Novel immortal human cell lines reveal subpopulations in the nucleus pulposus
- Guus GH van den Akker1, 2,
- Don AM Surtel1,
- Andy Cremers1,
- Ricardo Rodrigues-Pinto3, 4,
- Stephen M Richardson3,
- Judith A Hoyland3,
- Lodewijk W van Rhijn1,
- Tim JM Welting†1 and
- Jan Willem Voncken†2Email author
© van den Akker et al.; licensee BioMed Central Ltd. 2014
Received: 27 August 2013
Accepted: 19 June 2014
Published: 27 June 2014
Relatively little is known about cellular subpopulations in the mature nucleus pulposus (NP). Detailed understanding of the ontogenetic, cellular and molecular characteristics of functional intervertebral disc (IVD) cell populations is pivotal to the successful development of cell replacement therapies and IVD regeneration. In this study, we aimed to investigate whether phenotypically distinct clonal cell lines representing different subpopulations in the human NP could be generated using immortalization strategies.
Nondegenerate healthy disc material (age range, 8 to 15 years) was obtained as surplus surgical material. Early passage NP monolayer cell cultures were initially characterized using a recently established NP marker set. NP cells were immortalized by simian virus 40 large T antigen (SV40LTag) and human telomerase reverse transcriptase expression. Immortalized cells were clonally expanded and characterized based on collagen type I, collagen type II, α1 (COL2A1), and SRY-box 9 (SOX9) protein expression profiles, as well as on expression of a subset of established in vivo NP cell lineage markers.
A total of 54 immortal clones were generated. Profiling of a set of novel NP markers (CD24, CA12, PAX1, PTN, FOXF1 and KRT19 mRNA) in a representative set of subclones substantiated successful immortalization of multiple cellular subpopulations from primary isolates and confirmed their NP origin and/or phenotype. We were able to identify two predominant clonal NP subtypes based on their morphological characteristics and their ability to induce SOX9 and COL2A1 under conventional differentiation conditions. In addition, cluster of differentiation 24 (CD24)–negative NP responder clones formed spheroid structures in various culture systems, suggesting the preservation of a more immature phenotype compared to CD24-positive nonresponder clones.
Here we report the generation of clonal NP cell lines from nondegenerate human IVD tissue and present a detailed characterization of NP cellular subpopulations. Differential cell surface marker expression and divergent responses to differentiation conditions suggest that the NP subtypes may correspond to distinct maturation stages and represent distinct NP cell subpopulations. Hence, we provide evidence that the immortalization strategy that we applied is capable of detecting cell heterogeneity in the NP. Our cell lines yield novel insights into NP biology and provide promising new tools for studies of IVD development, cell function and disease.
Degenerative disc disease (DDD) poses a substantial socioeconomic burden in developed countries . Currently, treatment of DDD is primarily aimed at relieving symptoms because effective therapy to delay or prevent DDD is not available.
The intervertebral disc (IVD) consists of a central gelatinous nucleus pulposus (NP) encircled by an elastic, ligamentous annulus fibrosus (AF) and is flanked superiorly and inferiorly by cartilaginous endplates. NP cells are highly specialized and share some features with articular chondrocytes in terms of aggrecan (ACAN), collagen type II, α1 (COL2A1), and SRY-box 9 (SOX9) protein expression . However, compared to articular cartilage (AC), the NP maintains a unique extracellular matrix (ECM) with a higher glycosaminoglycan to hydroxyproline (GAG/OH-pro) ratio, and its native cells display distinctive gene expression signatures [3–5]. The initial stages of DDD correlate with reduced cellularity, aberrant cell function, loss of proteoglycans and concomitant tissue dehydration . As cells within the IVD are responsible for ECM maintenance and homeostasis, they play an important role in the degenerative process. The findings in an increasing number of studies support the idea that mature NP cells are derived from precursor notochordal cells (NCs), although NP cells differ from NCs morphologically and express different genes (reviewed in ). However, it is becoming increasingly clear that the NP comprises multiple cell subpopulations [8–11]. This cellular heterogeneity may reflect different stages of proliferation, differentiation and maturation; however, relatively little is known about these NP cell subpopulations. Successful development of cell replacement therapies and IVD regeneration is crucially dependent on an in-depth understanding of cellular and molecular characteristics of the functional IVD. To accomplish this, access to representative human cell models is pivotal. However, current research on primary cells is hampered by restricted availability of human cells, particularly from nondegenerate discs, where there is a relatively inherent low cellularity within the tissue. In addition, lack of well-defined cellular characteristics and differences in the origin of study material (for example, donor age, IVD degeneration status) underlies experimental variability and thus low reproducibility. To date, a few NP cell lines have been independently generated by Sakai et al.  and, more recently, by Liu and co-workers .
