Death Receptor 3 (TNFRSF25) Increases Mineral Apposition by Osteoblasts and Region Specific New Bone Formation in the Axial Skeleton of Male DBA/1 Mice

Collins, Fraser L.; Williams, Jessica O.; Bloom, Anja C.; Stone, Michael D.; Choy, Ernest; Wang, Eddie C. Y.; Williams, Anwen S.

doi:https://doi.org/10.1155/2015/901679

Journal of Immunology Research

On this page

Abstract Introduction Materials and Methods Results Discussion Acknowledgments References Copyright Related Articles

Special Issue

Pathogenesis of Bone Diseases: The Role of Immune System

View this Special Issue

Research Article | Open Access

Volume 2015 | Article ID 901679 | https://doi.org/10.1155/2015/901679

Death Receptor 3 (TNFRSF25) Increases Mineral Apposition by Osteoblasts and Region Specific New Bone Formation in the Axial Skeleton of Male DBA/1 Mice

Fraser L. Collins,¹Jessica O. Williams,¹Anja C. Bloom,¹Michael D. Stone,²Ernest Choy,¹Eddie C. Y. Wang,¹and Anwen S. Williams¹

Academic Editor: Giacomina Brunetti

Received17 Oct 2014

Revised01 Dec 2014

Accepted01 Dec 2014

Published03 May 2015

Abstract

Objectives. Genome wide association studies identified TNFSF member TNF-like protein 1A (TL1A, TNFSF15) as a potential modulator of ankylosing spondylitis (AS). TL1A is the only confirmed TNFSF ligand of death receptor 3 (DR3, TNFRSF25); however, its role in disease pathology is not characterised. We evaluated DR3’s role in controlling osteoblast- (OB-) dependent bone formation in vitro and in vivo. Methods. Osteoprogenitor cells and OB were cultured from male DR3-deficient () and wild-type () DBA/1 mice. DR3 and RANKL expression were tested by flow cytometry. Alkaline phosphatase and mineralization were quantified. Osteopontin, osteoprotegerin, and pro MMP-9 were measured by ELISA. A fluorescent probe (BoneTag) was used to measure in vivo mineralization in 10-month-old mice. Results. DR3 was expressed on osteoprogenitors and OB from mice. Alkaline phosphatase, osteopontin, and mineral apposition were significantly elevated in cultures. Levels of RANKL were comparable whilst osteoprotegerin was significantly increased in cultures. In vivo incorporation of BoneTag was significantly lower in the thoracic vertebrae of 10-month-old mice. Conclusions. These data identify new roles for DR3 in regulating OB-dependent bone mineral apposition. They potentially begin to explain the atypical pattern of new bone formation observed in the axial skeleton of grouped, aging DBA/1 mice.

1. Introduction

In a normal physiological state the process of bone remodeling is accomplished through the coupled activities of the osteoclast (OC) and the osteoblast (OB). The OC is responsible for the degradation of bone while the OB produces the organic matrix and aids in its mineralization [1, 2]. In certain pathological conditions, however, OC and OB activity can become uncoupled leading to an increase or decrease in bone resorption and bone formation. Increased bone formation is observed in the spondyloarthritides; delicate marginal syndesmophytes are common in ankylosing spondylitis (AS) whilst nonmarginal syndesmophytes are frequently observed in reactive arthritis and psoriatic arthritis (PsA) [3–5]. The cause of this excessive focal bone formation by OB is currently not clear. The immune system and increased expression of proinflammatory cytokines such as members of the tumour necrosis factor super family (TNFSF) and their receptors have been shown to be implicated [3]. Our study assesses the impact of the TNF receptor superfamily (TNFRSF) member death receptor 3 (DR3) upon OB-directed mineral apposition with a view to understanding how it modulates bone remodelling in the axial skeleton.

Identification of a link between the DR3/TL1A pathway and the spondyloarthritides was first demonstrated when single-nucleotide polymorphisms (SNPs) located in the direct vicinity of the TNFSF15 gene were shown to be strongly associated with predisposition to spondyloarthropathy [6]. Further evidence for a role of the DR3/TL1A pathway in AS was provided by Konsta et al., who identified that serum levels of TL1A are significantly elevated in AS patients over healthy controls [7]. The mechanism through which the DR3/TL1A pathway potentially drives the pathogenesis of the spondyloarthritides, however, is not clear. Expanded numbers of circulating CD8⁺ CD28⁻ T cells have been identified in AS patients, which correlated with a more severe course of disease [8]. A study by Twohig et al., demonstrated that TL1A signalling on TCR stimulated CD8⁺ T cells resulted in increased proliferation [9]. The indirect effect of DR3/TL1A signalling in CD8⁺ T cells upon the expansion of OBs or mineral apposition by OB, however, has not been resolved. Studies by Bu et al. [10] and Borysenko et al. [11] demonstrated the expression of DR3 on the surface of a human OB cell line and primary human OB. These findings imply that the DR3/TL1A signaling pathway could directly modulate apposition of bone matrix by OB, a notion that has not been investigated previously.

