Osteoprotegerin Prevents Development of Abdominal Aortic Aneurysms

Abdominal aortic aneurysms (AAAs), which commonly occur among elderly individuals, are accompanied by a risk of rupture and subsequent high mortality. Establishment of medical therapies for the prevention of AAAs requires further understanding of the molecular pathogenesis of this condition. This report details the possible involvement of Osteoprotegerin (OPG) in the prevention of AAAs through inhibition of Tumor necrosis factor-related apoptosis-inducing ligand (TRAIL). In CaCl2-induced AAA models, both internal and external diameters were significantly increased with destruction of elastic fibers in the media in Opg knockout (KO) mice, as compared to wild-type mice. Moreover, up-regulation of TRAIL expression was observed in the media by immunohistochemical analyses. Using a culture system, both the TRAIL-induced expression of matrix metalloproteinase-9 in smooth muscle cells (SMCs) and the chemoattractive effect of TRAIL on SMCs were inhibited by OPG. These data suggest that Opg may play a preventive role in the development of AAA through its antagonistic effect on Trail.


Introduction
An abdominal aortic aneurysm (AAA) is a progressive dilation of the aorta, which results in rupture with high mortality ratio. The infiltration of macrophages and disruption of medial elastic fibers that occur in this condition are believed to be associated with inflammation [1]. Since inflammation is a common underlying feature of both AAAs and atherosclerosis, these two conditions are considered to be closely related [2]. It has not yet been determined, however, whether the relationship between AAAs and atherosclerosis is causal or if these conditions merely share common risk factors, such as smoking, hypertension, and obesity [3].
Studies of human AAA tissue have shown extensive inflammatory infiltrates into both the tunica media and tunica adventitia, while atherosclerosis is primarily found within the tunica intima and tunica media. It has been suggested that AAA vascular tissue has a higher level of proteolytic activity, and a greater rate of inflammatory cell infiltration, as compared to atherosclerosis [4,5]. Proteolytic activities involved in the degradation of elastin in the supporting lamina of the aortic media depend on matrix metalloproteinase (MMP)-2 and MMP-9, as well as tissue inhibitor of metalloproteinase (TIMP)-1, the expression of which is elevated in the aneurysm tissues of both human and animal models [6][7][8][9][10][11][12]. MMPs are reportedly produced from macrophages and smooth muscle cells through the c-Jun NH2-terminal kinase (JNK) pathway [11,13]. These recent studies collectively suggest the involvement of several pathways for development of AAAs, although the pathogenesis of this condition has yet to be fully understood.
Osteoprotegerin (OPG, also referred to as TNFSF11B), a member of tumor necrosis factor (TNF) superfamily, has been shown to regulate the functions of many key genes for biological processes [14]. OPG was first identified as a main regulator of bone metabolism [15]. This soluble decoy receptor for the receptor activator of nuclear factor-kappaB ligand (RANKL, or TNFSF11) blocks the promotion of osteoclast differentiation and activation, which leads to bone resorption, by inhibiting RANKL binding to the activator of nuclear factor-kappaB (RANK, or TNFSF11A) [16]. OPG also works as a decoy receptor for the TNF-related apoptosis-inducing ligand (TRAIL, or TNFSF10) [14]. By signaling through death receptor-4 (DR4, or TNFRSF11A) and death receptor 5 (DR5, or TNFRSF11B), TRAIL is involved in two overlapping modes of signaling for cell death and cell survival, including transcriptional activation in normal tissues [17]. The function of this ligand in immune surveillance for tumors through the control of cell death signaling is well characterized. In the vascular system, studies using animal models have suggested that OPG plays a role in preventing arterial calcification and stabilizing plaque formation [18][19][20][21][22][23]. However, loss of the Opg gene has been reported to reduce Angiotensin II (AngII)-induced aneurysm formation in ApolipoproteinE (ApoE)-KO mice [24]. Clinical studies have shown positive correlations between serum OPG and the presence and progression of cardiovascular disease, including AAA [25,26]. However, whether the concentration of OPG in AAA tissue is up-regulated or down-regulated remains controversial [27,28]. Thus, while OPG may play an important biological role in the vascular system, its function remains ambiguous.
This study reports that loss of the Opg gene results in deterioration of AAAs, possibly through involvement of TRAIL in smooth muscle actin (SMA)-positive cells, including smooth muscle cells (SMCs) and myofibroblasts, in a CaCl 2 -induced AAA experimental model [13]. TRAIL has been shown to serve as a chemoattractant for SMCs and macrophages, as well as an inducer of Mmp-9 and Timp-1 transcription via the JNK and/or Nuclear factor-kappaB (NF-kB) pathways, leading to thickening of the medial layer and denaturation of the extracellular matrix (ECM) in the aortic wall. Thus, OPG may play an important role in the prevention of AAA formation via suppression of TRAIL signaling.

