Normal proliferation and differentiation of Hoxc-8 transgenic chondrocytes in vitro
© Cormier et al; licensee BioMed Central Ltd. 2003
Received: 20 December 2002
Accepted: 24 April 2003
Published: 24 April 2003
Hox genes encode transcription factors that are involved in pattern formation in the skeleton, and recent evidence suggests that they also play a role in the regulation of endochondral ossification. To analyze the role of Hoxc-8 in this process in more detail, we applied in vitro culture systems, using high density cultures of primary chondrocytes from neonatal mouse ribs.
Cultured cells were characterized on the basis of morphology (light microscopy) and production of cartilage-specific extracellular matrix (sulfated proteoglycans and type II Collagen). Hypertrophy was demonstrated by increase in cell size, alkaline phosphatase activity and type X Collagen immunohistochemistry. Proliferation was assessed by BrdU uptake and flow cytometry. Unexpectedly, chondrocytes from Hoxc-8 transgenic mice, which exhibit delayed cartilage maturation in vivo , were able to proliferate and differentiate normally in our culture systems. This was the case even though freshly isolated Hoxc-8 transgenic chondrocytes exhibited significant molecular differences as measured by real-time quantitative PCR.
The results demonstrate that primary rib chondrocytes behave similar to published reports for chondrocytes from other sources, validating in vitro approaches for studies of Hox genes in the regulation of endochondral ossification. Our analysis of cartilage-producing cells from Hoxc-8 transgenic mice provides evidence that the cellular phenotype induced by Hoxc-8 overexpression in vivo is reversible in vitro.
Endochondral ossification is the process by which mesenchymal cells condense at specific sites and differentiate into chondrocytes, forming the cartilage anlagen that are the model for the future bone. The cells in the center of the anlagen, which are initially immature, undergo an ordered differentiation program (also called chondrocyte maturation ): the chondrocytes proliferate, become pre-hypertrophic, and then undergo hypertrophy and matrix calcification. The calcified cartilage is then invaded by blood vessels that bring osteoblasts and osteoclasts, and bone is formed. Each step of cartilage maturation occurs in a precise and tightly regulated manner . Disruptions of this process cause abnormalities in cartilage and bone formation [5, 6]. Endochondral ossification occurs in embryonic skeletal formation, in skeletal growth and fracture healing.
Homeobox genes of the Hox class are required for proper patterning of skeletal elements . The functional role of Hox genes in skeletal growth and development has been clearly demonstrated, but how they control the differentiation of specific tissues is not well understood. Hox genes encode transcription factors that regulate the expression of yet unidentified target genes . In order to identify such target genes and to better understand the role of Hox genes in cartilage differentiation and maturation, we established in vitro culture systems for primary mouse rib chondrocytes.
Previously, we generated transgenic mice that overexpress the homeobox transcription factor Hoxc-8 in the thoracic region, where Hoxc-8 is normally expressed ( and unpublished results). The transgenic mice exhibit profound cartilage defects, predominantly in ribs and vertebral column, and severity of defects depends on transgene dosage. The abnormal cartilage is characterized by an accumulation of proliferating chondrocytes and reduced cartilage maturation. The structural rigidity of rib cartilage is greatly compromised, fatally interfering with pulmonary function, and vertebral cartilage is so weak that the skeleton often disassembles during skeletal preparation . These results suggest that Hoxc-8 continues to regulate skeletal development well beyond pattern formation in a tissue-specific manner, presumably by controlling the progression of cells along the chondrocyte differentiation pathway. We found a similar phenotype upon overexpression of Hoxd-4 in our transgenic system (Kappen, manuscript in preparation), whereas overexpression of the LIM-homeodomain transcription factor Isl-1 did not cause abnormalities in cartilage but other developmental defects [1, 9]. The observation that cartilage is affected by misregulation of Hoxc-8 and Hoxd-4, but not by a divergent homeobox gene, indicates that the capacity to regulate cartilage differentiation is specific to homeobox genes of the Hox subclass. It also suggests that Hox genes could be involved in human chondrodysplasias and other cartilage disorders. We envisioned that well-defined in vitro culture systems would allow us to further characterize the cellular and molecular basis of abnormal chondrocyte differentiation in Hox transgenic mice. Detailed knowledge of regulatory mechanisms in endochondral ossification will be essential for strategies to manipulate chondrocyte proliferation, differentiation and maturation in skeletal growth and development, osteochondrodysplasias and fracture healing.
