The avascular nature of the human intervertebral disc (IVD) is thought to play a major role in disc pathophysiology by limiting nutrient supply to resident IVD cells. In the human IVD, the central IVD cells at maturity are normally chondrocytic in phenotype. However, abnormal cell phenotypes have been associated with degenerative disc diseases, including cell proliferation and cluster formation, cell death, stellate morphologies, and cell senescence. Therefore, we have examined the relative influence of possible blood-borne factors on the growth characteristics of IVD cells in vitro.
Methods
Bovine IVD cells were cultured either in monolayer to encourage cell proliferation or in alginate to induce chondrocytic differentiation. In both culture systems, cells were maintained with or without 20% serum, with or without 320 mg/dL glucose, and in atmospheric levels (~21%) of oxygen or 1% oxygen. Cell proliferation and viability, cell senescence, and collagen immunopositivity were assessed after 7 days. Statistical differences in these growth characteristics were tested using nonparametric analyses (n = 4 samples).
Results
In both culture systems, serum deprivation significantly inhibited IVD cell proliferation and increased cell positivity for senescence-associated beta-galactosidase (SA-β-gal), a marker of cell senescence. Conversely, IVD cells cultured in the presence of serum, but deprived of glucose, proliferated significantly more rapidly. In alginate cultures, this enhanced cell proliferation (through glucose deprivation) led to the formation of IVD cell clusters. Serum-deprived cells in monolayer, but not in alginate, adopted a stellate appearance. Oxygen deprivation alone had little effect on IVD cell proliferation or survival. Oxygen and glucose deprivation also had no significant effect on SA-β-gal positivity. IVD cell viability was markedly and significantly decreased in serum-deprived alginate cultures, but in all other conditions remained at or greater than approximately 95%. Glucose deprivation, but not serum or oxygen deprivation, inhibited synthesis of type I and type II collagen, both in monolayer and alginate cultures.
Conclusion
This study demonstrates that factors present in serum interact with other nutrients, notably glucose, to play a major role in regulating the behaviour of IVD cells. These findings suggest that IVD cell phenotypes seen in degenerative disc disease may arise through the cells' response to altered vascularisation and nutrient supply.
Introduction
The intervertebral disc (IVD) is the largest avascular connective tissue in the human body. It is composed largely of a collagenous extracellular matrix that is sparsely interspersed by IVD cells (~6,000 mm-3) [1]. The activity of IVD cells is important to tissue function, and IVD cell death, along with decreased IVD cellularity, is associated with ageing and degenerative disc pathology [2, 3]. Abnormal cell behaviour seen in pathological human IVDs also includes increased cell proliferation and cluster formation [4], the appearance of stellate cells [5], and cell senescence [6–8]. The avascularity of the disc has long been considered to influence IVD cell function [1], a view supported by in vitro studies. Hence, Urban and colleagues [9] demonstrated that reduced levels of glucose and oxygen, combined with other environmental conditions present in the inner parts of human IVDs (that is, decreased pH and increased osmolarity), decrease the anabolic activity of IVD cells. Glucose deprivation, in particular, also results in increased IVD cell death, an effect that increases with increased cell density (see reviews [9, 10]). There are also clinical and experimental indications that factors affecting vascular function or glucose supply are associated with an increased risk of disc disease. For example, atherosclerosis [11] and smoking [12], along with diabetes [13, 14], have been linked to IVD degeneration, although the influence of insulin-dependent diabetes on susceptibility to human disc disease remains unproven [15].
Few studies have examined the influence of serum-derived factors on the growth and survival of IVD cells, even though these factors generally are considered to be essential for the survival of most normal cell types. This may be because workers in the field have considered it unlikely that growth factors enter the IVD's inner regions via diffusion from the peripheral vasculature. Indeed, one early study [16] demonstrated that the diffusion rate of molecules through the cartilage endplate, the major route of glucose and oxygen to the central nucleus pulposus (NP) [9, 10], was dependent on their size, charge, and shape, with larger, more globular proteins diffusing more slowly than smaller, more linear molecules. However, there is no direct evidence that serum-derived factors are restricted from entering the IVD. Furthermore, the IVD becomes increasingly vascularised as it degenerates or is damaged, with blood vessels particularly entering disrupted regions of the tissue [17–19]. Herniated discs are also frequently vascularised [20, 21]. Hence, the provision of serum-derived factors to IVD cells may increase in pathological IVDs and consequently play an important role in regulating IVD cell behaviour. In this study, we have examined the relative influence of serum, glucose, and oxygen supply, singly or combined, on the growth pattern of bovine IVD cells. Since the nutrient supply affects the NP more than the anulus fibrosus (AF), the response of NP disc cells was investigated.
