Search tips
Search criteria 


Logo of jcinvestThe Journal of Clinical Investigation
J Clin Invest. 2011 September 1; 121(9): 3492–3504.
Published online 2011 August 1. doi:  10.1172/JCI46406
PMCID: PMC3163961

Gsα enhances commitment of mesenchymal progenitors to the osteoblast lineage but restrains osteoblast differentiation in mice


The heterotrimeric G protein subunit Gsα stimulates cAMP-dependent signaling downstream of G protein–coupled receptors. In this study, we set out to determine the role of Gsα signaling in cells of the early osteoblast lineage in vivo by conditionally deleting Gsα from osterix-expressing cells. This led to severe osteoporosis with fractures at birth, a phenotype that was found to be the consequence of impaired bone formation rather than increased resorption. Osteoblast number was markedly decreased and osteogenic differentiation was accelerated, resulting in the formation of woven bone. Rapid differentiation of mature osteoblasts into matrix-embedded osteocytes likely contributed to depletion of the osteoblast pool. In addition, the number of committed osteoblast progenitors was diminished in both bone marrow stromal cells (BMSCs) and calvarial cells of mutant mice. In the absence of Gsα, expression of sclerostin and dickkopf1 (Dkk1), inhibitors of canonical Wnt signaling, was markedly increased; this was accompanied by reduced Wnt signaling in the osteoblast lineage. In summary, we have shown that Gsα regulates bone formation by at least two distinct mechanisms: facilitating the commitment of mesenchymal progenitors to the osteoblast lineage in association with enhanced Wnt signaling; and restraining the differentiation of committed osteoblasts to enable production of bone of optimal mass, quality, and strength.


Osteoporosis is one of the most common degenerative diseases of aging, with an estimated 50% of women experiencing an osteoporotic fracture during their lives. This skeletal fragility results from an imbalance between bone resorption and bone formation that is progressively exacerbated with age. At present the treatment of osteoporosis is largely dependent on antiresorptive agents, which increase bone density modestly and significantly reduce fracture risk, but cannot cure this degenerative disease (1). The ability to enhance the differentiation and function of osteoblasts would therefore be expected to have a profound impact on the treatment of osteoporosis. Indeed, recombinant parathyroid hormone (PTH) (teriparatide), the sole anabolic agent currently approved for clinical use in osteoporosis, is a potent stimulator of bone formation (2).

The actions of PTH on bone mass are complex and still incompletely understood. PTH is a ligand for the PTH/PTH-related peptide (PTHrP) receptor (PPR), a GPCR that activates multiple G protein–dependent signaling pathways (3). Signaling by the PPR has a significant effect on skeletal development, as targeted expression of the constitutively active mutant receptor to osteoblasts leads to a dramatic increase in the formation of trabecular bone (4). Activating mutations of the PPR, as found in Jansen metaphyseal chondrodysplasia, predominantly signal via the stimulatory G protein subunit Gsα in vitro (5). Gsα stimulates adenylyl cyclase and increases cAMP levels, resulting in activation of the PKA pathway (6). In humans, somatic activating mutations of Gsα are associated with fibrous dysplasia, expansile osteolytic lesions in which hematopoietic marrow is replaced by stromal cells of the osteoblast lineage, a phenotype reminiscent of the expansion of stromal cells seen in Jansen transgenic mice (7). When cells from fibrous dysplasia lesions are implanted subcutaneously, these cells, unlike normal cells from these patients, fail to differentiate into mature osteoblasts (8). Constitutive basal activation of Gsα by a modified GPCR has also been demonstrated to markedly increase the amount of trabecular bone in mice (9). These studies indicate that stimulation of Gsα-dependent signaling in osteoblasts can profoundly affect bone mass.

However, the mechanisms by which Gsα-dependent signaling regulates osteoblast differentiation remain obscure. Intermittent PTH increases osteoblast survival and differentiation (10). In contrast, continuous exposure to PTH in vitro significantly attenuates osteogenic differentiation, suggesting that under some circumstances PTH/PKA may inhibit osteoblast maturation (11, 12). In chondrocytes, ablation of either PPR or Gsα leads to accelerated chondrocyte differentiation and hypertrophy (1317), demonstrating that PKA-dependent pathways can inhibit cellular differentiation in some tissues.

The canonical Wnt signaling pathway is required for the commitment and differentiation of mesenchymal progenitors to the osteoblast lineage. Ablation of β-catenin, a central component of canonical Wnt signaling, in early mesenchymal progenitors or osteoblast precursors leads to a failure of osteoblast commitment and differentiation, with adoption of a chondrocytic fate instead (1820). In the skeleton, the PTH signaling pathway intersects with canonical Wnt signaling. For instance, PTH regulates several inhibitors of Wnt signaling (21). PTH suppresses expression of sclerostin, a canonical Wnt inhibitor encoded by Sost and produced by osteocytes, in a PKA-dependent manner (22, 23). MEF2 transcription factors acting on the Sost bone enhancer mediate this action of PTH (24). PTH also regulates dickkopf1 (Dkk1), another soluble Wnt inhibitor that blocks activation of the Wnt coreceptors Lrp5/6 (25). Although suppression of Dkk1 is not required for the anabolic effects of PTH (25, 26), overexpression of either Sost or Dkk1 results in osteopenia (27, 28). Conversely, targeted expression of a constitutively active PPR to osteocytes suppresses sclerostin expression and leads to high bone mass (29).

In addition to the PPR, several other GPCRs that signal via Gsα have been described in osteoblasts, including receptors for PGE2 (EP2R and EP4R) (30), thyroid-stimulating hormone (31), and β2-adrenergic agonists (32). Ablation of these receptors leads to varying and sometimes opposing skeletal consequences in mice. Since Gsα likely serves to mediate signaling downstream of multiple GPCRs in osteoblasts, we hypothesized that ablation of Gsα early in the osteoblast lineage would have significant effects on osteoblast differentiation. Ablation of Gsα in more differentiated cells of the osteoblast lineage results in reduced trabecular bone and increased cortical bone late in embryogenesis (33). However, craniofacial abnormalities and perinatal lethality have precluded the analysis of the role of Gsα in early postnatal development of the skeleton.

In an article describing the regulation of B lymphocyte development in the bone marrow by cells of the osteoblast lineage, we have previously reported that ablation of Gsα early in the osteoblast lineage results in postnatal growth retardation and early mortality, with a dramatic decrease in the bone surface covered with trabecular osteoblasts (34). We now demonstrate that absence of Gsα dramatically impairs bone formation, and we identify at least two distinct functions for Gsα in cells of the osteoblast lineage. First, differentiation of Gsα-deficient osteoblasts is significantly accelerated, resulting in the formation of predominantly woven bone that is highly susceptible to fractures. Second, in the absence of Gsα, expression of the Wnt inhibitors sclerostin and Dkk1 is significantly upregulated, with attenuation of Wnt signaling in osteoblasts. Consistent with previous reports that the commitment of mesenchymal progenitors to the osteoblast lineage is dependent upon canonical Wnt signaling (1820), we found that the frequency of osteoblast precursors is markedly decreased in mutant mice.


Deletion of Gsα in osteoprogenitors leads to profound osteoporosis.

Mice lacking Gsα in the osteoblast lineage (GsαOsxKO mice) were generated by ablation of Gsα in osterix-expressing (Osx-expressing) progenitors as previously described (34). Mutant mice were grossly similar to control littermates at birth, and skeletal preparations did not demonstrate significant differences in patterning of the axial skeleton on P1 (Supplemental Figure 1, A and B; supplemental material available online with this article; doi: 10.1172/JCI46406DS1). Histological analysis at E15.5 revealed normal vascular invasion, with subsequent formation of the bone marrow cavity (Supplemental Figure 1, C and D). However, fractures of ribs (Figure (Figure1,1, A and B) and long bones (Supplemental Figure 1, E and F) were identified in GsαOsxKO mice on P1. Perhaps as a consequence of early and extensive fractures, although other contributing factors have not been ruled out, GsαOsxKO mice exhibit early postnatal mortality (ref. 34 and Supplemental Figure 1G), with no mutant mice surviving until weaning. The fractures did not occur simply as a result of handling of the skeletons during isolation, as healing calluses were evident by 1 week of life (Supplemental Figure 1, H and I). The fractures were not present in utero (Supplemental Figure 1, J–L), suggesting that initial fractures were sustained during birth. However, delivery via Caesarian section failed to prevent early postnatal acquisition of fractures and did not reduce mortality (data not shown).

