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NADPH oxidase gp91phox contributes to RANKL-induced osteoclast differentiation by upregulating NFATc1

Scientific Reports volume 6, Article number: 38014 (2016) | Download Citation


Bone-marrow derived monocyte-macrophages (BMMs) differentiate into osteoclasts by M-CSF along subsequent RANKL stimulation possibly in collaboration with many other unknown cytokines released by pre- or mature osteoblasts. The differentiation process requires receptor activator of nuclear factor kappa-B ligand (RANKL)/RANK signaling and reactive oxygen species (ROS) such as superoxide anion (O2•−). Gp91phox, a plasma membrane subunit of NADPH oxidase (Nox), is constitutively expressed in BMMs and plays a major role in superoxide anion production. In this study, we found that mice deficient in gp91phox (gp91phox−/−) showed defects in osteoclast differentiation. Femurs of these mice produced osteoclasts at about 70% of the levels seen in femurs from wild-type mice, and accordingly exhibited excessive bone density. This abnormal bone growth in the femurs of gp91phox−/− mice resulted from impaired osteoclast differentiation. In addition, gp91phox−/− mice were defective for RANKL-induced expression of nuclear factor of activated T cells c1 (NFATc1). However, H2O2 treatment compensated for gp91phox deficiency in BMMs, almost completely rescuing osteoclast differentiation. Treating wild-type BMMs with antioxidants and superoxide inhibitors resulted in a differentiation defect resembling the phenotype of gp91phox−/− BMMs. Therefore, our results demonstrate that gp91phox-derived superoxide is important for promoting efficient osteoclast differentiation by inducing NFATc1 as a downstream signaling mediator of RANK.


Osteoclasts are multinucleated bone cells that originate from bone marrow-derived monocyte-macrophages (BMMs). Osteoclast differentiation from hematopoietic progenitor cells requires macrophage colony stimulating factor (M-CSF) and receptor activator of nuclear factor kappa-B ligand (RANKL)1,2. M-CSF induces the formation of BMMs and the expression of RANK in early-stage osteoclast precursor cells3. M-CSF activates osteoclast precursors during early phases of osteoclast differentiation. RANKL induces differentiation of osteoclast precursors into osteoclasts and suppresses osteoclast apoptosis through NF-κB and NFATc1 signaling4. Osteoclasts break down bone tissue by secreting proteases, a process known as bone resorption. This function is critical for normal bone repairing and remodeling. Cathepsin K (CTSK) is the major protease involved in degrading type I collagen and other noncollagenous proteins. Knockout of CTSK in mice leads to an osteopetrotic phenotype, which is partially compensated for by increased expression of other bone proteases. Bone resorption is a multistep process associated with many enzymatic activities including proteolytic degradation by CTSK. NFATc1-mediated CTSK gene expression is induced by RANKL stimulation5. CTSK is secreted by osteoclasts to degrade collagen and other matrix proteins during bone resorption. Therefore, bone density and especially bone resorption are tightly regulated by the RANK–RANKL signaling pathway.

In the last decade, studies have indicated that reactive oxygen species (ROS), including superoxide and hydrogen peroxide, are crucial components that regulate the differentiation process of osteoclasts (see6 for a review). Reactive oxygen species (ROS) mediate RANK–RANKL-induced signaling pathways and cellular events as a second messenger in osteoclast precursors7,8. Conversely, RANKL stimulation transiently increases intracellular ROS levels through NADPH oxidase (Nox), and ROS act as second messengers in RANKL-induced signaling pathways in osteoclast precursors, regulating their consequent differentiation into osteoclasts7,8,9,10. Similarly, M-CSF also transiently increases intracellular ROS levels through Nox3. These findings indicate that Nox-derived ROS are essential intracellular mediators throughout the osteoclast differentiation process.

Nox consists of integral membrane enzymes that produce superoxide (O2•−) by transporting electrons to oxygen from NADPH across the membrane. Nox1-5 have been described in mammals11. Among those, Nox1, Nox2, and Nox4 have been found in osteoclast precursors and osteoblasts. Gp91phox, also known as Nox2, is highly expressed in neutrophils and macrophages, where it generates superoxide that is essential for killing pathogens by the respiratory burst12. Upon cellular activation, three cytoplasmic subunits, p47phox, p67phox, and p40phox, translocate to the membrane and join together with membrane-bound flavocytochrome b, p91phox, and p22phox to form active Nox213.

Recently, it has been reported that cellular Nox2 levels are regulated by a protein called negative regulator of ROS (NRROS)14. NRROS is located in the endoplasmic reticulum, where it negatively regulates ROS generation by degrading Nox2 during the inflammatory response. More recently, Kim et al. reported that NRROS is increased during osteoclast differentiation and represses Nox1 and Nox2 expression, thereby attenuating RANKL-induced osteoclast differentiation15. These findings suggest that Nox2 expression and Nox2-derived ROS are tightly controlled by negative regulatory networks. Mitochondria are also known to regulate Nox2 activation. Mitochondrial ROS induce slower but long-lasting Nox2 activity, suggesting cross-talk between mitochondria and Nox216. More research is required in order to understand the precise regulatory networks that control Nox2 activity during osteoclast formation.

