Correspondence to: Mone Zaidi, Division of Endocrinology, Box 1055, Mount Sinai School of Medicine, 1 Gustave Levy Place, New York, NY 10029. Tel:(212) 241-8797 E-mail:mone.zaidi{at}smtplink.mssm.edu.
![]() |
Abstract |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
The multifunctional ADP-ribosyl cyclase, CD38, catalyzes the cyclization of NAD+ to cyclic ADP-ribose (cADPr). The latter gates Ca2+ release through microsomal membrane-resident ryanodine receptors (RyRs). We first cloned and sequenced full-length CD38 cDNA from a rabbit osteoclast cDNA library. The predicted amino acid sequence displayed 59, 59, and 50% similarity, respectively, to the mouse, rat, and human CD38. In situ RT-PCR revealed intense cytoplasmic staining of osteoclasts, confirming CD38 mRNA expression. Both confocal microscopy and Western blotting confirmed the plasma membrane localization of the CD38 protein. The ADP-ribosyl cyclase activity of osteoclastic CD38 was next demonstrated by its ability to cyclize the NAD+ surrogate, NGD+, to its fluorescent derivative cGDP-ribose. We then examined the effects of CD38 on osteoclast function. CD38 activation by an agonist antibody (A10) in the presence of substrate (NAD+) triggered a cytosolic Ca2+ signal. Both ryanodine receptor modulators, ryanodine, and caffeine, markedly attenuated this cytosolic Ca2+ change. Furthermore, the anti-CD38 agonist antibody expectedly inhibited bone resorption in the pit assay and elevated interleukin-6 (IL-6) secretion. IL-6, in turn, enhanced CD38 mRNA expression. Taken together, the results provide compelling evidence for a new role for CD38/ADP-ribosyl cyclase in the control of bone resorption, most likely exerted via cADPr.
Key Words: Ca2+ channel, ryanodine receptor, bone resorption, cADPr, osteoporosis
![]() |
Introduction |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
CD38/ADP-ribosyl cyclase is a key cellular enzyme that catalyses the cyclization of the intermediary metabolite, nicotinamide adenine dinucleotide (NAD+), to the putative second messenger, cyclic ADP-ribose (cADPr)1. The latter activates Ca2+ release from RyR-gated Ca2+ stores (
Apart from being an ADP-ribosyl cyclase, CD38 can function as a NAD+ glycohydrolase and an ADPr hydrolase (
It is now well established that the osteoclast, a cell that is unique in its ability to resorb bone, can monitor changes in its ambient Ca2+ level by means of a Ca2+ sensor (
Ca2+ sensing in the osteoclast is regulated by several systemic and local factors, namely calcitonin, interleukin-6 (IL-6), ambient pH, and membrane potential (
This study examines whether CD38/ADP ribosyl cyclase has a new role in the regulation of osteoclastic bone resorption. We first report the cloning and sequencing of cDNA encoding a novel CD38 homologue. Furthermore, we demonstrate that CD38 mRNA is expressed in the osteoclast; that immunoreactive CD38 is localized to the cell's plasma membrane; that the enzyme displays ADP ribosyl cyclase activity in the NGD+cGDPr assay; that, when activated, CD38 triggers a cytosolic Ca2+ signal through ryanodine receptor activation; and that the CD38-induced Ca2+ signal is associated with resorption inhibition and IL-6 release. We postulate that NAD+ couples an osteoclast's metabolic activity to its resorptive function using CD38 and cADPr as the sensor and signal, respectively.
![]() |
Materials and Methods |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
Osteoclast Cultures
Long bones obtained from neonatal Wistar rats killed by decapitation were curetted into Hepes-buffered Medium 199 containing Hank's salts (GIBCO-BRL) and heat-inactivated fetal bovine serum (FBS, 5% vol/vol; Sigma Chemical Co.) (M199-H). The resulting suspension was dispersed onto devitalized cortical bone slices or 22-mm, 0-grade, glass coverslips (Libro/ICN). Osteoclasts attached to the respective substrate within 15 min (37°C) and contaminating cells were removed by gentle rinsing. Osteoclasts were identified readily by their large size, multinuclearity, complex morphology, densely ruffling edges, and response to calcitonin (
Purified rabbit osteoclasts were prepared by the method of
Isolation and Sequencing of CD38 cDNA Clone from a Rabbit Osteoclast cDNA Library
A rabbit osteoclast cDNA library containing 1 x 1010 independent clones was used for PCR amplification ( cells. 293 bp of pBS-CD38 insert was confirmed through the DNA Sequencing Facility at the University of Pennsylvania.