Materials and methods
Intervertebral disc cell culture
IVD cells were isolated from the NP of adult bovine caudal IVDs by enzymatic digestion and expanded in monolayer culture in standard Dulbecco's modified Eagle's medium (DMEM)/F-12 supplemented with 10% foetal calf serum (FCS), penicillin, and streptomycin, as described [22] (all reagents from Invitrogen Ltd., Paisley, UK). Freshly isolated NP cells are chondrocytic in phenotype, but during monolayer culture, they become adherent and fibroblast-like in morphology and enter the cell cycle to proliferate, a process that has been termed chondrocyte dedifferentiation [23]. At passage II, these fibroblastic cells were seeded into culture plates at a density of 2 × 103 cells per square centimetre in DMEM containing 10% FCS and left to adhere overnight. Following washes with phosphate-buffered saline, seeded cells were fed with DMEM (a) supplemented with or without 20% FCS, (b) supplemented with or without 320 mg/dL glucose, and (c) maintained in a humidified atmosphere containing atmospheric levels (~21%) of oxygen or 1% oxygen. Various combinations of serum, glucose, and oxygen supplementation were also examined. Alternatively, passage II IVD cells were seeded into alginate beads at a low cell density of 106 cells per millilitre and a final alginate concentration of 1.2%. The alginate beads were then incubated in combinations of medium supplemented with or without serum and glucose and in 21% or 1% oxygen, as described above. All culture medium was at pH 6.9 to 7.1 and approximately 312 to 321 mOsm/kg water. Cultures were fed at day 4 after the initial feeding and harvested on day 7. For all analyses, control cultures were designated as those maintained at atmospheric levels of oxygen and in medium supplemented with 20% FCS and 320 mg/dL glucose.
Cell proliferation and cell viability
Monolayers were harvested by trypsinisation and viable cell counts were performed using trypan blue. The proliferation status of cells was also examined by immunocytochemistry for the proliferation-associated Ki-67 antigen, as described [24]. Cell viability in alginate was assessed by 'live/dead' scoring, in which live cells fluoresce green and dead cells fluoresce red (Live/Dead; Invitrogen Ltd.) [25].
Cell senescence
Senescent cells express much greater levels of beta-galactosidase activity than nonsenescent cells such that its enzymic activity can be detected at the suboptimal pH of 6.0 [26]. Hence, senescence-associated beta-galactosidase (SA-β-gal) activity was examined, as described [6], and the proportion of SA-β-gal-positive cells was quantitated by scoring a minimum of 200 cells for each condition and each sample.
Collagen immunolocalisation
The production of type I and II collagens was examined by immunolocalisation of cytospins, as described [24]. In brief, formalin-fixed cytospins were incubated with antibodies specific for collagen type I (clone I-8H5; ICN Biomedical Ltd., now part of MP Biomedicals, Irvine, CA, USA) or collagen type II (clone C11C1; Developmental Studies Hybridoma Bank, Iowa City, IA, USA). Immunoreactivity was revealed using a commercial kit (Vectastain ABC Elite; Vecta Labs Ltd., Peterborough, UK) combined with streptavidin-FITC (fluorescein isothiocyanate) (Vecta Labs Ltd.) and counterstained with DAPI (4'-6-diamidino-2-phenylindole). Immunolocalisation was also performed using isotype-matched irrelevant antibodies (Dako, Ely, UK); this staining was negative. The presence of filamentous actin (F-actin) was assessed using fluorescently tagged phalloidin (FITC-phalloidin; Molecular Probes Inc., now part of Invitrogen Corporation, Carlsbad, CA, USA), as described [24].
Microscopy and image capture
Cultures were viewed using phase-contrast and fluorescence microscopy (Nikon Eclipse TS100; Nikon, Kingston-upon-Thames, UK). Digitized images were captured with a Hamamatsu (C4742-95; Hamamatsu Corporation, Bridgewater, NJ, USA) or Nikon digital camera and examined using IP Lab software (version 3.6; Nikon).