Generation of a Mouse Model for AAAs
Seven-week-old male wild-type and Opg-KO mice of the C57BL/6J strain (CLEA Japan, Inc.) underwent AAA induction via peri-aortic application of 0.5M CaCl 2 . For the control (sham) group, saline was used instead of CaCl 2 (S1 Fig). After AAA induction, a time-course aortic analysis (from day one to week six) was performed. Under anesthesia, mice were perfusionfixed with 4% paraformaldehyde in phosphate buffered saline (PBS) at physiological perfusion pressure. Abdominal aortas were then excised from the mice for histological examinations after images were taken. For RNA isolation, aortas were harvested after perfusion with PBS and stored in RNAlater solution (Ambion). This experimental protocol was approved by the Committee of Animal Experimentation at Hiroshima University (A08-32) and carried out in accordance with this protocol. All surgery was performed under sodium pentobarbital anesthesia, and all efforts were made to minimize suffering during and after surgery. At the end of each experiment, animals were sacrificed either by anesthetic overdose or intracardiac perfusion under anesthesia.

Serum Opg Analysis
Serum Opg and Trail concentrations in wild-type mice at six weeks after AAA induction were measured using an ELISA kits (R&D Systems and RayBiotech).

Morphological Examination
Paraffin-embedded aortic tissues were used to create 6-μm thick sections, which were subsequently stained with hematoxylin & eosin (HE), Elastica van Gieson (EVG), Aniline Blue-Azan, and von Kossa, using standard protocols. The maximum aortic diameter, which included thickened adventitia with inflammation, was measured as the external aortic diameter. For widths of the medial layers of the aorta, the maximum values on the sides to which CaCl 2 was applied were measured. The averages of the maximum and minimum measurements of the internal cross-section of the aorta were calculated for the internal diameters of the aorta. All measurements were performed using Photoshop (Adobe Systems) and Image-J (NIH).

Cell Culture
Mouse aortic SMCs were isolated from the abdominal aorta (from the diaphragm to the bifurcation) in 5-week-old wild-type male mice as previously described [29], and maintained in Dulbecco's Modified Eagle Medium (DMEM) with 10-20% fetal bovine serum (FBS). Cells were growth arrested at 70-80% confluence via incubation in serum-free medium for 48 hours before stimulating cells with rh-TRAIL (CD253; AbD Serotec). Different concentrations of rh-OPG (Peprotech) were used to block TRAIL; MG-132 (Calbiochem) or BAY11-7082 (Calbiochem) was used for inhibition of NF-kB activity, and AS-601245 (Enzo Life Sciences) or SP600125 (Calbiochem) for inhibition of JNK activity two hours before TRAIL induction.

Migration Assay
Migration assays were performed using the ThinCert cell culture insert (Greiner Bio One), a modified Boyden chamber equipped with a polycarbonate membrane filter with 8 μm pores. Mouse peritoneal macrophages were isolated from five-week-old male wild-type mice via intra-peritoneal injection of 3% Brewer thioglycollate medium (Sigma Aldrich) for four days prior to isolation. Samples were maintained and frozen in Roswell Park Memorial Institute (RPMI) medium, as previously described [30]. Mouse aortic SMCs, isolated from the abdominal aorta, or macrophage cells from intraperitoneal fluid were seeded on top of the membranes at a density of 1x10 5 cells, with the bottom of the membrane immersed in 1 μg/ml of rh-TRAIL, 100 ng/ml of rh-MCP-1 (R&D Systems), or 0.5 μg/ml of PDGF (Sigma-Aldrich) in DMEM. Different concentrations of rh-OPG (Peprotech) were also added for inhibition of TRAIL-induced migration. After incubation of macrophages for 90 minutes or SMCs for six hours at 37°C in 5% CO 2 , tops of the membranes were wiped with an absorbent cotton to remove non-migratory cells and then stained with Diff-Quick staining solution (Sysmex). Migrated cells on the bottom surface of the membranes were counted in 10 microscopic fields as previously described [31,32].