To obtain the full-length CD38 cDNA, the 293-bp CD38 coding region DNA fragment was used as probe to screen our osteoclast cDNA library (by a method described by Sambrook, 1989). For this, the probe was labeled with -[32P]CTP (3,000 Ci/mmol) (NENTM Life Science Products Inc.) using the Redprime Random Prime Labeling Kit (Amersham Pharmacia Biotech Inc.). Duplicate filters, which covered 1 x 107 independent clones, were then hybridized overnight at 42°C with prehybridization solution (50% formamide, 6x SSC, 5x Denhardt's, 0.5% SDS, 0.1 mg/ml denatured fragmented salmon sperm DNA) to which a labeled probe was added 3 h later. After a high-strigency wash at 68°C for 1 h, the filters were exposed to x-ray film with intensifying screens for 20 h at -70°C. Positive recombinant plaques were purified from phage plate lysates according to the Lambda ZAP II library's instruction manual (Stratagene). The DNA clones were confirmed by PstI-KpnI restriction analysis and direct nucleotide sequencing.
CD38 mRNA Expression in Single Osteoclasts Revealed by In Situ RT-PCR Cytoimaging
We and others have recently applied in situ RT-PCR cytoimaging successfully to study IL-6 and IL-6 receptor expression in osteoblasts, osteoclasts, and bone marrow stromal cells (
Osteoclasts were incubated on glass coverslips (22 mm, 0 grade) in Medium 199 with Earle's salts (6.6 mM Na2CO3, M199-E) for 6 h (37°C, 5% humidified CO2, pH 7.4). In separate experiments, the cells were incubated with either vehicle or IL-6 (10 ng/liter or 10 µg/liter). The cultures were washed with M199-E, fixed with paraformaldehyde (4% vol/vol) in phosphate-buffered saline (PBS) (20 min, 4°C), and washed twice with cold PBS. The fixed cells were treated with 0.2 N-HCl (20 min, 20°C), washed with DEPC-water (Sigma Chemical Co.), and treated with proteinase-K (5 mg/liter in 10 mM Tris-HCl, pH 8, 15 min, 37°C) and cold paraformaldehyde (4% vol/vol, 30 min, 4°C). Before being air-dried, the cells were dehydrated by sequential 1-min immersions in graded aqueous ethanol solutions, 70, 80, 90, and 100% (vol/vol). They were then incubated overnight (37°C) with RNase-free DNase I (1,500 units/ml; Boehringer Mannheim) to remove genomic DNA. The DNase I was finally washed out with DEPC-water and inactivated by heating (90°C, 10 min).
First-strand cDNA was synthesized by incubating cultures with RT mixture (50 µl) comprising 1 mM dNTP, 0.01 M DTT, 400 nM reverse primer (above), DEPC-water, and 14 U/ml Superscript RT II (GIBCO-BRL) (42°C, 60 min). An AmpliCover disc was used to cover each sample. The samples were then treated separately with PCR mixture (50 µl) comprising 0.2 mM dNTP, PCR buffer, 2.5 mM MgCl2, 0.1 U/µl Taq polymerase, 400 nM forward and reverse primers, 10 µM digoxigenin (DIG)-labeled-11-dUTP (Boehringer Mannheim), and DEPC-water. Each sample was then covered gently with an AmpliCover disc ensuring the absence of air bubbles. The GeneAmp In situ PCR System 1000 (Perkin Elmer) was programmed as follows. A 4-min soak at 94°C was followed by 40 cycles of: 94°C for 1 min, 55°C for 2 min, and 72°C for 3 min.
