Physioxia Promotes the Articular Chondrocyte-Like Phenotype in Human Chondroprogenitor-Derived Self-Organized Tissue

Abstract

Introduction:

Biomaterial-based tissue engineering has not successfully reproduced the structural architecture or functional mechanical properties of native articular cartilage. In scaffold-free tissue engineering systems, cells secrete and organize the entire extracellular matrix over time in response to environmental signals such as oxygen level. In this study, we investigated the effect of oxygen on the formation of neocartilage from human-derived chondrogenic cells.

Materials

and Methods: Articular chondrocytes (ACs) and articular cartilage progenitor cells (ACPs) derived from healthy human adults were guided toward cell condensation by centrifugation onto plate inserts that were uncoated or coated with either agarose or fibronectin. Neocartilage discs were cultured at hyperoxic (20%) or physioxic (5%) oxygen levels, and biochemical, biomechanical, and molecular analyses were used to compare the cartilage produced by ACs versus ACPs.

Results:

Fibronectin-coated inserts proved optimal for growing cartilaginous discs from both cell types. In comparison with culture in hyperoxia, AC neocartilage cultured at physioxia exhibited a significant increase in chondrogenic gene expression, proteoglycan production, and mechanical properties with a concomitant decrease in collagen content. At both oxygen levels, ACP-derived neocartilage produced tissue with significantly enhanced mechanical properties and collagen content relative to AC-derived neocartilage. Both ACs and ACPs produced substantial collagen II and reduced levels of collagens I and X in physioxia relative to hyperoxia. Neocartilage from ACPs exhibited anisotropic organization characteristic of native cartilage with respect to collagen VI of the pericellular matrix when compared with AC-derived neocartilage; however, only ACs produced abundant surface-localized lubricin.

Discussion and Conclusions:

Guiding human-derived cells toward condensation and subsequent culture in physioxia promoted the articular cartilage tissue phenotype for ACs and ACPs. Unlike ACs, ACPs are clonable and highly expandable while retaining chondrogenicity. The ability to generate large tissues utilizing a scaffold-free approach from a single autologous progenitor cell may represent a promising source of neocartilage destined for cartilage repair.

Introduction

Cartilage pathologies are the most common cause of chronic disability among adults in the United States, and early intervention to repair focal defects is key to restoring tissue integrity before chronic degeneration.^1–3 Unfortunately, successful surgical repair remains a challenge as the resultant tissues are usually fibrocartilaginous and cannot meet the functional demands of the joint.⁴ The limited long-term success of current strategies suggests a need for tissue engineering approaches to recapitulate the structural and biomechanical properties of articular cartilage.

In cartilage tissue engineering, biomaterials are used to provide initial structure; however, the resultant tissue phenotype is constrained by biomaterial influences.⁵ Over the past decade, a number of scaffold-free methods have emerged: self-assembled tissues, which form through cell interaction and condensation in the absence of external stimuli,^6–11 and self-organizing models relying on external cues to guide the cells toward condensation. For the latter, cells are typically centrifuged and/or cultured onto substrates such as porous polymer^12–17 or protein-coated membranes.^18–21 One goal of the current work was to develop a reliable and repeatable method to produce large-scale, scaffold-free neocartilage constructs. To this end, we hypothesized that fibronectin, which is the earliest extracellular matrix protein produced following cell condensation,^22,23 would provide necessary cues to drive cell condensation toward a defined geometry during in vitro tissue culture.

The selection of a cell type with high chondrogenic and anabolic capacities is essential to generate scaffold-free cartilage. Stem and progenitor cell populations mitigate the challenges of availability of primary chondrocytes and their phenotypic modulation during expansion. Articular cartilage progenitor cells (ACPs) are postulated to reside in the upper zone of adult cartilage after forming the tissue through appositional growth.^24–27 They can be clonally expanded in vitro and maintain differentiation potential following extended population doublings with minimal differentiation toward hypertrophy compared with mesenchymal stem cells (MSCs).^28,29 To date, tissue engineering utilizing human ACPs is limited to scaffold-based systems.^30,31

While cells within a scaffold-free tissue will determine tissue phenotype, the culture environment will guide tissue development. Without a blood supply, native articular chondrocytes (ACs) reside in physioxia ranging from 1% to 5% oxygen (8–40 mmHg).^32,33 We have previously shown that lowering oxygen from hyperoxia (20% O₂) to physioxia significantly enhances chondrogenesis of expanded human chondrocytes.³⁴ We have more recently discovered that the responses to altered oxygen tension for both MSCs and ACPs are dependent on the intrinsic chondrogenicity of the cells, and physioxia drives differentiation toward the stable phenotype for highly chondrogenic cells.³⁵ Thus, we sought to develop scaffold-free neocartilage from adult human cells in physioxia with optimization of medium volume and cell density to maintain tissue viability. The ACP clones used were chosen from those characterized in our prior work as highly chondrogenic.³⁵ We hypothesized that in comparison with heterogeneous ACs, clonal ACPs would generate tissue closer to the articular cartilage phenotype and that lowered oxygen tension would facilitate its extracellular matrix maturation.

