matrix metalloproteinase-9 (MMP-9) via a converging plasmin/stromelysin-1 cascade enhances tumor cell invasion. J Biol Chem. 1999, 274: 13066-13076. 10.1074/jbc.274.19.13066.
Karsdal MA, Larsen L, Engsig MT, Lou H, Ferreras M, Lochter A, Delaissé J-M, Foged NT: Matrix metalloproteinase-dependent activation of latent transforming growth factor-beta controls the conversion of osteoblasts into osteocytes by blocking osteoblast apoptosis. Journal of Biological Chemistry. 2002, 277: 44061-44067. 10.1074/jbc.M207205200.
Schönbeck U, Mach F, Libby P: Generation of biologically active IL-1β by matrix metalloproteinases: a novel caspase-1-independent pathway of IL-1β processing. Journal of Immunology. 1998, 161: 3340-3346.
Gearing AJ, Beckett P, Christodoulou M, Churchill M, Clements J, Davidson AH, Drummond AH, Galloway WA, Gilbert R, Gordon JL: Processing of tumour necrosis factor-alpha precursor by metalloproteinases. Nature. 1994, 370: 555-557. 10.1038/370555a0.
McQuibban GA, Gong J-H, Wong JP, Wallace JL, Clark-Lewis I, Overall CM: Matrix metalloproteinase processing of monocyte chemoattractant proteins generates CC chemokine receptor antagonists with anti-inflammatory properties in vivo. Blood. 2002, 100: 1160-1167.
Steen Van den PE, Wuyts A, Husson SJ, Proost P, Damme JV, Opdenakker G: Gelatinase B/MMP-9 and neutrophil collagenase/MMP-8 process the chemokines human GCP-2/CXCL6, ENA-78/CXCL5 and mouse GCP-2/LIX and modulate their physiological activities. European Journal of Biochemistry. 2003, 270: 3739-3749. 10.1046/j.1432-1033.2003.03760.x.
Li Q, Park PW, Wilson CL, Parks WC: Matrilysin shedding of syndecan-1 regulates chemokine mobilization and transepithelial efflux of neutrophils in acute lung injury. Cell. 2002, 111: 635-646. 10.1016/S0092-8674(02)01079-6.
Zhou Z, Apte SS, Soininen R, Cao R, Baaklini GV, Rauser RW, Wang J, Cao Y, Tryggvason K: Impaired endochondral ossification and angiogenesis in mice deficient in membrane-type matrix metalloproteinase I. Proceedings of the National Academy of Sciences. 2000, 97: 4052-4057. 10.1073/pnas.060037197.
Bruner-Tran KL, Zhang Z, Eisenberg E, Winneker RC, Osteen KG: Down-regulation of endometrial matrix metalloproteinase-3 and -7 expression in vitro and therapeutic regression of experimental endometriosis in vivo by a novel nonsteroidal progesterone receptor agonist, tanaproget. J Clin Endocrinol Metab. 2006, 91: 1554-1560. 10.1210/jc.2005-2024.
Zhang X, Christenson LK, Nothnick WB: Regulation of MMP-9 expression and activity in the mouse uterus by estrogen. Mol Reprod Dev. 2007, 74: 321-331. 10.1002/mrd.20582.
Keller NR, Sierra-Rivera E, Eisenberg E, Osteen KG: Progesterone exposure prevents matrix metalloproteinase-3 (MMP-3) stimulation by interleukin-1alpha in human endometrial stromal cells. J Clin Endocrinol Metab. 2000, 85: 1611-1619. 10.1210/jc.85.4.1611.
Rawdanowicz TJ, Hampton AL, Nagase H, Woolley DE, Salamonsen LA: Matrix metalloproteinase production by cultured human endometrial stromal cells: identification of interstitial collagenase, gelatinase-A, gelatinase-B, and stromelysin-1 and their differential regulation by interleukin-1 alpha and tumor necrosis factor-alpha. J Clin Endocrinol Metab. 1994, 79: 530-536. 10.1210/jc.79.2.530.
Osteen KG, Bruner KL, Sharpe-Timms KL: Steroid and growth factor regulation of matrix metalloproteinase expression and endometriosis. Seminars in Reproductive Endocrinology. 1996, 14: 247-255. 10.1055/s-2007-1016334.