This study is the first to specifically investigate the functional role of DR3 on mineral apposition by OB in vitro and in vivo using male DBA/1 mice lacking the DR3 gene (). The spontaneous development of ankylosing enthesopathy has been reported previously in aging male DBA/1 mice and our study provides the first insight to DR3’s role in controlling new bone formation by OB in the axial skeleton [12]. Here we report that OB-derived DR3 increases expression of the early OB differentiation marker alkaline phosphatase, increases expression of the transcription factors Runx2 and OSX, and regulates mineral apposition. MMP-9 and OPN production by OB were measured as surrogate markers of increased OB activation. OB and OC cross talk is an important factor in bone homeostasis. We measured OB-derived RANKL and OPG production to determine the role of DR3 in regulating OC differentiation by OB. These findings examine potentially important, hitherto unknown, mechanisms whereby DR3 regulates OB-dependent bone homeostasis.

2. Materials and Methods

2.1. Animals

All experiments were undertaken in male DBA/1 DR and DR mice generated in a DR × DR colony. The DBA/1 DR strain was generated through backcrossing C57BL/6 DR mice [13] with DBA/1 wild-type mice for 7 generations. All DBA/1 DR and DR animals were generated in-house. Animals used for in vitro experiments were 8–12 weeks of age. Animals for the in vivo BoneTag experiments were 10 months of age. Animals were housed in filter top cages at a constant temperature and humidity on a 12-hour light/dark cycle. Food and water were available ad libitum. All procedures were approved by the Local Research Ethics Committee and performed in strict accordance with Home Office approved license PPL 30/2361.

2.2. OPC and OB Cell Culture

To obtain osteoprogenitors (OPCs) bone marrow was isolated from the femora of DR () and DR () DBA/1 mice and cultured in αMEM supplemented with 20% foetal calf serum, 50 μg/mL Penicillin-Streptomycin (control medium) and 5% CO₂ at 37°C. At confluence OPCs were detached from the culture vessel by scraping and were replated in a 12-well plate at a density of 4 × 10⁴ cells/well in control medium. Osteoblasts were subsequently differentiated from OPCs by addition of αMEM supplemented with 10% foetal calf serum, 50 μg/mL Penicillin-Streptomycin, 10 mM β-glycerophosphate, 50 μg/mL ascorbic acid, and 10 nM dexamethasone (mineralisation medium). Osteoblasts were maintained for up to 26 days (5% CO₂ at 37°C) with medium changes every 3-4 days.

2.3. Cellular Staining and Flow Cytometry

OPCs (DR, DR) and OB (DR, DR) were cultured for 15 days using the method described above. Cells were removed from the culture vessel and incubated with Fc block (BD Pharmingen, CA, USA) for 15 min followed by a 30 min block with 2% normal goat serum. Cells were stained with either polyclonal α-mouse DR3-biotin (BAF 2437; R&D Systems, MN, USA) followed by SA-APC (Molecular Probes, OR, USA) or PE-conjugated α-mouse RANKL mAb (IK22/5; Santa Cruz Biotechnology Inc., TX, USA). Data were acquired on a BD Accuri C6 flow cytometer and analysed with CFlow software (BD Biosciences).

2.4. TL1A RT-PCR

RNA was extracted from OPCs and mineralising OB (DR, DR) using RNeasy (QIAGEN) following manufacturer’s instructions and converted to cDNA using SuperScript II Reverse Transcriptase (Life Technologies). RT-PCR was performed according to standard Life Technologies protocols. PCR primers were as follows: TL1A, forward 5′-CAG CAG AAG GAT GGC AGA-3′ and reverse 5′-CTC TGG CCT GTG TCT ACA-3′, giving a 91-bp product; and β-actin, forward 5′-CGG CCA GGT CAT CAC TAT TG-3′ and reverse 5′-CTC AGT AAC CCG CCT AG-3′, giving a 450-bp product. The PCR comprised 33 cycles with an annealing temperature of 59°C. The PCR products were size fractionated by agarose gel electrophoresis and analysed using a UVP BioDoc It imaging system (Cambridge, UK).