Figure 1
Deletion of Gsα in the osteoblast lineage leads to severe osteoporosis.

Sakamoto et al. reported that ablation of Gsα in differentiated osteoblasts using collagen Iα1 promoter Cre transgenic mice resulted in reduced trabecular bone at E18.5 (33). We found that deletion of Gsα earlier in the osteoblast lineage also led to reduced trabecular bone in the primary spongiosa at E18.5 (Figure (Figure1,1, C and D). By 1 week of age, von Kossa staining demonstrated further loss of mineralized trabecular bone (Figure (Figure1,1, E and F). Cortical bone was markedly irregular and thinned in the few mice surviving past the second week of life, and in places was almost completely absent (Figure (Figure1,1, G and H). Histomorphometric analysis of the tibial metaphysis revealed a 71% decrease in trabecular bone volume, with decreased trabecular thickness and number and increased trabecular spacing (Figure (Figure1I). 1I).

Decreased bone mass in the absence of Gsα is due to impaired bone formation rather than enhanced bone resorption.

Micro-CT demonstrated reduced cortical bone and increased cortical porosity at 1 week (Figure (Figure2,2, A–D). To determine whether the porosity might result from enhanced bone resorption by osteoclasts, we performed TRAP staining at E18.5, when cortical bone had not yet thinned significantly in GsαOsxKO mice (Figure (Figure2,2, E and F). As previously reported for ablation of Gsα in differentiated osteoblasts (33), there was a marked decrease in the number of endocortical osteoclasts at E18.5 (Figure (Figure2,2, G and H). Furthermore, at no time during early postnatal development was there evidence for increased numbers of TRAP+ osteoclasts in trabecular bone of mutant mice (data not shown). Osteoclast surface was not increased in trabecular bone of 1-week-old mutant mice (Figure (Figure2I),2I), and there was no increase in the level of serum TRACP 5b, a marker of bone resorption, despite the presence of fractures (Figure (Figure2J).2J). These findings suggest that the dramatic decrease in GsαOsxKO bone mass cannot be attributed to increased bone resorption.

Figure 2
Decreased bone mass in the absence of Gsα is due to inadequate bone formation.

If the decreased bone mass in GsαOsxKO mice was not the result of enhanced bone resorption, then bone formation must have been inadequate. Consistent with this, histomorphometry revealed an 85% reduction in osteoblast surface (34) and an equally dramatic decrease in osteoblast number in GsαOsxKO mice (Figure (Figure2K).2K). Serum osteocalcin, a marker of bone formation, was also significantly decreased in early postnatal mutant mice (Figure (Figure2L).2L). In an attempt to calculate bone formation rate by dynamic histomorphometry, we performed double calcein labeling 1 and 4 days prior to analysis on P7. In control mice this allowed visualization of two distinct mineralization fronts (Figure (Figure2M).2M). In contrast, bones from mutant mice were diffusely labeled with fluorochrome, indicating the formation of woven bone during the labeling period and precluding analysis of bone formation rate (Figure (Figure2N).2N). Indeed, when tibiae of 2-week-old mice were analyzed under polarized light, the cortical bone of control mice exhibited lamellar organization, while mutant cortical bone revealed markedly disorganized arrangement of collagen fibrils (Figure (Figure2,2, O and P). Together these results indicate that the loss of Gsα early in the osteoblast lineage leads to formation of disorganized bone of insufficient mass, strength, and quality, as evidenced by the occurrence of fractures.

Intramembranous bone formation is defective in GsαOsxKO mice.

While long bones are formed by the process of endochondral ossification, craniofacial bones are more commonly derived by intramembranous ossification, in which cells of mesenchymal condensations differentiate directly into osteoblasts without a cartilage template. Skeletal preparations on P1 demonstrated a dramatic impairment in mineralization of intramembranous cranial bones. While the parietal bone of control mice exhibited relatively homogenous mineralization and well-formed sutures (Figure (Figure3A),3A), the parietal bone in GsαOsxKO mice displayed patchy mineralization in a reticular pattern with ragged sutures (Figure (Figure3B).3B). Histological analysis of control calvariae at P4 and 2 weeks revealed 1–2 layers of osteoblasts along the bone surfaces and orderly lamellar bone (Figure (Figure3,3, C and E). In contrast, multiple layers of stromal cells and preosteoblasts were found lining the periosteal surface of GsαOsxKO mice (Figure (Figure3,3, D and F). Like cortical bone, the calvarial bone of GsαOsxKO mice was woven, as indicated by misshapen osteocyte lacunae and irregular collagen fibril deposition (Figure (Figure3,3, G and H). Likewise, porosity was dramatically increased in GsαOsxKO calvarial bones at 2 weeks (Figure (Figure3I).3I). Therefore ablation of Gsα early in the osteoblast lineage resulted in abnormal trabecular, cortical, and intramembranous bone that was evident at birth, indicating that Gsα plays a crucial role during embryonic skeletogenesis.

Figure 3
Intramembranous bone formation is defective in GsαOsxKO mice.

Osteogenic differentiation is accelerated in the absence of Gsα.

To assess osteoblast differentiation in vivo in the absence of Gsα, we analyzed the expression of gene markers of osteoblast differentiation. We found that during embryonic development, mRNA levels of genes expressed early in the osteoblast lineage, such as alkaline phosphatase (ALP) and collagen Iα1, were similar in GsαOsxKO mice and littermate controls at E15.5 and P1 (Figure (Figure4A).4A). In contrast, expression of osteocalcin mRNA, a marker of terminally differentiated osteoblasts initially detectable in WT mice at P1, was nearly absent in mutant bones by P9 (Figure (Figure4A).4A). By this time collagen Iα1 expression was also noticeably decreased, likely reflecting the dramatic decrease in osteoblast numbers (Figure (Figure2K).2K). Since osteocalcin mRNA expression is at least partly dependent on PKA-mediated gene transcription (35), its absence could reflect reduced PKA activation in osteoblasts lacking Gsα. Consistent with this, expression of another PKA target gene, Mmp13 (36), was also reduced in bones from GsαOsxKO mice (Figure (Figure4,4, B and C) as well as Gsα-deficient osteoblasts (Figure (Figure4D).4D). However, given the markedly reduced osteoblast number in mutant mice, the absence of osteocalcin expression might also reflect failure of terminal differentiation into mature osteoblasts in the absence of Gsα.

Figure 4
Osteogenic differentiation is not impaired in GsαOsxKO mice.

In order to evaluate osteoblast differentiation directly, we isolated primary calvarial osteoblastic cells from GsαOsxKO mice and control littermates, and subjected these cells to osteogenic differentiation in vitro. Unexpectedly, GsαOsxKO cells consistently demonstrated accelerated ALP expression as well as earlier and more extensive mineralization than cells from WT mice (Figure (Figure4,4, E and F). To demonstrate that the accelerated differentiation occurred in cells in which Cre recombinase had been active, we crossed GsαOsxKO mice to R26 reporter mice (37). In Osx1-GFP::Cre;Gsαfl/fl;R26 mice, cells stained blue by X-gal reflect expression of Cre recombinase and therefore likely ablation of Gsα. We have previously shown that expression of Cre recombinase efficiently reduces Gsα mRNA levels by greater than 90% (34). We found that calvarial osteoblasts from Osx1-GFP::Cre;Gsαfl/fl;R26 mice, as well as control Osx1-GFP::Cre;Gsαfl/+;R26 mice, formed mineralized nodules in which the majority of cells in the nodule were also blue (Figure (Figure4,4, G and H). Therefore, in calvarial osteoblasts isolated from GsαOsxKO mice and subjected to osteogenic differentiation, the enhanced mineralization was a direct effect of Gsα deficiency in cells of the osteoblast lineage.