Incorporated DIG-11-dUTP in the PCR product was detected by an alkaline phosphatase (AP)-conjugated anti-DIG antiserum and AP substrates, 4-nitroblue tetrazolium chloride (NBT) and 5-bromo-4-chloro-3-indoyl-phosphate (BCIP) using a DIG Nucleic Acid Detection Kit (Boehringer Mannheim) per manufacturer's protocol. Negative controls, in which primers were omitted, were run in parallel. Messenger RNA expressing cells stained dark purplish brown, while negative controls did not stain.
We then performed an analysis of the staining intensity using a blinded observer. Osteoclasts were scored on a scale from 0 to 4 (no staining to intense staining, see legend to Figure 4). The results from three experiments were plotted as a frequency histogram. This allowed us to determine the proportion of cells that lay in a certain intensity range. A similar analysis has been used by us previously (
|
|
|
|
Antibodies
Dr. F. Malavasi (Torino, Italy) kindly provided the monoclonal anti-CD38 antibody, A10. A10 was raised by immunizing mice with Burkitt's lymphoma Daudi cells (
Immunocytochemistry and Confocal Microscopic Analysis
Osteoclasts were incubated with normal goat serum (in 10 mM PBS, 1:10, pH, 7.4, 15 min) in multiwell dishes and washed with HBSS (GIBCO-BRL). The cells were either incubated without antibody, or with nonimmune mouse IgG, Ab34 (anti-RyR antibody) (all controls), or A10 (anti-CD38 antibody) (in M199-H, 1:100). In the same experiment, CD38-negative fibroblasts were also incubated with the same antibodies. The coverslips were rinsed gently with HBSS, drained, reincubated with goat antimouse FITC (Sigma Chemical Co.; 1:100, in HBSS, 60 min), washed gently, and finally, drained. The number of fluorescent osteoclasts was first determined in a laser confocal scanning microscope, at ex = 495 nm and
em = 525 nm (Leica Inc.). To localize staining to the osteoclast membrane, 1-µm-thick optical sections were obtained in the cell's coronal plane in selected experiments. Finally, trypan blue (1 mM, 961 Da; Sigma Chemical Co.) was applied to exclude membrane damage that could allow antibody access into the cell.
Membrane Isolation and Western Blot Analysis
For isolation of plasma membranes, cells were first scraped and homogenized in TKM solution (50 mM Tris-HCl, pH 7.5, 25 mM KCl and 5 mM MgCl2) supplemented with 0.25 mM sucrose. The homogenate was centrifuged (3,000 g, 10 min), the pellet resuspended in sucrose (70% wt/vol), and then rehomogenized (12 strokes) with a glass/Teflon homogenizer. The sucrose solution was then layered as follows: the homogenate was overlaid with 12 ml of 48% (wt/vol) sucrose, followed by 6 ml of 42% (wt/vol) sucrose. This was then centrifuged at 27,700 rpm for 70 min in a SW-28 swinging bucket rotor. The plasma membrane fraction banding at the interface of 70%/48% sucrose was collected and suspended in 70% (wt/vol) sucrose solution. The entire process was repeated twice to purify the plasma membranes.
SDS-PAGE was performed using 12% separating and 4% stacking polyacrylamide gels using a minigel system (BioRad Laboratories). Plasma membranes prepared from osteoclasts and osteoblasts (30 µg protein) were heated for 5 min at 95°C in Laemelli's sample buffer (2% SDS, 2% ß-mercaptoethanol, 10% vol/vol glycerol and 50 mg/liter bromophenol blue in 0.1 M Tris-HCl buffer, pH 6.8). Electrophoresis was performed at 20 mAmps per gel. The proteins thus resolved were stained with Coomassie Brilliant Blue (Sigma Chemical Co.) or transferred electrophoretically onto OPTITRAN-supported nitrocellulose membrane (Schleicher and Schuell) at 15°C for 1 h at 100 volts. The membranes were blocked with Tween 20 (0.3% vol/vol) in PBS at 20°C and incubated with the anti-CD38 antibody (1:3,000) (Sigma Chemical Co.). After rinsing, the blot was incubated for 1 h with HRP-conjugated antimouse antibody. The blot was developed using Pierce SuperSignal Ultra Chemiluminescence Kit, per manufacturer's instructions.