2.5. Quantitative PCR

RNA was extracted from OPCs and OB and converted to cDNA as described above (DR, DR ). Quantitative PCR was performed using the iCycler iQ system (Bio-Rad) with RT2 Real Time SYBR green PCR master mix (SA Biosciences) following the recommended protocol for SYBR green (Bio-Rad). Assays were run in duplicate. mRNA levels were determined using the comparative C_t method and normalized to β-actin mRNA levels. Primers used for quantitative PCR were as follows: RUNX2, forward 5′-CCCTGAACTCTGCACCAAGT-3′ and reverse 5′-TGGCTCAGATAGGAGGGGTA-3′; OSX, forward 5′-TCTCCATCTGCCTGACTCCT-3′ and reverse 5′-CAGGGGACTGGAGCCATAGT-3′; β-actin as above.

2.6. Alkaline Phosphatase and Mineralisation Staining

Alkaline phosphatase (ALP) activity was determined in OB cultures (DR, DR) using SigmaFast BCIP/NBT stain (Sigma). The mineralized matrix was stained for calcium deposition by Alizarin-red staining. Briefly, at time points indicated in results, cultures were fixed with a 4% formaldehyde/PBS solution for 15 min. Cultures were then incubated with either SigmaFast BCIP/NBT solution or Alizarin-red (1% solution in water) for 30 minutes. Cultures stained for mineral apposition were washed with 50% methanol to remove nonspecific background. Plates were air-dried and scanned and the percentage of the well was covered by ALP positive cells or mineral calculated with Image J (NIH).

2.7. Measurement of Soluble Mediators in Cell Culture Supernatant

Expression of soluble mediators in cell culture supernatants was analysed by ELISA using mouse osteoprotegerin (OPG), pro MMP-9, receptor activator of nuclear factor kappa-B ligand (RANKL) and osteopontin (OPN) DuoSet kits (all R&D Systems).

2.8. In Vivo Imaging

DBA/1 male mice were housed together as previously described [12]. Animals at 10 months (DR, DR) of age were subjected to either an intraperitoneal injection with IRDye 680 BoneTag optical probe (0.08 nmol/g) or equal volume of PBS as control. After 24 hours animals were sacrificed by CO₂ asphyxiation. Images were taken using the Xenogen IVIS 200 (excitation wavelength 676 nm, emission wavelength 698 nm, f-stop 1) and rectangular regions of interest of fixed dimensions were selected at the thoracic spine, knee, and tail. Total efficiency of the marker was analyzed using the Live Image software, version 2.50.2 (Caliper). The efficiency values obtained from the PBS control animals were subtracted from the values obtained with BoneTag, to account for background autofluorescence.

2.9. Statistical Analysis

Data are expressed as mean ± SEM and statistical analysis performed using the Mann-Whitney test for nonparametric data, unpaired -test for parametric data, or 2-way analysis of variance (ANOVA) using GraphPad Prism software (GraphPad, San Diego, CA, USA). values of ≤0.05 were considered significant and values of ≤0.01 were considered highly significant.

3. Results

3.1. Expression of DR3 and TL1A by OPCs and OB

Expression of DR3 on the human MG63 osteosarcoma cell line has previously been demonstrated by Borysenko et al. [11]. Here we investigated DR3 expression on primary, murine OPCs and OB using flow cytometry. The signal from the surface of DR OPCs was -fold higher than the isotype control (Figure 1(a)) and was significantly higher than from DR OPCs (). Levels of DR3 signal were reduced on DR mineralising OB (-fold increase) compared to the OPCs. RT-PCR analysis of DR- and DR-derived OPCs and OB showed constitutive expression of TL1A mRNA across a 15 day time course (Figure 1(b)).

(a)

(b)

(c)

Figure 1

Expression of DR3 by murine OPCs and OBs. (a) DR () and DR () OPCs and OB (DR , DR ) were analysed for DR3 signal by flow cytometry. DR3 signal was observed on DR OPCs and OBs. A small subpopulation of DR OPCs displayed higher levels of DR3 signal (shaded area = isotype control, black outline = DR3 antibody). (b) RNA was extracted from DR and DR OPCs and OB and tested for TL1A mRNA by RT-PCR. A 91 bp band corresponding to TL1A mRNA was detected at all time-points demonstrating constitutive expression of TL1A mRNA by DR and DR OPCs and OB. (c) Samples (DR , DR ) were tested by qPCR at time points indicated to determine whether DR3 signalling modulates (i) Runx2 or (ii) OSX gene expression. Increased expression of Runx2 was detected at day 7 and day 14 while increased OSX expression was only detected at day 14 in the DR compared to the DR.