Western Blotting
Cell lysate was prepared from growth-arrested VSMCs, which were stimulated with rh-TRAIL and lysed in radio-immunoprecipitation assay (RIPA) lysis buffer [31,32]. Samples containing equal amounts of protein were separated by SDS-PAGE and transferred onto a nitrocellulose membrane. The membrane was incubated with a primary antibody (Mmp-9, goat polyclonal, 1:1000, R&D Systems; Timp-1, goat polyclonal, 1:1000, LSBio; OPG, rabbit polyclonal, 1:1000, Abcam) and subsequently with an appropriate secondary antibody. Signals were visualized using the ECL system (Amersham-Pharmacia Co, UK). Images were captured using Photoshop (Adobe Systems) and densitometry was performed with Image J software (NIH).

Statistical analysis
One-way analysis of variance (ANOVA) with Fisher's post-hoc analysis, was used (if not indicated otherwise), provided that Bartlett's test (p<0.05) showed homogeneity of variances. A nonparametric analysis, the Mann-Whitney's U-test or Kruskal-Wallis test with Scheffe's and Steel-Dwass post-hoc analyses was used. These analyses were performed with Ekuseru-Toukei 2012 software (Social Survey Research Information Co., Ltd.). Multiple regression analyses with spline functions were also performed for external diameter, internal diameter, and medial layer. All data are expressed as mean ± standard deviation (SD). P<0.05 was considered statistically significant.

Absence of Opg Gene-Enhanced AAA Formation
We first tested whether the loss of Opg genes would affect AAA development, which was induced by application of CaCl 2 to the abdominal aorta [13]. In wild-type mice, significant enlargement of the external aortic diameters was found at one week after AAA induction, and was retained at six weeks after induction (Fig 1A and 1B). In Opg-KO mice, the external aortic diameter was also enlarged at one week, and showed gradual dilation afterward. At six weeks after AAA induction, the external aortic diameters of Opg-KO mice were larger than those of wild-type mice. Sham operations did not result in significant changes at any point (S1 Fig). Hematoxylin and eosin (HE) staining of sections showed thinning of the medial layer and enlargement of the internal diameter at one week in both wild-type and Opg-KO mice (Fig 1C, 1D and 1E). However, at six weeks, thickening of the medial layer and dilatation of the internal diameter were evident in Opg-KO mice (Fig 1C, 1D and 1E). Through the application of multiple regression analyses with spline functions, statistically significant increases in the external diameter, medial layer, and internal diameter were also detected in Opg-KO mice at six weeks (S2 Fig).
Elastica van Gieson (EVG) and Azan staining showed typical wavy lamellae of elastic and collagen fibers at regular intervals in the medial layer of wild-type and Opg-KO mice at day zero and at six weeks after the sham operation ( Fig 1F). However, after AAA induction, elastic fibers appeared to have flattened lamellae at thinner intervals, but never disappeared in wildtype mice. In contrast, partial or entire disappearance of the medial elastic lamellae and accumulation of collagen fibers were observed in Opg-KO mice ( Fig 1F). These observations suggest that aortic properties of the extracellular matrix, especially in the media, were severely altered in Opg-KO mice.

Up-Regulation of Opg Expression in Response to AAA Formation
To investigate the role of Opg in AAA formation, its expression was measured in the serum and aortic tissue of wild-type mice. There was no significant difference in serum Opg concentration between sham operation and AAA operation groups (Fig 2A). Instead, the expression level of Opg mRNA in the aorta was up-regulated in response to AAA induction in wild-type mice (Fig 2B). In order to determine whether Opg is produced by aortic SMCs as previously reported [33], we performed western blot analysis and found that Opg protein was only detected in lysates of cultured SMCs from wild-type mice, but not from the Opg-KO mice, with or without rh-TRAIL (S3A Fig). These results suggest that aortic SMCs are the primary source of Opg and its expression increases during development and progression of AAAs.