ADP-Ribosyl Cyclase (NGD+cGDPr) Assay
ADP-ribosyl cyclase activity was measured in osteoclast plasma membranes isolated as above. We measured the cyclization of the NAD+ surrogate, NGD+, to its fluorescent derivative, cGDPr. Plasma membranes (25 µg) were incubated, for 20 min at 37°C, in 20 mM Tris-HCl (pH 7.4) with 100 µM NGD+. The reaction was stopped with 5 µl of 100% (vol/vol) trichloroacetic acid. Fluorescence in the supernatant was measured using a high-sensitivity spectrofluorometer (ex = 300 nm;
em = 410 nm). The amount of cGDPr formed was plotted as mean ± SD in nmol/ml/mg protein. To establish specificity of the assay, we incubated membranes in with anti-CD38 antibody (1:1,000; Sigma Chemical Co.) and NAD+ (400 µM). Mouse IgG5 was used as control.
Measurement of Cytosolic Ca2+ in Single Osteoclasts
Glass coverslips containing freshly isolated osteoclasts were incubated in serum-free medium (30 min, 37°C) with 10 µM fura 2/AM (Molecular Probes), then washed in M199-H and transferred to a Perspex bath positioned on the microspectrofluorometer stage. The latter was previously constructed from an inverted microscope (Diaphot; Nikon) (s of 340 or 380 nm. The emitted fluorescence was deflected through a 400-nm dichroic mirror and subsequently filtered at 510 nm. The signal was converted to 25 ns, 5V transistor-transistor-logic (TTL) pulses in a photomultiplier tube (PM28B; Thorn EMI). The resulting pulses were counted by a dual photon counter (Newcastle Photometrics) and recorded every second to give a ratio of emitted intensities at excitation
s of 340 and 380 nm, F340/F380.
The cytosolic Ca2+ measuring system was calibrated using an established protocol for intracellular calibration (Shankar et al., 1993). In brief, fura 2loaded osteoclasts were bathed in Ca2+-free, EGTA-containing solution containing 130 mM NaCl, 5 mM KCl, 5 mM glucose, 0.8 mM MgCl2, 10 mM Hepes, and 0.1 mM EGTA. 5 µM ionomycin was first applied to obtain the minimum ratio due to lowest cytosolic Ca2+ (Rmin) and the maximum fluorescence intensity at 380 nm (Fmax). 1 mM CaCl2 was then applied with 5 µM ionomycin to obtain values of the maximum ratio due to an elevated cytosolic Ca2+ (Rmax) and the minimum fluorescence intensity at 380 nm (Fmin). The dissociation constant Kd for Ca2+ and fura 2 is 224 nM (20°C, 0.1 M, pH 6.85). The values were substituted into the equation: [Ca2+] = Kd x [(R - Rmin)/(Rmax - R)] x [(Fmax/Fmin)]. Mean changes () in the cytosolic Ca2+ concentration ([Ca2+]) were then calculated by subtracting peak from basal cytosolic [Ca2+]. Statistical comparisons of cytosolic
[Ca2+] were made by Analysis of Variance (ANOVA) with Bonferroni's Correction for Inequality.
Bone Resorption Assay
Bone resorption was measured using the pit assay (
The slices were incubated for 24 h in humidified CO2 (5%) (pH 6.9), after which they were fixed with glutaraldehyde (10% vol/vol) and stained for the presence of tartrate-resistant acid phosphatase (TRAP) using a kit (Kit 386A; Sigma Chemical Co.). The number of osteoclasts with two or more nuclei was determined on each slice using a light microscope (Olympus). The cells were removed by treating the slices with NaOCl (5 min), and the slices rinsed with distilled water followed by acetone, and then air-dried. The slices were stained subsequently with toluidine blue (1% vol/vol, in 1% wt/vol borate, 5 min). The number of resorption pits was determined on each slice by light microscopy. Notably, each experiment was performed with osteoclasts obtained from three animals with five or six bone slices per treatment. The number of pits or osteoclasts per bone slice was expressed as a mean ± SEM. Student's unpaired t test was used to analyze the effect of treatment, which was considered significant at P < 0.05.
