The 146-kDa Pasteurella multocida toxin (PMT) is the main virulence factor to induce P. multocida-associated progressive atrophic rhinitis in various animals. PMT leads to a destruction of nasal turbinate bones implicating an effect of the toxin on osteoblasts and/or osteoclasts. The toxin induces constitutive activation of Gα proteins of the Gq/11-, G12/13- and Gi-family by deamidating an essential glutamine residue. To study the PMT effect on bone cells, we used primary osteoblasts derived from rat calvariae and stromal ST-2 cells as differentiation model. As marker of functional osteoblasts the expression and activity of alkaline phosphatase, formation of mineralization nodules or expression of specific transcription factors as osterix was determined. Here, we show that the toxin inhibits differentiation and/or function of osteoblasts by activation of Gαq/11. Subsequently, Gαq/11 activates RhoA via p63RhoGEF, which specifically interacts with Gαq/11 but not with other G proteins like Gα12/13 and Gαi. Activated RhoA transactivates the mitogen-activated protein (MAP) kinase cascade via Rho kinase, involving Ras, MEK and ERK, resulting in inhibition of osteoblast differentiation. PMT-induced inhibition of differentiation was selective for the osteoblast lineage as adipocyte-like differentiation of ST-2 cells was not hampered. The present work provides novel insights, how the bacterial toxin PMT can control osteoblastic development by activating heterotrimeric G proteins of the Gαq/11-family and is a molecular pathogenetic basis for understanding the role of the toxin in bone loss during progressive atrophic rhinitis induced by Pasteurella multocida.
Bone tissue is a common target for bacterial infections. Diseases like caries, periodontitis or osteomyelitis are due to infections by Streptococcus mutans, Actinobacillus actinomycetemcomitans or Staphylococcus aureus inter alia. The mechanism of bacterial-induced bone damage may be caused by factors released from pathogens, which interact with bone matrix or affect bone cells, or by bacteria which directly invade bone cells to initiate pathological changes [1]. One of the skeleton affecting bacteria is Pasteurella multocida, which causes various diseases in men and an`imals. As a commensal P. multocida is found mainly in the nasal/pharyngeal space of domesticated and wild animals and is frequently isolated from cat and dog bites [2]. P. multocida is directly or as a supportive factor connected to several diseases like haemorrhagic septicaemia in hoofed animals, avian cholera or snuffles in rabbits [3]. In the case of the economically important progressive atrophic rhinitis P. multocida has a central role [4]. Atrophic rhinitis is characterized by drastic degeneration of nasal turbinate bones, leading to a shortening and/or twisting of the snout accompanied by growth retardation of young pigs. Besides domesticated pigs, rabbits, wild pigs and cattle show atrophic rhinitis-like symptoms [3]. The causative agent of atrophic rhinitis is Pasteurella multocida toxin (PMT), which is produced by capsular type D and some type A strains [5]. Inoculation of PMT alone is sufficient to generate all symptoms of atrophic rhinitis in animals [6]. Bone tissue is constantly rebuilt by the action of osteoblasts and osteoclasts [7]. Accordingly, analysis of nasal turbinates in atrophic rhinitis disclosed effects of PMT on both types of cells. Besides bone resorption areas, a depletion of osteoblasts was reported [8]. In in vitro models the toxin inhibits osteoblastic differentiation and stimulates the differentiation of osteoclasts [9]–[11]. Moreover, a PMT-induced activation of RhoA seems to be important for the blockade of osteoblast differentiation [12]. Notably, PMT induces bone destruction but exhibits no obvious cytotoxicity [3], [13]. Up to date a detailed analysis of PMT-activated signaling pathways in osteoblasts was hampered by the fact that the intracellular substrate of the toxin was unknown. Recently, we identified the molecular mechanism of PMT. The toxin stimulates heterotrimeric G protein signaling. In the switch II region of the α-subunit of heterotrimeric G proteins, PMT deamidates a specific Gln residue, which is involved in GTP hydrolysis [14], [15]. Once the α-subunits are deamidated, they have a constitutive active phenotype. PMT targets α-subunits of the Gαq/11-, Gα12/13- and Gαi-family [16]–[20]. A consequence is the activation of multiple signal transduction pathways, leading in a cell type specific manner to strong mitogenicity, anti-apoptotic effects or restructuring of the cytoskeleton [21], [22]. Differentiation and activity of osteoblasts and osteoclasts are tightly regulated. Osteoblast differentiation is stimulated by various factors like BMP, PTH or growth factors as IGF or TGF, acting on different types of receptors [23]. In addition, previous studies showed that various heterotrimeric G proteins and G protein-coupled receptors are involved in the regulation of osteoblast differentiation. Thereby, Gαs and Gαi signaling appear to control differentiation of bone cells in an opposite manner [24], [25]. The opposing effects of Gαs and Gαi on osteoblasts depend at least partly on the regulation of adenylyl cyclase [26]. Furthermore, it was shown that a constitutive active mutant of Gαq blocked differentiation of osteoblasts. Transgenic mice, expressing this mutant in osteoblast progenitors, developed osteopenia [27]. Also the mitogen-activated protein kinase (MAPK) pathway contributes to bone development. However, the data available are inconsistent, because studies provide evidence for positive as well as for negative effects on bone cell development upon MAPK activation [28]–[31]. Elucidation of the molecular mechanism of PMT and recent progress in the understanding of bone cell development prompted us to analyze the effects of PMT on osteoblasts and osteoblast precursors in more detail. Here we present evidence that PMT controls the differentiation of osteoblasts by constitutive activation of Gαq/11, subsequent stimulation of RhoA/Rock pathway via p63RhoGEF and transactivation of MAPK cascade.