Since calvariae from GsαOsxKO mutant mice exhibit impaired mineralization (Figure (Figure3B),3B), we considered the possibility that the results of Figure Figure4,4, E and F, might be explained by an artifact: perhaps serial collagenase digestion would more easily recover differentiated osteoblasts from mutant calvariae than from control calvariae, thereby favoring the onset of mineralization in cells isolated from mutant mice. To control for the distribution of osteoblast lineage populations at varying stages of differentiation, we harvested primary calvarial osteoblasts from Col2.3::GFP;Gsαfl/fl mice, in which GFP is under the control of the 2.3-kb rat type I collagen promoter and therefore expressed in differentiated osteoblasts (38). In cells isolated from calvariae of these mice, expression of GFP serves as a marker for osteogenic differentiation (12, 38). Equal numbers of calvarial cells from Col2.3::GFP;Gsαfl/fl mice were infected with either adenovirus encoding Cre recombinase to ablate Gsα expression or with control adenovirus encoding either β-gal or YFP. Gsα expression was efficiently reduced within 24 hours (Supplemental Figure 2A), and functional loss of Gsα was confirmed by the decrease in basal cAMP levels after 48 hours (Supplemental Figure 2B), after which cells were placed in osteogenic differentiation media. Cre-infected Gsα-deficient cells displayed robust mineralization as early as 6 days after differentiation, while mineralization of control cells was not detectable until 9 days in culture (Figure (Figure5,5, A and B). The Col2.3::GFP+, and in particular the GFPhi, population was enriched in cells that expressed markers of mature osteoblasts (ALP, collagen Iα1, and osteocalcin) (Supplemental Figure 2, C and D). GFP expression was significantly increased in Cre-infected cells by day 6 and remained persistently elevated relative to control cells throughout the course of differentiation (Figure (Figure5C).5C). Mineralization in vitro can be affected by cell density; however, we confirmed that the enhanced mineralization of Cre-infected Gsα-deficient calvarial osteoblasts was independent of cell number. When plated at low cell density such that there was a moderate increase in cell number in Gsα-deficient cells only after 12 days in culture (Supplemental Figure 2E), there was already a significant increase in both alizarin deposition (Supplemental Figure 2F) and the frequency of Col2.3::GFPhi cells (Supplemental Figure 2G) after 6 days of culture. These differences were even more pronounced after 12 days in culture. To determine whether Gsα deletion accelerated the differentiation only of committed osteoprogenitors, we sorted ALP Col2.3::GFP Gsαfl/fl cells, which do not yet express markers of osteogenic commitment (Supplemental Figure 2D), infected them with adeno-Cre or adeno–β-gal, and subjected them to osteogenic differentiation. Even among uncommitted progenitors, ablation of Gsα led to enhanced osteogenic differentiation (Figure (Figure5D).5D). Finally, the accelerated osteogenic differentiation in cells lacking Gsα was not unique to calvarial osteoblasts. Bone marrow stromal cells (BMSCs) isolated from Col2.3::GFP;Gsαfl/fl mice and infected with adeno-Cre also demonstrated dramatic enhancement of osteogenic differentiation (Figure (Figure5,5, E and F).

Figure 5
Osteogenic differentiation is accelerated in the absence of Gsα.

We next analyzed markers of osteoblast differentiation in cultured calvarial osteoblasts (Figure (Figure5G).5G). After 6 days of culture under osteogenic conditions, Gsα mRNA expression remained significantly reduced by adeno-Cre infection. Accelerated maturation was reflected by the significant increase in expression of the osteoblast markers ALP and collagen Iα1 in Gsα-deficient cells relative to control cells. However, we did not detect any significant differences in the mRNA levels of the osteogenic transcription factors Runx2, Osx, or Atf4. Together these data demonstrate that osteogenic differentiation is dramatically accelerated when Gsα is deleted early in the osteoblast lineage.

Osteoblast differentiation is accelerated in vivo in GsαOsxKO mice.

In order to assess the fate of Gsα-deficient cells of the osteoblast lineage in vivo, we crossed GsαOsxKO to Rosa26 reporter mice (37). Staining with X-gal revealed abundant cells in GsαOsxKO bone that were descended from Osx-expressing precursors, including osteocytes (Figure (Figure6,6, A and B). Osteocytes are derived from terminally differentiated osteoblasts (39, 40) and are embedded in the mineralized matrix. Indeed, inspection of H&E-stained sections of both cortical and calvarial bones revealed a significant increase in osteocyte density in GsαOsxKO mice (Figure (Figure6,6, C–E, and data not shown). To determine whether accelerated osteoblast maturation might contribute to the increased osteocyte density in GsαOsxKO mice, we performed a pulse-chase with BrdU. Four hours after BrdU injection, no BrdU+ osteocytes were identified, consistent with their postmitotic state. In contrast, 24 hours after BrdU injection, we found a significantly higher proportion of BrdU+ osteocytes in GsαOsxKO mice relative to littermate controls (Figure (Figure6,6, F and G). Since osteocytes themselves do not proliferate and therefore do not incorporate BrdU, BrdU+ osteocytes must have been derived from labeled pre-osteoblasts/osteoblasts that subsequently differentiated into osteocytes. We could find no discernible increase in BrdU+ frequency in GsαOsxKO mature osteoblasts on the bone surface at either 4 or 24 hours after injection, suggesting that enhanced differentiation rather than increased proliferation of osteoblasts leads to the increased frequency of BrdU+ osteocytes in GsαOsxKO mice (Figure (Figure6,6, F and G). To further investigate osteoblast proliferation in vivo, we isolated Osx1-GFP::Cre+ osteoblasts by FACS sorting from WT and GsαOsxKO mice. Cell cycle analysis demonstrated that the distribution of cells in cell cycle stages G1, S, and G2/M was the same in Osx1-GFP::Cre+ cells from control (Osx1-GFP::Cre+;Gsα+/+) and GsαOsxKO mice, again indicating similar rates of proliferation of these cells in vivo (Supplemental Figure 3A). Finally, TUNEL staining for the presence of apoptosis did not reveal any significant increase in apoptosis of GsαOsxKO osteoblasts in tibiae at 1 week (Supplemental Figure 3, B and C).

Figure 6
Accelerated osteogenic differentiation occurs in vivo in GsαOsxKO mice.

In vitro, expression of osteocytic markers coincides with mineralized nodule formation (41). We therefore examined expression of osteocyte-specific genes in calvarial osteoblasts cultured under osteogenic conditions, and found that after only 1 week in culture, expression of the osteocyte-specific genes Dmp1 and Phex was upregulated in mutant calvarial osteoblasts, coincident with the early appearance of mineralization (Figure (Figure6H).6H). Similarly, Dmp1 and Phex mRNA levels were dramatically increased over 2 weeks of osteogenic differentiation of Gsα-deficient BMSCs (Figure (Figure6I).6I). In summary, these data indicate that both in vitro and in vivo, absence of Gsα leads to accelerated osteoblast differentiation in a cell-autonomous manner. The rapid maturation of differentiated osteoblasts into osteocytes therefore contributes to the small size of the mature osteoblast pool in GsαOsxKO mice.

GsαOsxKO mice have woven bone and abnormal osteocytes.