Statistical analysis
The nonparametric Mann-Whitney U test was used to assess significant differences between control cultures and cultures deprived of nutrient factors for the following parameters: (a) the harvested cell number, (b) the proportion of Ki-67-immunopositive cells, (c) cell viability, and (d) the proportion of SA-β-gal-positive cells. All data shown are presented as mean ± standard error of the mean, where NP cell cultures were established from caudal IVD obtained from four bovine tails (that is, n = 4). Significance differences were accepted at a P value of less than 0.05.
Results
Growth kinetics of monolayer cultures
From a seeding population of 20 × 103 cells per well (in six-well plates), control monolayer cultures expanded to 166 ± 37 × 103 cells per well by day 7. In contrast, monolayer cultures in serum-free medium increased only to 37 ± 6 × 103 cells per well. Monolayers in glucose-deprived medium expanded to 403 ± 60 × 103 cells per well over the same time period (Figure 1a). These significant differences in cell harvests were reflected in the proportions of Ki-67-immunopositive cells (Figure 1b). The proliferative response of IVD cells to glucose deprivation was abrogated when cultures were further deprived either of serum or oxygen such that only 60 ± 9 × 103 cells per well or 198 ± 47 × 103 cells per well were harvested, respectively. Oxygen deprivation alone did not significantly alter the harvested cell number or the Ki-67 index. Day 7 cell harvests of serum-deprived cultures which were also further deprived of oxygen (31 ± 8 × 103 cells per well) or of oxygen and glucose (53 ± 21 × 103 cells per well) were not significantly different from those cultures deprived of serum alone. In all of these experiments, there was no evidence of monolayered cells becoming nonadherent and cell viability remained at 98% to 99%, except for glucose-deprived cultures in which viability by day 7 had decreased slightly, but significantly, to 94.8% ± 0.6% (Mann-Whitney U test; P = 0.0286). Hence, serum deprivation was associated with IVD cell growth arrest, whereas glucose deprivation (in the presence of serum and oxygen) resulted in IVD cell proliferation.
Figure 1
The growth of intervertebral disc cells in monolayer culture. (a) Compared with control cultures, cell numbers at day 7 were significantly decreased in serum-deprived cultures and increased in glucose-deprived cultures. Oxygen deprivation had no significant effect. (b) The proportions of Ki-67-immunopositive cells were also significantly decreased in serum-deprived cultures and increased in glucose-deprived cultures. Oxygen deprivation had no significant effect. Data are presented as mean ± standard error of the mean. *P < 0.05.
Morphology and senescence
Serum-deprived IVD cells in monolayer, but not control or glucose- or oxygen-deprived cells, exhibited a stellate morphology, with many cells extending several branching cell processes (Figure 2a). Furthermore, the proportion of SA-β-gal-positive cells was significantly greater in serum-deprived cultures (46% ± 8%) compared with control or glucose- or oxygen-deprived cultures (~0.5%) (Figure 2b, c). However, there was no clear relationship between cell morphology and cell senescence. Increased SA-β-gal positivity was not seen in cultures deprived of glucose and/or oxygen, nor was it seen to any greater extent in serum-deprived cultures that were further deprived of glucose and/or oxygen (data not shown).
Figure 2
Serum deprivation of intervertebral disc cells in monolayer cultures was associated with the adoption of a stellate morphology and increased cell senescence. (a) Representative images of control (left panel) and serum-deprived (right panel) cells at day 7; stellate cells are indicated with arrows (original magnification ×200). (b) Representative images of control (left panel) and serum-deprived (right panel) cultures stained for senescence-associated beta-galactosidase (SA-β-gal) activity at day 7 (original magnification ×100). (c) The proportion of SA-β-gal-positive cells was significantly increased in serum-deprived cultures compared with control cultures but was unaffected by glucose or oxygen deprivation. Data are presented as mean ± standard error of the mean. *P < 0.05.