To study the effects of PMT on osteoblast differentiation, we used the established cell culture model of ST-2 cells. ST-2 cells are characterized by their potency to differentiate into osteoblast or adipocyte lineages. Thus, in respect to differentiation, the cells are comparable to osteoblast progenitor cells. The primary effect of PMT is the activation of heterotrimeric G proteins by deamidation of a conserved glutamine. Recently, a monoclonal antibody was described, which selectively recognizes the PMT-deamidated G proteins but not the unaffected ones [32]. By using this antibody, we could demonstrate that the toxin-induced deamidation takes place also in ST-2 cells (Fig. 1A). Thus, we studied osteoblastic differentiation by measuring the activity of alkaline phosphatase (ALP) after 10 d, which is an early marker of osteoblasts and indicates proper differentiation. As shown in Figure 1B, PMT but not the catalytically inactive mutant PMTC1165S inhibited the osteoblast formation. Moreover, as determined by the concentration dependent blockade of ALP activity, the toxin was found to be a strong inhibitor of osteoblastic differentiation. 10 pM PMT nearly abolished osteoblastic differentiation (Fig. 1C). Additionally, osteoblastic differentiation can be visualized by using the phosphatase substrate enzyme labeled fluorescence (ELF) 97, which specifically stains ALP. Control cells showed strong staining with ELF97, indicating proper osteoblast differentiation, whereas no alkaline phosphatase staining was visible in PMT-treated cells (Fig. 1D). To exclude that PMT induces degradation of ALP, we quantified mRNA levels. In PMT-treated cells ALP expression levels decreased as compared to cells solely cultured in osteoblastic differentiation medium. In contrast, PMTC1165S exhibited no effect on mRNA levels (Fig. 1E). Because ST-2 cells possess the potency to differentiate to diverse lineages, we tested whether PMT also affects differentiation into the adipocyte lineage. Induction of adipocyte differentiation was monitored by the formation of lipid vacuoles. ST-2 cells were incubated for 6 d with adipocyte differentiation medium and lipid droplets were visualized by Oil Red O staining. As shown in Figure 2A, coincubation with PMT did not impair adipocyte differentiation. In contrast, PMT but not PMTC1165S, even increased lipid droplet formation compared to the induction by differentiation medium alone (Fig. 2B). The increase in Oil Red O staining could be due to more intense staining or more cells showing staining. To address this question we counted positive- and un-stained cells. PMT treatment significantly increased the total cell number (adipocyte differentiation medium (adm) 183, ±21 SD; adm+PMT 255, ±20 SD, p<0. 01, n = 8) and the relative portion of Oil Red O-positive cells (adm 30. 5%, ±4% SD; adm+PMT 38. 0%, ±3. 8% SD, p<0. 01, n = 8). Adipocytes are characterized by the expression of several marker proteins, such as peroxisome proliferator-activated receptor γ (PPARγ) or CCAAT/enhancer-binding family of proteins (C/EBPα). Congruently, quantification of mRNA expression levels of those markers showed no inhibitory effects of PMT (Fig. 2C). To exclude the possibility that PMT is not able to activate heterotrimeric G proteins under adipogenic conditions, we verified G protein deamidation in an immunoblot. PMT but not PMTC1165S led to deamidation under these conditions (Fig. 2D). A system of primary osteoblasts from calvariae of neonatal rats was used to strengthen our studies. Also these primary osteoblasts were directly targeted by PMT as shown by deamidation of heterotrimeric G proteins (Fig. 3A). For functional studies, primary osteoblasts were cultivated for 4–10 d and ALP activity was determined by the ALP activity assay or the ELF97 staining, respectively. As found for the differentiation of ST-2 cells to the osteoblastic lineage, PMT inhibited ALP activity of primary osteoblasts at picomolar concentrations (Fig. 3B). In the PMT-treated primary osteoblasts no ALP staining was detectable with ELF97 (Fig. 3C). In accordance with the diminished ALP activity, also mRNA levels of ALP were reduced by PMT. Specific transcription factors, e. g. runt-related transcription factor 2 (Runx2) or osterix (SP7) regulate osteoblast differentiation. qPCR analysis of SP7 and Runx2 expression revealed that PMT treatment significantly reduced the expression of SP7 but not Runx2 in primary osteoblasts (Fig. 3D). The formation of mineralization nodules is another marker for osteoblasts. Also mineralization nodules, detected by van Kossa staining, were nearly abolished in PMT-treated samples (Fig. 3E). The small GTPase RhoA is one of the downstream effectors of PMT-activated heterotrimeric G proteins [17]. Furthermore, it was shown that RhoA is involved in inhibition of osteoblastic differentiation [12]. Therefore, we tested whether the direct activation of RhoA is sufficient to block osteoblastogenesis. To this end, we utilized cytotoxic necrotizing factor (CNF) y from Yersinia pseudotuberculosis, which is a specific activator of RhoA [33]. PMT