3.2. DR3/TL1A Signalling Promotes RUNX2 and OSX Expression

To identify whether DR3 signalling in OPCs and OB modulates Runx2 and OSX expression qPCR was performed on differentiating OB across a 14-day time course (Figure 1(c)). No difference in RUNX2 and OSX levels was detected between the DR and DR cultures after the first 3 days of differentiation. At day 7 an increase in Runx2 gene expression was observed in the DR cultures. At day 14 both Runx2 and OSX expression levels were elevated in the DR cultures compared to the DR cultures.

3.3. Effect of DR3 on OB Differentiation, OPN and Pro MMP-9 Expression and Mineral Apposition

To assess the effect of DR3 on OB differentiation and mineral apposition, mineralization assays were performed and expression of the early OB differentiation marker ALP was studied. At the earliest time point assessed (day 17), the percentage area of the wells demonstrating ALP-positive cells was elevated in the DR (%) versus DR (%) cultures. These levels did not vary significantly across the 26-day time course, translating into significantly increased levels of ALP staining in DR cultures (; Figure 2(a)).

(a)

(b)

(c)

(d)

Figure 2

Expression of ALP, OPN, pro MMP-9, and mineral apposition in DR and DR osteoblast cultures. (a) DR () and DR () derived OB were cultured and the percentage of well area covered by ALP⁺ cells was calculated. ALP staining was significantly higher in the DR compared to the DR cultures across the 26-day time course (). Supernatants from OB cultures were tested for soluble levels of (b) OPN and (c) pro MMP-9. Across the time course significantly increased levels of OPN were detected in DR versus DR cultures (). (d) Levels of mineral apposition in the cultures were tested by alizarin-red staining. Significantly increased levels of mineralization were observed in the DR cultures at days 23 and 26 () compared to the DR. This translated into a significant increase in the level of mineral apposition across the 26-day time course ().

To see whether the increase in DR ALP expression was accompanied by an increase in OB activation markers, levels of the Ca²⁺ binding osteoid protein (OPN) and a regulator of bone matrix maturation (pro MMP-9) were measured in culture supernatants [14, 15]. Levels of OPN were significantly elevated in DR cultures compared to DR cultures over the 26-day time course (; Figure 2(b)). Levels of OPN peaked at day 17 in the DR ( ng/mL) and at day 23 in the DR cultures ( ng/mL). Levels of pro MMP-9 were initially higher at day 3 in the DR cultures versus DR ( ng/mL versus ng/mL; ). DR pro MMP-9 levels peaked at day 7 ( ng/mL) and decreased over the duration of the time course to ng/mL. In contrast, expression of pro MMP-9 in the DR cultures increased over the culture period and peaked at day 20 ( ng/mL; Figure 2(c)).

To identify whether the increase in DR OB differentiation and OPN expression correlated with an effect on mineral apposition, levels of mineralization in the cultures were evaluated. At day 17 comparable levels of mineralization were observed between the DR (%) and DR (%) cultures. Mineral apposition was significantly increased in the DR cultures at day 23 (%; ) and day 26 (%; ) when compared to DR cultures (% and %, resp.). This resulted in significantly increased levels of mineral apposition across the time course in the DR cultures (; Figure 2(d)). Having demonstrated that DR3 affects OB differentiation and mineral apposition, in vitro, we investigated whether it could have a potential effect on OB control of osteoclast formation.

3.4. Effect of DR3 on OB-Derived RANKL and OPG

To investigate whether DR3 had a role in regulating OB control of OC formation, levels of OB-derived RANKL and OPG were studied. OPC and OB cell surface RANKL expression were comparable between DR and DR cells (Figure 3(a)). No soluble RANKL was detected in any culture supernatants (data not shown). In contrast, significantly increased levels of OPG were detected across the 26-day time course in DR compared to DR cultures (; Figure 3(b)). Levels of OPG peaked at day 14 ( ng/mL) in DR cultures, while in DR cultures OPG levels reached a peak of ng/mL on day 17.