Alginate cultures
IVD cells cultured in alginate were markedly less proliferative than those in monolayer. Hence, whereas 24% ± 2% of cells in control monolayers were Ki-67-immunopositive, only 3% ± 0.8% of cells were positive in control alginate cultures. None of the cells in serum-deprived alginate cultures was Ki-67-immunopositive. The proportion of Ki-67-immunopositive cells was significantly greater in glucose-deprived alginate cultures (8% ± 1.3%) compared with controls, whereas oxygen deprivation had no significant effect (Figure 3a). Therefore, and similar to our observations in monolayer, serum deprivation of alginate cultures induced IVD cell growth arrest whereas glucose deprivation was associated with increased proliferation. This enhanced cell proliferation was also evidenced by the formation of viable IVD cell clusters (Figure 3a, inset). Cytochemical positivity for SA-β-gal was significantly increased in serum-deprived alginate cultures (24% ± 3%) in comparison with all other conditions (Figure 3b). However, there was no evidence of serum-deprived cells in alginate becoming stellate, with all cells appearing spherical or ovoid. There was a significant decrease in cell viability in serum-deprived alginate cultures, in which only 63% ± 6% of cells remained alive at day 7 (see Additional file 1). Cell viability remained at approximately 95% in all other conditions (that is, in control or glucose- or oxygen-deprived cultures).
Figure 3
The growth and senescence of intervertebral disc (IVD) cells in alginate culture. (a) Compared with control cultures, the proportion of Ki-67-immunopositive cells was significantly decreased in serum-deprived cultures and increased in glucose-deprived cultures. Oxygen deprivation had no significant effect. Inset: representative images of glucose-deprived alginate cultures, showing a viable cell cluster, and Ki-67-immunopositive cells following harvest (arrow) (original magnification ×200). (b) The proportion of senescence-associated beta-galactosidase (SA-β-gal)-positive IVD cells was significantly increased in serum-deprived cultures compared with control cultures but was unaffected by glucose or oxygen deprivation. Data are presented as mean ± standard error of the mean (n = 4). *P < 0.05.
Collagen production
Collagen type I immunopositivity in IVD cells was more prevalent in control monolayer cultures compared with control alginate cultures. Conversely, collagen type II was largely absent in monolayered IVD cells but was more prevalent in cells in alginate (Figure 4a). Serum or oxygen deprivation appeared to have little effect on these patterns of immunopositivity (data not shown). However, glucose deprivation was associated with a drastic reduction in the immunopositivity of both collagen type I and II, whether in monolayer or alginate cultures (Figure 4b). Staining for F-actin was used as an indicator of protein production. Hence, F-actin positivity was seen to similar extents in control and glucose-deprived IVD cells (Figure 4c).
Figure 4
Collagen production by intervertebral disc (IVD) cells in monolayer and alginate cultures. Immunocytochemistry of cytospins was used to examine collagen production at day 7; representative images are shown. (a) In monolayer control cultures (left panels), collagen type I-immunopositive IVD cells were markedly more prevalent than collagen type II-immunopositive cells, indicative of a dedifferentiated phenotype [22]. This pattern of immunopositivity was reversed in alginate control cultures (right panels), suggesting that the cells in alginate had redifferentiated toward a chondrocytic phenotype [22]. (b) Immunopositivity for both types of collagen was markedly decreased in glucose-deprived cultures, both in monolayer (left panels) and alginate (right panels) culture. (c) Phalloidin-fluorescein isothiocyanate staining of IVD cells following monolayer (left panel) and alginate (right panel) culture in conditions of glucose-deprivation at day 7, demonstrating that the presence of filamentous actin (F-actin) was not markedly different in either condition (original magnification ×200).
The predominant phenotypic changes seen in IVD cells when cultured in the presence or absence of serum or glucose, both in monolayer and alginate culture systems, are summarised in Table 1. The minimal influence of oxygen levels on IVD cell growth and behaviour is omitted from this summary.
Table 1
The major phenotypes of bovine intervertebral disc cells in response to altered culture conditions
Serum
Glucose
Monolayer
With
Without
With
Without
Cell proliferation
↑↑↑
↓↓
↔
↑↑↑↑
Cell senescence
↔
↑↑↑
↔
↔
Cell death
↔
↔
↔
↔
Collagen synthesis
↑↑↑ Type I ↓ Type II
↔ Type I ↔ Type II
↔ Type I ↔ Type II
↓↓↓ Type I ↓ Type II
Serum
Glucose
Alginate
With
Without
With
Without
Cell proliferation
↓↓
↓↓↓
↔
↑
Cell senescence
↔
↑↑
↔
↔
Cell death
↔
↓↓
↔
↔
Collagen synthesis
↓ Type I ↑↑ Type II
↔ Type I ↔ Type II
↔ Type I ↔ Type II
↔ Type I ↓↓ Type II
↑, increased; ↓, decreased; ↔, no change (from control conditions).