Gomez DE, Alonso DF, Yoshiji H, Thorgeirsson UP: Tissue inhibitors of metalloproteinases: structure, regulation and biological functions. European Journal of Cell Biology. 1997, 74: 111-122.
Kleiner DE, Stetler-Stevenson WG: Structural biochemistry and activation of matrix metalloproteinases. Current Opinion in Cell Biology. 1993, 5: 891-897. 10.1016/0955-0674(93)90040-W.
Kaitu'u-Lino TJ, Morison NB, Salamonsen LA: Neutrophil depletion retards endometrial repair in a mouse model. Cell Tissue Res. 2007, 328: 197-206. 10.1007/s00441-006-0358-2.
Hunt J: Immunologically relevant cells in the uterus. Biology of Reproduction. 1994, 50: 461-466. 10.1095/biolreprod50.3.461.
Kachkache M, Acker GM, Chaouat G, Noun A, Garabedian M: Hormonal and local factors control the immunohistochemical distribution of immunocytes in the rat uterus before conceptus implantation: effects of ovariectomy, fallopian tube section, and injection. Biology of Reproduction. 1991, 45: 860-868. 10.1095/biolreprod45.6.860.
Kaushic C, Frauendorf E, Rossoll R, Richardson J, Wira C: Influence of the estrous cycle on the presence and distribution of immune cells in the rat reproductive tract. American Journal of Reproductive Immunology. 1998, 39: 209-216.
Di Nezza LA, Misajon A, Zhang J, Jobling T, Quinn MA, Ostor AG, Nie G, Lopata A, Salamonsen LA: Presence of active gelatinases in endometrial carcinoma and correlation of matrix metalloproteinase expression with increasing tumor grade and invasion. Cancer. 2002, 94: 1466-1475. 10.1002/cncr.10355.
Tchernitchin A, Roorijck J, Tchernitchin X, Vandenhende J, Galand P: Dramatic early increase in uterine eosinophils after oestrogen administration. Nature. 1974, 248: 142-10.1038/248142a0.
Zheng Y, Zhou ZZ, Lyttle CR, Teuscher C: Immunohistochemical characterization of the estrogen-stimulated leukocyte influx in the immature rat uterus. Journal of Leukocyte Biology. 1988, 44: 27-36.
Bigsby RM: Progesterone and dexamethasone inhibition of estrogen-induced synthesis of DNA and complement in rat uterine epithelium: effects of antiprogesterone compounds. J Steroid Biochem Mol Biol. 1993, 45: 295-301. 10.1016/0960-0760(93)90345-W.
Markaverich BM, Upchurch S, Clark JH: Progesterone and dexamethasone antagonism of uterine growth: a role for a second nuclear binding site for estradiol in estrogen action. Journal of Steroid Biochemistry. 1981, 14: 125-132. 10.1016/0022-4731(81)90164-3.
Rhen T, Grissom S, Afshari C, Cidlowski JA: Dexamethasone blocks the rapid biological effects of 17β-estradiol in the rat uterus without antagonizing its global genomic actions. FASEB J. 2003, 17: 1849-1870. 10.1096/fj.02-1099com.
Stewart PJ, Zaloudek CJ, Inman MM, Webster RA: Effects of dexamethasone and indomethacin on estrogen-induced uterine growth. Life Sciences. 1983, 33: 2349-2356. 10.1016/0024-3205(83)90269-2.
Velardo JT, Hisaw FL, Bever AT: Inhibitory action of desoxycorticosterone acetate, cortisone acetate, and testosterone on uterine growth induced by estradiol-17β. Endocrinology. 1956, 59: 165-169. 10.1210/endo-59-2-165.
Tibbetts TA, Conneely OM, O'Malley BW: Progesterone via its receptor antagonizes the pro-inflammatory activity of estrogen in the mouse uterus. Biol Reprod. 1999, 60: 1158-1165. 10.1095/biolreprod60.5.1158.