As no cell lines are available that represent the reported different subpopulations in adult human NP cells, we set out to generate in vitro cell models for human NP cells. Our approach using immortalization, clonal selection and outgrowth allowed us to address NP cell heterogeneity. Here we provide a molecular and cellular characterization of the first immortal human NP cellular subpopulations.
Isolation of intervertebral disc cells, cell culture and immortalization
Intervertebral disc donor characteristics and clones a
Age b, yr
T mRNA primary isolates
Retroviral transduction and generation of immortal clones
The simian virus 40 large T antigen (SV40LTag) and human telomerase reverse transcriptase (hTERT) cDNAs were cloned into pBABE-hygro  and pBMN-IRES-NEO vectors, respectively. Production of viral particles was performed as described previously . Viral titres were sufficiently high to achieve nearly 100% infection. Retrovirally transduced P5 AF and NP cells from donors 4 and 5 were selected with 400 μg/ml G418 and 25 μg/ml hygromycin B (PAA Laboratories/GE Healthcare Life Sciences, Somerset, UK). Immediately following selection, clones were generated by plating less than 1 cell (that is, ±0.5) per well in 96-well plates in reduced selection medium (200 μg/ml G418 and 12 μg/ml hygromycin B). After 1 week of culture, small colonies became discernible. Culture wells with more than one colony were omitted from further study to ensure single picks. Single clones were expanded under continued antibiotic selection pressure and expanded for three more passages (P1 to P4) for cryogenic storage and screening experiments. Selected clones were expanded and remained stable for 8 months or 328 additional population doublings.
Telomeric repeat amplification protocol
To measure TERT activity, a telomeric repeat amplification protocol assay was performed according to the manufacturer’s instructions (TRAPeze Telomerase Detection Kit; Millipore, Amsterdam, the Netherlands) . Briefly, 1 μg of total protein input was used to produce tandem TAAGGG repeats (extension step at 30°C for 30 minutes); these repeats were amplified by PCR using telomere-specific primers (30 cycles), which typically generated a ladder of products with 6-bp increments starting at 50 nucleotides (for example, 50, 56, 62, 68).
Aggrecan coating differentiation assays
To assess NP clonal responses to a relevant proteoglycan in the NP ECM, ACAN was used to coat culture dishes. In brief, we added 5 μg of purified bovine ACAN (Sigma-Aldrich A1960) in 200 μl of solution to 24-well culture plates. The continuously agitated solution was allowed to evaporate overnight at ambient temperature under sterile conditions as described previously . Plates were washed twice with phosphate-buffered saline (PBS), and 200,000 cells/well suspended in Dmed were seeded. Media were changed every other day.
Matrigel cell culture assays
To assess increases in NP clonal behaviour in a three-dimensional environment, we established a Matrigel hydrogel system to support chondrogenesis of articular chondrocytes. Briefly, 90 μl of growth factor–reduced Matrigel (BD Biosciences, San Jose, CA, USA) was dispensed into 12-well culture plates (Greiner Bio-One, Monroe, NC, USA). NP cells (N = 68,400) were grown for 7 days under conventional (that is, articular chondrocyte) differentiation conditions (in Dmed). mRNA samples were taken at 7 days and isolated using the mirVana mRNA Isolation Kit (Ambion, Austin, TX, USA) for whole RNA extraction according to the manufacturer’s instructions.