Discussion
Pathological conditions of the human IVD are associated with changes in IVD cell behaviour, including increased cell death [2, 3], cell division [4], the appearance of stellate cells [5], and cell senescence [6–8]. What leads to these phenotypes is currently unclear; however, it is generally thought that nutritional deprivation may limit the capacity of IVD cells to function. Here, we have demonstrated that depriving IVD cells of serum, glucose, or oxygen has a variable influence on their growth and survival. Serum supplementation was required for continued IVD cell proliferation in monolayer cultures but was insufficient to drive proliferation to the same extent (as delineated by the Ki-67 index) in alginate cultures. Conversely, serum deprivation of monolayer cultures had no significant effect on cell viability but was associated with increased cell death in alginate cultures. In both culture systems, serum deprivation led to IVD cell growth arrest. These findings fit the general observation of various cell types that serum withdrawal induces cell growth arrest and/or apoptosis [27, 28] whereas cell adhesion promotes cell survival [29]. We also found that serum deprivation was associated with increased SA-β-gal positivity in both culture systems and with the appearance of stellate cells in monolayer cultures. Both of these phenotypes have been linked with cell senescence or cellular adaptations to extracellular stresses [26, 30]. As SA-β-gal staining was seen in cell populations that had undergone growth arrest, it can be concluded that this may be indicative of premature cell senescence. It remains to be determined how these findings relate to pathological human discs, where SA-β-gal-positive cells were seen most frequently in cell clusters [6] and have been associated with an increased catabolic activity [8]. In addition, Gruber and colleagues [31] have demonstrated increased levels of apoptosis in cells isolated from pathological human AF tissue in response to serum deprivation over a 10-day culture period of monolayer culture (from 0.1% to approximately 1%); this induction of cell death was inhibited by insulin-like growth factor-1 or platelet-derived growth factor. Zhao and colleagues [32] recently found that serum deprivation also induces apoptosis in rat AF cells, an effect that was exacerbated by interleukin-1-β. Hence, it is possible that the initial growth arrest and senescence that we have documented in response to serum deprivation may be followed by apoptotic cell death. Alternatively, NP cells and AF cells may require serum-derived survival factors to different extents. These areas warrant further investigation, as do the actions of individual growth and survival factors that may enter the disc from the vascular supply or that may be synthesised by IVD cells themselves [33].
The availability of oxygen and glucose to IVD cells is dependent on their transport from blood vessels and therefore on the degree of disc vascularisation (reviewed in [9, 10]). As this varies according to age and pathology [17–21], the influence of oxygen and glucose on IVD cell growth may also be expected to vary. However, depriving IVD cells of oxygen alone had no marked effect on their growth or survival in vitro, either in monolayer or alginate culture. Risbud and colleagues [34] have shown that rat, sheep, and human IVD cells express hypoxia inducible factor-1-alpha (HIF-1-α), a transcription factor that is responsive to oxygen availability, even in normoxia. HIF-1-α expression was also only minimally induced and activated following hypoxia in culture. Furthermore, the same authors demonstrated that NP cells in rat discs, which are notochordally derived, do not appear to rely upon oxygen for their metabolism in vivo [35]. Although the central regions of the human IVD are more hypoxic than its periphery [36] (which may not be the case in smaller rat discs), one interpretation of the studies of Risbud and colleagues, along with our present findings, is that NP cells are adapted not to respond to hypoxia as readily as other cell types.
Depriving IVD cells of glucose resulted in increased cell proliferation, so long as serum (and to a lesser extent oxygen) was present, but a clear decrease in collagen production. The reasons for these responses are currently unclear; however, a similar relationship between glucose levels and proliferation was reported recently in Chinese hamster ovary (CHO) cells, which expanded in a low-glucose environment (6 mM) at a rate 1.7 times that seen in high-glucose conditions (33 mM) [37]. Similarly, exposure to higher levels of glucose (greater than 15 mM) was shown to inhibit cell proliferation in fibroblasts [38]. In our experiments, the proliferative response to glucose deprivation was dependent on the presence of serum, which in itself will contain glucose. As normal blood glucose levels vary between 4 and 8 mM (equating to 70 to 150 mg/dL), it may be assumed that the glucose levels in culture medium supplemented with 20% FCS will contain approximately 14 to 30 mg/dL. Hence, the precise relationships between levels of glucose and of other serum-derived factors in regulating IVD cell proliferation and collagen synthesis remain to be fully elucidated. It is noteworthy, however, that the increased cell proliferation seen in glucose-deprived alginate cultures resulted in the formation of NP cell clusters, which also form through increased cell proliferation in the NP in vivo and have been suggested to form part of an ineffective response to tissue damage [4].