The osteocytes in GsαOsxKO mice that result from accelerated osteoblast differentiation display numerous abnormalities characteristic of woven bone. E11 is a marker of early osteocytes and/or late osteoblasts and plays a role in the elongation of osteocytic dendrites (42). In tibiae of control mice, expression of E11 protein in cortical bone was restricted to a single layer of cells, representing terminally differentiated osteoblasts and/or immature osteocytes, at the edge of the mineralizing matrix, highlighting the dendritic processes that form the osteocyte lacuno-canalicular network (Figure (Figure7A).7A). In contrast, expression of E11 in tibiae of mutant mice was found throughout the thickness of cortical bone in osteocytes with a notable paucity of dendrites (Figure (Figure7B).7B). We confirmed disruption of the normal osteocyte lacuno-canalicular network with Bodian staining, which revealed a well-established network in control mice but the absence of a well-organized canalicular network in mutant bones (Figure (Figure7,7, C and D). Furthermore, osteocyte morphology was abnormal in GsαOsxKO bones, with rounded nuclei and increased perilacunar space (Figure (Figure7,7, E and F). Transmission electron microscopy further demonstrated that whereas control cells have abundant cytoplasm containing rough endoplasmic reticulum, mutant osteocytes have scant cytoplasm (Figure (Figure7,7, G and H). The findings of increased osteocyte density, aberrant E11 expression, and absence of a lacuno-canalicular network are all consistent with the presence of woven bone, normally associated with pathologic states of rapid ossification (43).

Figure 7
Accelerated osteoblast maturation in GsαOsxKO mice is associated with woven bone and abnormal osteocytes.

Consistent with the model that overly rapid maturation of osteoblast maturation results in formation of woven bone, expression of bone sialoprotein (BSP), a gene expressed at high levels in woven bone (44), was upregulated almost 20-fold in differentiating Gsα-deficient calvarial osteoblasts as compared with control osteoblasts in vitro (Figure (Figure7I).7I). Thus, in the absence of Gsα, osteoblast differentiation was accelerated and resulted in production of mainly woven bone, with a failure of production of normal lamellar bone. We suggest that the presence of predominantly woven bone (Figure (Figure2P2P and Figure Figure3H)3H) contributes to the remarkable fragility of GsαOsxKO bones.

Inhibition of canonical Wnt signaling is associated with reduced mesen­chymal commitment to the osteoblast lineage in GsαOsxKO mice.

Despite the profound osteoporosis and the scarcity of osteoblasts seen in GsαOsxKO mice, we have paradoxically found that osteoblast differentiation is dramatically enhanced by the absence of Gsα. Since there was no detectable difference in apoptosis by TUNEL staining (Supplemental Figure 3, B and C), and no defect in proliferation of Gsα-deficient osteoblasts (Figure (Figure6F6F and Supplemental Figure 3A), accelerated differentiation into osteocytes should have led to the depletion of the osteoblast population. However, osteoblast numbers were so dramatically reduced (by >80%) in mutant mice (Figure (Figure2K)2K) that we hypothesized that there might also be a decrease in the population of osteoblast precursors. To determine whether osteoblast precursors are reduced in GsαOsxKO mice, we plated BMSCs and calvarial cells isolated from GsαOsxKO and control mice at low density, and counted cells capable of initiating fibroblastic colonies (CFU-F) as well as cells capable of initiating osteogenic colonies (CFU-ALP). We found that both CFU-F and CFU-ALP were reduced by greater than 3-fold in GsαOsxKO BMSCs (Figure (Figure8A).8A). In calvarial cells, while the number of CFU-F was not significantly decreased, the number of CFU-ALP was also markedly lower in GsαOsxKO mice (Figure (Figure8B). 8B).

Figure 8
GsαOsxKO mice have reduced Wnt signaling in the osteoblast lineage and a depleted osteoprogenitor pool.

Canonical Wnt signaling positively regulates osteoblast commitment and differentiation (1820). Several groups have demonstrated that sclerostin and Dkk1, two inhibitors of Wnt signaling, are potently suppressed by PTH (22, 23, 25). Since Gsα mediates the activation of PKA by PTH stimulation of the PPR, we hypothesized that sclerostin and/or Dkk1 expression would be increased in the absence of Gsα. Indeed, Sost mRNA, which encodes sclerostin, was markedly increased in calvariae and long bones of GsαOsxKO mice (Figure (Figure8C8C and data not shown). Immunohistochemical staining of cortical bone of tibiae at 3 weeks demonstrated abundant sclerostin protein in GsαOsxKO osteocytes (Figure (Figure8,8, D and E). Since the increased Sost mRNA levels in GsαOsxKO bones might have at least partially reflected the increase in osteocyte density, we examined expression of Sost as well as Dkk1 mRNAs in cultured calvarial osteoblasts plated at equal numbers. In differentiating calvarial osteoblasts, mRNA levels of both Sost and Dkk1 were dramatically upregulated in Gsα-deficient osteoblasts after only 6 days in culture (Figure (Figure8F).8F). Therefore, absence of Gsα in the osteoblast lineage is associated with increased expression of at least two inhibitors of canonical Wnt signaling.

To examine the consequences of upregulation of sclerostin and Dkk1 on Wnt signaling in osteoblasts lacking Gsα, we quantitated the expression of the Wnt target genes Axin2 and Lef1. Expression of Axin2 and Lef1 mRNAs was significantly reduced in Gsα-deficient osteoblasts (Figure (Figure8G).8G). To further evaluate Wnt-dependent signaling in Gsα-deficient osteoblasts in vivo, we crossed GsαOsxKO mice to TopGal reporter mice, in which multiple TCF response elements regulate expression of β-gal (45). Quantitative real-time PCR analysis of mRNA from GsαOsxKO bones revealed decreased expression of the Wnt reporter TopGal in the absence of Gsα (Figure (Figure8H).8H). Thus, absence of Gsα in the osteoblast lineage leads to increased expression of sclerostin and Dkk1, which may feed back to decrease canonical Wnt signaling in the osteoblast lineage. Since canonical Wnt signaling is required for commitment of mesenchymal progenitors into the osteoblast lineage, attenuated Wnt signaling likely contributes to the reduction of committed osteoprogenitors in GsαOsxKO mice.


The role of Gsα in governing osteoblast differentiation is of particular relevance for several human skeletal disorders (46). Heterozygous loss-of-function mutations in Gsα result in Albright hereditary osteodystrophy (AHO), with short stature, brachydactyly, and obesity. A subset of patients with AHO, frequently those with paternal inheritance of the mutated allele, experience ectopic ossifications that can involve subcutaneous or deep soft tissues as well as skeletal muscle (progressive osseous heteroplasia). Conversely, activating somatic mutations of Gsα are found in fibrous dysplasia, skeletal lesions that can occur alone or in association with other endocrinopathies (McCune-Albright syndrome). Fibrous dysplasia lesions are characterized by impaired osteoblast differentiation and woven bone. Therefore Gsα plays a crucial role in osteoblast development and function, and understanding the molecular mechanisms will be of great clinical significance.

To that end we have generated mice with conditional deletion of Gsα early in the osteoblast lineage. GsαOsxKO mice have severe osteoporosis characterized by impaired endochondral and intramembranous ossification. The dramatic reduction in bone mass is accompanied by a failure of normal bone formation, with production of predominantly woven bone of inadequate mass and strength, and a marked decrease in osteoblast number. Gsα is downstream of multiple GPCRs and therefore may participate in various signaling pathways. We have identified at least two distinct mechanisms that may underlie the diminished osteoblast number in GsαOsxKO mice: (a) accelerated differentiation of osteoblasts into osteocytes and (b) decreased commitment of mesenchymal progenitors to the osteoblast lineage, in association with attenuated Wnt signaling that results at least in part from increased expression of the Wnt inhibitors sclerostin and Dkk1.