Materials and Methods

Cell isolation

Normal human femoral condyles were obtained postmortem (n = 5 for AC, n = 3 for ACP) with Institutional Review Board approval at Oregon Health & Science University (Portland, OR) and the NHS Blood and Tissue bank (Liverpool, United Kingdom). Full-thickness human articular cartilage was dissected, minced, and digested as described previously.³⁵ Following digestion, ACs were expanded in low-glucose DMEM, 10% (v/v) fetal bovine serum (FBS), and 1% (v/v) penicillin/streptomycin (P/S). ACPs were isolated from separate donor tissue in the same manner as ACs through sequential pronase (70 U/mL for 20 min at 37°C) and type I collagenase (300 U/mL for 4 h at 37°C) digestion. Directly following cell isolation from tissue, ACPs were selected from the total chondrocyte population through differential adhesion to fibronectin,²⁷ and clonal populations were isolated with cloning rings. Colonies were expanded in monolayer in low-glucose DMEM/F12 (1:1), 10 mM HEPES, 10% (v/v) FBS, 1% (v/v) P/S, 0.1 mM ascorbic acid 2-phosphate (Wako), 1 ng/mL transforming growth factor β1 (TGF-β1; PeproTech), and 5 ng/mL FGF-2 (PeproTech). ACs and ACPs were plated at 1 × 10⁶ cells and expanded in atmospheric oxygen and 5% CO₂ through two passages. At final cell harvest, ACPs had undergone 22–24 population doublings from a single-cell origin and ACs had undergone 4 population doublings from a heterogeneous population.

Tissue culture

Both ACs and ACPs were passaged with TrypLE reagent (Life Technologies) and resuspended at a density of 2 × 10⁶ cells per 200 μL in serum-free chondrogenic differentiation medium.³⁶ Cell density was selected based on initial experiments with 1, 1.5, 2, or 3 × 10⁶ cells per tissue, whereby 2 × 10⁶ of each cell type reliably produced a tissue of maximum thickness; void tissue cores developed at higher cell seeding densities. Cell suspensions were pipetted into Transwell inserts (6.5 mm diameter, 0.4 μm pore size, polyester; Corning, Inc.), which were either uncoated, coated with 2% agarose (w/v), or coated with 50 μg/mL fibronectin (CalBioChem, Merck). The cell-laden inserts were centrifuged at 200 g for 5 min in 24-well plates with 1 mL medium below the membrane. Two days later, the inserts were suspended in 12-well plates containing 4.8 mL medium and cultured on an orbital shaker at 1 Hz frequency at 5% oxygen (physioxia) or at 20% oxygen (hyperoxia) and 5% CO₂. Medium was changed twice weekly, with physioxia maintained in a low oxygen chamber (BioSpherix) with pregassed medium. After 10 days, tissues were released from the membrane into free swelling culture in 0.9% w/v poly-2-hydroxyethylmethacrylate (poly-HEMA) (Sigma-Aldrich)-coated 12-well plates containing 3 mL differentiation medium, a minimum volume optimized for high cell densities based on our prior work. Cultures were maintained for 28 days with the originally membrane-oriented side facing upward.

Biochemical analysis

Triplicate samples from each condition were weighed, rinsed with phosphate-buffered saline (PBS), and digested overnight at 60°C in 4 U/mL papain (Sigma-Aldrich) in PBS containing 6 mM Na₂-ethylenediaminetetraacetic acid and 6 mM L-cysteine (papain buffer, pH 6.0). Total DNA and sulfated glycosaminoglycan (GAG) content were quantified using Hoechst dye and 1,9-dimethymethylene blue (DMMB) assays, respectively, as described previously.³⁴ Hydroxyproline content was quantified using an adaptation of the chloramine-T hydrate oxidation/p-dimethylaminobenzaldehyde method as described previously.³⁴

Biomechanical analysis

Mechanical properties of three replicates from each condition were tested in unconfined compression.³⁷ Sample dimensions were measured with a digital micrometer, and the tissue was subjected to a creep test under 0.02 N load until equilibrium was reached at ∼300 s. Upon equilibrium, iterative stress relaxation tests were performed at 1 mm/s to 10%, 20%, 30%, and 40% compressive strain to derive the equilibrium compressive Young's modulus at each ramp. Between each stress relaxation ramp, a dynamic test was carried out by applying 1% oscillatory strain at 1 Hz frequency to derive the dynamic modulus.