Conclusion
This study demonstrates that factors present in serum interact with other nutrients, notably glucose, to play a major role in regulating the behaviour of IVD cells. Furthermore, by manipulating the nutrient and serum supply to IVD cells in vitro, we have observed a number of cellular phenotypes akin to those seen in pathological human IVDs [2–7]. Hence, this study supports the conclusion that many of the cellular changes associated with IVD degeneration are likely to arise through the cells' response to altered vascularisation and nutrient supply.
Abbreviations
AF:
anulus fibrosus
DMEM:
Dulbecco's modified Eagle's medium
F-actin:
filamentous actin
FCS:
foetal calf serum
FITC:
fluorescein isothiocyanate
HIF-1-α:
hypoxia inducible factor-1-alpha
IVD:
intervertebral disc
NP:
nucleus pulposus
SA-β-gal:
senescence-associated beta-galactosidase.
Declarations
Acknowledgements
This work was funded by the Biotechnology and Biological Sciences Research Council, UK.
Authors’ Affiliations
(1)
Centre for Spinal Studies, Robert Jones and Agnes Hunt Orthopaedic Hospital
(2)
Institute for Science and Technology in Medicine, Keele University
References
Maroudas A, Stockwell RA, Nachemson A, Urban J: Factors involved in the nutrition of the human lumbar intervertebral disc: cellularity and diffusion of glucose in vitro. J Anat. 1975, 120: 113-130.PubMed CentralPubMedGoogle Scholar
Gruber HE, Hanley EN: Analysis of aging and degeneration of the human intervertebral disc. Comparison of surgical specimens with normal controls. Spine. 1998, 23: 751-757. 10.1097/00007632-199804010-00001.View ArticlePubMedGoogle Scholar
Boos N, Weissbach S, Rohrbach H, Weiler C, Spratt KF, Nerlich AG: Classification of age-related changes in lumbar intervertebral discs: 2002 Volvo Award in basic science. Spine. 2002, 27: 2631-2644. 10.1097/00007632-200212010-00002.View ArticlePubMedGoogle Scholar
Johnson WE, Eisenstein SM, Roberts S: Cell cluster formation in degenerate lumbar intervertebral discs is associated with increased disc cell proliferation. Connect Tissue Res. 2001, 42: 197-207. 10.3109/03008200109005650.View ArticlePubMedGoogle Scholar
Johnson WE, Roberts S: Human intervertebral disc cell morphology and cytoskeletal composition: a preliminary study of regional variations in health and disease. J Anat. 2003, 203: 605-612. 10.1046/j.1469-7580.2003.00249.x.PubMed CentralView ArticlePubMedGoogle Scholar
Roberts S, Evans EH, Kletsas D, Jaffray DC, Eisenstein SM: Senescence in human intervertebral discs. Eur Spine J. 2006, 15: S312-316. 10.1007/s00586-006-0126-8.View ArticlePubMedGoogle Scholar
Gruber HE, Ingram JA, Norton HJ, Hanley EN: Senescence in cells of the aging and degenerating intervertebral disc: immunolocalization of senescence-associated beta-galactosidase in human and sand rat discs. Spine. 2007, 32: 321-327. 10.1097/01.brs.0000253960.57051.de.View ArticlePubMedGoogle Scholar
Le Maitre CL, Freemont AJ, Hoyland JA: Accelerated cellular senescence in degenerate intervertebral discs: a possible role in the pathogenesis of intervertebral disc degeneration. Arthritis Res Ther. 2007, 9: R45-10.1186/ar2198.PubMed CentralView ArticlePubMedGoogle Scholar
Urban JP, Smith S, Fairbank JC: Nutrition of the intervertebral disc. Spine. 2004, 29: 2700-2709. 10.1097/01.brs.0000146499.97948.52.View ArticlePubMedGoogle Scholar