RNA isolation and quantitative real-time PCR
Quantitative PCR primer list a
Carbonic anhydrase XII
Collagen type I, collagen α1
Collagen type II, collagen α1
Cartilage oligomeric matrix protein
Cluster of differentiation 24
Forkhead box F1
Paired box 1
Protein extraction and immunoblotting
Protein extraction and immunoblotting were performed and analysed as described previously with minor adjustments . For extraction, cells were lysed in radioimmunoprecipitation assay buffer (50 mM Tris, pH 8.0, 150 mM NaCl, 0.1% SDS, 5 mM ethylenediaminetetraacetic acid (EDTA), 0.5% w/v sodium deoxycholate and 1% Nonidet P-40) supplemented with protease and phosphatase inhibitors (Roche Diagnostics, Indianapolis, IN, USA). Lysates were sonicated on ice using the Soniprep 150 Plus ultrasonic disintegrator (MSE, London, UK) at amplitude 10 for 14 cycles (1 second on, 1 second off). Insoluble material was removed by centrifugation (10 minutes at 16,000 × g and 4°C). Protein concentration was determined using a bicinchoninic acid protein assay kit (Pierce/Thermo Scientific, Rockford, IL, USA). Protein samples were separated by SDS-PAGE and immobilized on nitrocellulose membranes. Membranes were blocked for 1 hour in 5% nonfat dry milk powder (FrieslandCampina, Amersfoort, the Netherlands) at ambient temperature and then incubated with primary antibodies overnight at 4°C. Antisera used were polyclonal goat anti-COL2A1 (1320-01; Southern Biotech, Birmingham, AL, USA), polyclonal goat collagen type I, α1 (anti-COL1A1) (1310-01; SouthernBiotech), polyclonal goat anti-SOX9 (ab3697; Abcam, Cambridge, UK), rabbit polyclonal antibody against brachyury T (hereafter ‘T’) (H-210 and SC-20109; Santa Cruz Biotechnology, Santa Cruz, CA, USA), mouse monoclonal anti-SV40LTag (Pab 108, sc-148; Santa Cruz Biotechnology), rabbit polyclonal anti-TERT (R1187; Acris Antibodies, San Diego, CA, USA), mouse monoclonal β-actin (clone C4, 08691001; MP Biomedicals, Santa Ana, CA, USA), mouse monoclonal α-tubulin (clone B-5-1-2, T6074; Sigma-Aldrich), rabbit polyclonal KAP-1 (A300-275A; Bethyl Laboratories, Montgomery, TX, USA). Secondary antisera used were polyclonal rabbit anti-goat (P0449; Dako Cytomation, Glostrup, Denmark), rabbit anti-mouse (P0260; Dako) and donkey anti-rabbit (711-035-152; Jackson ImmunoResearch Laboratories, West Grove, PA, USA). Signals were detected using enhanced chemiluminescence (Pierce/Thermo Scientific).
Flow cytometry was performed as described previously . Cell surface markers analysed were cluster of differentiation 44 (CD44), CD73, CD90 and CD105 (Miltenyi Biotec, San Diego, CA, USA); gangliosidase 2 (GD2) (Santa Cruz Biotechnology); and CD24 (BioLegend, San Diego, CA, USA). Briefly, antibody incubation (10 minutes at 4°C in the dark) was followed by washes.
Cell proliferation assays
Cells were seeded at 6,400 cells/cm2, allowed to attach overnight (t 0; baseline) and grown in 12-well plates for 12 days. At the indicated time points (cf. Figure 2C), cells were washed in PBS, fixed in 3.7% formaldehyde in PBS solution for 10 minutes at ambient temperature and rinsed with demineralized water. Nuclear DNA was stained (0.1% Crystal violet, 30 minutes, ambient temperature), after which cells were washed extensively with demineralized water. Crystal violet was extracted at a fixed volume of 10% acetic acid. Absorbance was determined at 590 nm (Benchmark microplate reader; Bio-Rad Laboratories, Hercules, CA, USA).