(a)

(b)

Figure 3

Effect of DR3 on OB-derived RANKL and OPG. (a) Cell surface expression of RANKL was analyzed on DR- and DR-derived OPCs and OB by flow cytometry. Both DR and DR OPCs displayed a 3-fold increase in RANKL signal over isotype control. RANKL signal increased to 5-fold over isotype in DR and DR OB. (b) Levels of soluble OPG were measured in culture supernatants by ELISA (DR , DR ). Expression of OPG was significantly elevated in the DR compared to DR OB cultures over the 26-day time course ().

3.5. Assessing the Impact of DR3 on Bone Formation In Vivo

In vitro DR3 has been shown to regulate OB differentiation and mineral apposition while promoting expression of the antiosteoclastogenic cytokine OPG. To identify what effect this would have on in vivo bone formation male DBA/1 mice were aged for 10 months as a spontaneous model of ankylosing enthesopathy [12]. Bone formation over a 24-hour period was measured at three sites (knee, tail, and thoracic vertebra) via the incorporation of the fluorescent probe BoneTag. Significantly increased fluorescence efficiency values were observed in the DR thoracic spine (; ) compared to the DR thoracic spine (; Figure 4(c)), suggesting DR mice exhibit some resistance to the long-term development of spontaneous ankylosing enthesopathy observed in DBA/1 strain wild-type animals.

(a)

(b)

(c)

4. Discussion

Spondyloarthritides such as AS and PsA are characterized by the formation of syndesmophytes [3–5]. Mechanisms that control this increased aberrant bone apposition are not clear. This study provides the first direct evidence of DR3’s involvement in OB-dependent new bone formation in vitro and in vivo. We demonstrate (using DR mice) that DR3 has an important role in the differentiation of OB and subsequent mineralization of the organic matrix by OB. We also reveal a novel pathway whereby DR3 increases OPG production by OB thereby potentially decreasing OC differentiation. In vivo, we show that gene deletion of DR3 protects the axial skeleton against excessive bone formation, a bone phenotype previously observed in aging DBA/1 male mice [12].

In the current study we reveal that DR3 is expressed on the cell surface of primary murine OPCs and OBs. DR3 expression on mouse OPC was shown to be comparable to that reported on the human OB MG63 cell line [11]. Cell surface expression of DR3 was reduced on mineralizing OB suggesting that DR3 may be temporally regulated during OB differentiation. In addition to DR3, the current study identified for the first the time expression of TL1A mRNA by primary OPCs and OB. These data suggest a potential autocrine role for the DR3/TL1A pathway in modulating OB differentiation and mineral apposition.

The notion that DR3 signalling has a role in OB differentiation was supported by the mineralization assay results. Levels of ALP expression and mineral apposition were significantly increased in the DR cultures. This could be explained by DR3 signalling increasing either OB differentiation or proliferation, as has been described for effector T cells [16–18]. Total OB cell numbers at experiment end-point were, however, comparable between the DR and DR cultures (data not shown), suggesting that the increase in ALP expressing cells was due to DR3 promoting differentiation. This result is at odds with data described by Borysenko et al. [11], who demonstrated that cross-linking of DR3 with an antibody on MG63 cells induced apoptosis and inhibited differentiation. However, Borysenko and colleagues were unable to reproduce their results with TL1A or in primary human OB, suggesting that activation following receptor cross-linking may differ from actions of the natural ligand. Further support for DR3 having a role in the regulation of OB differentiation is provided by the analysis of Runx2 and OSX gene expression. Runx2 and OSX are critical transcription factors involved in OB differentiation, the absence of which results in the maturational arrest of the OB [19–21]. In the present study both Runx2 and OSX were elevated in the DR, but not DR, cultures at later time points. These data suggest a possible mechanism through which OB-dependent DR3 signalling potentially modulates OB differentiation.