RANK is a TNF receptor family member that recognizes RANKL through cell-to-cell interaction with stromal cells, and promotes the differentiation of osteoclast precursors into osteoclasts in the presence of M-CSF17. RANK expression is induced in osteoclast precursors by M-CSF3. RANKL stimulation recruits adaptor molecules such as TNF receptor-associated factor 6 (TRAF6), and activates downstream signaling cascades including MAPKs, PI3K, and NF-κB18. These intracellular signaling pathways consequently upregulate osteoclastogenic transcription factors, including NFATc119,20. NFATc1 expression in RANKL-stimulated osteoclast precursors is crucial for osteoclast differentiation, as NFATc1 induces the expression of osteoclast-specific genes such as tartrate-resistant acid phosphatase (TRAP), CTSK17,21,22 and osteoclast-associated receptor (OSCAR)23,24. NFATc1-deficient embryonic stem cells fail to differentiate into osteoclasts in response to RANKL stimulation. Ectopic expression of NFATc1 allows osteoclast precursors to undergo efficient differentiation in the absence of RANKL signaling. Thus, NFATc1 may represent the master switch that functions downstream of RANKL to regulate osteoclast differentiation.

Fusion of osteoclast precursors is a critical cellular event for osteoclast differentiation, and understanding its regulation will have an important impact on the development of a new therapy to control bone loss. Osteoclast fusion is regulated by various factors. Dendritic cell–specific transmembrane protein (DC-STAMP), a putative seven-transmembrane protein has been identified as an essential factor for osteoclast fusion in bone homeostasis and RANKL is a strong inducer of DC-STAMP production25,26. Although osteoclast differentiation is known to require RANKL and M-CSF, non-canonical pathways of osteoclast formation were reported in which cytokines/growth factors can substitute for RANKL to induce osteoclast formation27. Substitutes for RANKL include LIGHT, TNF-α and interleukins 6, 11 and 828. Recently, RANKL has been reported that it can even suppress osteoclast differentiation by binding leucine-rich repeat-containing G-protein-coupled receptor 4 (LGR4, also called GPR48), another receptor for RANKL to compete RANK. RANKL binding to LGR4 activates the Gαq and GSK3-β signaling pathway, an action that suppresses the expression and activity of NFATc1 during osteoclastogenesis29.

In this study, we demonstrate that gp91phox is involved in osteoclast differentiation by enhancing RANKL-induced NFATc1 expression in osteoclast precursors. This suggests that gp91phox-derived superoxide is crucial for osteoclast precursors to differentiate into osteoclasts in collaboration with RANKL/ NFATc1 signal pathways.


Superoxide production was impaired in gp91phox−/− osteoclasts

Although ROS are clearly linked to osteoclast differentiation, we wanted to test if gp91phox-derived superoxide participates in osteoclast differentiation and bone resorption. Thus, we compared superoxide production between osteoclast precursors derived from gp91phox−/− mice and osteoclast precursors derived from wild-type mice after stimulation with 200 ng/mL phorbol 12-myristate 13-acetate (PMA) (Fig. 1A) or 50 ng/mL RANKL (Fig. 1B) for 10 min and 30 min, respectively, by isoluminol chemiluminescence assay. In contrast to wild-type cells, gp91phox-deficient osteoclast precursors showed decreased superoxide production in response to PMA or RANKL. We stimulated osteoclast precursors with M-CSF plus RANKL for an additional 4 days to produce osteoclasts and examined intracellular ROS levels in fully differentiated osteoclasts from gp91phox−/− mice and wild-type mice after PMA stimulation. As shown by fluorescence microscopic images visualized with DCF-DA (Fig. 1C), osteoclasts derived from gp91phox−/− mice did not produce ROS in response to PMA as readily as osteoclasts from wild-type mice. These results indicate that gp91phox is an essential Nox homologue for ROS production in both osteoclast precursors and osteoclasts in response to RANKL and PMA stimulation.

Figure 1: Impaired RANKL-induced ROS production in osteoclast precursors and osteoclasts from gp91phox−/− mice.
Figure 1

Osteoclast precursors were incubated with (A) PMA or (B) RANKL after preloading with isoluminol, and superoxide production was measured. Result represent the mean ± SD of 6 (A) and 3 (B) independent experiments, *p < 0.05 and **p < 0.01 (paired t-test). (C) Osteoclasts obtained from wild-type and gp91phox−/− mice were pretreated with DCF-DA and observed under fluorescence microscope at the magnitudes designated after PMA treatment for 10 min. The fluorescent images are representative of least 3 independent experiments, each performed in triplicate.

Gp91phox−/− mice defective osteoclast formation had elevated bone volume

Since BMMs from gp91phox−/− mice showed defects in ROS production, we tested the ability of BMMs from gp91phox−/− mice to differentiate into osteoclasts. To accomplish this, we compared osteoclast populations and bone density between femurs from gp91phox−/− mice and femurs from wild-type mice. We detected osteoclasts in the femurs by staining TRAP, an osteoclast marker (Fig. 2A) and then counted TRAP-positive cells in the histological sections (Fig. 2B). We found that gp91phox−/− femurs displayed only about 68% of the number of osteoclasts seen in wild-type femurs (34.7 ± 3.1 for wild-type vs. 23.3 ± 5.0 for gp91phox−/− femurs). As superoxide is crucial for osteoclast differentiation3,9,10,12,30,31,32,33, the lower number of osteoclast in gp91phox−/− femurs might be due to a lack of gp91phox-derived superoxide. Osteoclasts degrade bone, a phenomenon referred to as bone resorption34,35. Thus, we tested if the decreased number of osteoclasts in the femurs of gp91phox−/− mice corresponded to an increase in bone mass. Radiographic μCT analyses indicated that femurs from gp91phox−/− mice showed greater bone density than femurs from wild-type mice (Fig. 2C). These data were plotted as % of bone volume fraction (BV/TV); trabecular bone volume (BV) to total volume (TV) ratio. The femurs from gp91phox−/− appeared higher in bone density by 24% than those from wild-type femurs (Fig. 2D). Although we did not definitely verify causative links between the impaired superoxide and osteoclast productions and the higher bone density in gp91phox−/− femurs, these concurrent events strongly suggest that higher bone density developed by gp91phox−/− mice compared to wild-type mice was due to their defective osteoclast differentiation by BMMs. There were no significant differences in body weight between gp91phox−/− mice and wild-type mice (Fig. 2E). Thus, the differences in bone density observed between gp91phox−/− femurs and wild-type mice were not due to differences in total body weight.