Biochemical matrix assays
Total sulphated GAG content was determined in papain-digested samples by using 1,9-dimethylmethylene blue stain (DMB) (Polysciences, Eppelheim, Germany) . Briefly, cell cultures were washed with 0.9% NaCl and incubated at 60°C for 16 hours in digestion buffer (100 mM sodium phosphate, pH 6.5, 5 mM L-cysteine HCl, 5 mM EDTA) containing 125 to 140 μg/ml papain (Sigma-Aldrich P3125). Samples were collected and centrifuged at 12,000 rpm for 5 minutes, and the supernatants were incubated with DMB solution (46 μM DMB, 40.5 mM glycine, 40.5 mM NaCl, pH 1.5). An absorption ratio of 540 nm/595 nm was determined within 5 to 10 minutes of adding DMB solution. A standard curve of chondroitin sulphate (Sigma-Aldrich) was included as a reference. OH-pro quantification was performed using a chloramine-T assay and compared to a trans-4-hydroxyproline standard essentially as described previously . Both GAG and OH-pro content were normalized against cellular DNA content. DNA concentration in papain-digested samples was determined using SYBR Green stain (Eurogentec, Fremont, CA, USA) as described previously . Quantification of DNA concentration was analysed against a genomic control DNA standard (calf thymus; Invitrogen).
Statistical significance (P < 0.05) was determined by two-tailed Student’s t-test. To test for normal distribution of input data, D’Agostino–Pearson omnibus normality tests were performed. All quantitative data sets presented passed the normality tests. The results of gene expression analyses are reported as means with standard deviations where indicated. The P-values given in the figure legends are for comparisons between AF and NP for all donors combined or between clonal subtypes (NP-R vs NP-nR). P-values for every statistical calculation are presented in Additional file 1: Tables S1 to S4.
Phenotypic characterization of primary nucleus pulposus cultures
Cell isolates D4 and D5 were expanded to P5 for comparative analysis and cloning (Figure 1C). The chondrocyte phenotype is known to be unstable in vitro [28, 29]. We therefore tested the differentiation capacity of primary IVD cell cultures. AF and NP cell isolates (P5) from two independent donors showed low amounts of COL2A1 and comparable COL1A1 protein levels (Figure 1D). Dmed induced SOX9 protein expression in primary NP and AF cultures (Figure 1E). In addition, COL2A1 was induced in Dmed in NP as well as AF isolates. Importantly, COL2A1 induction was clearly more prominent in NP cultures (Figure 1E), whereas COL1A1 expression was higher in AF cells (Figure 1E).
NP marker mRNA analysis for CA12, CD24, FOXF1, PAX1, PTN and cytokeratin 19 (KRT19) clearly discriminated between AF and NP cultures in samples from three independent donors (Figure 1F). KRT19 mRNA was higher in NP compared to AF cultures (4- to 70-fold), as were CA12 (1.5- to 3-fold), CD24 (2- to 2.5-fold), FOXF1 (1.9- to 2.3-fold), PAX1 (1.2- to 15-fold) and PTN (2- to 3-fold). These six markers initially appeared stable in pools P0 to P5, although expression diminished thereafter, at P10 (data not shown). Of note, neither T mRNA nor protein was detected in the primary NP isolates of the donors, except for the youngest donor (D1, age 8 years) (Table 1). T is specifically expressed in the notochord and in NCs in the IVD. As such, this finding suggests that the primary isolates that we used for cell line generation were free of NCs. These combined phenotypic analyses confirmed the respective tissues of origin of the primary NP and AF cell isolates and suggest that differentiation capacity was maintained in primary NP cultures. Taken together, these findings provide a solid basis for experimental immortalization and clonal cell line generation.
Phenotypic characterization of immortalized nucleus pulposus clones
We next examined the differentiation capacity of 20 individual immortalized D5 NP clones (Table 1). Expanded clones were induced to differentiate using a standard AC protocol with Dmed, and marker expression was evaluated at the level of proteins (SOX9, COL2A1 and COL1A1).