Kaitu'u TJ, Shen J, Zhang J, Morison NB, Salamonsen LA: Matrix metalloproteinases in endometrial breakdown and repair: functional significance in a mouse model. Biol Reprod. 2005, 73: 672-680. 10.1095/biolreprod.105.042473.
Lathbury LJ, Salamonsen LA: In-vitro studies of the potential role of neutrophils in the process of menstruation. Mol Hum Reprod. 2000, 6: 899-906. 10.1093/molehr/6.10.899.
Zhang J, Nie G, Jian W, Woolley DE, Salamonsen LA: Mast cell regulation of human endometrial matrix metalloproteinases: A mechanism underlying menstruation. Biol Reprod. 1998, 59: 693-703. 10.1095/biolreprod59.3.693.
Fu X, Kassim SY, Parks WC, Heinecke JW: Hypochlorous acid oxygenates the cysteine switch domain of pro-matrilysin (MMP-7). A mechanism for matrix metalloproteinase activation and atherosclerotic plaque rupture by myeloperoxidase. Journal of Biological Chemistry. 2001, 276: 41279-41287. 10.1074/jbc.M106958200.
Fu X, Kassim SY, Parks WC, Heinecke JW: Hypochlorous acid generated by myeloperoxidase modifies adjacent tryptophan and glycine residues in the catalytic domain of matrix metalloproteinase-7 (matrilysin): an oxidative mechanism for restraining proteolytic activity during inflammation. Journal of Biological Chemistry. 2003, 278: 28403-28409. 10.1074/jbc.M304739200.
Weiss SJ, Peppin G, Ortiz X, Ragsdale C, Test ST: Oxidative autoactivation of latent collagenase by human neutrophils. Science. 1985, 227: 747-749. 10.1126/science.2982211.
McQuibban GA, Gong JH, Tam EM, McCulloch CA, Clark-Lewis I, Overall CM: Inflammation dampened by gelatinase A cleavage of monocyte chemoattractant protein-3. Science. 2000, 289: 1202-1206. 10.1126/science.289.5482.1202.
Van Lint P, Libert C: Chemokine and cytokine processing by matrix metalloproteinases and its effect on leukocyte migration and inflammation. J Leukoc Biol. 2007, 82: 1375-1381. 10.1189/jlb.0607338.
Russo LA, Calabro SP, Filler TA, Carey DJ, Gardner RM: In vivo regulation of syndecan-3 expression in the rat uterus by 17 beta-estradiol. J Biol Chem. 2001, 276: 686-692. 10.1074/jbc.M004106200.
Suva LJ, Harm SC, Gardner RM, Thiede MA: In vivo regulation of Zif268 messenger RNA expression by 17 beta-estradiol in the rat uterus. Mol Endocrinol. 1991, 5: 829-835. 10.1210/mend-5-6-829.
Thiede MA, Harm SC, Hasson DM, Gardner RM: In vivo regulation of parathyroid hormone-related peptide messenger ribonucleic acid in the rat uterus by 17 beta-estradiol. Endocrinology. 1991, 128: 2317-2323. 10.1210/endo-128-5-2317.
Wang X, Fu X, Brown PD, Crimmin MJ, Hoffman RM: Matrix metalloproteinase inhibitor BB-94 (batimastat) inhibits human colon tumor growth and spread in a patient-like orthotopic model in nude mice. Cancer Res. 1994, 54: 4726-4728.
Curry TE, Osteen KG: The matrix metalloproteinase system: changes, regulation, and impact throughout the ovarian and uterine reproductive cycle. Endocr Rev. 2003, 24: 428-465. 10.1210/er.2002-0005.
Snoek-van Beurden PA, Hoff Von den JW: Zymographic techniques for the analysis of matrix metalloproteinases and their inhibitors. Biotechniques. 2005, 38: 73-83. 10.2144/05381RV01.
Stack MS, Johnson DA: Human mast cell tryptase activates single-chain urinary-type plasminogen activator (pro-urokinase). J Biol Chem. 1994, 269: 9416-9419.
Zhou L, Yan C, Gieling RG, Kida Y, Garner W, Li W, Han YP: Tumor necrosis factor-alpha induced expression of matrix metalloproteinase-9 through p21-activated kinase-1. BMC Immunol. 2009, 10: 15-10.1186/1471-2172-10-15.