Up-Regulation of Trail in the media of AAAs in Opg-KO Mice
Given the role of OPG as a decoy receptor for TRAIL, we first tested whether its expression is up-regulated in aortic tissue. Although the aortic expression of Trail mRNA at six weeks after AAA induction tended to be higher in Opg-KO mice than in wild-type mice, the difference was not significant (Fig 2E). Moreover, no difference was found in the serum concentration of Trail between wild-type and Opg-KO mice at six weeks after AAA induction (data not shown).
We next determined whether Trail is up-regulated in SMCs, or macrophages, by doubleimmunofluorescent staining using antibodies that recognize SMA and macrophages (F4/80). At six weeks after AAA induction, Trail was detected weakly in most SMCs of the media of Opg-KO mice, but strongly in some SMCs, particularly those located at the peripheral edge of the medial layer and elastic fibers, in both wild-type ( Fig 2C- . This suggests that Trail is expressed in SMCs, macrophages, and myofibroblasts in the aorta. In order to determine whether Trail would be up-regulated in the absence of OPG, we measured the Trail-positive area in the media (S4 and S6 Figs) and found that this area in Opg-KO mice was significantly larger than that in wild-type mice (Fig 2D).
Since TRAIL enhances apoptosis in cancer [17], we determined whether apoptosis would be detected after AAA induction by immunohistochemical detection of Caspase-9, a marker of apoptosis. Caspase-9 was not detected in the aortic wall six weeks after AAA induction in either wild-type or Opg-KO mice, suggesting that Trail may not be involved in apoptosis in this context (S5 Fig). We also tested whether TRAIL could induce SMC proliferation, given previous reports that it enhances SMC proliferation [34]. An increase in the BrdU-positive SMCs was observed after AAA induction in the medial layer and adventitia of Opg-KO mice compared to wild-type mice (data not shown). However, rh-TRAIL did not induce significant growth, despite a trend for an increased number of cells in SMCs culture system. Thus, whether Trail enhances SMC proliferation during AAA formation remains inconclusive.

Trail is a Chemoattractant for SMCs and Macrophages
As TRAIL has been reported to induce chemotactic migration of monocytes toward the site of inflammation [31], it was hypothesized that TRAIL also functions as a chemoattractant for SMCs. Since Trail was detected in the elastic fibers and the peripheral edge of the medial layer (Fig 2C), this property could be responsible for the accumulation of SMCs in the media. A cell culture-based migration assay confirmed that rh-TRAIL could induce migration of mouse abdominal macrophages, with dose-dependent repression by rh-OPG application (Fig 3A and  3B). Similarly, rh-TRAIL induced the migration of mouse aortic SMCs, with dose-dependent inhibition by rh-OPG (Fig 3C and 3D). These results suggest that the release of a larger quantity of TRAIL induced a greater amount of SMC migration in Opg-KO mice.

Trail Can Induce Its Own Expression
Due to the continuous up-regulation of Trail expression in the absence of Opg, it was hypothesized that Trail could induce its own expression. Within a SMC culture system, incubation with rh-TRAIL induced up-regulation of the expression of Trail mRNA, but not Opg mRNA (S3B and S3C Fig). Trail up-regulation was inhibited by pre-incubation with rh-OPG, whereas rh-OPG had no effect on Trail expression (S3D and S3E Fig). These results suggest that TRAIL-induced Trail mRNA production may be a cause of continuous Trail up-regulation in the development of AAAs in Opg-KO mice.
Mmp-9 and Timp-1 Co-localize with Trail in the Media of AAA Since imbalanced production of MMPs and TIMPs has been suggested to cause changes in medial elastic fibers, we assessed whether Mmp-9 and Timp-1 mRNA levels were altered in the AAA model. Mmp-9 mRNA expression was up-regulated in the aorta of wild-type and Opg-KO mice, as assessed by qRT-PCR (Fig 4A). Timp-1 mRNA expression was continuously up-regulated in both wild-type and Opg-KO mice after AAA induction (Fig 4B). In order to determine whether Mmp-9 and Timp-1 are up-regulated in the media, we measured the Mmp-9-and Timp-1-positive areas in the media by immunofluorescent staining (S6A and S6B Fig). The Mmp-9-and Timp-1-expressing areas in Opg-KO mice were significantly larger than those in wild-type mice (Fig 4C and 4D).
Next, to determine whether Trail regulates Mmp-9 and Timp-1 expression, we performed double immunohistochemical analysis. At six weeks, the expression of Mmp-9 was reduced in wild-type mice (Fig 4EA), while Timp-1 was still expressed with Trail in the medial layer as well as the adventitia (Fig 4EB). In contrast, in Opg-KO mice, focal expression of Mmp-9 was still observed in the medial layer (Fig 4EC), and Timp-1 was expressed mainly in the adventitia (Fig 4ED). These results indicate that focal expression of Mmp-9 in the medial layer of Opg-KO mice, regardless of the continuous expression of Timp-1, could be the main cause of elastic fiber disappearance and might be regulated by Trail.