To determine whether any of the NP markers described above could discriminate between the clonal subtypes (NP-R vs nR), we evaluated differences in mRNA levels of KRT19, CA12, CD24, PTN, FOXF1 and PAX1. In addition, we included cartilage oligomeric matrix protein (COMP), a gene previously shown to be expressed in rat AC and NP cells and in human NP cells [30, 31]. Comparative gene expression analysis of two groups of six representative chondrogenic NP-R and NP-nR clones revealed a clear segregation between the two subtypes. Of these markers, CA12 and FOXF1 levels were significantly higher at t 0 in NP-R clones (Figure 4B; see Additional file 1: Table S2). CD24 showed a trend towards lower expression in NP-R clones under maintenance conditions, whereas COMP mRNA levels tended to be higher in this NP subtype under the same conditions; however, these differences did not reach significance (P = 0.056 and P = 0.099, respectively). KRT19, PAX1 and PTN mRNA levels were not significantly different between NP-R and nR clones at t 0. Exposing NP subtypes to differentiation conditions induced distinct responses (that is, marker gene expression) between the NP subtypes. CA12 mRNA levels significantly decreased in both NP-R and NP-nR clones, which eliminated the original differences (that is, at t 0) between these subtypes (7 days in Dmed) (Figure 4B). In contrast, FOXF1 and COMP significantly changed in NP-R clones, but not in NP-nR clones, in Dmed. Conversely, PAX1 levels significantly dropped in NP-nR clones, but not in NP-R clones, in Dmed. Remarkably, all seven markers tested displayed enhanced differences in expression levels in NP-R versus NP-nR clones under Dmed conditions, three of which reached significance (FOXF1 (P = 0.008), PTN (P = 0.01) and COMP (P = 0.02)). The remaining four markers showed consistent trends (CA12 (P = 0.069), CD24 (P = 0.073), PAX1 (P = 0.066) and KRT19 (P = 0.056)) (Figure 4B). CD24 excepted, expression of all markers was reduced in NP-nR clones under these conditions. The induction of important ECM structural protein-encoding mRNAs such as COL2A1 and ACAN was relatively low at the transcriptional level and did not correlate with cell morphology (data not shown).
In summary, the results of our analyses demonstrate clear differentiation-induced COL2A1 and SOX9 protein detection in NP-R clones that correlate well with the described morphological characteristics. The phenotypic differences between NP-R and NP-nR clones are further substantiated by differential NP marker gene expression profiles, under both nondifferentiation and differentiation conditions, and suggest functional phenotypic differences between the immortalized clonal subtypes.
Cell surface characterization of nucleus pulposus clones
Extracellular matrix molecules in nucleus pulposus cell differentiation
We next tested the differentiation capacity of NP-R and NP-nR cells on Matrigel, as this was recently shown to support differentiation of induced pluripotent stem cells (iPSCs) to NP-like cells . In addition, we examined the effect of ACAN coating on NP subtype differentiation. ACAN is an important constituent of the NP ECM, and ACAN coating has been applied to assist differentiation of meniscus-derived fibrochondrocytes and MSCs into chondrocyte-like cells [39, 40]. We cultured NP-R and nR cells in the presence of either Matrigel or ACAN for 3 to 7 days under differentiation conditions and compared induction of SOX9, COL2A1, ACAN and COMP expression. COL1A1 expression was low under all conditions and was not induced (data not shown). SOX9 mRNA levels were comparable between the NP subtypes under all conditions tested. Interestingly, COMP induction was consistently higher in NP-R cells, whereas, conversely, ACAN induction was consistently higher in NP-nR cells, providing further support for the maintenance of distinct functional properties between the NP-R and NP-nR clones. Only on Matrigel was COL2A1 induced significantly greater in NP-R cells (Figure 6B). Remarkably, Matrigel and ACAN coating had dramatic effects on differentiation-induced COMP and COL2A1 expression levels, respectively. These combined results support the idea that ECM is a determining factor in NP cell differentiation responses and suggest that distinct NP cell types differentially respond to the presence of ECM molecules.
The variation in differentiation capacity between NP-R and NP-nR clones suggested a possible difference in differentiation status or maturity between NP cellular subtypes. As relatively immature porcine NC and NP cells were shown to form spheroids on Matrigel , we compared NP-R and NP-nR clones for their ability to form spheroids structures under similar conditions. NP-R clones produced spheroid structures on Matrigel, whereas growth of NP-nR clones appeared to be restricted to small adherent colonies (Figure 6C). Remarkably, on ACAN, the NP subtypes revealed similar responses: NP-R clones showed poor attachment and readily formed floating spheroids (Figure 6D). Spheroid formation occurred within 24 hours and was most prominent at 72 hours postplating. In contrast, NP-nR clones maintained surface adherence, and spheroid formation (that is, adherence) appeared only sporadically (see, for example, Figure 6D). These collective findings suggest that distinct biological responses are triggered in NP subtypes in the presence of ECM and that Matrigel and ACAN evoke gene-specific transcriptional responses in NP cells compared to standard monolayer differentiation assay conditions.