The DR3-dependent increase in OB differentiation in the DR was associated with increasing mineral apposition in the cultures. This elevation in mineral apposition corresponded with a significant increase in OPN expression in the DR cultures. OPN is suggested to play a role in osteogenesis by attachment of the OB to the organic matrix and to regulate crystal size during mineralization [14, 22]. Interestingly OPN is in part transcriptionally regulated by Runx2 [22, 23] suggesting that in OBs, DR3 modulates OPN expression indirectly via this transcription factor. Before the OB can commence with the formation of newly mineralized bone the organic matrix must first undergo a maturation process. In a study by Filanti et al. [15] members of the matrix metalloproteinase (MMP) family, including MMP-2, -9, and -14, were increased in OB cultures at the time of nodule formation suggesting that they play a significant role in this matrix maturation process. Previous studies have demonstrated that DR3 signalling has a role in MMP-9 production; the THP-1 cell line has been shown to increase MMP-9 expression following treatment with TL1A [24, 25]. In addition, a study by Wang et al. [26] described significantly lower levels of MMP-9 in the joints of DR mice with antigen induced arthritis compared to their DR counterparts during the early stages of disease. In the present study we sought to determine whether OB-dependent DR3 signalling affected osteoblastic MMP-9 expression, which would potentially modulate OB mineral apposition. A difference in the MMP-9 expression pattern was observed between the DR and DR cultures; with higher levels of pro MMP-9 observed at the early time points in the DR cultures. This early expression of MMP-9 shows similarity to the phenotype described by Wang et al. [26] and taken together the results suggest that DR3 signalling has a central role in controlling levels of MMP-9. Unpublished work from our laboratory also suggests that the DR3 pathway may have a key role in the activation of MMP-9 from the pro form.

In addition to an OB specific effect, we have shown in vitro that OB DR3-dependent signalling results in significantly elevated expression of the soluble RANKL inhibitor OPG. This data suggests that OB DR3 signalling has the potential to in-directly modulate OC formation; where the increased OB-derived OPG inhibits OC formation and subsequently bone resorption [27]. This is in contrast to the direct contribution of DR3 signalling on osteoclastogenesis during inflammatory arthritis where DR3 has been revealed to enhance OC formation [28]. Interestingly, significantly increased levels of OPG have been detected in the serum from AS patients and are linked to poor physical mobility [29].

To investigate whether DR3 regulation of OB differentiation and mineral apposition could contribute towards the increased bone formation associated with the spondyloarthritides, we examined the effect of DR3 on in vivo bone formation in the spontaneous ankylosing enthesopathy model [12]. The results from the 10-month-old mice are consistent with the hypothesis that OB-dependent DR3 signalling has a significant role in regulating the atypical bone formation observed in the axial skeleton of mice with spontaneous ankylosing enthesopathy. The increased bone formation observed in the thoracic spine of DBA/1 DR mice is analogous to the pattern of marginal/nonmarginal syndesmophyte formation observed in the spine of PsA and AS patients [30, 31]; thus this observation could have important implications in the understanding of the pathogenesis of these diseases.

The results from the present study provide the first evidence for a functional role for DR3 signalling in new bone formation. We have shown that cell surface DR3 is temporally expressed by OPCs and OB while TL1A mRNA is constitutively expressed and that an autocrine signalling loop may promote Runx2 and OSX expression, consequently modulating OB differentiation and mineral apposition. OB-dependent DR3 signalling increased levels of the soluble inhibitor OPG and could, therefore, indirectly regulate OC formation and bone resorption. Finally, in vivo, the absence of DR3 leads to differences in bone formation compared to wild-type DBA/1 mice, which in 10-month-old animals suggest resistance to the development of spontaneous ankylosing enthesopathy that has been previously described in this strain [12]. These data, taken with the study by Konsta et al. [7], suggest that OB-dependent DR3 signalling could be an important contributory factor in the atypical bone pathology associated with diseases such as PsA and AS.

Conflict of Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.

Authors’ Contribution

Eddie C. Y. Wang and Anwen S. Williams contributed equally to this work and are cosenior authors.

Acknowledgments

Fraser L. Collins and this work were funded by an Arthritis Research UK PhD studentship (Grant Code: 18598) awarded to Anwen S. Williams, Eddie C. Y. Wang, and Michael D. Stone. Eddie C. Y. Wang was additionally funded by MRC Project Grant G0901119. Funding for open access was kindly provided by Cardiff University.