Supernatant IL-6 Measurements by ELISA
Osteoclasts on coverslips were bathed in a multiwell dish containing 500 µl M199-E (with 10% FBS vol/vol) for 6 h in the presence of either vehicle or anti-CD38 antibody (1:500) and NAD+ (1 mM). The culture medium was removed and its IL-6 level was measured with an ELISA kit (M6000; R&D). In brief, 96-well plates coated with a polyclonal antimouse IL-6 antiserum were used to accommodate 50 µl of assay diluent (buffered protein) and 50 µl of standard, control, or sample. After incubation (20°C, 2 h), the wells were aspirated, washed repeatedly, and loaded with 100 µl horseradish peroxidaseconjugated antiIL-6 antibody. After a further incubation (20°C, 2 h), 100 µl of substrate solution containing H2O2 and tetramethylbenzidine, was added to each well. Finally, a further incubation (30 min) was followed by the addition of 100 µl of dilute HCl to stop the reaction. The optical density of each sample was measured at 450 nm on a microplate reader (BioRad). IL-6 was estimated from the standard curve in triplicate experiments and represented as mean ± SEM. Differences between control and treatment were assessed by the Student's unpaired t test.
![]() |
Results |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
Isolation and DNA Sequence Analysis of a 2.8-kb Rabbit Osteoclast CD38 cDNA
To obtain full-length CD38 cDNA clones, a rabbit osteoclast cDNA library was screened. A 293-bp CD38 cDNA coding region DNA fragment was initially cloned and used as probe. A single positive cDNA clone was identified after screening 1 x 107 independent phage recombinants; this contained a 2.8-kb EcoRI-XhoI insert in the plasmid pBluescript-SK (termed SL385). The sequence of the full-length SL385 CD38 insert was obtained. Sequence analysis confirmed the presence of the CD38 coding sequence and extended into 3'-untranslated region (Figure 1). The osteoclast CD38 cDNA sequence was 71, 69, and 66% similar to corresponding full-length CD38 cDNA sequences of mouse, rat, and human CD38 (obtained from the GenBank database) (Figure 1). No significant homology was found, however, between the sequence of the insert and any other sequence in the GenBank database. Figure 2 shows the predicted amino acid sequence of the full-length rabbit osteoclastic CD38. There was a 59, 59, and 50% similarity between this sequence and that of mouse, rat, and human CD38 (GenBank), respectively. The relative sequence divergence suggests that the amplified DNA product codes for a yet uncharacterized member of the CD38 family of cyclases.
CD38 mRNA in Single Osteoclasts Demonstrated by In Situ RT-bPCR Cytoimaging
CD38 mRNA expression in isolated single osteoclasts was investigated by in situ RT-PCR cytoimaging using the same primers as used for PCR cloning (above). Figure 3 shows light micrographs of histostained osteoclasts after RT-PCR. Panel i shows an unstained osteoclast (negative controls) in an experiment in which primers were omitted from the reaction mixture. Panels ii and iii show osteoclasts in which the intense bluish-brown staining represents, respectively, mRNA expression for cathepsin K (cell-specific positive control) or GAPDH (housekeeping gene). Panels iv to vi show intense CD38 mRNA histostaining in osteoclasts that were either incubated with vehicle (iv), 10 ng/liter IL-6 (v), or 10 µg/liter IL-6 (vi).