The application of human IVD material as a potential source of cell lines to date has been limited. Sakai et al. published their first immortalized HNPSV-1 cell line in 2004 . The authors of a recent report  described the generation of an NP cell line utilizing a distinct immortalization strategy that we employed in our present study. Despite the low number of studies in which investigators have utilized immortalized NP cell lines, such models provide valuable tools with which to study important aspects, such as the developmental origins of NP, NP cell biology disc degeneration, and can also aid in drug development and drug testing. In this report, we present the generation and thorough initial characterization of novel clonal human NP cell lines. We have established multiple NP cell lines starting from immortalized primary (P5) NP cultures derived from two independent donors. Importantly, analysis of immortal NP clones shows that multiple clonal subtypes can be distinguished based on morphological characteristics, marker gene expression and their diverse responses to differentiation conditions. We also report that ECM-assisted culture models further segregate the NP-R and nR phenotypes based on their spheroid-forming capacity in culture.
Nucleus pulposus marker expression
Several reported NP markers expressed by our immortal cell clones are consistent with a human NP phenotype and hence distinguish our primary NP and AF cultures. NP cell cultures typically synthesize COL2A1, ACAN and SOX9, whereas AF cells predominantly produce COL1A1 and considerably less COL2A1 . Cytokeratin 8 (CK8) and cytokeratin 19 (KRT19) have been suggested as potential NP markers [5, 33, 43]. Indeed, our NP primary cultures clearly segregated from AF cultures based on KRT19 mRNA expression. In line with the report of cell surface marker CD24 being able to identify the immature NP , we found CD24 expression in primary NP cells. Although none of the markers used in the present or previously published analyses are exclusively linked to AF, NP or AC tissue, the consistency of the quantitative differences we detected between AF- and NP-derived cultures further substantiates correspondence to their tissue of origin.
We report here, for the first time to the best of our knowledge, that the significant differences in marker expression between immortal NP subtypes isolated from immortalized primary cultures (CA12, CD24, FOXF1, PTN, PAX1 and COMP) discriminate human NP subtypes from two independent donors in primary monolayer cultures. Relevantly, the CA12, CD24, FOXF1 and KRT19 genes have been used successfully to study IVD-like differentiation of MSCs . Of note, throughout the present study, we used differentiation conditions that have previously been established for AC models. As the most optimal conditions for NP cell differentiation are currently unknown, some caution is warranted in direct translation of this data to the in vivo situation. Likewise, numerous animal studies have revealed NP markers that either fail as human NP markers or have not been evaluated in human IVD tissue. Thus, despite recent advances, a consistent definition of a NP marker signature for human cells in vivo is currently lacking [7, 46]. Investigators in recent gene expression array studies have identified additional markers that distinguish human NP cells from AC and/or AF cells [3, 5]. Similarly, gene expression analysis of distinctive immortalized cellular subtypes may prove useful in refinement of NP marker definition and is also expected to contribute to the development of robust differentiation protocols. Clearly, additional functional analyses are required to determine the role of NP markers in the development and pathology of the IVD.
Nucleus pulposus cell models and differentiation protocols
Using primary tissue from scoliosis patients as starting material justifies the question whether the primary culture and the immortalized cell cultures may contain degenerate cells. Although we cannot formally exclude this possibility based on our marker analysis, the IVD material we used for these studies was mainly obtained from the convex (that is, noncompressed) side of scoliotic discs. Of note, all available donors were relatively young. In addition, although the number of studies on DDD in the context of scoliosis are limited, DDD is rarely detected at this age, with the exception of cases with associated morbidity (for example, concurrent congenital spinal stenosis, body mass index >30, athletics) .