The in vitro chondrocyte culture systems we utilized here consisted of high-density cultures of primary rib chondrocytes from neonatal mice. The micromass culture system  provides the three-dimensional environment needed for chondrogenesis, cartilage maturation and hypertrophy. The system also allows the investigation of the continuous program of differentiation, maturation and hypertrophy in the same culture. The cellular phenotype in culture was characterized by morphology and extra-cellular matrix (ECM) production. Chondrocyte maturation was assessed on the basis of cell proliferation, cellular hypertrophy, alkaline phosphase activity and expression of Collagen type II and type X. Apoptosis was investigated by TUNEL (terminal deoxynucleotidyl transferase-mediated deoxyuridine triposphate nick end labeling). High density bulk cultures were used to assess the capacity of chondrocytes from Hoxc-8 transgenic mice for cell proliferation and differentiation. Proliferation of chondrocytes in vivo was assayed by BrdU incorporation, and gene expression was analyzed by real-time quantitative PCR.
We previously reported  that Hoxc-8 transgenic mice exhibit profound defects in cartilage, particularly in the rib cage and vertebral column. The cartilage is structurally insufficient and weak, contains fewer hypertrophic chondrocytes, displays much reduced staining for sulfated proteoglycans, and consists predominantly of immature chondrocytes, with a high fraction of proliferating cells. These results point to a role of Hoxc-8 in regulation of cartilage maturation and chondrocyte differentiation. A similar phenotype is found in Hoxd-4 transgenic mice ( and Kappen, manuscript in preparation) indicating that Hox transcription factors regulate chondrocyte development. To examine this function in more detail, we employed a culture system that facilitates chondrocyte maturation and cartilage formation, and closely recapitulates the in vivo situation . The micromass system has been used extensively for studies of cartilage formation from limb mesenchyme [10–13] and also for culture of chondrocytes in high density . Here, we have adapted the system to neonatal mouse rib chondrocytes, to study the role of Hoxc-8 in chondrocyte maturation.
Interestingly, when primary chondrocytes from Hoxc-8 transgenic mice were assayed, they showed the same cell cycle kinetics as chondrocytes from control animals. Essentially similar proportions of cells in S phase were found in all cultures (Figure 7, Panel B). This was regardless of levels of expression of the Hoxc-8 transgene (Figure 7, Panel B) which increases with increasing transgene dosage [1, 23]. These data indicate that, after appropriate time in culture, transgenic chondrocytes were able to proliferate normally, at least over the 24 hours duration of the assay.