Grunhagen T, Wilde G, Soukane DM, Shirazi-Adl SA, Urban JP: Nutrient supply and intervertebral disc metabolism. J Bone Joint Surg Am. 2006, 88: 30-35. 10.2106/JBJS.E.01290.View ArticlePubMedGoogle Scholar
Kauppila LI, McAlindon T, Evans S, Wilson PW, Kiel D, Felson DT: Disc degeneration/back pain and calcification of the abdominal aorta. A 25-year follow-up study in Framingham. Spine. 1997, 22: 1642-1647. 10.1097/00007632-199707150-00023.View ArticlePubMedGoogle Scholar
Holm S, Nachemson A: Nutrition of the intervertebral disc: acute effects of cigarette smoking. An experimental animal study. Ups J Med Sci. 1988, 93: 91-99.PubMedGoogle Scholar
Ziv I, Moskowitz RW, Kraise I, Adler JH, Maroudas A: Physicochemical properties of the aging and diabetic sand rat intervertebral disc. J Orthop Res. 1992, 10: 205-210. 10.1002/jor.1100100207.View ArticlePubMedGoogle Scholar
Robinson D, Mirovsky Y, Halperin N, Evron Z, Nevo Z: Changes in proteoglycans of intervertebral disc in diabetic patients. A possible cause of increased back pain. Spine. 1998, 23: 849-855. 10.1097/00007632-199804150-00001.View ArticlePubMedGoogle Scholar
Videman T, Battié MC, Gibbons LE, Kaprio J, Koskenvuo M, Kannus P, Raininko R, Manninen H: Disc degeneration and bone density in monozygotic twins discordant for insulin-dependent diabetes mellitus. J Orthop Res. 2000, 18: 768-772. 10.1002/jor.1100180514.View ArticlePubMedGoogle Scholar
Roberts S, Urban JP, Evans H, Eisenstein SM: Transport properties of the human cartilage endplate in relation to its composition and calcification. Spine. 1996, 21: 415-420. 10.1097/00007632-199602150-00003.View ArticlePubMedGoogle Scholar
Kauppila LI: Ingrowth of blood vessels in disc degeneration. Angiographic and histological studies of cadaveric spines. J Bone Joint Surg Am. 1995, 77: 26-31.PubMedGoogle Scholar
Johnson WE, Evans H, Menage J, Eisenstein SM, El Haj A, Roberts S: Immunohistochemical detection of Schwann cells in innervated and vascularized human intervertebral discs. Spine. 2001, 26: 2550-2557. 10.1097/00007632-200112010-00007.View ArticlePubMedGoogle Scholar
Nerlich AG, Schaaf R, Wälchli B, Boos N: Temporo-spatial distribution of blood vessels in human lumbar intervertebral discs. Eur Spine J. 2007, 16: 547-555. 10.1007/s00586-006-0213-x.PubMed CentralView ArticlePubMedGoogle Scholar
Pai RR, D'sa B, Raghuveer CV, Kamath A: Neovascularization of nucleus pulposus. A diagnostic feature of intervertebral disc prolapse. Spine. 1999, 24: 739-741. 10.1097/00007632-199904150-00002.View ArticlePubMedGoogle Scholar
Ozaki S, Muro T, Ito S, Mizushima M: Neovascularization of the outermost area of herniated lumbar intervertebral discs. J Orthop Sci. 1999, 4: 286-292. 10.1007/s007760050105.View ArticlePubMedGoogle Scholar
Johnson WE, Wootton A, El Haj A, Eisenstein SM, Curtis AS, Roberts S: Topographical guidance of intervertebral disc cell growth in vitro : towards the development of tissue repair strategies for the anulus fibrosus. Eur Spine J. 2006, 15: S389-396. 10.1007/s00586-006-0125-9.View ArticlePubMedGoogle Scholar
Benya PD, Shaffer JD: Dedifferentiated chondrocytes reexpress the differentiated collagen phenotype when cultured in agarose gels. Cell. 1982, 30: 215-224. 10.1016/0092-8674(82)90027-7.View ArticlePubMedGoogle Scholar
Gargiulo BJ, Cragg P, Richardson JB, Ashton BA, Johnson WE: Phenotypic modulation of human articular chondrocytes by bistratene A. Eur Cell Mater. 2002, 3: 9-18.PubMedGoogle Scholar