Figure 4 shows a semi-quantitative analysis of staining intensity using a method modified from that reported by
CD38 Localization to the Osteoclast Plasma Membrane
We next examined whether our highly specific anti-CD38 antibody, A10, bound to the surface of intact live osteoclasts. This agonist antibody has previously been shown to bind to, and activate, the CD38 antigen in several systems (Funaro et al., 1990). Figure 5 (BD) shows confocal microscopic images taken at 1-µm intervals in the coronal plane of CD38-positive osteoclasts. Intense, strictly peripheral, immunostaining was visualized distinctly reminiscent of plasma membrane staining. Notably, CD38-negative fibroblasts were found not to stain with the antibody (not shown). Also of note is that every one of the ~20 osteoclasts examined in each different experiment showed positive staining. Furthermore, all cells remained negative for trypan blue, excluding membrane damage that would otherwise permit antibody access into the cytosol.
|
Control experiments were performed by (a) not including the anti-CD38 antibody (not shown); (b) using preimmune mouse IgG instead of the antibody (not shown); (c) using an irrelevant anti-ryanodine receptor antibody, Ab34 (Figure 5 A). That osteoclasts did not stain with any such treatment provided clear evidence for specificity. Note that Ab34 was raised against a cytosolic calmodulin-binding sequence of the RyR, and hence, is known not to stain the surface of nonpermeabilized osteoclasts (
We further confirmed that the CD38 protein was present in isolated osteoclast plasma membranes by Western blotting using a different antagonist anti-CD38 antibody (Sigma Chemical Co.). A ~46 kD band was observed when plasma membranes purified by sucrose gradient centrifugation were electrophoresed and immunoblotted (Figure 6). A further, significantly weaker, band of a smaller molecular weight (~39 kD) was also seen; this may represent a degradation product, but we are unclear of its identity. The latter band was not obvious when post-nuclear membranes from osteoblastic MC3T3-E1 cells were similarly immunoblotted. Note that the purity of the osteoclastic preparations was >99% based on TRAP staining (see Materials and Methods).
|
ADP Ribosyl Cyclase Activity in Osteoclast Plasma Membranes in the NGD+cGDPr Assay
CD38 is not only an ADP-ribosyl cyclase that converts NAD+ to cADPr, but is also an ADP hydrolase converting active cADPr to inactive ADP-ribose. It is difficult to separate the two reactions that proceed simultaneously. We have therefore used an assay that monitors cyclization of NGD+ to cGDPr, a nonhydrolyzable cADPr surrogate. Thus, the rate of cGDPr formation, in the absence of its breakdown, will more accurately reflect the ADP-ribosyl cyclase activity of CD38. Furthermore, cGDPr is a fluorescent compound that can be quantitated by fluorimetry. We found that osteoclast plasma membranes synthesized cGDPr at a rate of 4.3 nmoles/min/mg protein (Figure 7). The anti-CD38 antagonist antibody (Sigma Chemical Co.) inhibited cGDPr formation significantly, thus attributing the observed ADP ribosyl cyclase activity to CD38. Enzyme activity was also inhibited significantly by addition of NAD+ (400 µM), indicating a possible competition between the two nucleotides. Similar results were obtained from postnuclear membranes prepared MC3T3-E1 osteoblasts (not shown).
|
Cytosolic Ca2+ Signals Triggered through CD38 Activation and cADPr Generation
Having established the presence of CD38 in the osteoclast plasma membrane, we next investigated the effects of its activation by the agonist anti-CD38 antibody. Thus, we measured changes in cytosolic [Ca2+] in response to application of NAD+ (substrate) in the presence of the agonist antibody. Expectedly, only in the presence of the antibody (1:500), did 1 mM NAD+ trigger a cytosolic [Ca2+] elevation (Figure 8 A). This result was consistent with an activated CD38/ADP-ribosyl cyclase that catalyses cADPr generation from NAD+. In separate experiments, the anti-CD38 antibody itself, in the absence of NAD+, did not elevate cytosolic [Ca2+], indicating that the substrate, NAD+, was necessary for CD38-induced Ca2+ signaling (not shown). Finally, 1 mM NAD+ failed to trigger a cytosolic Ca2+ signal in the presence of the control anti-RyR antibody, Ab34, further confirming response specificity.
|
At higher, 10 mM, NAD+ concentrations, a marked elevation in cytosolic [Ca2+] was noted even in the absence of the antibody (Figure 8 A). This response was significantly different (P = 0.013) to the control response (1 mM NAD+ alone), but did not differ significantly (P = 0.22) from the response triggered by 1 mM NAD+ with antibody (Figure 8 A).