It is important to note that the application of immortal cell lines is restricted to in vitro analyses. Experimental application may be limited as a direct consequence of the immortalization procedure itself. For example, SV40LTag interferes with pRB and TP53 function; both proteins are involved in the programming of senescence, which may be relevant for the degeneration process [48–52]. However, the establishment of distinct NP clonal phenotypes reported herein (for the first time, to the best of our knowledge) provides access to a source of human NP cell models that will enable us to exploit differences in aspects such as cell surface marker expression to study NP cell biology. These immortalized NP cell models should thus be viewed as powerful complementary models to primary isolates.
The identification of distinct cell phenotypes among our immortalized NP cell clones reflects the cellular heterogeneity in vivo and provides important avenues for further study. Our observations reported herein support the notion that it is possible to fix different epigenetic states (that is, functional cellular heterogeneity) in the NP by means of immortalization procedures. Indeed, others have observed that cellular phenotypes are retained by immortalization . It is relevant to note that NP-R and NP-nR clonal outgrowth may have been subject to selection bias, as integration of retroviral DNA is dependent on active de novo DNA replication; as such, the heterogeneity in NP tissue may not be limited to the two subtypes described herein.
Many differentiation protocols have been optimized for SOX9, COL2A1 or GAG expression in AC cultures, and such protocols have been used to differentiate bone marrow– or adipose tissue–derived MSCs towards an NP-like phenotype . Also, TGFβ3 supplementation reproducibly promotes collagen and GAG synthesis in primary NP cells [31, 55]; yet, the exact conditions that faithfully support NP differentiation (and appropriately functioning matrix formation) have been reported throughout the literature to vary and thus appear not to be fully optimized (a parameter that is dependent on consensus definitions of NP phenotypes). Our observation that TGFβ3 repressed expression of novel NP markers in primary cells and cell clones is consistent with a recent report . Coculture experiments employing MSCs or conditioned media indicate that as yet unknown factors contribute to NP differentiation and/or phenotype stabilization [56–59]. The presence of Matrigel or ACAN produced a stronger induction of conventional chondrogenic markers in our clonal NP cell lines. Similarly, ACAN coating has been reported to induce a chondrocyte-like phenotype in primary fibroblasts, which upregulated COL2A1 and SOX9 but not ACAN, and primary meniscus fibrochondrocytes induced ACAN expression but not COL2A1 and SOX9 [19, 39]. Also, bone marrow stromal cells express ACAN in response to ACAN coating culture . Remarkably, we found that Matrigel and ACAN enhanced induction of COMP and COL2A1 expression, respectively. Although the mechanism by which ACAN affects differentiation is currently unclear, it is possible that ACAN functions to enhance growth factor signalling, as was recently shown for COMP . In this light, it would be of interest to determine the effect of ACAN coating on NP phenotype stability. Clearly, a much improved definition of NP maintenance and differentiation conditions is needed.
Nucleus pulposus cellular subpopulations
Evidence for the existence of a progenitor population in the adult human disc in vivo is accumulating [3, 10, 61, 62]. The immature NP contains NCs that harbour stem cell–like properties, and their lifelong presence in small laboratory animals, in contrast to humans, is thought to support tissue repair and thus prevent disc degeneration [63, 64]. NCs are replaced by smaller, rounded, chondrocyte-like cells in early human adulthood . As increasing evidence points to an ontogenic relationship between the notochord and the NP, , expression analysis of the NC marker T was of relevance to pinpointing the exact nature of our cell cultures. We found that T mRNA and T protein expression were very low and undetectable, respectively, in the primary isolates from which the immortal clones were derived. Only the primary NP isolate (D1P0) from the youngest donor (8 years old) had detectable T mRNA levels (Table 1). These data are consistent with reports that T expression disappears during human IVD maturation and is virtually undetectable from 10 years of age onwards [7, 67]. In keeping with this, the low or absent T expression in our immortal clones suggests that not NCs, but rather more mature NP cells, were immortalized.