The biological corollaries of changes in gene expression profiles are noteworthy in that they may provide evidence on the molecular targets of Hox genes in cartilage, as well as on the consequences of Hox gene overexpression. In Hoxc-8 transgenic chondrocytes, we found increased expression of Collagen II splice form A mRNA . This is consistent with our earlier finding of at least 2-fold increased Collagen II mRNA expression by in situ hybridization and increased numbers of immature chondrocytes in Hoxc-8 transgenic mice . Sox-5, which is normally expressed in proliferating chondrocytes [25, 26], is elevated in Hoxc-8 transgenic cells, again consistent with accumulation of immature chondrocytes. Unexpected was the elevated expression of Collagen X mRNA, a marker for hypertrophic cells. As fewer hypertrophic cells are present in Hoxc-8 transgenics, and cartilage maturation is delayed in Hoxc-8transgenic animals , one would expect to see decreased Collagen X mRNA levels . Yet, the data clearly indicate that mRNA expression is elevated in transgenic rib chondrocytes. This could be either from increased Collagen X mRNA transcription within prehypertrophic and hypertrophic cells or from ectopic activation of Collagen X transcription in proliferating chondrocytes. Whether either of these possibilities would also increase Collagen X expression at the protein level remains to be investigated. Interestingly, Collagen X expression has been shown to be induced by Bmp-2 , which is overexpressed in our transgenic mice. Bmp-2 signaling has a positive effect on chondrocyte proliferation , and can induce Indian hedgehog (Ihh) expression in responsive cells . We find Ihh mRNA elevated in Hoxc-8 transgenic chondrocytes (see Figure 8). Ihh can induce Bmp expression in proliferating cells, further increasing positive effects on chondrocyte proliferation . At the same time, Ihh decreases the rate of progression to hypertrophy [32, 33], again consistent with an accumulation of proliferating cells in our transgenic animals. Whether the elevated Ihh mRNA levels originate from increased expression in cells that make Ihh normally (prehypertrophic and hypertrophic chondrocytes) or from ectopic activation by the Hox transcription factors in proliferating cells, remains to be investigated. Greater numbers of prehypertrophic cells are unlikely to account for elevated expression of prehypertrophic cell markers: histological sections from Hoxc-8 transgenic animals show no increase in prehypertrophic cells , and PTHrP receptor mRNA levels are unchanged in cells from transgenic animals (see Figure 8). These data also suggest that PTHrP signaling [34–36] is only moderately affected by overexpression of Hoxc-8. We found the expression of p107 mRNA and Bmp-4 mRNA to be decreased, which, if reflected in reduced protein levels, would be consistent with the phenotype of delayed cartilage maturation in Hox transgenic animals: As Bmp-4 was shown to have a positive effect on hypertrophy and inhibitory effect on proliferation [37, 38], decreased Bmp-4 expression would be expected to promote chondrocyte proliferation. p107 has been shown to be required for exit from the cell cycle [39, 40], and reduced p107 expression is associated with deregulated proliferation. Also, chondrocytes without p107 expression fail to respond to inhibitory signals from FGFs . The relationship to elevated Fgf receptor 3 mRNA levels in Hoxc-8 transgenic cells, however, remains to be clarified. The same caveat applies to elevated expression in Hoxc-8 transgenic cells of p130, which is also known to be linked to cell cycle exit and FGF response . While the profile of gene expression changes in Hoxc-8 transgenic mice is suggestive of interactions between the various gene products, further studies will be required to mechanistically link the gene expression differences to the maturational delay in the Hoxc-8 transgenic cartilage.
In summary, the gene expression profiles of primary chondrocytes from Hoxc-8 transgenic animals display notable differences in the expression of regulators of chondrocyte maturation in a pattern largely consistent with delayed chondrocyte maturation in vivo. These results now allow us to investigate whether any of these molecules is directly regulated by Hox transcription factors in chondrocytes. It is also remarkable, as apparent from our cell culture results, that cells with obvious molecular differences downstream of Hoxc-8 expression can be modulated to resemble a normal chondrocyte phenotype after a few days in culture.