Figure 2: Osteopetrotic phenotypes of gp91phox−/− mice.
Figure 2

(A~D) Data are expressed as the mean ± SD, *p < 0.05 (paired t-test). (A) TRAP expression in femurs from 6 mice (24-week-old, wild-type male = 3; gp91phox−/− male = 3, n = 3 independent replicates) detected from histological sections. (B) Osteoclasts from femurs per selected field were counted (n = 3 independent replicates). (C) Microcomputed tomography of femurs from wild-type and gp91phox−/− mice was assessed (6-week-old, wild-type male = 4; gp91phox−/− male = 4, n = 4 independent replicates). (D) Trabecular bone volumes of wild-type (male = 4) and gp91phox−/− (male = 4) mice were compared by quantitative μCT as % of bone volume fraction (BV/TV). (E) Body weights of 42 wild-type (male = 19, female = 23) and 41 gp91phox−/− mice (male = 22, female = 19) were compared for 100 days after birth. Data were analyzed by one-way ANOVA and expressed as the mean ± SD.

Gp91phox may play an important role for osteoclast precursors to differentiate into osteoclasts

Osteoclasts contain vacuoles filled with TRAP and CTSK. We utilized this to assess osteoclast differentiation by staining for TRAP as mature osteoclast marker. We counted the number of TRAP-positive multinucleated cells (more than three nuclei) which represent mature osteoclasts. Histological analysis revealed that BMMs from gp91phox−/− mice displayed a significantly decreased number of TRAP-positive osteoclasts after stimulation with RANKL (~60% compared to wild-type cells) (Fig. 3A,B). Additionally, TRAP-positive osteoclasts from gp91phox−/− mice were significantly smaller than osteoclasts from wild-type cells (Fig. 3A,C). We compared heterozygous gp91phox+/− mice with littermate gp91phox−/− mice for the osteoclast numbers, TRAP and CTSK expression after RANKL stimulation. Heterozygous gp91phox+/− mice displayed significantly more osteoclasts (Fig. 3D~136% compared to knockout mice), expression levels of TRAP (Fig. 3E)and CTSK (Fig. 3F) compared to littermate gp91phox−/− mice.

Figure 3: Impaired RANKL-induced osteoclast differentiation in gp91phox−/− mice.
Figure 3

Data are expressed as the mean ± SD, *p < 0.05 and **p < 0.01 (paired t-test). (A–C) Degree of RANKL/MCSF-induced osteoclast differentiation from wild-type and gp91phox−/− BMMs was assessed on 8th day following RANKL stimulation by histological examination (A), cell numbers per well (B), and relative osteoclast areas (C). Result represent the mean ± SD of 3 independent experiments, each performed in triplicate. (D) Osteoclast numbers from 8 littermates (6-week-old, gp91phox+/− female = 4; gp91phox−/− male = 4) were determined (n = 4 independent replicates). Expression of TRAP (E) and CTSK (F) were measured by qPCR during osteoclast differentiation (n = 5 independent experiments, each performed in duplicate). (G) TRAP activity in osteoclasts was determined by measuring acid phosphatase activity (n = 3 independent experiments, each performed in triplicate). (H) BMMs from wild-type and gp91phox−/− were differentiated into osteoclasts. Resulting cells were assessed for resorption activity (n = 3 independent experiments, each performed in triplicate). (I) Relative resorption areas were calculated and plotted as % of wild-type control (n = 3 independent experiments, each performed in triplicate).

Consistent with the decreased number of TRAP-positive cells, gp91phox−/− osteoclasts contained lower TRAP activity (~67% of wild-type) after stimulation with RANKL than wild-type osteoclasts (Fig. 3G). TRAP activity is abundant in osteoclasts. Since we calculated TRAP activity per cell, the data suggest that a large portion of BMMs from gp91phox−/− mice might remain undifferentiated even in the presence of M-CSF and RANKL. We do not rule out the possibility that osteoclasts derived from of gp91phox−/− mice were much smaller with less TRAP than those from wild-type mice. Femurs from gp91phox−/− mice showed less resorptive area than femurs from wild-type mice as observed by histochemical images (Fig. 3H,I). Taken together, these results suggest that gp91phox may play an important role during the differentiation of osteoclast precursors into osteoclasts.