We have found that the population of osteoblast precursors (CFU-ALP) was significantly decreased among both BMSCs and calvarial cells of GsαOsxKO mice, suggesting reduced commitment of mesenchymal progenitors to the osteoblast lineage. Wnt signaling is required for osteoblast commitment and early osteoblast differentiation (1820), and PKA signaling downstream of the PPR can suppress expression of the canonical Wnt inhibitors sclerostin and Dkk1. Sclerostin was overexpressed in calvariae of GsαOsxKO mice, and both Sost and Dkk1 mRNA levels were increased in calvarial osteoblasts from GsαOsxKO mice, with a concomitant decrease in expression of Wnt target genes in these same cells. Therefore, the inhibition of Wnt signaling may contribute to the dramatic decrease in the pool of osteoprogenitors in GsαOsxKO mice. In addition to sclerostin and Dkk1, several laboratories have demonstrated other points of interaction between the PTH/PPR/PKA and Wnt signaling pathways (21, 47). PTH is able to activate β-catenin targets in osteoblasts even in the absence of Dkk1 suppression (25, 26), implicating other actions downstream of the PPR in regulating Wnt signaling. Indeed, several potential mechanisms have been identified, including direct interactions between PPR and the Wnt coreceptor LRP6 (48), as well as phosphorylation of β-catenin by PKA (49). Therefore, the effects of PKA on Wnt signaling may be both indirect, mediated by soluble inhibitors such as sclerostin and Dkk1, as well as cell autonomous, by direct phosphorylation of components of the Wnt signaling pathway. More detailed investigations into the effects of Gsα ablation on Wnt signaling in GsαOsxKO mice are underway.

Once mesenchymal progenitors are committed to the osteoblast lineage, however, the loss of Gsα somewhat paradoxically results in accelerated osteogenic maturation. Although the near absence of osteocalcin mRNA initially suggested a failure of osteoblast differentiation, instead the reduced expression of osteocalcin mRNA reflected attenuated PKA signaling in osteoblasts lacking Gsα. In support of this, expression of Mmp13 mRNA, another PKA target gene, was also reduced in GsαOsxKO bones, while other markers of osteogenic differentiation were still expressed.

Although the number of mature osteoblasts was markedly reduced in GsαOsxKO mice, this was not due to complete failure of osteoblast differentiation, as these mice have abundant osteocytes, which are derived from terminally differentiated osteoblasts (40). Rather, we have shown that in the absence of Gsα, cells of the osteoblast lineage differentiate rapidly into osteocytes. Whereas PTH has been demonstrated to decrease apoptosis in osteoblasts in adult mice (50), we could find no discernible alteration in osteoblast apoptosis in early postnatal GsαOsxKO mice in vivo. The effects of PTH on osteoblast apoptosis vary greatly by anatomic location (51) as well as means of administration (10). During early postnatal growth, a time of rapid bone formation, perhaps changes in apoptosis may have lesser effects on cell numbers. In addition, there was no evidence of increased proliferation of Gsα-deficient osteoblasts in vivo. Thus, accelerated differentiation results in depletion of osteoblasts and accumulation of osteocytes in GsαOsxKO mice. It therefore appears that in cells of the osteoblast lineage, Gsα restrains cellular differentiation. Of note, the bone that is present in GsαOsxKO mice is mainly woven bone. By regulating the pace of osteoblast differentiation, Gsα may function to promote the formation of a larger number of osteoblasts and production of more orderly lamellar bone. In the absence of Gsα, the resulting bone is largely woven, typically associated with embryonic development and states of pathologically rapid bone formation such as fracture repair.

Our data are in keeping with the findings that continuous exposure of osteoblasts to PTH inhibits differentiation (11, 12). Moreover, in chondrocytes, ablation of either PPR or Gsα leads to accelerated chondrocyte differentiation and hypertrophy, with adverse consequences for skeletal development (1317). Whether similar mechanisms underlie the effects of Gsα and PKA in inhibiting differentiation of both osteoblasts and chondrocytes is under investigation.

The mechanisms mediating the effects of Gsα on osteoblast lineage commitment and differentiation are distinct and involve both Wnt-dependent and Wnt-independent effects. In particular, like Wnt signaling and perhaps through its effects on Wnt signaling, Gsα favors osteogenic commitment of mesenchymal progenitors. In contrast, whereas Wnt signaling positively regulates osteoblast differentiation, osteoblast maturation is accelerated in GsαOsxKO mice even in the face of reduced Wnt signaling, suggesting that absence of Gsα can override the inhibition of Wnt signaling in driving osteoblast differentiation forward. The accelerated differentiation of osteoblasts into osteocytes in the absence of Gsα is unlikely to be related to alterations in Wnt signaling. In differentiated osteoblasts, manipulation of Wnt signaling does not affect bone formation, but only affects bone resorption via disruption of osteoprotegerin expression (52, 53). Furthermore, reduced Wnt signaling in osteocytes due to either ablation of β-catenin or overexpression of Dkk1 in osteoblasts does not lead to an increase in osteocyte density or woven bone (25, 27, 54). Together these studies suggest that Wnt signaling probably does not regulate differentiation of osteoblasts into osteocytes.

The actions of Gsα on both commitment to and differentiation of the osteoblast lineage are at work in both intramembranous and endochondral bone. When plated at low cell densities, osteoprogenitor numbers, as determined by CFU-ALP, were reduced in both BMSCs and calvarial cells of GsαOsxKO mice. In cells committed to the osteoblast lineage, however, the absence of Gsα resulted in accelerated osteoblast differentiation. In keeping with a similar role for Gsα in both types of cells, when equal numbers of osteoprogenitors were plated in vitro, followed by ablation of Gsα, mineralization was dramatically increased in both BMSCs and calvarial cells. Therefore, we conclude that Gsα acts to enhance osteoblast lineage commitment but restrain osteoblast differentiation in both intramembranous and endochondral bone.

The relevant receptors upstream of Gsα are of great interest. The PPR is a prime candidate, since PTH has important effects on osteoblasts, and many of these are mediated by Gsα (10). In vitro, deletion of the PPR in calvarial osteoblasts also resulted in accelerated osteogenic differentiation; however, ablation of the PPR in osteoprogenitors did not lead to the presence of fractures at birth (data not shown). Therefore, other GPCRs may well be involved. Other Gsα-coupled GPCRs reported in osteoblasts include TSHR and β2AR. However, ablation of TSHR leads to a high-turnover osteoporosis (31), while deletion of β2AR results in high bone mass (32). Thus, the actions of these receptors are unlikely, at least during embryonic development, to be the predominant GPCRs signaling to Gsα in early cells of the osteoblast lineage. PGE2 also has anabolic effects on bone (55, 56), and in osteoblasts the PGE2 receptors EP2 and EP4 are coupled to Gsα and may serve crucial functions in regulating bone formation.

In summary, our studies demonstrate that Gsα signaling early in the osteoblast lineage is crucial for the formation of normal bone. In the absence of Gsα, decreased commitment of mesenchymal progenitors to the osteoblast lineage and pathologically accelerated osteogenic differentiation yield bone of striking fragility. That Gsα mediates multiple functions in osteoblasts suggests that more specific targeted interventions may be possible to increase bone mass, quality, and strength.


Experimental animals.

Osx1-GFP::Cre (20) and Gsαfl/fl (57) mice have been described previously. Col2.3::GFP mice (38) were provided by David Rowe (University of Connecticut Health Center, Farmington, Connecticut, USA). R26 reporter mice were obtained from The Jackson Laboratory. Since GsαOsxKO mice are of a mixed genetic background (C57BL/6 and CD1), littermate controls (Gsαfl/fl, except where otherwise specified) were used for all experiments described. Genotyping was performed on genomic DNA isolated from tails, using previously published protocols (34). All animals were housed in the Center for Comparative Medicine at the Massachusetts General Hospital, and all experiments were approved by the hospital’s Subcommittee on Research Animal Care.

Skeletal preparations.

Skeletons were fixed in 95% ethanol, then stained overnight in 0.015% alcian blue in acetic acid/ethanol. Soft tissues were cleared in 1% KOH, then stained overnight in 0.01% alizarin red.

Serum TRACP 5b and osteocalcin.

Serum levels of TRACP 5b were measured by ELISA using the MouseTRAP assay (Immunodiagnostic Systems). Serum osteocalcin levels were determined by ELISA (Biomedical Technologies Inc.) according to the manufacturer’s protocol.

Histological analysis.