Our studies of chondrocytes from Hoxc-8 transgenic mice reveal several interesting results: in vivo, chondrocytes remain relatively immature, with few progressing to hypertrophy in Hoxc-8 transgenic mice. Combined with the fact that some, albeit fewer, hypertrophic cells are present, the accumulation of proliferating chondrocytes suggests that Hoxc-8 regulates the rate of progression of chondrocytes to maturity . In line with this interpretation, the in vivo BrdU incorporation assays suggested that cell cycle progression of chondrocytes may be decreased in transgenic animals with higher Hoxc-8 transgene expression levels. If fewer immature cells enter the cell cycle in a given time interval, this is consistent with, and would explain the increased steady-state numbers of chondrocytes upon Hoxc-8 overexpression. This could occur through two different mechanisms: (i) Hoxc-8 actively recruits cells into the chondrocyte lineage and maintains them in the proliferating state; or (ii) Hoxc-8 inhibits a specific step in chondrocyte maturation. In order to distinguish between these possibilities, we sought to employ cell culture assays with well-established parameters for chondrocyte differentiation and maturation. Interestingly, chondrocytes from Hoxc-8 tansgenic animals behaved undistinguishable from control cells under all conditions tested. No differences were found in capacity to differentiate in micromass (see Figure 3), or in high density cultures (not shown), and proliferative indices are comparable (see Figure 7), irrespective of transgene dosage. The latter could be explained by the fact that the FACS analyses were done at the time of greatest proliferation, three days after culture initiation, which may allow transgenic cells to recover to a normal phenotype. However, we did not detect any differences in the first few days of culture by microscopy or histology. Cellular differences must exist at the time the cells are taken from the animal (which would be expected to die as a Hoxc-8 transgenic), and indeed molecular differences exist (see Figure 8). Yet, the cell culture conditions either quickly reverse cellular phenotype or support normal chondrocyte maturation. Alternatively, it is conceivable that the Hoxc-8 transgene could be silenced as cells are isolated from the animal, returning cells to their normal phenotype. There is little evidence to support this possibility as Hoxc-8 is expressed normally in our chondrocyte cultures (data not shown), and the promoter used to drive the transgene contains a cartilage-specific element (Cormier and Kappen, unpublished results) that is active in chondrocytes. Yet, even if transgene expression was reduced in culture, the important implication of our results is that the downstream biological effects of at least 6 days of Hoxc-8 overexpression in vivo are reversible. From these results, we postulate that the cartilage defect in Hoxc-8 transgenic mice is mediated by absence of factors/signals that are present in the culture medium. Serum-free conditions and supplementation with candidate molecules would be one strategy to investigate this further. An interesting, albeit preliminary, finding from our gene expression studies is that chondrocytes from Hoxc-8 transgenic animals display gene expression profiles that are indicative for immature chondrocytes, but not totally identical. This suggests that both Hox transcription factors may, in addition to the delay in chondrocyte maturation, induce specific changes in gene expression. By extending the collection of candidate genes, or screening on microarrays, it may thus be possible to identify specific targets for Hox transcription factors in chondrocytes.
Our results support the conclusion that factors in serum-containing medium provide the environment in which Hoxc-8 transgenic chondrocytes are capable of reverting to a normal cellular phenotype. Thus, Hoxc-8 induced changes in chondrocytes are reversible under certain conditions. This has important implications for the identification of the transcriptional targets of Hox transcription factors. In our system, the biological effects of Hox genes in chondrocytes can be modulated by external factors, and this finding points to the importance of gene-environment interactions as modulators of Hox gene function.
Preparation of mouse rib chondrocytes
The preparation of primary rib chondrocytes from neonatal mice is a modification of the method used by Lefebvre et al. . Briefly, newborn FVB mice were sacrificed, and the ventral regions of rib cages were dissected in sterile conditions to release soft tissues. Rib cages were transferred to phosphate buffered saline (PBS) and washed extensively. Cells were dissociated in 50 ml tubes by enzymatic digestion with 0.25% Collagenase (Worthington Biochemical, Collagenase Type 2 – CLS 2) and 0.25% Trypsin/EDTA (Invitrogen/Gibco BRL) for 1 hour at 37°C, or until the soft tissues were floating in the solution. The solution was aspirated, leaving the rib cages on the bottom of the tube. The ribcages were washed with PBS, and fresh 0.25% Collagenase in PBS was added for 1 hour at 37°C, or until the rib cages were dissociated. The enzymatic reaction was stopped with an equal volume of tissue culture medium containing 10% FCS. The cells were filtered through a 70 μm cell strainer (Becton Dickinson) and pelleted by centrifugation in 50 ml conical tubes (maximum volume 25 ml) at 1200 rpm for 5 minutes. The pellet was washed with PBS, cells were counted, and adjusted for desired cell density.