We further demonstrated CD38-specificity of the NAD+-induced cytosolic Ca2+ response by preincubating osteoclasts with the anti-CD38 antagonist antibody (Sigma Chemical Co.) before application of 10 mM NAD+. The antagonist antibody attenuated the magnitude of the cytosolic Ca2+ response significantly (Figure 8 C).
To determine whether NAD+ triggered the release of Ca2+ from intracellular stores, we carried out experiments with 10 mM NAD+ in the presence or absence of 2 mM EGTA (to chelate extracellular Ca2+ to near-nanomolar levels) or thapsigargin (a microsomal membrane Ca2+-ATPase inhibitor that is known to deplete intracellular Ca2+ stores). The response to 10 mM NAD+ in Ca2+-free, EGTA-containing medium remained unchanged compared with that to 10 mM NAD+ in 1.25 mM Ca2+ (P = 0.335). Furthermore, Figure 8 B shows that when cells were treated with 4 µM thapsigargin, there was a significant attenuation of the cytosolic Ca2+ response to 10 mM NAD+. However, it is notable that thapsigargin did not completely abolish the cytosolic Ca2+ response to NAD+ suggesting that the Ca2+ signal was not completely dependent upon the fullness of intracellular Ca2+ stores. Taken together, the results suggested that NAD+ primarily triggered the release of Ca2+ from intracellular Ca2+ stores, although Ca2+ influx may also play a role.
We next attempted to test the hypothesis that NAD+-induced cADPr generation resulted in the activation of intracellular ryanodine receptors. For this, we examined whether the known cell permeant ryanodine receptor modulators, ryanodine and caffeine, inhibited the response to applied NAD+. Both ryanodine (5 µM) and caffeine (250 µM and 1 mM) significantly inhibited the cytosolic Ca2+ response to NAD+ (P values, see legend to Figure 8). Taken together, the results suggest that RyR-gated Ca2+ stores were being emptied in response to NAD+, implicating, though not proving, a direct role of cADPr as a second messenger. This is consistent with our direct demonstration of cADPr-forming, ADP-ribosyl cyclase activity in the osteoclast plasma membrane as assessed by the NGDcGDPr assay (Figure 7). It should be emphasized that thapsigargin, ryanodine, and caffeine have all been used as tools to understand the mechanism of NAD+-induced Ca2+ signaling, and in view of their other cellular actions would not be expected to reverse the effect of NAD+ on bone resorption and IL-6 release.
Inhibition of Bone Resorption and Enhancement of IL-6 Release by CD38 Activation
We have shown that while a cytosolic Ca2+ change triggers resorption inhibition, it elevates IL-6 synthesis and release (
|
![]() |
Discussion |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
The multifunctional ectoenzyme, CD38, is known to modulate lymphocyte functions as critical as adhesion, proliferation and cytokine production (
CD38 catalyzes the cyclization of NAD+ not only to cADPr (
The observed effect of CD38 activation in inhibiting bone resorption and elevating IL-6 release thus mirrors that of Ca2+. Notably, both agents act by elevating cytosolic Ca2+. Interestingly, however, cADPr-induced Ca2+ release also mediates the effect of CD38 in inducing other cytokines, including IL-6, interferon-, granulocyte-macrophage colony stimulating factor (GM-CSF), and IL-10 (
The Ca2+-like effects of CD38 might also be relevant physiologically in the metabolic control of bone resorption via NAD+. It is noteworthy that the energy requirement of a resorbing osteoclast is high due to its active secretion of acid and enzymes and its intense motile activity. It is therefore possible that large amounts of NAD+ are being generated intracellularly during resorption. Significant amounts of this NAD+ may indeed extrude from the osteoclast. Indeed,
Our evidence for the production of cADPr through NAD+ catalysis by CD38 is twofold. First, we have directly demonstrated that osteoclast plasma membranes that are positive for CD38 immunoreactivity contain ADP-ribosyl cyclase activity. This has been assessed using an assay that allows for the catalytic conversion of the NAD+ surrogate, NGD+, to its nonhydrolyzable and fluorescent derivative, cGDPr. We showed that the observed ADP-ribosyl cyclase activity could be inhibited noncompetitively by an antagonist antibody to CD38, confirming directly, a role for CD38 in cGDPr formation. That NAD+ also significantly inhibited NGD+ catalysis confirmed further that the two molecules most likely shared the same substrate-binding site. cGDPr formation in osteoclast plasma membranes thus appears truly reflective of the ADP-ribosyl cyclase activity of CD38. Second, and in line with the above, we have shown that NAD+ application to osteoclasts triggers cytosolic Ca2+ release mostly from intracellular stores that are sensitive to inhibition by RyR modulators, ryanodine and caffeine. This, albeit indirect, demonstration for a role of RyRs in NAD+-induced Ca2+ release further suggests a second messenger role for the generated cADPr.