References

G. Karsenty, H. M. Kronenberg, and C. Settembre, “Genetic control of bone formation,” Annual Review of Cell and Developmental Biology, vol. 25, pp. 629–648, 2009.
View at: Google Scholar
S. L. Teitelbaum, “Osteoclasts: what do they do and how do they do it?” The American Journal of Pathology, vol. 170, no. 2, pp. 427–435, 2007, http://www.ncbi.nlm.nih.gov/pmc/articles/PMC1851862/?tool=pmcentrez.
View at: Publisher Site | Google Scholar
M. A. Khan, “Update on spondyloarthropathies,” Annals of Internal Medicine, vol. 136, no. 12, pp. 896–907, 2002.
View at: Google Scholar
E. Dakwar, J. Reddy, F. L. Vale, and J. S. Uribe, “A review of the pathogenesis of ankylosing spondylitis,” Neurosurgical Focus, vol. 24, no. 1, p. E2, 2008.
View at: Publisher Site | Google Scholar
P. Ory, “Radiography in the assessment of musculoskeletal conditions,” Best Practice & Research Clinical Rheumatology, vol. 17, no. 3, pp. 495–512, 2003.
View at: Publisher Site | Google Scholar
E. Zinovieva, C. Bourgain, A. Kadi et al., “Comprehensive linkage and association analyses identify haplotype, near to the TNFSF15 gene, significantly associated with spondyloarthritis,” PLoS Genetics, vol. 5, no. 6, Article ID e1000528, 2009.
View at: Publisher Site | Google Scholar
M. Konsta, G. Bamias, M. G. Tektonidou, P. Christopoulos, A. Iliopoulos, and P. P. Sfikakis, “Increased levels of soluble TNF-like cytokine 1A in ankylosing spondylitis,” Rheumatology, vol. 52, no. 3, pp. 448–451, 2013.
View at: Publisher Site | Google Scholar
M. Schirmer, C. Goldberger, R. Würzner et al., “Circulating cytotoxic CD8⁺ CD28⁻ T cells in ankylosing spondylitis,” Arthritis Research, vol. 4, no. 1, pp. 71–76, 2002.
View at: Google Scholar
J. P. Twohig, M. Marsden, and S. M. Cuff, “The death receptor 3/TL1A pathway is essential for efficient development of antiviral CD4⁺ and CD8⁺ T-cell immunity,” The FASEB Journal, vol. 26, no. 8, pp. 3575–3586, 2012, http://www.pubmedcentral.nih.gov/articlerender.fcgi?artid=3460213&tool=pmcentrez&rendertype=abstract.
View at: Publisher Site | Google Scholar
R. Bu, C. W. Borysenko, Y. Li, L. Cao, A. Sabokbar, and H. C. Blair, “Expression and function of TNF-family proteins and receptors in human osteoblasts,” Bone, vol. 33, no. 5, pp. 760–770, 2003.
View at: Publisher Site | Google Scholar
C. W. Borysenko, V. García-Palacios, R. D. Griswold et al., “Death receptor-3 mediates apoptosis in human osteoblasts under narrowly regulated conditions,” Journal of Cellular Physiology, vol. 209, no. 3, pp. 1021–1028, 2006.
View at: Google Scholar
R. J. U. Lories, P. Matthys, K. De Vlam, I. Derese, and F. P. Luyten, “Ankylosing enthesitis, dactylitis, and onychoperiostitis in male DBA/1 mice: a model of psoriatic arthritis,” Annals of the Rheumatic Diseases, vol. 63, no. 5, pp. 595–598, 2004.
View at: Publisher Site | Google Scholar
E. C. Wang, A. Thern, A. Denzel, J. Kitson, S. N. Farrow, and M. J. Owen, “DR3 regulates negative selection during thymocyte development,” Molecular and Cellular Biology, vol. 21, no. 10, pp. 3451–3461, 2001.
View at: Google Scholar
P. Robey and A. Boskey, “Extracellular matrix and biomineralisation of bone,” in Primer on the Metabolic Bone Diseases and Disorders of Mineral Metabolism, pp. 12–19, 2006.
View at: Google Scholar
C. Filanti, G. R. Dickson, D. Di Martino et al., “The expression of metalloproteinase-2, -9, and -14 and of tissue inhibitors-1 and-2 is developmentally modulated during osteogenesis in vitro, the mature osteoblastic phenotype expressing metalloproteinase-14,” Journal of Bone and Mineral Research, vol. 15, no. 11, pp. 2154–2168, 2000.
View at: Publisher Site | Google Scholar
F. Meylan, T. S. Davidson, E. Kahle, M. Kinder, K. Acharya, and D. Jankovic, “The TNF-family receptor DR3 is essential for diverse T cell-mediated inflammatory diseases,” Immunity, vol. 29, no. 1, pp. 79–89, 2008.
View at: Publisher Site | Google Scholar