Primary chondrocyte high density bulk cultures
For analysis of cell cycle parameters, we kept primary chondrocytes in high density bulk cultures, as this allows for recovery of cells for flow cytometry. These cultures undergo chondrocyte maturation with differentiation to hypertrophy and formation of cartilage modules. Briefly, cells were plated on 35 mm dishes coated with 0.1% gelatin at a final concentration of 3 × 105/dish, in DMEM, high glucose, 10% FCS and 25 μg/ml L-ascorbic acid. Removal of cells was done by trypsinization. For Alcian Blue staining, cells were fixed in 70% Ethanol for 30 minutes and then incubated for one hour with the Alcian Blue staining solution, which consisted of 15 mg Alcian Blue 8GX (Sigma) in 30 ml of 95% Ethanol and 20 ml Glacial acetic acid. Cells were rinsed again with 70% Ethanol, and dehydrated through an Ethanol series before coverslipping on the dish.
Primary high density micromass cultures
For micromass cultures , cell density was adjusted to 25 × 106 cells/ml. 103 l of cell suspension was plated in the center of a culture well (24-well plate, Midwest Scientific). The cultures were incubated at 37°C in a humidified incubator with 5% CO2 for 1 1/2 to 2 hours to allow for cell adhesion and attachment. Medium was added very slowly and consisted of a 1:1 mixture of DMEM and F12 (Life Technologies/Gibco BRL) supplemented with 10% fetal calf serum (Hyclone), 5000 U/ml Penicillin, 53 g/ml Streptomycin (Life Technologies/Gibco BRL), 25 μg/ml L-ascorbic acid (Life Technologies/Gibco BRL) and 10 mM β-Glycerophosphate (Sigma). Medium was replaced with fresh medium every other day [11, 13, 42].
Assessment of morphological and histological parameters of micromass cultured cells
During the first 2 or 3 days, micromass cultures were observed directly by phase contrast light microscopy. After that, cultures were harvested, washed in PBS, fixed in 4% Paraformaldehyde for 45 minutes, dehydrated in graded series of Ethanol and paraffin-embedded for subsequent analysis. We used histochemical staining with Hematoxylin and Eosin to ascertain cell morphology; and Alcian Blue at pH 1  to detect cartilage matrix sulfated glucosaminoglycans as described before . The production of Collagen type II was assessed by immunohistochemistry using a monoclonal antibody against mouse type II Collagen (Chemicon), and secondary antibody and colorimetric reaction kit (Histostain Plus, Zymed). Cell proliferation was assessed by BrdU incorporation. Cells were incubated with 3 mM of BrdU (Sigma), harvested after 24 hrs and paraffin-embedded. Cells with BrdU incorporation were detected by immunohistochemistry with a monoclonal antibody against BrdU (BrdU staining kit, Zymed). Cell size was determined by measuring cell diameter microscopically, and mean cell size was calculated. Alkaline phosphatase activity was measured as follows: Cells were rinsed in cold TBS (Tris-buffered Saline), scrapped from the plate, homogenized in 0.05% Triton X-100 in Tris-HCl (pH 7.5) on ice, and the sample was centrifuged at 1200 rpm for 5 minutes at 4°C. Protein concentration in the supernatant was assessed by Micro BCA assay (Pierce Chemicals). Alkaline phosphatase activity in the supernatant was determined spectrophotometrically at 405 nm wavelength as the amount of p-nitrophenol released from the substrate p-nitrophenyl phosphate (ALP10, Sigma). Type X Collagen deposition in extracellular matrix was analyzed by immunohistchemistry using a monoclonal antibody against mouse type X Collagen (Research Diagnostics, Inc.) and the same secondary reagents as described above. Apoptosis was assessed by terminal deoxynucleotidyl transferase-mediated deoxyuridine triphosphate (dUTP) nick end labeling (TUNEL) (In situ Cell Death Detection Kit, POD, Boehringer-Manheim).