and CNFy activate RhoA as shown by effector pulldown of activated RhoA (Fig. 4A). Treatment of ST-2 cells with increasing concentration of CNFy blocked osteoblastogenesis as measured by the activity of the ALP (Fig. 4B). RhoA activates several effector proteins like the Rho-associated, coiled-coil containing protein kinase (Rock). Pharmacological inhibition of Rock with Y27632 abrogated the inhibitory effect of PMT on osteoblast differentiation (Fig. 4C). In ST-2 cells Y27632 not only reversed the effect of PMT but also increased osteoblastic differentiation. This pro-osteoblastic effect of Y27632 was already previously described [34] and might be due to the reduction of RhoA/Rock signaling below the basal activity level. Our results demonstrate that active RhoA/Rock-signaling inhibits osteoblastogenesis. In turn blockade of RhoA/Rock impairs the PMT effect on differentiation. The small GTPase RhoA can be stimulated by members of the Gαq/11- and Gα12/13-family of heterotrimeric G proteins. Via different Rho guanine nucleotide exchange factors (GEF) like p115RhoGEF or p63RhoGEF the heterotrimeric G proteins are linked to RhoA [35], [36]. To determine the Gαq/11 dependent portion of PMT-induced RhoA activity, we utilized a specific inhibitor of Gαq/11 signaling, YM-254890 [37]. In the presence of YM-254890 the PMT-stimulated RhoA activity was strongly diminished (Fig. 4D). The pivotal role of Gαq/11 in PMT-induced RhoA activity prompted us to study the effect of Gαq/11 inhibition on osteoblast differentiation. Blockade of PMT-induced Gαq/11 activation by YM-254890 abrogated the toxins effect on ALP activity and expression in ST-2 cells (Fig. 4E). Congruently, in primary osteoblasts pharmacological inhibition of RhoA/Rock or Gαq/11 prevent the PMT effect on osteoblast differentiation as measured by ALP activity (Fig. 4C/E). A specific RhoGEF protein, which couples Gαq/11 to RhoA, is p63RhoGEF [36]. This RhoGEF is not ubiquitously expressed [38], however, we detected its expression in ST-2 cells and primary osteoblasts. Next, we addressed the question whether p63RhoGEF is involved in PMT-induced inhibition of osteoblastogenesis. To this end, we depleted endogenous p63RhoGEF by sh-RNA, using an adenoviral transfection system [39]. As shown in Fig. 5 A/B, sh-p63RhoGEF effectively reduced the endogenous content of p63RhoGEF in stromal ST-2 cells and rat primary osteoblasts. Both types of p63RhoGEF-knockdown cells exhibited declined RhoA activity as compared to control cells after PMT treatment (Fig. 5C/D). These results indicated that a predominant portion of PMT-induced RhoA activity depends on the Gαq/11-p63RhoGEF axis. Moreover, we analyzed the ability of PMT to inhibit osteoblast function in primary osteoblasts after p63RhoGEF-knockdown. In control cells PMT inhibited ALP activity as measured by the ELF97 staining. In contrast, in p63RhoGEF-knockdown cells the inhibitory effect of PMT on osteoblastogenesis was significantly abrogated as shown by strong activity of ALP (Fig. 5E/F). By this approach we confirmed that the Gαq/11-p63RhoGEF-RhoA axis is of major importance for PMT-dependent inhibition of osteoblast differentiation. The mitogen-activated protein kinase (MAPK) pathway has been implicated in regulation of osteogenesis [40]. Therefore, we tested whether PMT stimulates the MAPK pathway in osteoblasts by measuring phosphorylation of the extracellular signal-regulated kinase (ERK) 1/2. To this end serum-starved stromal ST-2 cells were incubated with PMT and ERK activity was determined by an immunoblot approach. PMT strongly enhanced ERK activity as shown in Fig. 6A. Additionally, we studied the effect of the specific RhoA activator CNFy. Similar to PMT treatment, the RhoA activation by CNFy increased ERK phosphorylation. Next, we asked whether PMT-induced MAPK activation is involved in the inhibition of osteoblast differentiation. The MEK-1 inhibitor PD98059 effectively abrogated the PMT effect on osteoblastogenesis in ST-2 cells and primary osteoblasts as measured by ALP activity. PD98059 also blocked PMT-induced ERK phosphorylation (Fig. 6B/C). The MAPK/ERK pathway depends on the small GTPase Ras, which is the major switch between MAPK cascade and the growth hormone receptor. We addressed the question, whether the PMT-dependent MAPK activation depends on Ras. To this end, we utilized TpeL (toxin perfringens large), a toxin produced by Clostridium perfringens. TpeL mono-O-GlcNAcylates specifically Ras and inhibits thereby Ras signaling and Ras-Raf interaction [41]. However, at higher concentrations TpeL is also known to affect Rac1. Therefore, we confirmed that in ST-2 cells and at utilized concentrations TpeL only acts on Ras but not on Rac1 (Protocol S1 and Figure S1). For further experiments a Ras-selective concentration of TpeL was used. Preincubation of ST-2 cells with TpeL inhibited PMT- and CNFy-induced ERK phosphorylation, demonstrating that MAPK activation by PMT and CNFy depends on functional Ras (Fig. 6A). This result prompted us to study, whether the activation of MAPK depends directly on PMT-induced RhoA activity. Y27632, a known inhibitor of the RhoA-regulated Rock I and II, impaired ERK phosphorylation in ST-2 cells and primary osteoblasts (Fig. 6C). Additionally, the Gαq/11- induced MAPK activation was studied by using the inhibitor YM-254890 and the p63RhoGEF knockdown cells. YM-254890 abolished PMT-induced ERK phosphorylation. Most interestingly, also the knockdown of p63RhoGEF decreased PMT-induced MAPK signaling in stromal ST-2 cells (Fig. 6D). Both results implicate a Gαq/11 dependent transactivation of the MAPK cascade via the p63RhoGEF-RhoA-Rock axis. This signaling pathway negatively controls osteoblastogenesis.