G. Bamias, M. Mishina, M. Nyce, W. G. Ross, G. Kollias, and J. Rivera-Nieves, “Role of TL1A and its receptor DR3 in two models of chronic murine ileitis,” Proceedings of the National Academy of Sciences of the United States of America, vol. 103, no. 22, pp. 8441–8446, 2006.
View at: Google Scholar
T. J. Slebioda, T. F. Rowley, J. R. Ferdinand et al., “Triggering of TNFRSF25 promotes CD8⁺ T-cell responses and anti-tumor immunity,” European Journal of Immunology, vol. 41, no. 9, pp. 2606–2611, 2011.
View at: Publisher Site | Google Scholar
T. Komori, H. Yagi, S. Nomura et al., “Targeted disruption of Cbfa1 results in a complete lack of bone formation owing to maturational arrest of osteoblasts,” Cell, vol. 89, no. 5, pp. 755–764, 1997.
View at: Publisher Site | Google Scholar
P. Ducy, R. Zhang, V. Geoffroy, A. L. Ridall, and G. Karsenty, “Osf2/Cbfa1: a transcriptional activator of osteoblast differentiation,” Cell, vol. 89, no. 5, pp. 747–754, 1997.
View at: Publisher Site | Google Scholar
K. Nakashima, X. Zhou, G. Kunkel, Z. Zhang, J. M. Deng, and R. R. Behringer, “The novel zinc finger-containing transcription factor osterix is required for osteoblast differentiation and bone formation,” Cell, vol. 108, no. 1, pp. 17–29, 2002.
View at: Publisher Site | Google Scholar
Q. Shen and S. Christakos, “The vitamin D receptor, Runx2, and the Notch signaling pathway cooperate in the transcriptional regulation of osteopontin,” The Journal of Biological Chemistry, vol. 280, no. 49, pp. 40589–40598, 2005.
View at: Google Scholar
C. K. Inman and P. Shore, “The osteoblast transcription factor Runx2 is expressed in mammary epithelial cells and mediates osteopontin expression,” The Journal of Biological Chemistry, vol. 278, no. 49, pp. 48684–48689, 2003, http://www.ncbi.nlm.nih.gov/pubmed/14506237.
View at: Publisher Site | Google Scholar
Y.-J. Kang, W.-J. Kim, H.-U. Bae et al., “Involvement of TL1A and DR3 in induction of pro-inflammatory cytokines and matrix metalloproteinase-9 in atherogenesis,” Cytokine, vol. 29, no. 5, pp. 229–235, 2005.
View at: Google Scholar
S. H. Kim, W. H. Lee, B. S. Kwon, G. T. Oh, Y. H. Choi, and J. E. Park, “Tumor necrosis factor receptor superfamily 12 may destabilize atherosclerotic plaques by inducing matrix metalloproteinases,” Japanese Circulation Journal, vol. 65, no. 2, pp. 136–138, 2001.
View at: Publisher Site | Google Scholar
E. C. Y. Wang, Z. Newton, O. A. Hayward et al., “Regulation of early cartilage destruction in inflammatory arthritis by death receptor 3,” Arthritis & Rheumatology, vol. 66, no. 10, pp. 2762–2772, 2014.
View at: Publisher Site | Google Scholar
S. L. Teitelbaum, “Bone resorption by osteoclasts,” Science, vol. 289, no. 5484, pp. 1504–1508, 2000.
View at: Google Scholar
M. J. Bull, A. S. Williams, Z. Mecklenburgh et al., “The death receptor 3-TNF-like protein 1A pathway drives adverse bone pathology in inflammatory arthritis,” The Journal of Experimental Medicine, vol. 205, no. 11, pp. 2457–2464, 2008.
View at: Publisher Site | Google Scholar
C.-H. Chen, H.-A. Chen, H.-T. Liao, C.-H. Liu, C.-Y. Tsai, and C.-T. Chou, “Soluble receptor activator of nuclear factor-kappaB ligand (RANKL) and osteoprotegerin in ankylosing spondylitis: OPG is associated with poor physical mobility and reflects systemic inflammation,” Clinical Rheumatology, vol. 29, no. 10, pp. 1155–1161, 2010.
View at: Publisher Site | Google Scholar
F. Cantini, L. Niccoli, C. Nannini, O. Kaloudi, M. Bertoni, and E. Cassarà, “Psoriatic arthritis: a systematic review,” International Journal of the Rheumatic Diseases, vol. 13, no. 4, pp. 300–317, 2010.
View at: Publisher Site | Google Scholar
I. van Echteld, A. Cieza, A. Boonen et al., “Identification of the most common problems by patients with ankylosing spondylitis using the International Classification of Functioning, Disability and Health,” Journal of Rheumatology, vol. 33, no. 12, pp. 2475–2483, 2006.
View at: Google Scholar

Copyright

Copyright © 2015 Fraser L. Collins et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

PDF Download Citation

Download other formats

Order printed copies

Views

1362

Downloads

1019

Citations