Mmp-9 and Timp-1 Are Up-Regulated via the JNK and NF-kB Signaling Pathways
TNF-α has been reported to up-regulate Mmp-9 expression via the JNK signaling pathway [35]. Given that TRAIL is a member of the TNF superfamily, we tested whether Trail induces Mmp-9 expression. Within a SMC culture system, Mmp-9 was up-regulated by rh-TRAIL  (Fig 5A and 5B). The distribution of Mmp-9 overlapped with that of phosphorylated JNK in the adventitia (Fig 5C). Mmp-2 expression was also up-regulated by rh-TRAIL via the JNK signaling pathway (S7D and S7E Fig).
TRAIL also induced Timp-1 expression, which was inhibited by rh-OPG (S7C, S7F and S7G Fig). TRAIL-induced Timp-1 mRNA expression was blocked by inhibitors of the NF-kB signaling pathway, MG-132 and BAY11-7082 (Fig 5D and 5E). Timp-1 distribution overlapped with phosphorylated NF-kB (Fig 5F), rather than with phosphorylated JNK (data not shown), suggesting that Trail may induce the expression of Timp-1 via the NF-kB signaling pathway in vivo.

Discussion
In this study, we found that dilation of the abdominal aorta was enhanced with complete destruction/disappearance of elastic fibers in the medial layer of Opg-KO mice by using a CaCl 2 -induced AAA model. Continuous Trail expression was observed in the medial layer of Opg-KO mice and overlapped with the expression of Mmp-9 and Timp-1. In the SMC culture system, TRAIL induced the expression of Mmp-9 and Timp-1 mRNA. Induction of Mmp-9 by TRAIL occurred via the JNK pathway, and Timp-1 was induced via NF-kB and the JNK pathway. Given that Mmp-9 is known to be the primary cause of elastic fiber disruption [9] [36] [37] [38], extracellular matrix remodeling in the medial layer could be associated with dilation of the abdominal aorta. Previous studies have also shown that MMP9 is induced via activation of the JNK pathway in AAA models [13] and that TRAIL has non-apoptotic functions, such as activation of JNK and NF-kB signaling in HeLa and human embryonic kidney 293 cell lines [39,40], although no downstream target genes related to these non-apoptotic aspects have been identified. In the present study, we identified downstream targets of Trail, which is under the control of Opg, suggesting that the Opg-Trail cytokine system could be implicated in the maintenance of medial layer integrity.
Accumulation of myofibroblasts was apparent in the adventitia of Opg-KO mice at six weeks after CaCl 2 treatment. Trail distribution was widely observed in myofibroblasts and colocalized with Mmp9 and Timp1 at one week after treatment (data not shown). However, Trail expression later shifted to a region where cells exist at high density with up-regulated expression of Timp1 in the adventitia. We speculate that Timp1 expression causes ECM accumulation, depriving myofibroblasts of their mobility. In wild-type mice, the accumulation of myofibroblasts in the adventitia was also seen after one week of CaCl 2 treatment, but was attenuated afterwards. On the other hand, in Opg-KO mice, proliferation and accumulation of myofibroblasts lasted up to six weeks after CaCl 2 treatment (data not shown). Myofibroblasts are mainly involved in ECM production and modification, secretion of angiogenic and pro-inflammatory factors, and generation of tensile force [41]. Thus, Opg may also play an important role in maintaining vascular integrity in the adventitia.
In the present study, Opg mRNA levels were up-regulated in the aortic tissue of wild-type mouse AAAs. Our results are consistent with human studies showing an increased tissue concentration of OPG in AAA [27,28]. Recently, Moran et al. reported that aortic dilation and Peritoneal macrophages (arrows in panel a) and aortic SMCs (c) that have migrated to the membrane surface are seen in violet. Chambers were immersed in monocyte chemotactic protein-1 (MCP-1) (100 ng/ml), platelet-derived growth factor (PDGF) (0.5 μg/ml), or rh-TRAIL (1.0 μg/ml). The concentration of rh-OPG was 0.25-1.0 μg/ml. (b, d) Measurements of macrophages (b) or aortic SMCs (d) that have migrated per one mm 2 of membrane area. Data are presented as mean ± SD (at least 3 independent experiments were performed); *p<0.05 or **p<0.01, as compared to controls or TRAIL alone.