ROS are indispensable for the differentiation of BMMs into osteoclasts

Lee et al.9 identified a crucial role for ROS in RANKL-induced murine BMM differentiation into osteoclasts. Thus, we treated the mouse BMMs with various antioxidants such as superoxide dismutase (SOD), N-acetylcysteine (NAC), and diphenyleneiodonium (DPI) to see whether these ROS scavengers can prevent M-CSF- and RANKL-induced differentiation of osteoclast precursors into osteoclasts. SOD plays a crucial role in the superoxide detoxification process. NAC is a potent oxidant scavenger, and DPI is an inhibitor of flavoprotein, a Nox constituent. All the antioxidants used in this experiment inhibited osteoclast formation in a dose-dependent manner (Fig. 4). These parallel relationships of ROS levels with the potentials of BMMs to differentiate into osteoclasts support our view that intracellular ROS play important role for the differentiation of BMMs into osteoclasts.

Figure 4: Effect of antioxidants and ROS inhibitors on osteoclast differentiation.
Figure 4

BMMs were treated with SOD, NAC, and DPI at different concentrations and then osteoclast differentiation was induced. Resulting cells were visually examined for osteoclast production under a microscope. Osteoclast numbers per well were counted from histological images and plotted along the designated ROS inhibitor concentrations. Data are expressed as the mean ± SD of 3 independent experiments, each performed in triplicate, *p < 0.05 and **p < 0.01 (paired t-test).

H2O2 rescued the osteoclast differentiation defect of gp91phox−/− BMMs

Membrane-bound gp91phox is one component of the Nox2 complex that generates superoxide anions from oxygen. Superoxide spontaneously forms H2O2, which undergoes further reactions to generate ROS. Thus, we tested if H2O2 treatment could rescue the osteoclast differentiation defect of gp91phox knockout BMMs. To accomplish this, gp91phox−/− BMMs were subjected to RANKL-induced osteoclast differentiation in the presence or absence of H2O2, and we evaluated osteoclast differentiation. As shown in Fig. 5, 0.1 μM H2O2 completely rescued the defective osteoclast differentiation in gp91phox−/− BMMs to levels seen in wild-type BMMs.

Figure 5: Differential effects of H2O2 on osteoclast differentiation in wild-type and gp91phox−/− BMMs.
Figure 5

BMMs were treated with H2O2 at the indicated concentrations osteoclast differentiation was induced. (A) Effects of H2O2 on osteoclast differentiation were visually observed under a microscope. (B) Numbers of osteoclasts per well were counted and plotted along the concentrations of H2O2. Data are expressed as the mean ± SD of 3 independent experiments, each performed in triplicate, *p < 0.05 and **p < 0.01 (paired t-test).

Gp91phox-derived superoxide enhanced RANKL-induced NFATc1 expression in osteoclasts

RANKL signaling activates multiple downstream signaling pathways required for osteoclast differentiation including NFATc1, NF-κB and AP-1. In particular, NFATc1 represents the master switch for osteoclast differentiation downstream of RANKL. Thus, we measured expression levels of NF-κB, AP-1, and NFATc1 in gp91phox−/− and wild-type BMMs during RANKL-induced osteoclast differentiation. BMMs were incubated with M-CSF for 3 days to induce differentiation to osteoclast precursors. Osteoclast precursors were cultured with 30 ng/mL M-CSF and 50 ng/mL RANKL for an additional 4 days to promote differentiation into mature osteoclasts. We monitored NFATc1 and NF-κB protein levels by western blotting during this process. As expected, BMMs from wild-type mice expressed NFATc1 in response to RANKL, reaching a maximum level on day 6 and declining afterwards. In sharp contrast, BMMs from gp91phox−/− mice showed blunted NFATc1 expression during RANKL stimulation (Fig. 6A,B). However, we did not notice a significant difference in NF-κB levels between wild-type and gp91phox−/− BMMs upon RANKL stimulation (Fig. 6A,B). These results indicate that NF-κB expression is not affected by gp91phox deficiency during RANKL-induced osteoclast differentiation. Although RANKL induces other osteoclast-specific genes including AP-1 and MAPKs during osteoclast differentiation21,22,36, we did not detect any noticeable effects of gp91phox on the levels of AP-1 and phosphorylated MAPKs in both osteoclast precursors and osteoclasts regardless in the presence and absence of RANKL during differentiation culture (data not shown), suggesting that MAPKs and AP-1 may be regulated independently of gp91phox-derived superoxide signaling pathways.

Figure 6: Effect of H2O2 on NFATc1 and NF-κB expression in osteoclasts from wild-type and gp91phox−/− mice during RANKL-induced osteoclast differentiation.
Figure 6

Data are expressed as the mean ± SD of 3 independent experiments, each performed in triplicate, *p < 0.05 and **p < 0.01 (paired t-test). (A,B) Differential NFATc1 expression between wild-type and gp91phox−/− cells during osteoclast differentiation is shown by western blotting. (C) BMMs from wild-type and gp91phox−/− mice were subjected to RANKL-induced osteoclast differentiation following treatment with or without 0.1 μM H2O2. After 4 (osteoclast precursor) and 8 (osteoclast) days, expression of NFATc1 and NF-κB was assessed by western blotting.

We then asked whether gp91phox cells defect in RANKL-induced NFATc1 expression could be rescued by H2O2 treatment. To address this, we monitored NFATc1 expression in differentiating osteoclasts in the presence or absence of 0.1 μM H2O2. Addition of H2O2 to gp91phox−/− BMMs greatly raised NFATc1 expression levels upon RANKL stimulation to levels almost comparable to the wild-type BMMs on day 8 (Fig. 6C). This suggests that ROS play a critical role in inducing NFATc1 expression in response to RANKL stimulation. H2O2 treatment did not significantly affect wild-type BMMs.