Atrophic rhinitis is characterized by increased bone resorption by osteoclasts and a lack of bone regeneration by osteoblasts [8], [42]. In this study we focused on the effect of the causative agent of atrophic rhinitis, PMT, on osteoblast differentiation and activity. Osteoblasts develop from mesenchymal stem cells [43]. These stem cells are multipotent cells, having the potential to differentiate amongst others to adipocytes, osteoblasts or chondrocytes [44]. Therefore, we utilized stromal ST-2 cells derived from murine bone marrow as a cell culture model [45]. Like primary mesenchymal stem cells, ST-2 cells give rise to different cell lineages like adipocytes [46], osteoblasts [47], or hematopoiesis supporting cells [48]. Under osteogenic conditions ST-2 cells differentiate into osteoblasts. This can be determined by the measurement of various specific markers of osteoblasts like alkaline phosphatase activity. We found that PMT is able to inhibit osteogenic differentiation of stromal cells as measured by the activity and mRNA expression of the alkaline phosphatase. This effect completely depended on the catalytic action of PMT as the inactive mutant (PMTC1165S) exhibited no inhibitory effect on osteoblastic differentiation of ST-2 cells. The high potency of PMT is reflected by the low concentrations sufficient for impairment of cell differentiation. Because of the high potency and effectiveness of PMT to block osteogenic differentiation, we were prompted to test, whether the toxin inhibits any kind of differentiation in stromal ST-2 cells; e. g. osteogenic and/or adipogenic differentiation. Therefore, we cultured stromal ST-2 in a medium forcing adipogenesis. Interestingly, PMT was not able to reduce differentiation of the adipocyte lineage. In line with these findings, the toxin was not able to reduce the mRNA levels of PPARγ and C/EBPα, which typically increase during adipogenesis of ST-2 cells. However, PMT even increased Oil Red O staining. Whether the observed rise in cell number completely accounts for increased Oil Red O staining or the increased expression of transcription factors like C/EBPα is additionally involved, should be clarified in further studies. If the toxin even enhances adipocyte development should also be addressed in a subsequent work. The data indicate that PMT is not a general inhibitor of any type of differentiation but a specific inhibitor of osteoblastic but not adipogenic differentiation in stromal cells like ST-2. In another cell culture model PMT inhibited adipogenesis [49]. However, a different cell type (NIH3T3-L1) was used, which is hardly comparable with ST-2 cells. Primary osteoblasts from newborn rat calvariae were used to verify the results obtained with the cell culture model ST-2. Martineau-Doizè and colleagues previously demonstrated that PMT-challenged rats develop atrophic rhinitis like symptoms [50]. Therefore, our model system of primary osteoblasts from rat calvariae should provide insights into the pathogenesis under veterinarian conditions. As observed for ST-2 cell differentiation, PMT strongly impaired the osteogenic development of primary osteoblasts as measured by early markers (ALP) or late markers of osteoblastogenesis (mineralization nodules). Osteoblast development is under the control of specific transcription factors. For example RUNX2 and osterix (SP7) are well known regulators of osteogenic differentiation, RUNX2 as an early transcription factor and SP7 as a late one [44]. PMT induced a significant down regulation of the transcription factor SP7, indicating that not only expression of osteoblast specific proteins, like ALP, is down regulated, but also master regulators of osteoblast differentiation are affected by PMT. However, PMT affected SP7 much stronger as compared to RUNX2. This might be due to the differentiation status of primary osteoblasts, which already undergo differentiation. Therefore, the late transcription factor SP7 might be more active and can be more efficiently regulated by PMT. PMT reportedly affects primary osteoblasts and osteoclasts in various in vitro systems. Mulan and coworkers performed studies with co-cultures of osteoblasts and osteoclasts. They discussed the question whether both osteoblasts and osteoclasts are directly affected by PMT or whether the toxin targets one cell type to induce effects in the other cell type in a paracrine manner [51]. To unambiguously clarify that PMT directly acts on Gα proteins in