doi:10.1371/journal.pone.0147088.g003 rupture was limited in Angiotensin (Ang) II-treated ApoE/Opg double KO (dKO) mice, compared to those of similarly treated ApoE single KO mice, suggesting that Opg could attenuate AAA formation in their model system [24]. One possible explanation for the discrepancy between their results and ours is the different amount of circulating AngII. With continuous infusion of AngII, Opg may accelerate the progression of AAA. However, without AngII addition, Opg may prevent AAA formation through our proposed mechanism. This may suggest that OPG functions as a double-edged sword depending on surrounding conditions. The important role of AngII in the formation of AAA provides us with insight regarding the use of AngII blockers in humans.
In animal studies, the function of Opg in the formation of arteriosclerosis has been a source of controversy. A few studies have demonstrated the promotion of arteriosclerosis by Opg [42,43], yet most studies have reported a preventive role of Opg in cardiovascular disease models [18][19][20][21]42]. Clinical studies have shown elevated serum OPG levels in cardiovascular diseases [25][26][27][28]44], and it is suggested that increased serum OPG levels in humans may be caused by a self-defensive compensatory response to inflammation. In the present study, while Opg mRNA levels were up-regulated in the aortic tissue of wild-type mouse AAAs, serum levels remained the same. In humans, the entire vasculature is involved in inflammation, whereas in a mouse model, lesion areas induced by CaCl 2 application are relatively small. This may be a reason why serum Opg levels remained unchanged in the present wild-type mouse AAA model. Our results support the preventive role of Opg in AAA pathogenesis.
Based on this study, a model for AAA induction is proposed (S8 Fig). After focal application of CaCl 2 , some SMCs are released from the medial layer. In wild-type mice, residual SMCs expressed Trail, which then induced Mmp-9 and Timp-1 expression. The balanced enhancement of these factors may result in the flattening of wavy lamella structure within the media, which resembles vascular remodeling [45]. Until six weeks, SMCs express Opg, attenuate the function of Trail, and continue to proliferate in the medial layer (data not shown), resulting in recovery of the medial layer. In contrast, the loss of Opg may lead to continuous Trail mRNA expression in SMCs via an autocrine mechanism. Prolonged up-regulation of both Mmp-9 and Timp-1, causing a local imbalance, could result in complete destruction of the elastic lamella. After this loss of elastic lamella, proliferation of SMCs was delayed but continued in the medial layer (data not shown), leading to thickening of the medial layer. Thus, in the aortas, OPG may function as an anti-inflammatory molecule.
In the adventitia, small populations of SMCs might migrate and attract macrophages by secreting Trail. The accumulation of SMA/Vimentin-positive cells might be attributed to continuous Trail secretion from SMCs and macrophages, or myofibroblasts derived from macrophages, as well as fibroblasts [46]. This process may be accompanied by a significant increase in adventitia volume. Taken together, Trail could be considered a cytokine that triggers inflammatory responses. Opg, as an antagonist of Trail, may prevent excessive inflammation. Thus, Opg and Trail together may contribute to the integrity of the vascular wall. In humans, OPG may also function as an inhibitor of TRAIL; if this inhibitory effect is insufficient, formation