Rhen T, Cidlowski JA: Estrogens and glucocorticoids have opposing effects on the amount and latent activity of complement proteins in the rat uterus. Biol Reprod. 2006, 74: 265-274. 10.1095/biolreprod.105.045336.
Jones RL, Kelly RW, Critchley HO: Chemokine and cyclooxygenase-2 expression in human endometrium coincides with leukocyte accumulation. Hum Reprod. 1997, 12: 1300-1306. 10.1093/humrep/12.6.1300.
Salamonsen LA, Hannan NJ, Dimitriadis E: Cytokines and chemokines during human embryo implantation: roles in implantation and early placentation. Semin Reprod Med. 2007, 25: 437-444. 10.1055/s-2007-991041.
McQuibban GA, Gong JH, Wong JP, Wallace JL, Clark-Lewis I, Overall CM: Matrix metalloproteinase processing of monocyte chemoattractant proteins generates CC chemokine receptor antagonists with anti-inflammatory properties in vivo. Blood. 2002, 100: 1160-1167.
Manicone AM, McGuire JK: Matrix metalloproteinases as modulators of inflammation. Semin Cell Dev Biol. 2008, 19: 34-41. 10.1016/j.semcdb.2007.07.003.
Schroen DJ, Brinckerhoff CE: Nuclear hormone receptors inhibit matrix metalloproteinase (MMP) gene expression through diverse mechanisms. Gene Expr. 1996, 6: 197-207.
Brach MA, Gruss HJ, Riedel D, Asano Y, De Vos S, Herrmann F: Effect of antiinflammatory agents on synthesis of MCP-1/JE transcripts by human blood monocytes. Mol Pharmacol. 1992, 42: 63-68.
Bini A, Wu D, Schnuer J, Kudryk BJ: Characterization of stromelysin-1 (MMP-3), matrilysin (MMP-7), and membrane type 1 matrix metalloproteinase (MT1-MMP) derived fibrin(ogen) fragments D-dimer and D-like monomer: NH2-terminal sequences of late-stage digest fragments. Biochemistry. 1999, 38: 13928-13936. 10.1021/bi991096g.
Lijnen HR: Plasmin and matrix metalloproteinases in vascular remodeling. Thrombosis Haemostasis. 2001, 86: 324-333.
Lopez-Boado YS, Wilson CL, Hooper LV, Gordon JI, Hultgren SJ, Parks WC: Bacterial exposure induces and activates matrilysin in mucosal epithelial cells. Journal of Cell Biology. 2000, 148: 1305-1315. 10.1083/jcb.148.6.1305.
We offer sincere thanks to Dr. Norman R. Dollahon and Ms. Sally Shrom (Villanova University) for their transmission electron microscopy patience and expertise and to Ms. Suzanne Muscella for her excellent animal care.
The authors declare that they have no competing interests.
LAR participated in the design of the study, in directing and completing all experimental analyses and in writing the manuscript. BJP participated in MMP mRNA analyses, in TEM tissue preparations and in writing the manuscript. SPT contributed significantly to generation of TEM data, mRNA analyses, and figure preparations. TDC developed the TEM quantitative method and participated in cytokine analyses to assess temporal changes in response to E2. BAO completed initial analyses of MMP expression and batimastat inhibitor studies. JAC contributed to quantitative TEM analysis for dexamethasone studies. ARS and OV participated in animal treatments and tissue preparations for MMP expression analysis. RMG participated in planning experiments and contributed to drafting of the manuscript. All authors have read and approved the final manuscript.
Authors’ original submitted files for images
Below are the links to the authors’ original submitted files for images.
About this article
Cite this article
Russo, L.A., Peano, B.J., Trivedi, S.P. et al. Regulated expression of matrix metalloproteinases, inflammatory mediators, and endometrial matrix remodeling by 17beta-estradiol in the immature rat uterus. Reprod Biol Endocrinol 7, 124 (2009). https://doi.org/10.1186/1477-7827-7-124
- Matrix Remodel
- Stromal Collagen
- Matrix Processing
- Uterine Growth
- Stromal Matrix