NFATc1 represents the master switch for regulating osteoclast differentiation, functioning downstream of RANKL. Thus, our results indicate that gp91phox-derived superoxide induces NFATc1 expression in response to RANKL stimulation, implicating gp91phox in promoting osteoclast differentiation downstream of RANKL. Although RANKL induces other osteoclast-specific genes including AP-1 and MAPKs during osteoclast differentiation21,22,36,37, we did not detect any noticeable effects of gp91phox on the levels of AP-1 and phosphorylated MAPKs (data not shown), suggesting that MAPKs and AP-1 are regulated independently of gp91phox-derived superoxide signaling pathways.


Although ROS have been shown to act as a cellular secondary messengers, the involvement of ROS signaling pathways in RANKL-mediated osteoclast differentiation remain unclear. In this study, we demonstrated that gp91phox−/− -derived superoxide participates in osteoclast differentiation from BMMs. These conclusions were verified by in vivo observations that the femurs from gp91phox−/− mice had fewer osteoclasts and higher bone density than femurs from wild-type mice. Levels of osteoclast-specific markers and TRAP activity were assessed in osteoclasts differentiating in response to M-CSF/RANKL. Consistent with the in vivo results, the osteoclasts from gp91phox−/− mice expressed significantly lower levels of osteoclast markers compared to osteoclasts from wild-type mice. We also noticed that upon RANKL stimulation, the BMMs from gp91phox−/− mice could not efficiently upregulate NFATc1, the master switch for regulating osteoclast differentiation. Addition of H2O2 to the differentiation cultures rescued the differentiation defects of BMMs from gp91phox−/−, by raising osteoclast numbers and RANKL-induced NFATc1 expression almost to wild-type levels. Conversely, antioxidants or ROS scavengers hampered osteoclast differentiation. These data clearly suggest that gp91phox−/− -derived superoxide contributes to osteoclast differentiation by enhancing NFATc1 expression, and serves as a secondary messenger downstream of RANKL.

Nox-derived ROS are crucial for RANKL-induced osteoclast differentiation. Several Nox isoforms, such as Nox1, Nox2 (gp91phox), and Nox4 are known to mediate osteoclastogenesis in BM macrophages and osteoclasts. However, it is not known which isoforms participate in the specific stages of osteoclast differentiation. Yang et al.38 were the first to identify Nox4 as an NADPH oxidase expressed in BM-derived osteoclasts. They reported that Nox4 expression was increased during the course of osteoclastogenesis. These authors also demonstrated that Nox4, but not Nox2, is involved in RANKL-induced ROS formation, showing that antisense Nox4 oligonucleotides reduced osteoclastic superoxide generation and resorption pit formation30,38. Consistent with these results, Nox4−/− mice showed reduced osteoclast numbers and markers, with higher bone density31. In contrast, Sasaki et al. reported that Nox4 siRNA did not affect RANKL-dependent osteoclast differentiation33. Consistent with their results, Nox4 does not seem to be involved in acute TRAF6-mediated RANKL-induced signaling.

Nox4 is upregulated and becomes detectable in BMMs only after stimulation with RANKL/M-CSF, and thereby differentiation into osteoclasts30,31,33. Nox4 expression is a separate, later event during the course of differentiation31,33. In contrast to Nox4, Nox2 mRNA expression is highest in early stages of differentiation and reduces as RANKL-induced differentiation proceeds. As Nox2 expression decreases, reciprocal upregulation of Nox1 and Nox3 transcripts occurs32. In contrast to these findings, earlier reports indicated that Nox2 levels were higher in mature osteoclasts compared to precursors as determined through RT-PCR and immunocytochemistry9,39. These studies reported that Nox1, not Nox2, is the main producer of ROS during osteoclastogenesis. In general, previous reports on the roles of Nox isoforms in osteoclast differentiation are controversial. Unlike BM-derived osteoclast precursors, the mouse macrophage cell line, RAW 264.7 cells constitutively express abundant Nox2 mRNA at a level 1,000 times greater than Nox1 in response to RANKL, and Nox4 is not detectable32.

The reported discrepancies in Nox isoform expression levels during osteoclast differentiation may be mainly due to dynamic expression kinetics of each Nox isoform. Such conflicting findings may indicate that different Nox isoforms contribute to osteoclast differentiation at distinct timings, and therefore Nox isoforms may play non-overlapping or sequential roles for osteoclast formation depending on the differentiation stage. In fact, knockdown of any one Nox isoform often fails to cause noticeable changes in RANKL-mediated ROS production or osteoclast formation. For example, BMMs from Nox1 as well as Nox2 knockout mice generated ROS in response to RANKL and also differentiated into osteoclasts to the same degree as wild-type cells33. This results seemingly contrast our observations. Interestingly, Nox1 and Nox2 siRNAs significantly suppressed ROS generation and osteoclast formation in Nox2−/− and Nox1−/− cells, respectively. Therefore, there may be a flexible compensatory mechanism between Nox isoforms to facilitate osteoclast differentiation32. Thus, we are in favor of the view that Nox2 is involved in osteoclast differentiation from osteoclast precursor as a downstream mediator of RANKL, and is especially involved in NFATc1 induction. Therefore, Nox2 may play a unique role in differentiation by enhancing NFATc1-mediated transcriptional activity. Nakanishi et al.3 provided some evidence that Nox2 is essential for RANK expression in rat BMMs. Furthermore, mitochondrial redox signaling cross-talks with Nox complexes16. Considering that pre-osteoclast mitochondria produce ROS upon RANKL stimulation, it is possible that RANKL-mediated ROS formation is impaired in Nox2-deficient cells. Therefore, Nox2 may play a distinct role from other Nox homologs by providing mitochondrial ROS to BMMs during osteoclast differentiation. Supplementary H2O2 may substitute for Nox2 deficiency by enhancing RANKL-induced NFATc1 expression.