of where [z] + = (z+ | z |) / 2, β 0 , β 1 , β 2 , β 3 and τ are unknown parameters to be estimated. The terms ε i , i = 1,. . ., n, represent errors, which are mutually independent normal distributions with means of zero and variances of σ 2 . These unknown parameters were estimated with the least square method. The resultant estimates are:b 0 ¼ 0:2333;b 1 ¼ À0:0040;b 2 ¼ À0:0993;b 3 ¼ 0:3795; andt ¼ 3:02: The difference in time-trends between the two groups, which is expressed byb 3 ¼ 3:795; was highly statistically significant (p = 1.64×10 −11 ). (b) Using a similar method to the analysis of external diameter data (a), the following regression model was applied to medial layer data: log(y i ) = β 0 + β 1 t i + β 2 s i + β 3 s i × t i + ε i , i = 1,. . ., n. The resulting unknown parameters were as follows:b 0 ¼ À3:698;b 1 ¼ 0:0191;b 2 ¼ 0:1347; ðp ¼ 0:0027Þ;b 3 ¼ 0:0090 ðp ¼ 2:39 Â 10 À6 Þ: (c) Using a similar method to that discussed above, the following regression model was applied to internal diameter measurement data: log(y i ) = β 0 + β 1 t i + β 2 (t i − τ) 2 + β 3 s i ×[t i -τ] + + ε i , i = 1,. . ., n.   Mmp-9 (a, b) and Timp-1 (d, e) mRNA in mouse aortic SMCs within a culture system induced by rh-TRAIL (10 ng/ml). SP-600125 (3-30 μM) (a) and AS-601245 (0.2-20 μM) (b) were used to inhibit the JNK signaling pathway. MG-132 (0.2-20 μM) (d) and BAY11-7082 (1-10 μM) (e) were used to inhibit the NF-kB pathway. Data are presented as mean ± SD; *p<0.05 or **p<0.01, as compared to controls or TRAIL alone. Samples were in triplicate for each group. (c, f) Representative double immunofluorescent staining images of abdominal aortas in wild-type and Opg-KO mice at six weeks, with pJNK (panels A-b, B-b, and C-b in c) or pNF-kB (panels D-b, E-b, and F-b in f) in green, and Mmp-9 (panels A-c, B-c, and C-c in c) or Timp-1 (panels D-c, E-c, and F-c in f) in red. pJNK signal merged with Mmp-9 (panels A-d, B-d, and C-d in c). pNF-kB signal merged with Timp-1 (panels A-d, B-d, and C-d in f). Rectangles in panels B and E show magnified areas in C and F, respectively. Nuclei are stained with DAPI in blue (m: medial layer; a: adventitia). Scale bars in panels A, B, D, and E represent 100 μm. Scale bars in panels C and F represent 50 μm. of Trail (b, d, e) and Opg mRNA (c) in a mouse aortic SMC culture system. Specific concentrations of rh-TRAIL (1-100 ng/ml) were used for induction of Trail (b) and Opg (c) expression. (d) Trail mRNA expression induced by rh-TRAIL (10 ng/ml) was inhibited by rh-OPG (5-50 ng/ml). (e) Trail mRNA expression was not affected by OPG alone (5-50 ng/ml). Samples were in triplicate for each group. Data are presented as mean ± SD, ÃÃ p<0.01, Ã p<0.05 compared to control or rh-TRAIL alone. , and Timp-1 (f, g) mRNA in mouse aortic SMCs culture system. The indicated concentrations of rh-TRAIL (1-100 ng/ml) were used to induce Mmp-9 (a), Mmp-2 (d) and Timp-1 (f). Mmp-9 (b) as well as Timp-1 (g), induced by rh-TRAIL (10 ng/ml), are inhibited by rh-OPG (5-50ng/ml). Mmp-2 (e), induced by rh-TRAIL (10 ng/ml), is inhibited by a JNK inhibitor, SP-600125 (3-30 μM). (c) Mmp-9 and Timp-1 protein are induced by rh-TRAIL (10 ng/ml) after 2 and 0.5 hours, respectively. Samples were in triplicate (or more) for each group. Data are presented as mean ± SD; Ã p<0.05 or ÃÃ p<0.01, as compared to controls or rh-TRAIL alone. (EPS) In the acute phase, dilation of internal aortic dimensions, thinning of the medial layer (red arrows), and thickening of the adventitia occur. (c) In the late phase, vascular size appears to be recovered, but linear elastic lamella structure remains within the media and inflammatory cells are found in the adventitia of wild-type mice. In contrast, increased vascular size and thickening of both the media and adventitia is observed continuously in Opg-KO mice. EC: endothelial cells; SMC: smooth muscle cells. (EPS)