The generation of Hoxc-8 transgenic mice and the characterization of their phenotype have been published . Briefly, Hoxc-8 expressing mice are generated in a binary transgenic mouse system  by crossing a transactivator strain (harboring a transgene in which expression of the transcriptional transactivator VP16 is under control of the Hoxc-8 promoter; ) to a transresponder strain (that carries as a transgene the Hoxc-8 cDNA linked to the ICP4 immediate early gene promoter, which is silent in mice in the absence of VP16; [45, 46]). Upon combination of both transgenes, the Hoxc-8 transresponder transgene is activated, and Hoxc-8 becomes overexpressed . This system also allows the generation of transgenic mice with increased gene dosage by superimposition of transgene loci to homozygosity [23, 44]. For the studies reported here, we used the T239 transactivator and the IE-c8-254 transresponder strains. All procedures involving animals were reviewed and approved by the Institutional Animal Care and Use Committee at UNMC.
Hoxd-4 transgenic mice were generated using the same transactivator strain crossed to the IE-d4-70 transresponder strain . Maintenance and genotyping of transgenic mice was done as described before [1, 23]. Unless otherwise noted, cells and samples were obtained from animals hemizygous for both transgenes.
All transgenes were maintained on a homogenous FVB inbred genetic background, and normal FVB mice were used as controls unless mentioned otherwise.
In vivo BrdU incorporation
To assess chondrocyte proliferation in Hoxc-8 transgenic mice, we performed in vivo BrdU labeling experiments. BrdU labeling reagent (Amersham RPN202) in PBS was injected into pregnant females at 0.01 ml/gr body weight. Four hours later, dams were sacrificed, embryos were isolated and fixed in 4% paraformaldehyde overnight at 4°C. They were then dehydrated through an alcohol series and embedded in paraffin for histological sectioning. Sections of 10 μm thickness were rehydrated and incubated for 10 minutes with one part 30% H2O2: 9 parts MeOH and processed in HIER (Biotek Solutions), denaturing and blocking solutions following the manufacturer's protocol. Staining of sections for BrdU incorporation was done using the Zymed BrdU staining kit with Horseradish Peroxidase, and development with DAB for 5 minutes. Counterstaining was done with Hematoxylin for one minute. Sections of vertebral structures were matched between pairs of embryos from the same litter according to anatomical landmarks of other tissues on the same section. Cells in skeletal structures were counted from at least 5 (samples 1,2,7,8) and more than 10 (all other samples) consecutive slides for each animal and cell counting was done independently by two technologists without knowledge of sample genotype. Data were collected from three independent experiments and were averaged to cells/section to normalize for potential growth differences between litters. Exponential trendlines were added by regression analysis as implemented in Microsoft Excel.
Assessment of cell proliferation in vitro by BrdU incorporation and flow cytometry
Primary rib chondrocytes were prepared as described above and 3 × 105 cells/well were placed into culture in 6-well plates. Medium was changed daily. Proliferation was assessed by cell counting, and maturation was ascertained visually as cartilage nodule formation, and histochemically by Alcian Blue staining. Cell cycle kinetics were measured by BrdU incorporation and flow cytometry for DNA content at various time points after initiation of the cultures. Cells that had not been incubated with any reagents or cells that were exposed only to anti-BrdU antibody and Propidium Iodide served as controls. For BrdU incorporation studies, BrdU labeling reagent (Amersham) was diluted 1:1000 in medium to a final concentration of 10 μM BrdU and 1 μM FdU, and sterilized through a 0.22 μm filter. 2 ml of staining solution were added to each well of a 6-well plate, followed by incubation for 0, 6, 12, 18, or 24 hours as indicated. To remove the cells, wells were washed with PBS, and 2 ml Trypsin-EDTA (Gibco/BRL) was added for at least five minutes at 37°C. The reaction was inactivated by an equal volume of serum-containing medium, and after vigorous pipetting, cells were collected into Falcon 2052 (12 × 75 mm, Becton-Dickinson) tubes. Cells were pelleted at 400 g for five minutes without brakes, the supernatant was decanted and the pellet was loosened by vortexing at setting 4. Cells were washed with 1% BSA/PBS and repelleted. During cell resuspension, 1 ml ice-cold 70% Ethanol was added, in which cells were either stored at -20°C for up to three days, or processed after 20 minute fixation by repelleting. Resuspension was done in 1 ml 2 N HCl/0.5% Triton X-100, and samples were incubated for 30 minutes at room temperature with vortexing every five minutes, followed by repelleting. After removal of the supernatant, nuclei were resuspended in 1 ml 0.1 M Na2B4O7 (pH 8.5) for two minutes at room temperature, and washed with 1 ml 0.5% Tween-20/1% BSA/PBS. Then, 20 μl FITC-coupled anti-BrdU antibody (Becton-Dickinson) was added, followed by 30 minute incubation at room temperature in the dark. After another wash with 1 ml 0.5% Tween-20/1% BSA/PBS, nuclei were resuspended in 0.25 ml PBS containing 5 μg/ml Propidium Iodide, filtered through 1.2 ml Costar cluster tubes (Costar #4410), or 6 ml tubes with 35 μm strainer cap (Falcon 2235, Becton-Dickinson) in case of volumes greater than 0.5 ml. Flow cytometry was done on a FACScan (Becton-Dickinson) and results were analyzed using FlowJo software (TreeStar).