RANKL stimulation is coupled with NFATc1 activation, and a sustained NFATc1-dependent transcriptional program may represent the master switch for regulating osteoclast differentiation downstream of RANKL. In line with this, NFATc1-deficient embryonic stem cells fail to differentiate into osteoclasts in response to RANKL stimulation, and ectopic NFATc1 expression allows efficient osteoclast differentiation in the absence of RANKL signaling. We found that gp91phox deficiency markedly attenuated RANKL-induced NFATc1 expression and led to impaired osteoclast differentiation. Based on these results, we conclude that gp91phox-derived superoxide participates in osteoclast differentiation by assuring a sustained NFATc1-dependent transcriptional program. Further studies are necessary to determine the precise mechanism by which gp91phox-derived superoxide cooperates with RANK signaling pathways to enhance NFATc1 activity.

Materials and Methods


Wild-type C57BL/6 J mice (Jackson Lab.) and those lacking the gp91phox gene40 were housed under specific pathogen-free conditions at the animal facility of Inha University. All procedures were conducted in accordance with institutional guidelines approved by the Animal Care and Use Committee of Inha University (INHA 131217-255). Mice used in these experiments were 6–8 - week - old males unless otherwise stated.

Histologic and μCT analysis

For histological studies, bones were fixed in buffered formalin and subjected to μCT analysis (SkyScan, Brucker, Belgium), or decalcified in 10% EDTA, embedded in paraffin, sectioned, and stained for H&E and TRAP. Bone volume and density in a standard zone were determined using 6.5-μm voxel size at 80 kV and 80 μA. Bone samples were taken at 3000 msec per projection (500 total projections) and trabecular bone parameters (thickness, separation, and number) were analyzed by μCT41. Mouse body weight and bone weight were measured before experiments.

Osteoclast formation

Bone marrow cells were isolated from 6–8-week-old male mice and cultured overnight in α-MEM (Hyclone) supplemented with 10% fetal bovine serum, 100 U/mL penicillin, 100 μg/mL streptomycin, and 10 ng/mL recombinant murine M-CSF (Peprotech). Subsequently, nonadherent cells were separated and adherent cells (2 × 104 cells/96-well and 5 × 104 cells/48-well) continuously cultured with 30 ng/mL M-CSF for 3 additional days to induce differentiation into osteoclast precursors. Osteoclast precursors were cultured for an additional 4 days with a combination of 30 ng/mL M-CSF and 50 ng/mL RANKL (Peprotech). Osteoclast formation was assessed by counting TRAP-positive cells with more than three nuclei. For ROS-related experiments, BMMs were treated with H2O2 or various antioxidants such as SOD, NAC, or DPI.

TRAP staining

TRAP-positive cells were detected with a Leukocyte Acid Phosphatase Assay kit (Sigma) by following the manufacturer’s instructions. Briefly, cells were washed with PBS and fixed with a fixing solution containing citrate, acetone, and formaldehyde. Fixed cells were incubated with TRAP-staining solution for 1 h at 37 °C in the dark. After washing with water, cells were counterstained with hematoxylin. TRAP-positive cells containing three or more nuclei were counted under a light microscope.

TRAP activity

Cells were incubated in 50 mM citrate buffer (pH 4.5) containing 10 mM sodium tartrate and 5 mM 4-nitrophenyl phosphate in 96-well plates for 30 min at 37 °C. The reaction mixtures were then transferred to a new 96-well plate containing an equal volume of 0.1 N NaOH. Absorbance was measured at 405 nm using Versamax microplate reader (Molecular Devices) equipped with SoftMax software (Molecular Devices).

Quantitative real time PCR

Total RNA was extracted from cells using TRI reagent (MRC) according to the manufacturer’s instructions. Reverse transcription of total RNA was performed according to the protocol provided by Takara (Takara). PCR amplification of cDNA was carried out on an Applied Biosystems StepOne unit using SYBR Green PCR Master Mix and the following primers (forward and reverse, respectively): TRAP, 5′-ACG GCT ACT TGC GGT TTC A-3′ and 5′-TCC TTG GGA GGC TGG TCT T-3′; CTSK, 5′-GAA GAA GAC TCA CCA GAA GCA G-3′ and 5′-TCC AGG TTA TGG GCA GAG ATT-3′; GAPDH, 5′-CCT TCC GTC CTA CCC C-3′ and 5′-CCC AAG ATG CCC TTC ATG-3′. Amplification data were analyzed using the sequence detection software provided by Applied Biosystems.