Despite our molecular and biochemical demonstration of functionally active CD38/ADP ribosyl cyclase in the osteoclast plasma membrane, it remains unclear how any cADPr synthesized extracellularly could act on intracellular RyRs. Two explanations have been offered in other models (
We have provided evidence that the NAD+-induced Ca2+ signal is made up of two components, Ca2+ release from RyR-gated intracellular stores, and Ca2+ influx possibly through the uniquely positioned plasma membrane RyR-2. The role of ryanodine receptors has been generally confirmed through experiments demonstrating that the cytosolic Ca2+ response to NAD+ is inhibited strongly by both ryanodine and caffeine (Figure 8). However, these experiments have not allowed us to determine whether the respective modulators block the intracellular RyRs, or the surface RyR-2, or both. Nonetheless, we show here that the NAD+-induced cytosolic Ca2+ response is maintained in Ca2+-free, EGTA-containing medium, suggesting its dependence on intracellular Ca2+ release. Our experiments with thapsigargin, a microsomal membrane Ca2+-ATPase inhibitor known to deplete intracellular Ca2+ stores, appear more conclusive. These results show that thapsigargin attenuates, but does not abolish the cytosolic Ca2+ signal, suggesting that there is a component of extracellular Ca2+ influx. This, however, remains to be established.
In conclusion, we have documented a new function for osteoclastic CD38. We believe that its activation at the osteoclast plasma membrane results in cytosolic Ca2+ release from RyR gated intracellular Ca2+ stores via cADPr generation from NAD+. The released Ca2+ then signals a reduction in bone resorption and a paradoxical elevation of IL-6 release. It is therefore possible that the CD38/Ca2+/IL-6 pathway may have a critical role in coupling an osteoclast's metabolic activity with its resorptive function. Our current studies with CD38-/- mice should shed more light on the function of CD38 in osteoclast control (
![]() |
Footnotes |
---|
L. Sun and O.A. Adebanjo contributed equally to this paper.
![]() |
Acknowledgements |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
The authors are grateful to Professor Iain MacIntyre (William Harvey Research Institute, London, UK) for his encouragement and support; Christopher L.-H. Huang (Physiological Laboratory, Cambridge, UK) for helpful discussion; Qinwu Lin (Wistar Institute, Philadelphia, PA) for assistance with confocal microscopy; Jerry Rosenzweig (Geriatrics Department, Veterans Affairs Medical Center, Philadelphia, PA) for assistance in grant management; and Stacey Marshall (University of Pennsylvania, Philadelphia, PA) for illustrations.
M. Zaidi acknowledges the support of the National Institutes of Health (RO1-AG14702-01) and the Department of Veteran's Affairs.
Submitted: 8 October 1998
Revised: 14 July 1999
Accepted: 26 July 1999
1.used in this paper: BCIP, 5-bromo-4-chloro-3-indoyl-phosphate; cADPr, cyclic ADP-ribose; IL-6, interleukin 6; NBT, 4-nitroblue tetrazolium chloride; RyRs, ryanodine receptors; TRAP, tartrate-resistant acid phosphatase
![]() |
References |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|