Mouse limbs were fixed in 10% buffered formalin, paraffin embedded, and sectioned. In situ hybridization was performed according to published protocols (4). Immunohistochemical analysis was performed on deparaffinized sections using biotinylated mouse anti-Sost antibody (R&D Systems) and anti-E11 (eBioscience). Bodian staining to highlight the osteocytic lacuno-canalicular network was performed as described previously (58). For transmission electron microscopy, limbs were fixed in EM fixative (2.5% glutaraldehyde, 2.0% PFA, 0.025% calcium chloride in a 0.1 M sodium cacodylate buffer [pH 7.4]) and processed for EM. Samples were examined with a Phillips 301 transmission electron microscope, and digital images were captured using an Advanced Microscopy Techniques CCD camera.

Histomorphometry and micro-CT analysis.

Double calcein labeling was performed by injection of mice with 20 mg/kg calcein on P3 and P6. Mice were sacrificed on P7, and bones were fixed in 10% buffered formalin and embedded in methylmethacrylate as previously described (59). Histomorphometry was carried out in the lower primary spongiosa of the proximal tibia, starting 150 μm below the growth plate and extending for 750 μm, according to standard procedures. Osteocyte density per bone area was quantitated on high-power fields of cortical bone using OsteoMeasure software (Osteo­Metrics). For micro-CT analysis, mid-diaphysis areas of femurs were scanned to evaluate cortical bone microarchitecture using a desktop high-resolution micro-CT instrument (μCT40, SCANCO Medical), as described previously (60). In brief, a total of 30 slices for the cortical region were measured at the mid-diaphysis of each femur using an X-ray energy of 70 KeV, integration time of 200 ms, and a 12-μm isotropic voxel size. Cortical shells were contoured across the 30 slices excluding the bone marrow cavity, and the ratio of cortical bone area to the total cross-sectional area was calculated.

Cell culture.

Calvarial osteoblasts were harvested from GsαOsxKO and control mice by serial collagenase digestion as previously described (61), plated at 5 × 103 to 10 × 103 cells/cm2, and induced to undergo osteogenic differentiation in the presence of ascorbic acid (50 μg/ml) and β-glycerol phosphate (10 mM). Gsαfl/fl calvarial osteoblasts were harvested and subjected to adenoviral infection with adeno-Cre or adeno–β-gal, then induced to undergo osteogenic differentiation as above. For measurement of cAMP accumulation, cells grown in 24-well plates were incubated at 37°C for 15 minutes in a buffer containing 2 mM isobutyl methylxanthine (an inhibitor of phosphodiesterase activity). Intracellular levels of cAMP were determined by radioimmunoassay as previously described (62).

BMSCs were harvested from neonatal mice by crushing hind limbs in PBS containing 2% fetal bovine serum. Bone marrow cells were filtered and plated at 0.5 × 106 to 1 × 106 cells/cm2 and subjected to osteogenic differentiation as described above.

CFU assays.

BMSCs and calvarial cells from WT and KO mice were seeded at 50 × 103 cells/cm2 and 100 cells/cm2, respectively, on Primaria cell culture plates (BD Falcon). For CFU-F assays, colonies were cultured for 7 days in α-MEM plus 10% fetal bovine serum, then fixed with formalin and stained with methylene blue. For CFU-ALP assays, colonies were cultured in osteogenic media containing 10 mM β-glycerol phosphate and 50 μg/ml ascorbic acid (both from Sigma-Aldrich). After 7 days colonies were fixed in formalin and stained for ALP activity as described previously (63).

Flow cytometry.

Osteoblastic cells were harvested from neonatal calvariae of Col2.3::GFP;Gsαfl/fl mice by serial collagenase digestion (61). Fractions 3–6 were pooled and resuspended in PBS with 2% fetal bovine serum. Cells were stained with biotinylated anti-ALP antibody (64) (courtesy of Mark Horowitz, Yale University, New Haven, Connecticut, USA) and streptavidin-APC (eBioscience), then analyzed on a FACSCalibur flow cytometer (BD Biosciences).

Quantitative real-time PCR.

Total RNA was isolated using the RNeasy kit (QIAGEN), and cDNA was synthesized with the SuperScript III First Strand synthesis system for real-time PCR (Invitrogen). Quantitative real-time PCR was performed using primers for Gsα (13), Runx2 (65), ALP (65), Osx (65), Col1a1 (66), Atf4 (66), Sost (67), TopGal (25), Dmp1 (67), Phex (67), and BSP (65) according to previously published protocols, with mRNA levels normalized to β-actin expression. Total RNA samples subjected to cDNA synthesis reactions in the absence of reverse transcriptase were included as negative controls.


Statistical analyses were performed using a 2-tailed Student’s t test. All values are expressed as mean ± SEM. P values less than 0.05 were considered significant.

Supplementary Material

Supplemental data:


We thank David Rowe for providing the Col2.3::GFP transgenic mice; Mark Horowitz for providing the ALP antibody; James Oh, Jackie McConnell, and Rhiannon Chubb for technical assistance; the MGH Center for Comparative Medicine staff for care of the mice; and the Dana Farber Cancer Institute and Harvard Stem Cell Institute flow cytometry cores. This work was supported in part by NIH grants AR053781 (to J.Y. Wu) and DK117940 (to H.M. Kronenberg) and by the National Institute of Diabetes and Digestive and Kidney Diseases’ Intramural Research Program (to M. Chen and L.S. Weinstein).


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

Citation for this article: J Clin Invest. 2011;121(9):3492–3504. doi:10.1172/JCI46406.