Poole CA, Brookes NH, Clover GM: Keratocyte networks visualised in the living cornea using vital dyes. J Cell Sci. 1993, 106: 685-691.PubMedGoogle Scholar
Dimri GP, Lee X, Basile G, Acosta M, Scott G, Roskelley C, Medrano EE, Linskens M, Rubelj I, Pereira-Smith O, Peacocke M, Campisi J: A biomarker that identifies senescent human cells in culture and in aging skin in vivo. Proc Natl Acad Sci USA. 1995, 92: 9363-9367. 10.1073/pnas.92.20.9363.PubMed CentralView ArticlePubMedGoogle Scholar
Preston GA, Lang JE, Maronpot RR, Barrett JC: Regulation of apoptosis by low serum in cells of different stages of neoplastic progression: enhanced susceptibility after loss of a senescence gene and decreased susceptibility after loss of a tumor suppressor gene. Cancer Res. 1994, 54: 4214-4223.PubMedGoogle Scholar
Gos M, Miloszewska J, Swoboda P, Trembacz H, Skierski J, Janik P: Cellular quiescence induced by contact inhibition or serum withdrawal in C3H10T1/2 cells. Cell Prolif. 2005, 38: 107-116. 10.1111/j.1365-2184.2005.00334.x.View ArticlePubMedGoogle Scholar
Qi J, Fox AM, Alexopoulos LG, Chi L, Bynum D, Guilak F, Banes AJ: IL-1beta decreases the elastic modulus of human tenocytes. J Appl Physiol. 2006, 101: 189-195. 10.1152/japplphysiol.01128.2005.View ArticlePubMedGoogle Scholar
Gruber HE, Norton HJ, Hanley EN: Anti-apoptotic effects of IGF-1 and PDGF on human intervertebral disc cells in vitro. Spine. 2000, 25: 2153-2157. 10.1097/00007632-200009010-00002.View ArticlePubMedGoogle Scholar
Zhao CQ, Liu D, Li H, Jiang LS, Dai LY: Interleukin-1beta enhances the effect of serum deprivation on rat annular cell apoptosis. Apoptosis. 2007, 12: 2155-2161. 10.1007/s10495-007-0137-x.View ArticlePubMedGoogle Scholar
Li H, Zou X, Baatrup A, Lind M, Bünger C: Cytokine profiles in conditioned media from cultured human intervertebral disc tissue. Implications of their effect on bone marrow stem cell metabolism. Acta Orthop. 2005, 76: 115-121. 10.1080/00016470510030436.View ArticlePubMedGoogle Scholar
Risbud MV, Guttapalli A, Stokes DG, Hawkins D, Danielson KG, Schaer TP, Albert TJ, Shapiro IM: Nucleus pulposus cells express HIF-1alpha under normoxic culture conditions: a metabolic adaptation to the intervertebral disc microenvironment. J Cell Biochem. 2006, 98: 152-159. 10.1002/jcb.20765.View ArticlePubMedGoogle Scholar
Lee DC, Adams CS, Albert TJ, Shapiro IM, Evans SM, Koch CJ: In situ oxygen utilization in the rat intervertebral disc. J Anat. 2007, 210: 294-303. 10.1111/j.1469-7580.2007.00692.x.PubMed CentralView ArticlePubMedGoogle Scholar
Bartels EM, Fairbank JC, Winlove CP, Urban JP: Oxygen and lactate concentrations measured in vivo in the intervertebral discs of patients with scoliosis and back pain. Spine. 1998, 23: 1-7. 10.1097/00007632-199801010-00001.View ArticlePubMedGoogle Scholar
Takuma S, Hirashima C, Piret JM: Dependence on glucose limitation of the pCO2 influences on CHO cell growth, metabolism and IgG production. Biotechnol Bioeng. 2007, 97: 1479-1488. 10.1002/bit.21376.View ArticlePubMedGoogle Scholar
Hehenberger K, Hansson A: High glucose-induced growth factor resistance in human fibroblasts can be reversed by antioxidants and protein kinase C-inhibitors. Cell Biochem Funct. 1997, 15: 197-201. 10.1002/(SICI)1099-0844(199709)15:3<197::AID-CBF740>3.0.CO;2-7.View ArticlePubMedGoogle Scholar
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