Measurement of NADPH oxidase activity

Superoxide production was measured by an isoluminol chemiluminescence assay42 in 96-well plates using a SpectraMax L microplate reader (Molecular Devices). Osteoclast precursors (1 × 105) in PBSG (PBS with 0.9 mM CaCl2, 0.5 mM MgCl2, and 7.5 mM glucose) were added to each well of a 96-well plate with 125 μM isoluminol (Sigma) in 80 μL PBSG and 100 units HRP (Sigma) in 40 μL PBSG. After cells were incubated at 37 °C for 10 min, either 200 ng/mL PMA or 50 ng/mL RANKL was then injected into the wells by the automatic injector of the microplate reader. Chemiluminescence was detected as relative luminescence units by fast kinetic mode, and the amount of superoxide produced was determined using SoftMax PRO software. ROS levels in RANKL-treated osteoclasts were detected with 2′,7′-dichlorofluorescein diacetate (DCF-DA) as described previously43. DCF, a highly fluorescent compound formed from DCF-DA as a result of exposure to ROS, was detected by fluorescence spectroscopy with maximum excitation and emission spectra of 495 nm and 529 nm, respectively. The DCF-DA stained cells were also examined under a fluorescence microscope (Carl Zeiss, Oberkochen, Germany).

Western blot analysis

Cell lysates were prepared as described previously44 and 20–30 μg of total protein was separated with SDS-PAGE. Resolved proteins were transferred onto polyvinylidene fluoride membranes (BioRad) which were probed with specific Abs against MAPKs (Cell Signaling), Akt (Cell Signaling), NF-κB (Santa Cruz), AP-1 (Santa Cruz), NFATc1 (Santa Cruz), or β-actin (Sigma). The membranes were incubated with the appropriate secondary antibody and then signals were developed using the ECL method (Amersham).

Bone resorption assay

Cells were seeded on calcium phosphate plates (Corning osteo assay, Corning) and then cultured for 4 days with 30 ng/mL M-CSF and 50 ng/mL RANKL. Osteoclasts were removed using 0.2% Triton X-100 in 1 M NaCl to visualize resorption pits. Photographs of decalcified area were obtained under a light microscope at 40× magnification, and decalcified areas were measured using Image-Pro plus 4.5 software (MediaCybernetics).

Statistical analysis

Two-tailed Student’s t-test (paired) or one-way ANOVA for Fig. 2E were performed using SigmaPlot11 software (Systat Software). Results were expressed as mean ± SD, and p values less than 0.05 were considered statistically significant.

Additional Information

How to cite this article: Kang, I. S. and Kim, C. NADPH oxidase gp91phox contributes to RANKL-induced osteoclast differentiation by upregulating NFATc1. Sci. Rep. 6, 38014; doi: 10.1038/srep38014 (2016).

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  1. 1.

    , , & Essential role of macrophage colony-stimulating factor in the osteoclast differentiation supported by stromal cells. J. Exp. Med. 173, 1291–1294 (1991).

  2. 2.

    & The molecular understanding of osteoclast differentiation. Bone 40, 251–264 (2007).

  3. 3.

    , , & A crucial role for reactive oxygen species in macrophage colony-stimulating factor-induced RANK expression in osteoclastic differentiation. Int. J. Mol. Med. 31, 874–880 (2013).

  4. 4.

    , & Osteoclasts have multiple roles in bone in addition to bone resorption. Crit. Rev. Eukaryot. Gene Expr. 19, 171–180 (2009).

  5. 5.

    et al. Identification of NFAT binding sites that mediate stimulation of cathepsin K promoter activity by RANK ligand. Gene 446, 90–98 (2009).

  6. 6.

    & Reactive oxygen species and oxidative stress in osteoclastogenesis, skeletal aging and bone diseases. J. Bone Miner. Metab. 33, 359–370 (2015).

  7. 7.

    , , , & Involvement of hydrogen peroxide in the differentiation of clonal HD-11EM cells into osteoclast-like cells. J. Cell Physiol. 176, 574–587 (1998).

  8. 8.

    , , & Participation of oxidative stress in the process of osteoclast differentiation. Biochim. Biophys. Acta. 1157, 318–323 (1993).

  9. 9.

    et al. A crucial role for reactive oxygen species in RANKL-induced osteoclast differentiation. Blood 106, 852–859 (2005).

  10. 10.

    et al. Reactive oxygen species mediate RANK signaling in osteoclasts. Exp. Cell Res. 301, 119–127 (2004).

  11. 11.

    & The NOX family of ROS-generating NADPH oxidases: physiology and pathophysiology. Physiol. Rev. 87, 245–313 (2007).

  12. 12.

    , , & NADPH-oxidase expression and in situ production of superoxide by osteoclasts actively resorbing bone. J. Cell Biol. 126, 765–772 (1994).

  13. 13.

    NADPH oxidase: an update. Blood 93, 1464–1476 (1999).

  14. 14.

    et al. NRROS negatively regulates reactive oxygen species during host defense and autoimmunity. Nature 509, 235–239 (2014).

  15. 15.

    , , , & NRROS negatively regulates osteoclast differentiation by inhibiting RANKL-mediated NF-κB and reactive oxygen species pathways. Mol. Cells 38, 904–910 (2015).

  16. 16.

    Redox signaling (cross-talk) from and to mitochondria involves mitochondrial pores and reactive oxygen species. Biochim. Biophys. Acta. 1797, 897–906 (2010).

  17. 17.

    et al. Modulation of osteoclast differentiation and function by the new members of the tumor necrosis factor receptor and ligand families. Endocr. Rev. 20, 345–357 (1999).

  18. 18.

    & Signal transduction by receptor activator of nuclear factor kappa B in osteoclasts. Biochem. Biophys. Res. Commun. 305, 211–214 (2003).

  19. 19.

    et al. c-Fos: a key regulator of osteoclast-macrophage lineage determination and bone remodeling. Science 266, 443–448 (1994).