osteoblasts, we utilized a monoclonal antibody, which selectively detects a PMT-induced deamidation [32]. This toxin-induced modification of Gα subunits was observed in osteoblastic cells indicating a direct action of PMT. Although PMT did not impair adipocytic differentiation of ST-2 cells, we could also verify the toxin activity under adipocytic conditions. Therefore, we conclude that PMT specifically inhibits the osteoblastic differentiation of stromal ST-2 cells but not adipocytic differentiation, although G proteins are deamidated under both conditions. To analyze the signal transduction pathway of PMT-induced blockade of osteoblastogenesis, the role of Rho proteins was studied. RhoA is a common effector of Gα12/13 and Gαq/11 and PMT was shown to stimulate RhoA via both G protein families [17], [52]. Because previous studies gave evidence for an important role of RhoA in PMT-induced blockade of osteoblast differentiation [12], we started to investigate the pathway utilized by PMT to induce RhoA activation. We observed an increased RhoA activity, after treatment of ST-2 cells and primary osteoblasts with PMT. Interestingly, a specific inhibitor of Gαq/11, YM-254890 [37], inhibited toxin-induced RhoA activation. These results indicate that in the cells studied, RhoA stimulation is predominantly dependent on Gαq/11 but not on Gα12/13. In a next step we studied the effect of Gαq/11 inhibition on PMT-dependent blockade of osteoblast differentiation. Gαq/11 inhibition by YM-254890 abolished the inhibitory effect of PMT on the expression of osteoblast markers (e. g. , alkaline phosphatase) during osteoblast differentiation. These results confirmed the important role of Gαq/11 in PMT-induced effects. Moreover, our results are in line with the studies of Ogata et al. showing that ectopical expression of a constitutive active mutant of Gαq impairs differentiation and induces osteopenia [27], [53]. In addition, inhibition of Rock abrogated the effects of PMT on osteoblast differentiation in stromal ST-2 cells and primary osteoblasts reconfirming the pivotal role of active RhoA/Rock as a negative regulator of osteoblastic differentiation [12], [34]. Because RhoA and Gαq/11 play pivotal roles in PMT-induced osteoblast impairment, we were encouraged to elucidate the missing link between these signaling factors. Heterotrimeric G proteins activate RhoA via RhoGEF proteins, e. g. p115RhoGEF (Gα12/13) or LARG (Gα12/13, Gαq/11) [35], [54], [55]. Moreover, p63RhoGEF specifically couples Gαq/11 but not Gα12/13, to RhoA activation [36]. By immunoblot analysis we detected expression of several splice variants of p63RhoGEF in stromal ST-2 cells and primary osteoblasts. To clarify the involvement of p63RhoGEF in PMT-induced inhibition of osteoblastogenesis, we utilized an adenoviral shRNA knockdown of p63RhoGEF. p63RhoGEF knockdown in osteoblasts dramatically diminished PMT-induced RhoA activity. These findings indicate that a major portion of RhoA activation depends on the Gαq/11-p63RhoGEF axis. Therefore the Gαα12/13-induced RhoA activation via other RhoGEFs may represent only a minor part of entire RhoA activity. Finally, the inhibitory effect of PMT on osteoblastogenesis in primary osteoblasts was compared to p63RhoGEF knockdown cells. Primary osteoblasts depleted for p63RhoGEF were not affected by PMT, whereas differentiation of control cells was inhibited by PMT intoxication. These results strongly suggest that Gαq/11 activity is inhibitory to osteoblast differentiation. Furthermore, RhoA stimulation due to the Gαq/11-specific p63RhoGEF is sufficient for this effect. The contribution of MAPK signaling in osteoblast differentiation is under discussion [40]. Inhibition of MAPK cascade at the level of growth factor receptor, MEK-1 or ERK leads to an increased differentiation of osteoblasts in different models as primary calvaria-derived osteoblasts or in pre-osteoblastic cell lines [28], [29]. It is known that PMT induces mitogenic signaling via MAPK-pathway in various cell lines as rat fibroblasts or HEK293 cells [13], [21]. Therefore, we analyzed the effect of PMT on the MAPK pathway in osteoblastic cells by measuring ERK phosphorylation. PMT was found to be a strong activator of MAPK signaling in ST-2 cells and primary osteoblasts. In line with our observation, it is described that MAPK activation blocks osteoblast differentiation. Congruently, inhibition of PMT-induced ERK phosphorylation abrogated the toxin' s effect on osteoblastogenesis. Utilizing various approaches, we examined the PMT-utilized pathway to stimulate MAPK signaling in ST-2 cells and primary osteoblasts. Inhibition of Gαq/11, Rock and knockdown of p63RhoGEF blocked the toxin-induced ERK phosphorylation. This indicates, that PMT-activated Gαq/11 leads via p63RhoGEF, RhoA and Rock to a transactivation of the MAPK cascade. Inhibition of Ras by TpeL toxin, which inactivates Ras by GlcNAcetylation [41], supported the hypothesis that the transactivation of the MAPK cascade by PMT depends on functional Ras. Moreover, direct activation of RhoA by CNFy was sufficient to transduce