Gene expression studies
To measure gene expression quantitatively, RNA was extracted from primary rib chondrocytes as follows: cells were harvested as described above, rinsed in PBS and kept in Trizol at -80°C. Extracts were thawed, homogenized in a PowerGen 125 homogenizer for 1 minute, centrifuged at 2000 rpm for 30 seconds. The supernatant was transferred to fresh tubes, 20% of volume of chloroform was added, and the sample was vortexed for 20 seconds, followed by centrifugation at 12000 rpm for 5 minutes at 4°C. The top layer was removed to fresh tubes for precipitation with 0.5 ml Isopropyl Alcohol, and centrifuged at 12000 rpm for 10 minutes at 4°C. The supernatant was removed and the pellet was washed three times with 75% EtOH. After final removal of supernatant, the pellet was air dried for 1–2 minutes and dissolved in nanopure H2O by gentle pipetting and, where necessary, by incubation at 37°C for 10 minutes. RNA concentration was measured by spectrophotometry. Reverse transcription of RNA was performed using the Superscript II first strand synthesis system for RT-PCR (Gibco BRL), following the supplier's instructions. Purification of cDNA was done using the Qiagen PCR Purification Kit, and cDNA concentration was measured by spectrophotometry. Primers for amplification were designed using Primer Express software (ABI) with the following parameters: TM requirements: min. TM 58°C, max. TM 60°C, optimal TM 59°C; GC content requirements: min. % GC 20, max.% GC 80; length requirements: min. length 9, max length 40, optimal length 20; amplicon requirements: min. TM 0°C, max. TM 85°C, min. length 50, max. length 150. The following primer pairs (Genbank accession numbers and coordinates on the mRNA sequence given in brackets) were used to amplify the specific cDNAs for
Bcl-2 (NM_009741); forward primer: 5'-CGGAGACGAGTTCAACGAAAC-3'(681–701); reverse primer: 5'-TGTAAGATAACCATTTGAGGGTGG-3'(770–747).
Bone Morphogenetic Protein-2 (Bmp-2; NM_007553); forward primer: 5'-CCTCAAGTCCAGCTGCAAGAG-3'(1223–1243); reverse primer: 5'-GGTGCCACGATCCAGTCATT-3'(1300–1281).
Bone Morphogenetic Protein-4 (Bmp-4; D14814); forward primer: 5'-GCACTGCCGCAGCTTCTC-3'(5630–5647); reverse primer: 5'-CACTGACAGAAAACAAGGCATATAATAA-3'(5727–5700).
Collagen II splice form A (NM_001844); forward primer: 5'-AATGGGCAGAGGTATAAAGATAAGGA-3'(24–49); reverse primer: 5'-CATTCCCAGTGTCACACACACA-3'(99–78).