On the basis of their morphology and ability to induce SOX9 and/or COL2A1 expression, we hypothesize that our different immortalized subtypes may represent more differentiated (NP-nR, cobblestone) or more progenitor-like (NP-R, wavelike) cell types. Importantly, we found both subtypes in two independent patient isolates (one male, one female). Both subtypes were CD44+, CD73+, CD90+ and CD105+, consistent with previously published data . CD24 and GD2 appeared to be more prominently present in our NP-nR clones than in NP-R clones, again supporting NP cell heterogeneity. Future characterization is needed to ascertain the ontogeny of the cloned cells.
The enhanced capacity to form spheroids under Matrigel and ACAN-supported culture conditions favours the notion that the NP-R cells represent a more progenitor or immature cell. Spheroid formation in culture is believed to mirror stem and progenitor capacity in any cell population. Lung-derived bronchospheres (or neurospheres, pancreatic) were previously shown to have stem cell– and progenitor-like characteristics [68, 69]. Indeed, spheroid formation was also recently used to identify progenitor cell presence in the IVD . The NP-R and NP-nR clones classify as GD2−/CD24− and GD2+/CD24+, respectively, and the spheroid-forming capacity of a subset of primary NP cells was recently used to propose a differentiation map for Tie2, GD2 and CD24 . Whether the phenotypes (chondrocyte-like, spheroid-forming and/or repopulating cells vs fibroblast-like cells) match our NP-R and NP-nR phenotypes and what role they fulfil in human NP development and disease remain to be determined. At this point, it is also premature to speculate about the ontogeny of these cells.
We report, for the first time to the best of our knowledge, the generation of phenotypically distinct immortal subclones from primary human NP tissue. Characterization of these clones suggests they correspond to discrete subpopulations in the NP, which differ in terms of morphology, cell surface NP marker expression and differentiation capacity. Interestingly, AC cell lines generated in the 20th century continue to provide important new insights into fundamental issues relating to AC cell biology ; thus, similarly immortal NP cell lines are expected to provide vital tools with which to study molecular mechanisms of NP cell ontogeny and cell function in the healthy and diseased IVD. It has become clear that the NP chondrocyte differs from AC; yet, there is currently no comprehensive, descriptive consensus regarding the NP phenotype. We advocate a systematic analytical coverage of isolation procedures, culture conditions and NP marker expression. The environmental interplay between chondrogenic factors and ECM proteins provides clues for further research. How to define the NP cell and how to faithfully mimic the NP microenvironment in vitro remain crucial questions to be resolved in the IVD field. Such issues will determine the success of cell replacement therapy and/or tissue engineering approaches to treating DDD.
Carbonic anhydrase XII
Cluster of differentiation 24
Collagen type I, α1
Collagen type II, α1
Cartilage oligomeric matrix protein
Degenerative disc disease
Forkhead box F1
Human telomerase reverse transcriptase
Induced pluripotent stem cell
Notochordal (precursor) cell
Nonresponder nucleus pulposus
Responder nucleosus pulposus
Paired box 1
Real-time quantitative polymerase chain reaction
Simian virus 40 large T antigen
Angiopoietin-1, tyrosine kinase receptor 2
Transforming protein 53.
The authors thank R Bernards (Netherlands Cancer Institute (NKI), Amsterdam, the Netherlands) for hTERT cDNA, S Brüderlein (University of Ulm, Germany) for the U-CH1 cell line, K Ito (Eindhoven University of Technology, the Netherlands) for useful discussions and sharing of protocols, R Bank (University of Groningen, the Netherlands) for suggestions on collagen detection and P Willems (Maastricht University Medical Centre, the Netherlands) for medical ethics reflections. Approval of all experimental sections of the present study and informed consent for publication of patient details and accompanying images were obtained as an integral part of approval 08-4-028 from Maastricht University Medical Centre/Maastricht Education and Research Centre. The approval is held by the authors and is available for review by the Editor-in-Chief of this journal. Funding was received from grant LLP14 from the Dutch Arthritis Foundation (to JWV and LWvR) and by a grant from the BMM-IDiDAS project (to LWvR and TJMW). RRP is supported by a grant from the Gulbenkian Programme for Advanced Medical Education, which is sponsored by the Calouste Gulbenkian Foundation, the Champalimaud Foundation, the Ministry of Health of Portugal and the Foundation for Science of Technology; and also by the Portuguese Association of the Pharmaceutical Industry.
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