MAPK activation in a Ras dependent manner. However, it is loosely understood how Rho/Rock signaling leads to Ras-dependent MAPK activation. It was suggested that actin dynamics provide a link between Rock and Ras activity [56]. Previously, RhoA-induced MAPK signaling has been implicated in osteoblastogenesis [40]. More recently, a genome wide analysis revealed the GEF Trio responsible for sustained MAPK pathway activation [57]. Trio contains a primary Rac-specific and a secondary Rho-specific GEF domain, of which the latter one is highly homologous to p63RhoGEF and can be activated by Gαq/11 [58]. Here, in osteoblastic cells, we identified p63RhoGEF as a Gq effector, involved in MAPK transactivation via RhoA. p63RhoGEF exhibits a restricted tissue distribution [38] and may represent a specific RhoGEF in osteoblastic cells, important for Gαq/11 dependent signaling. Thus, we suggest that PMT affects pre-/osteoblasts by activating the Gαq/11-p63RhoGEF-RhoA axis. This leads to transactivation of the MAPK pathway resulting in inhibition of the osteoblastogenesis. Besides Gαq/11 PMT activates α-subunits of the Gα12/13 and Gαi family [16]. Also these G proteins are associated with proliferative signaling, i. e. MAPK pathway stimulation [59], [60]. However, in the tested osteoblastic cells, stromal ST-2 cells and rat calvaria-derived primary osteoblasts the PMT-activated Gαq/11 pathway apparently prevails. The pivotal clinical symptom of atrophic rhinitis is the atrophy of nasal turbinate bones. Over the last decades it was discovered that infections with P. multocida and/or Bordetella bronchiseptica give rise to atrophic rhinitis [61]. The virulence factors of B. bronchseptica and P. multocida are dermonecrotic toxin (DNT) and PMT, respectively. DNT activates small GTPases of the Rho family like RhoA, Rac and Cdc42 by deamidation or polyamination and impairs osteoblastogenesis [61], [62]. Our results with the specific RhoA activator CNFy strengthen the hypothesis that DNT-induced activation of the small GTPase RhoA is the key for the observed effects on bone cells. However, combined effects of DNT, directly acting on Rho GTPases, and PMT, activating Rho GTPases via Gαq/11-p63RhoGEF, might account for the exacerbation of the disease in the case of coinfection. A single infection with B. bronchiseptica causes only moderate bone loss whereas coinfection with P. multocida induces more drastic effects called progressive atrophic rhinitis [61]. Moreover, de Jong and Nielson recognized P. multocida as the causative agent of progressive atrophic rhinitis without any coinfection necessary [4]. This drastic degradation of bone tissue might be explained by the synergy of the PMT-induced effects on bone cells. On the one hand, PMT specifically inhibits osteoblastic differentiation and function and, therefore, hinders new bone formation. For this purpose, PMT utilizes a distinct signaling pathway, which we present in this work. On the other hand, PMT stimulates osteoclast activity and induces thereby a reduction of bone mass [61]. Whether the effect of PMT on osteoclast activity and/or differentiation is direct or indirect is under discussion [51]. For example, osteoclast differentiation is regulated by osteoblast-derived factors. E. g. receptor activator of NF-κB ligand (RANKL) is a positive osteoblast-derived factor for osteoclastogenesis; whereas osteoprotegerin (OPG) is a negative regulator [63]. Therefore, PMT should at least indirectly affect osteoclast development by targeting osteoblasts. In further studies it would be of interest to clarify the effect of PMT on osteoclasts and osteocytes, which also participate in bone tissue renewal. Besides this obvious impact on bone tissue, the inhibition of osteoblastogenesis by PMT might result in a further pathogenetic advantage for P. multocida as a strong functional interaction of bone and the immune system takes place [64]. Recently, the involvement of osteoblasts in B cell differentiation was demonstrated [65], [66]. Additionally, it is known that PMT is a poor immunogene. Pigs suffering from atrophic rhinitis do not develop protective or specific immune response [67], [68]. Moreover, colonization of piglets with toxigenic but not with non-toxigenic strains of P. multocida reduces serum IgA and IgG response to ovalbumin [69], [70]. Whether the inhibition of osteoblast differentiation via the Gαq/11-p63RhoGEF axis is associated with these previously described immune modulatory effects of PMT should be analyzed in further studies. This would present an important function of PMT in addition to the manifest destruction of bone tissue. In summary, our findings indicate that PMT-induced Gαq/11 activation impairs osteoblastogenesis via a RhoA – MAPK pathway (Fig. 7). In pre-/osteoblasts, Gαq/11 and RhoA/Rock is linked by p63RhoGEF. PMT-induced RhoA/Rock activation leads to a Ras-dependent transactivation of the MAPK cascade, which is responsible for inhibition of osteoblastogenesis. Thus, the bacterial toxin PMT regulates the osteoblastic cell fate in a heterotrimeric G protein dependent manner.