Collagen X (X67348); forward primer: 5'-CAAACGGCCTCTACTCCTCTGA-3'(1937–1958); reverse primer: 5'-CGATGGAATTGGGTGGAAAG-3'(2065–2046).
Dlx 5 (NM_01156); forward primer: 5'-ACGCGCGGAGTTGGC-3'(437–451); reverse primer: 5'-CTTGATCTTGGATCTTTTGTTCTGAA-3'(518–493)
Fibroblast growth factor receptor 3 (Fgfr3; NM_008010); forward primer: 5'-GAGTCTACACCCACCAGAGTGATGT-3'(2200–2224); reverse primer: 5'-AGCCCCCCAGCGTAAAGAT-3'(2271–2253).
Glyceraldehyde 3-phosphate dehydrogenase (GAPDH; Xm_194302) forward primer: 5'-CCAGAACATCATCCCTGCATC-3'(674–694); reverse primer: 5'-GGTAGGAACACGGAAGGCC-3'(794–776)
Hoxc-8 (NM_010466); forward primer: 5'-CAACACTAACAGTAGCGAAGGACAAG-3' (595–620); reverse primer: 5'-CAAGGTCTGATACCGGCTGTAAGT-3' (727–704).
Indian hedgehog (Ihh; U85610); forward primer: 5'-CCCCAACTACAATCCCGACA-3'(543–562); reverse primer: 5'-TCATGAGGCGGTCGGC-3'(607–592).
p107 (U27177); forward primer: 5'-TGGATTATTGAAGTTCTCGATTTGC-3'(1624–1648); reverse primer: 5'-ATGCTGTTCAGATGTTTCACCATG-3'(1736–1713)
Parathyroid Hormone/Parathyroid hormone related peptide Receptor (PTH/PTHrP-R; L28108); forward primer: 5'-GAAAGAATAAAGCAAAAGCGAGACA-3'(232–256); reverse primer: 5'-AGGGAGCTCTGACATCGGG-3'(299–281).
Sox-5 (NM 011444); forward primer: 5'-ATGGTGTGGGCGAAAGATGA-3'(1802–1821); reverse primer: 5'-GGCGGGCCTGCTCCT-3'(1946–1932).
All real-time PCR reactions were performed in triplicate on an ABI Prism 7000 in SYBR Green Master Mix (Applied Biosystems), with denaturation at 94°C for 15 seconds, annealing at 55°C for one minute and extension at 60°C for one minute in a total of 40 cycles. 100 nM of each primer were used and 10 ng of template cDNA. Measurements were done in triplicate for each sample, and for each sample, the cycle number (Ct) was determined at which signal above threshold was detected. The values were averaged and standardized to measurements for GAPDH cDNA in the same sample by subtraction: CtGENE - CtGAPDH = ΔCt. This value for each gene in transgenic samples was then normalized for the value of the same gene in the control sample by a second subtraction: ΔCttransgenic - ΔCtcontrol = ΔΔCt. The value for "fold expression" relative to the control is obtained by the formula f = 2ΔΔCt. The resulting data were expressed as "fold change" relative to the gene expression level in the control which was prepared from an FVB mouse.
SAC performed the in vivo BrdU labeling studies and FACS analyses, MAM did the analyses involving micromass cultures, and CK conceived and supervised the studies, wrote the manuscript and secured funding from the Arthritis Foundation (to C.K.), the Aircast Foundation (to C.K.), NIH-F32AR008545 (to S.C.), NIH-NIAMS RO3-AR44945 (to C.K.), and NIH-NIDCR R21-DE014523-01 (to C.K.). We thank Diane Costanzo, Lauren Greenlee, Jean Kloss, Kristin Smith, Catherine Talmadge, Teresa Tinder and Hope West for technical assistance, M. Anita Jennings for histology, Jill Martin for cell sorting, and Saralyn Fisher for secretarial services. We also are grateful to Drs. Veronica Lefebvre, Benoit de Crombrugghe, H.K. (Tina) Dinh and J. Michael Salbaum for technical advice and discussions.
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