  20. 20.

    et al. Induction and activation of the transcription factor NFATc1 (NFAT2) integrate RANKL signaling in terminal differentiation of osteoclasts. Dev. Cell 3, 889–901 (2002).

  21. 21.

    , & Osteoclast differentiation and activation. Nature 423, 337–342 (2003).

  22. 22.

    , & Signaling crosstalk between RANKL and interferons in osteoclast differentiation. Arthritis Res. 4 Suppl 3, S227–232 (2002).

  23. 23.

    et al. Nuclear factor of activated T cells c1 induces osteoclast-associated receptor gene expression during tumor necrosis factor-related activation-induced cytokine-mediated osteoclastogenesis. J. Biol. Chem. 280, 35209–35216 (2005).

  24. 24.

    et al. NFATc1 regulation of the human beta3 integrin promoter in osteoclast differentiation. Gene 372, 92–102 (2006).

  25. 25.

    et al. DC-STAMP is essential for cell-cell fusion in osteoclasts and foreign body giant cells. J. Exp. Med. 202, 345–351 (2005).

  26. 26.

    , & Osteoclast fusion and regulation by RANKL-dependent and independent factors. World J. Orthop. 3, 212–222 (2012).

  27. 27.

    , , & Non-canonical (RANKL-independent) pathways of osteoclast differentiation and their role in musculoskeletal diseases. Clin. Rev. Allergy Immunol. 51, 16–26 (2016).

  28. 28.

    et al. The COP9 signalosome is required for light-dependent timeless degradation and Drosophila clock resetting. J. Neurosci. 29, 1152–1162 (2009).

  29. 29.

    et al. LGR4 is a receptor for RANKL and negatively regulates osteoclast differentiation and bone resorption. Nat. Med. 22, 539–546 (2016).

  30. 30.

    , , & Expression of Nox4 in osteoclasts. J. Cell Biochem. 92, 238–248 (2004).

  31. 31.

    et al. NADPH oxidase 4 limits bone mass by promoting osteoclastogenesis. J. Clin. Invest. 123, 4731–4738 (2013).

  32. 32.

    et al. NADPH oxidase-derived reactive oxygen species are essential for differentiation of a mouse macrophage cell line (RAW264.7) into osteoclasts. J. Med. Invest. 56, 33–41 (2009).

  33. 33.

    et al. Receptor activator of nuclear factor-kappaB ligand-induced mouse osteoclast differentiation is associated with switching between NADPH oxidase homologues. Free Radic. Biol. Med. 47, 189–199 (2009).

  34. 34.

    , , , & Isolated osteoclasts resorb the organic and inorganic components of bone. J. Cell Biol. 102, 1164–1172 (1986).

  35. 35.

    Bone resorption by osteoclasts. Science 289, 1504–1508 (2000).

  36. 36.

    et al. Critical roles of c-Jun signaling in regulation of NFAT family and RANKL-regulated osteoclast differentiation. J. Clin. Invest. 114, 475–484 (2004).

  37. 37.

    An essential role for free radicals and derived species in signal transduction. Faseb. J. 11, 118–124 (1997).

  38. 38.

    , , , & A new superoxide-generating oxidase in murine osteoclasts. J. Biol. Chem. 276, 5452–5458 (2001).

  39. 39.

    , & Nicotinamide adenine dinucleotide phosphate oxidase in the formation of superoxide in osteoclasts. Calcif. Tissue Int. 63, 346–350 (1998).

  40. 40.

    et al. Mouse model of X-linked chronic granulomatous disease, an inherited defect in phagocyte superoxide production. Nat. Genet. 9, 202–209 (1995).

  41. 41.

    et al. Guidelines for assessment of bone microstructure in rodents using micro-computed tomography. J. Bone Miner. Res. 25, 1468–1486 (2010).

  42. 42.

    & Respiratory burst in human neutrophils. J. Immunol. Methods 232, 3–14 (1999).

  43. 43.

    , , , & Taurine chloramine induces heme oxygenase-1 expression via Nrf2 activation in murine macrophages. Int. Immunopharmacol. 10, 440–446 (2010).

  44. 44.

    & Inhibition of LPS-induced NO production by taurine chloramine in macrophages is mediated through Ras-ERK-NF-κB. Biochem. Pharmacol. 70, 1352–1360 (2005).

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We thank MC Dinauer (Washington University, St. Louis) for supplying gp91phox−/− mice and helpful discussion, and YJ Kim (Indiana University, Indianapolis) for help in writing the manuscript. This research was supported by grants from NRF funded by the Korea MEST (2012R1A1A3007097 and 2014R1A1A2057148), and by a research grant from Inha University.

Author information


  1. Laboratory of Leukocyte Signaling Research, Department of Pharmacology, Inha University School of Medicine, Incheon 22212, Korea

    • In Soon Kang
    •  & Chaekyun Kim
  2. Convergent Research Center for Metabolism and Immunoregulation, Inha University, Incheon 22212, Korea

    • Chaekyun Kim


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Study design: C.K., Data collection and analysis: I.S.K. and C.K., Animal maintenance: I.S.K., Drafting manuscript: I.S.K. and C.K., Approving final version of manuscript: I.S.K. and C.K. I.S.K. and C.K. take responsibility for the integrity of the data analysis.

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The authors declare no competing financial interests.

Corresponding author

Correspondence to Chaekyun Kim.

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