PCR primers were from Apara (Denzlingen, Germany). All other reagents were of analytical grade and purchased from commercial sources. Murine stromal ST-2 cells were obtained from the Leibniz Institute DSMZ (German Collection of Microorganisms and Cell Cultures) and cultivated in RPMI 1640 supplemented with 10% FCS. ST-2 cells were incubated to differentiate into adipocytes or osteoblasts in the corresponding induction medium for 10 days. The adipocyte differentiation medium (adm) consisted of RPMI 1640 (Gibco) supplemented with 10 µg/mL insulin (Sigma) and 40 ng/mL dexamethasone (Sigma). The osteoblast differentiation medium (odm) consisted of RPMI 1640 (Gibco) supplemented with ascorbic acid (284 µM) and β-glycerophosphate (200 µM). Medium including supplements was changed every two days. Primary osteoblasts were isolated from 2–3 day old rats using collagenase digestion [71]. The crushed skulls were incubated at 37°C in RPMI 1640 Medium containing 0. 1% collagenase P for 15 min per digestion cycle. Extracted cells were harvested and resuspended in RPMI 1640 Medium containing 10% FCS. Fractions 2 to 5 were pooled and used for further experiments. After 3 days cultures were trypsinized and seeded for further experiments. Cell lysates were prepared as follows: Cells were grown to confluency and serum starved overnight. After 30 min preincubation with the indicated inhibitors the cells were incubated with PMT (1 nM, 5 h). Thereafter cells were lysed in RIPA buffer (50 mM Hepes, pH 7. 4,150 mM NaCl, 5 mM MgCl2,1 mM EDTA, 1% Nonidet P-40,0. 5% (w/v) deoxycholate and 0. 1% (w/v) SDS), containing complete protease inhibitor (Roche) and phosphatase inhibitor cocktail 2 and 3 (Sigma). Protein concentrations of the lysates were determined by Bradford measurement. Lysates with equalized amounts of protein were used for immunoblot analysis. PMTwt and the catalytically inactive mutant PMTC1165S were expressed and purified as described previously [72]. To perform the alkaline phosphatase assay cells were cultured for 10 (ST-2) or 4 (primary osteoblasts) days in odm. To measure alkaline phosphatase activity the cells were washed with PBS and then incubated with ALP assay solution (8 mM p-nitrophenylphosphate-6 H2O (Sigma), 12 mM MgCl2,0. 1 mM ZnCl2 and 100 mM glycine-NaOH, pH 10. 5) for 10 min at 37°C. The reaction was stopped by the addition of 200 mM NaOH. The absorption was determined at 405 nm. Alkaline phosphatase staining: On coverslips cultivated cells were fixed in 4% PFA for 30 min. To remove the PFA cells were washed twice with PBS. To stain the alkaline phosphatase the cells were incubated with ALP assay solution containing 5% (v/v) ELF97 (Life Techn.) in the absence of light for 15 min at 25°C. Again cells were washed twice with PBS and incubated for 1 h with a 0. 02% SYTO Green/PBS solution. Cells were mounted with Mowiol 4–88 (Carl-Roth). van Kossa staining: Cells were stained as described by Mukherjee et. al 2008 [73]. In brief, cells were fixed, washed and incubated with a 5% silver nitrate solution for 30 min. After washing the cells with water the microscopic pictures were obtained. Oil Red O staining: To detect lipid droplets, cells were stained with Oil Red O. Therefore, the cells were fixed in PFA and incubated with a saturated Oil Red O solution. Unbound Oil Red O was washed out with 70% (v/v) EtOH. To quantify the amount of Oil Red O bound to lipid droplets, the dye was extracted with a 4% (v/v) Nonidet P-40/isopropanol solution. The absorption was measured at 520 nm. Total RNA was extracted from either ST-2 cells or primary osteoblasts with the RNeasy Mini Kit (Qiagen). cDNA was prepared using the QuantiTect Reverse Transcription Kit (Qiagen). All Kits were used following the manufacturer' s manual. Quantitative PCR was performed using GoTaq qPCR Master Mix (Promega). The expression levels of the ribosomal Protein S29 (mouse) or HPRT (rat) were used as an internal control and fold changes were calculated using the ΔΔCt method. Values are shown as 2−ΔΔCt. The following primer pairs were used for analysis: mS29: forward-ATGGGTCACCAGCAGCTCTA, reverse-AGCCTATGTCCTTCGCGTACT, mALP: forward-AATGAGGTCACATCCATCCTG, reverse-CACCCGAGTGGTAGTCACAA, mPPARγ: forward-AAGACAACGGACAAATCACCA, reverse-GGGGGTGATATGTTTGAACTTG, mC/EBPα: forward-AAACAACGCAACGTGGAGA, reverse-GCGGTCATTGTCACTGGTC, rHPRT: forward-GACCGGTTCTGTCATGTCG, reverse-ACCTGGTTCATCATCACTAATCAC, rALP: forward-GCACAACATCAAGGACATCG, reverse-TCAGTTCTGTTCTTGGGGTACAT, rRUNX2: forward-CCACAGAGCTATTAAAGTGACAGTG, reverse-AACAAACTAGGTTTAGAGTCATCAAGC, rSP7: forward-CGTCCTCTCTGCTTGAGGAA, reverse-TGGAGCCACCAAACTTGC For immunoblot analysis proteins were subjected to SDS-polyacrylamide gel electrophoresis and transferred onto polyvinylidene difluoride-membrane. Anti RhoA-antibody (sc-418 (26C4) ) was purchased from Santa CruzBiotech (Heidelberg, Germany), anti p63RhoGEF-antibody (51004) from Proteintech, anti pERK-antibody (4370S) from New England Biolabs, anti tubulin-antibody (T9026) from Sigma Aldrich and anti p84-antibody (ab487) from Abcam. Deamidation specific antibody anti-Gαq Q209E (3G3) was kindly provided by Dr. Y. Horiguchi (Osaka University, Japan) [32]. Enhanced chemiluminescent detection reagent (100 mM Tris-HCl, pH 8. 0,1 mM luminol (Fluka), 0. 2 mM p-coumaric acid, 3 mM H2O2) was used to detect binding of the second horseradish peroxidase-coupled antibody with the imaging system LAS-3000 (Fujifilm). Quantifications of immunoblots were done using MultiGauge software. To detect the levels of activated RhoA a Rhotekin pulldown assay was performed as described previously [17]. In brief, cells were lysed after 4 h of treatment with indicated compounds. Rhotekin-coupled beads were incubated with the lysates for 1 h at 4°C. The amount of bound and therefore active RhoA was analyzed by immunoblot analysis. For adenoviral infection cells were seeded and directly supplemented with sh-virus suspension and 8 µg/mL polybrene. A specific p63RhoGEF shRNA was used and as control a specific GFP shRNA [39]. One day after infection cells were starved for 24 h in fresh medium containing sh-virus. Cells were cultured in 10% FCS for two more days for a maximal knockdown efficacy. On day four after viral infection of the cells the described assays were performed. Results are presented as means ± S. E. Significance was assessed by paired Student' s t test. p values<0. 05 were considered statistically significant (* = p<0. 05; ** = p<0. 01; ns, not significant). Multiple group comparisons were analyzed by ANOVA followed by Student' s t test. All animal experiments were performed in compliance with the German animal protection law (TierSchG). The animals were housed and handled in accordance with good animal practice as defined by FELASA (www. felasa. eu/guidelines. php) and the national animal welfare body GV-SOLAS (www. gv-solas. de). The animal welfare committees of the universities of Freiburg as well as the local authorities (Regierungspräsidium Freiburg, license X-09/31S) approved all animal experiments.
Pasteurella multocida causes as a facultative pathogen various diseases in men and animals. One induced syndrome is atrophic rhinitis, which is a form of osteopenia, mainly characterized by facial distortion due to degradation of nasal turbinate bones. Strains, which especially affect bone tissue, produce the protein toxin P. multocida toxin (PMT). Importantly, PMT alone is capable to induce all symptoms of atrophic rhinitis. To cause osteopenia PMT influences the development and/or activity of specialized bone cells like osteoblasts and osteoclasts. Recently, we could identify the molecular mechanism of PMT. The toxin constitutively activates certain heterotrimeric G proteins by deamidation. Here, we studied the effect of PMT on the differentiation of osteoblasts. We demonstrate the direct action of PMT on osteoblasts and osteoblast-like cells and as a consequence inhibition of osteoblastic differentiation. Moreover, we revealed the underlying signal transduction pathway to impair proper osteoblast development. We show that PMT activates small GTPases in a Gαq/11 dependent manner via a non-ubiquitously expressed RhoGEF. In turn the mitogen-activated protein kinase pathway is transactivated leading to inhibition of osteoblastogenesis. Our findings present a mechanism how PMT hijacks host cell signaling pathways to hinder osteoblast development, which contributes to the syndrome of atrophic rhinitis.
medicine
mitogenic signaling
host-pathogen interaction
microbiology
g-protein signaling
pasteurellosis
bacterial diseases
gtpase signaling
mapk signaling cascades
bacterial pathogens
erk signaling cascade
infectious diseases
signaling in cellular processes
pasteurella multocida
ras signaling
biology
pathogenesis
signal transduction
gram negative
molecular cell biology
signaling cascades
Pasteurella Multocida Toxin Prevents Osteoblast Differentiation by Transactivation of the MAP-Kinase Cascade via the Gαq/11 - p63RhoGEF - RhoA Axis