1. Raisz LG. Pathogenesis of osteoporosis: concepts, conflicts, and prospects. J Clin Invest. 2005;115(12):3318–3325. [PMC free article] [PubMed]
2. Neer RM, et al. Effect of parathyroid hormone (1-34) on fractures and bone mineral density in postmenopausal women with osteoporosis. N Engl J Med. 2001;344(19):1434–1441. doi: 10.1056/NEJM200105103441904. [PubMed] [Cross Ref]
3. Bringhurst FR, et al. Cloned, stably expressed parathyroid hormone (PTH)/PTH-related peptide receptors activate multiple messenger signals and biological responses in LLC-PK1 kidney cells. Endocrinology. 1993;132(5):2090–2098. doi: 10.1210/en.132.5.2090. [PubMed] [Cross Ref]
4. Calvi LM, et al. Activated parathyroid hormone/parathyroid hormone-related protein receptor in osteoblastic cells differentially affects cortical and trabecular bone. J Clin Invest. 2001;107(3):277–286. doi: 10.1172/JCI11296. [PMC free article] [PubMed] [Cross Ref]
5. Schipani E, Kruse K, Juppner H. A constitutively active mutant PTH-PTHrP receptor in Jansen-type metaphyseal chondrodysplasia. Science. 1995;268(5207):98–100. [PubMed]
6. Pearman AT, Chou WY, Bergman KD, Pulumati MR, Partridge NC. Parathyroid hormone induces c-fos promoter activity in osteoblastic cells through phosphorylated cAMP response element (CRE)-binding protein binding to the major CRE. J Biol Chem. 1996;271(41):25715–25721. doi: 10.1074/jbc.271.41.25715. [PubMed] [Cross Ref]
7. Weinstein LS, Yu S, Warner DR, Liu J. Endocrine manifestations of stimulatory G protein alpha-subunit mutations and the role of genomic imprinting. Endocr Rev. 2001;22(5):675–705. doi: 10.1210/er.22.5.675. [PubMed] [Cross Ref]
8. Bianco P, Kuznetsov SA, Riminucci M, Fisher LW, Spiegel AM, Robey PG. Reproduction of human fibrous dysplasia of bone in immunocompromised mice by transplanted mosaics of normal and Gsalpha-mutated skeletal progenitor cells. J Clin Invest. 1998;101(8):1737–1744. doi: 10.1172/JCI2361. [PMC free article] [PubMed] [Cross Ref]
9. Hsiao EC, et al. Osteoblast expression of an engineered Gs-coupled receptor dramatically increases bone mass. Proc Natl Acad Sci U S A. 2008;105(4):1209–1214. [PubMed]
10. Jilka RL. Molecular and cellular mechanisms of the anabolic effect of intermittent PTH. Bone. 2007;40(6):1434–1446. doi: 10.1016/j.bone.2007.03.017. [PMC free article] [PubMed] [Cross Ref]
11. Ishizuya T, et al. Parathyroid hormone exerts disparate effects on osteoblast differentiation depending on exposure time in rat osteoblastic cells. J Clin Invest. 1997;99(12):2961–2970. doi: 10.1172/JCI119491. [PMC free article] [PubMed] [Cross Ref]
12. Wang YH, Liu Y, Buhl K, Rowe DW. Comparison of the action of transient and continuous PTH on primary osteoblast cultures expressing differentiation stage-specific GFP. J Bone Miner Res. 2005;20(1):5–14. doi: 10.1359/JBMR.041016. [PubMed] [Cross Ref]
13. Bastepe M, et al. Stimulatory G protein directly regulates hypertrophic differentiation of growth plate cartilage in vivo. Proc Natl Acad Sci U S A. 2004;101(41):14794–14799. doi: 10.1073/pnas.0405091101. [PubMed] [Cross Ref]
14. Chung UI, Lanske B, Lee K, Li E, Kronenberg H. The parathyroid hormone/parathyroid hormone-related peptide receptor coordinates endochondral bone development by directly controlling chondrocyte differentiation. Proc Natl Acad Sci U S A. 1998;95(22):13030–13035. [PubMed]
15. Kozhemyakina E, Cohen T, Yao TP, Lassar AB. Parathyroid hormone-related peptide represses chondrocyte hypertrophy through a protein phosphatase 2A/histone deacetylase 4/MEF2 pathway. Mol Cell Biol. 2009;29(21):5751–5762. doi: 10.1128/MCB.00415-09. [PMC free article] [PubMed] [Cross Ref]
16. Lanske B, et al. PTH/PTHrP receptor in early development and Indian hedgehog-regulated bone growth. Science. 1996;273(5275):663–666. doi: 10.1126/science.273.5275.663. [PubMed] [Cross Ref]
17. Sakamoto A, Chen M, Kobayashi T, Kronenberg HM, Weinstein LS. Chondrocyte-specific knockout of the G protein G(s)alpha leads to epiphyseal and growth plate abnormalities and ectopic chondrocyte formation. J Bone Miner Res. 2005;20(4):663–671. doi: 10.1359/JBMR.041210. [PubMed] [Cross Ref]
18. Day TF, Guo X, Garrett-Beal L, Yang Y. Wnt/beta-catenin signaling in mesenchymal progenitors controls osteoblast and chondrocyte differentiation during vertebrate skeletogenesis. Dev Cell. 2005;8(5):739–750. doi: 10.1016/j.devcel.2005.03.016. [PubMed] [Cross Ref]
19. Hill TP, Spater D, Taketo MM, Birchmeier W, Hartmann C. Canonical Wnt/beta-catenin signaling prevents osteoblasts from differentiating into chondrocytes. Dev Cell. 2005;8(5):727–738. doi: 10.1016/j.devcel.2005.02.013. [PubMed] [Cross Ref]
20. Rodda SJ, McMahon AP. Distinct roles for Hedgehog and canonical Wnt signaling in specification, differentiation and maintenance of osteoblast progenitors. Development. 2006;133(16):3231–3244. doi: 10.1242/dev.02480. [PubMed] [Cross Ref]
21. Kulkarni NH, et al. Effects of parathyroid hormone on Wnt signaling pathway in bone. J Cell Biochem. 2005;95(6):1178–1190. doi: 10.1002/jcb.20506. [PubMed] [Cross Ref]
22. Bellido T, et al. Chronic elevation of parathyroid hormone in mice reduces expression of sclerostin by osteocytes: a novel mechanism for hormonal control of osteoblastogenesis. Endocrinology. 2005;146(11):4577–4583. [PubMed]
23. Keller H, Kneissel M. SOST is a target gene for PTH in bone. Bone. 2005;37(2):148–158. doi: 10.1016/j.bone.2005.03.018. [PubMed] [Cross Ref]
24. Leupin O, et al. Control of the SOST bone enhancer by PTH using MEF2 transcription factors. J Bone Miner Res. 2007;22(12):1957–1967. doi: 10.1359/jbmr.070804. [PMC free article] [PubMed] [Cross Ref]
25. Guo J, et al. Suppression of Wnt signaling by Dkk1 attenuates PTH-mediated stromal cell response and new bone formation. Cell Metabolism. 2010;11(2):161–171. [PMC free article] [PubMed]
26. Yao GQ, Wu JJ, Troiano N, Insogna K. Targeted overexpression of Dkk1 in osteoblasts reduces bone mass but does not impair the anabolic response to intermittent PTH treatment in mice. J Bone Miner Metab. 2011;29(2):141–148. doi: 10.1007/s00774-010-0202-3. [PMC free article] [PubMed] [Cross Ref]
27. Li J, et al. Dkk1-mediated inhibition of Wnt signaling in bone results in osteopenia. Bone. 2006;39(4):754–766. [PubMed]
28. Winkler DG, et al. Osteocyte control of bone formation via sclerostin, a novel BMP antagonist. Embo J. 2003;22(23):6267–6276. doi: 10.1093/emboj/cdg599. [PubMed] [Cross Ref]
29. O’Brien CA, et al. Control of bone mass and remodeling by PTH receptor signaling in osteocytes. PLoS One. 2008;3(8):e2942. doi: 10.1371/journal.pone.0002942. [PMC free article] [PubMed] [Cross Ref]
30. Suda M, et al. Prostaglandin E receptor subtypes in mouse osteoblastic cell line. Endocrinology. 1996;137(5):1698–1705. [PubMed]
31. Abe E, et al. TSH is a negative regulator of skeletal remodeling. Cell. 2003;115(2):151–162. doi: 10.1016/S0092-8674(03)00771-2. [PubMed] [Cross Ref]
32. Elefteriou F, et al. Leptin regulation of bone resorption by the sympathetic nervous system and CART. Nature. 2005;434(7032):514–520. doi: 10.1038/nature03398. [PubMed] [Cross Ref]
33. Sakamoto A, Chen M, Nakamura T, Xie T, Karsenty G, Weinstein LS. Deficiency of the G-protein alpha-subunit G(s)alpha in osteoblasts leads to differential effects on trabecular and cortical bone. J Biol Chem. 2005;280(22):21369–21375. doi: 10.1074/jbc.M500346200. [PubMed] [Cross Ref]
34. Wu J, et al. Osteoblastic regulation of B lymphopoiesis is mediated by Gsalpha-dependent signaling pathways. Proc Natl Acad Sci U S A. 2008;105(44):16976–16981. [PubMed]
35. Boguslawski G, et al. Activation of osteocalcin transcription involves interaction of protein kinase A- and protein kinase C-dependent pathways. J Biol Chem. 2000;275(2):999–1006. doi: 10.1074/jbc.275.2.999. [PubMed] [Cross Ref]
36. Selvamurugan N, Chou WY, Pearman AT, Pulumati MR, Partridge NC. Parathyroid hormone regulates the rat collagenase-3 promoter in osteoblastic cells through the cooperative interaction of the activator protein-1 site and the runt domain binding sequence. J Biol Chem. 1998;273(17):10647–10657. doi: 10.1074/jbc.273.17.10647. [PubMed] [Cross Ref]
37. Soriano P. Generalized lacZ expression with the ROSA26 Cre reporter strain. Nat Genet. 1999;21(1):70–71. [PubMed]
38. Kalajzic I, et al. Use of type I collagen green fluorescent protein transgenes to identify subpopulations of cells at different stages of the osteoblast lineage. J Bone Miner Res. 2002;17(1):15–25. doi: 10.1359/jbmr.2002.17.1.15. [PubMed] [Cross Ref]
39. Bonewald LF, Johnson ML. Osteocytes, mechanosensing and Wnt signaling. Bone. 2008;42(4):606–615. doi: 10.1016/j.bone.2007.12.224. [PMC free article] [PubMed] [Cross Ref]
40. Manolagas SC. Birth and death of bone cells: basic regulatory mechanisms and implications for the pathogenesis and treatment of osteoporosis. Endocr Rev. 2000;21(2):115–137. doi: 10.1210/er.21.2.115. [PubMed] [Cross Ref]
41. Dallas SL, et al. Time lapse imaging techniques for comparison of mineralization dynamics in primary murine osteoblasts and the late osteoblast/early osteocyte-like cell line MLO-A5. Cells Tissues Organs. 2009;189(1–4):6–11. doi: 10.1159/000151745. [PMC free article] [PubMed] [Cross Ref]
42. Zhang K, et al. E11/gp38 selective expression in osteocytes: regulation by mechanical strain and role in dendrite elongation. Mol Cell Biol. 2006;26(12):4539–4552. [PMC free article] [PubMed]
43. Hadjiargyrou M, Rightmire EP, Ando T, Lombardo FT. The E11 osteoblastic lineage marker is differentially expressed during fracture healing. Bone. 2001;29(2):149–154. [PubMed]
44. Gorski JP. Is all bone the same? Distinctive distributions and properties of non-collagenous matrix proteins in lamellar vs. woven bone imply the existence of different underlying osteogenic mechanisms. Crit Rev Oral Biol Med. 1998;9(2):201–223. doi: 10.1177/10454411980090020401. [PubMed] [Cross Ref]
45. DasGupta R, Fuchs E. Multiple roles for activated LEF/TCF transcription complexes during hair follicle development and differentiation. Development. 1999;126(20):4557–4568. [PubMed]
46. Weinstein LS, Chen M, Xie T, Liu J. Genetic diseases associated with heterotrimeric G proteins. Trends Pharmacol Sci. 2006;27(5):260–266. doi: 10.1016/ [PubMed] [Cross Ref]
47. Tobimatsu T, et al. Parathyroid hormone increases beta-catenin levels through Smad3 in mouse osteoblastic cells. Endocrinology. 2006;147(5):2583–2590. doi: 10.1210/en.2005-1627. [PubMed] [Cross Ref]
48. Wan M, et al. Parathyroid hormone signaling through low-density lipoprotein-related protein 6. Genes Dev. 2008;22(21):2968–2979. doi: 10.1101/gad.1702708. [PubMed] [Cross Ref]
49. Taurin S, Sandbo N, Qin Y, Browning D, Dulin NO. Phosphorylation of beta-catenin by cyclic AMP-dependent protein kinase. J Biol Chem. 2006;281(15):9971–9976. [PubMed]
50. Jilka RL, Weinstein RS, Bellido T, Roberson P, Parfitt AM, Manolagas SC. Increased bone formation by prevention of osteoblast apoptosis with parathyroid hormone. J Clin Invest. 1999;104(4):439–446. doi: 10.1172/JCI6610. [PMC free article] [PubMed] [Cross Ref]
51. Jilka RL, O’Brien CA, Ali AA, Roberson PK, Weinstein RS, Manolagas SC. Intermittent PTH stimulates periosteal bone formation by actions on post-mitotic preosteoblasts. Bone. 2009;44(2):275–286. doi: 10.1016/j.bone.2008.10.037. [PMC free article] [PubMed] [Cross Ref]
52. Glass DA 2nd, et al. Canonical Wnt signaling in differentiated osteoblasts controls osteoclast differentiation. Dev Cell. 2005;8(5):751–764. doi: 10.1016/j.devcel.2005.02.017. [PubMed] [Cross Ref]
53. Holmen SL, et al. Essential role of beta-catenin in postnatal bone acquisition. J Biol Chem. 2005;280(22):21162–21168. [PubMed]
54. Kramer I, et al. Osteocyte Wnt/beta-catenin signaling is required for normal bone homeostasis. Mol Cell Biol. 2010;30(12):3071–3085. doi: 10.1128/MCB.01428-09. [PMC free article] [PubMed] [Cross Ref]
55. Yoshida K, et al. Stimulation of bone formation and prevention of bone loss by prostaglandin E EP4 receptor activation. Proc Natl Acad Sci U S A. 2002;99(7):4580–4585. doi: 10.1073/pnas.062053399. [PubMed] [Cross Ref]
56. Zhang X, Schwarz EM, Young DA, Puzas JE, Rosier RN, O’Keefe RJ. Cyclooxygenase-2 regulates mesenchymal cell differentiation into the osteoblast lineage and is critically involved in bone repair. J Clin Invest. 2002;109(11):1405–1415. [PMC free article] [PubMed]
57. Chen M, et al. Increased glucose tolerance and reduced adiposity in the absence of fasting hypoglycemia in mice with liver-specific Gs alpha deficiency. J Clin Invest. 2005;115(11):3217–3227. doi: 10.1172/JCI24196. [PMC free article] [PubMed] [Cross Ref]
58. Inoue K, et al. A crucial role for matrix metalloproteinase 2 in osteocytic canalicular formation and bone metabolism. J Biol Chem. 2006;281(44):33814–33824. doi: 10.1074/jbc.M607290200. [PubMed] [Cross Ref]
59. Sims NA, Brennan K, Spaliviero J, Handelsman DJ, Seibel MJ. Perinatal testosterone surge is required for normal adult bone size but not for normal bone remodeling. Am J Physiol Endocrinol Metab. 2006;290(3):E456–E462. doi: 10.1152/ajpendo.00311.2005. [PubMed] [Cross Ref]
60. Bouxsein ML, Boyd SK, Christiansen BA, Guldberg RE, Jepsen KJ, Muller R. Guidelines for assessment of bone microstructure in rodents using micro-computed tomography. J Bone Miner Res. 2010;25(7):1468–1486. [PubMed]
61. Yang D, Guo J, Divieti P, Shioda T, Bringhurst FR. CBP/p300-interacting protein CITED1 modulates parathyroid hormone regulation of osteoblastic differentiation. Endocrinology. 2008;149(4):1728–1735. doi: 10.1210/en.2007-0826. [PubMed] [Cross Ref]
62. Aydin C, et al. Extralarge XL(alpha)s (XXL(alpha)s), a variant of stimulatory G protein alpha-subunit (Gs(alpha)), is a distinct, membrane-anchored GNAS product that can mimic Gs(alpha). Endocrinology. 2009;150(8):3567–3575. doi: 10.1210/en.2009-0318. [PubMed] [Cross Ref]
63. Aubin JE. Osteoprogenitor cell frequency in rat bone marrow stromal populations: role for heterotypic cell-cell interactions in osteoblast differentiation. J Cell Biochem. 1999;72(3):396–410. doi: 10.1002/(SICI)1097-4644(19990301)72:3<396::AID-JCB9>3.0.CO;2-6. [PubMed] [Cross Ref]
64. Strasser A. PB76: a novel surface glycoprotein preferentially expressed on mouse pre-B cells and plasma cells detected by the monoclonal antibody G-5-2. Eur J Immunol. 1988;18(11):1803–1810. doi: 10.1002/eji.1830181123. [PubMed] [Cross Ref]
65. Kenner L, et al. Mice lacking JunB are osteopenic due to cell-autonomous osteoblast and osteoclast defects. J Cell Biol. 2004;164(4):613–623. doi: 10.1083/jcb.200308155. [PMC free article] [PubMed] [Cross Ref]
66. Dobreva G, et al. SATB2 is a multifunctional determinant of craniofacial patterning and osteoblast differentiation. Cell. 2006;125(5):971–986. doi: 10.1016/j.cell.2006.05.012. [PubMed] [Cross Ref]
67. Tatsumi S, et al. Targeted ablation of osteocytes induces osteoporosis with defective mechanotransduction. Cell Metab. 2007;5(6):464–475. doi: 10.1016/j.cmet.2007.05.001. [PubMed] [Cross Ref]

Articles from The Journal of Clinical Investigation are provided here courtesy of American Society for Clinical Investigation