Gene expression analysis

RNA was isolated from three biological replicates in each condition. Tissues were pooled, snap-frozen, crushed, and lysed with buffer RLT (QIAGEN) containing 40 mM dithiothreitol (DTT). RNA isolation was performed with the RNeasy Mini Kit (QIAGEN) and reverse transcribed using qScript cDNA SuperMix (Quanta BioSciences). Quantitative polymerase chain reaction was performed with cDNA using a StepOnePlus thermal cycler (Life Technologies) with TaqMan Fast Advanced Master Mix and primers (Supplementary Table S1; Supplementary Data are available online at www.liebertpub.com/tea) according to previously reported parameters.³⁵

Histology and immunohistochemistry

Tissue from each condition was formalin-fixed, paraffin-embedded (FFPE), and sectioned or frozen in cold boiling hexanes, mounted in OCT, and sectioned. FFPE sections were deparaffinized, and frozen sections were fixed in 4% PFA at 4°C for 10 mins, before antigen retrieval. Toluidine blue (0.04% in 0.2 M acetate buffer, pH 4.0) was applied to visualize proteoglycans. For collagens I and II, pretreatment of FFPE sections with 1 mg/mL protease (Roche) in 1 × PBS for 30 min at room temperature was followed by 0.1% (w/v) hyaluronidase (Sigma-Aldrich) in 1X PBS for 45 min at 37°C. FFPE sections were pretreated with protease only for collagen X and frozen sections were pretreated with hyaluronidase only for perlecan. For lubricin and collagen VI, FFPE sections were pretreated in preheated citrate buffer (10 mM sodium citrate, 0.05% Tween-20, pH 6.0) for 5 min at 55°C and 550 Watts in a BioWave microwave (Ted Pella), followed by 0.1% hyaluronidase for 45 min at 37°C. All sections were blocked with 5% bovine serum albumin (BSA) in 1X PBS and incubated overnight at 4°C with primary antibodies to collagen I (1:200; kind gift from A Hollander, University of Bristol, Bristol, United Kingdom), collagen II (1:200; II-II6B3, Developmental Studies Hybridoma Bank, University of Iowa, Iowa City, IA), collagen X (1:300; kind gift from GJ Gibson, Henry Ford Hospital, Detroit, MI), perlecan (1:200; MAB1948P, Merck Millipore), lubricin (1:200; MABT401, Merck Millipore), or collagen VI (1:200; sc-20649, Santa Cruz Biotechnologies). Sections were washed with PBS and incubated for 45 min at room temperature with Oregon Green-conjugated goat anti-rabbit (1:250) or Alexa Fluor 596-conjugated goat anti-mouse (1:250) (Life Technologies) diluted in 1% BSA in 1 × PBS. Slides were mounted with ProLong Gold containing 4′,6-diamidino-2-phenylindole (DAPI; Life Technologies).

Collagen protein analysis

Enzyme-linked immunosorbent assays (ELISAs) were used to quantify collagens I and II. Discs were flash-frozen, pulverized, and lyophilized, then assayed according to manufacturer instructions (Chondrex; catalog #6018, #6021).

Statistical analysis

Three biological replicates were used for each ACP experiment (n = 3), five biological replicates were used for each AC experiment (n = 5), and three technical replicates were used for each analytical method. Normality for each condition in each cell type was assessed using a D'Agostino–Pearson omnibus K2 test, with normally distributed groups not meeting significance of p < 0.05 for distribution other than Gaussian. Comparison of biochemical parameters and gene expression between physioxia and hyperoxia within a given group was assessed using a paired t-test for normal data and Wilcoxon matched-pairs signed rank test for non-normal data, with significance set at p < 0.05. Comparison between normally distributed data of each cell type was performed with an unpaired t-test, with significance set at p < 0.05. Mean and standard deviation for fold change gene expression were calculated as physioxia relative to hyperoxia for each group.

Results

Fibronectin directs tissue geometry in scaffold-free constructs

Both ACs and ACPs formed flat discs of a defined geometry over 28 days of culture in a self-organization system through centrifugation, cell condensation on a fibronectin-coated membrane, and extracellular matrix elaboration (Fig. 1). In contrast, both cell types contracted into large pellets within 24 h of culture in inserts coated with 2% agarose, indicating that an adherent substrate was necessary to define tissue geometry in early scaffold-free constructs (Fig. 2). In agreement with prior work,¹⁸ ACs retained a flat disc morphology on uncoated porous polyester membranes, yet consistently lacked proteoglycans throughout the tissue depth. ACPs, however, contracted into large pellets within 24 h. When cultured on a fibronectin-coated porous polyester membrane, both cell types reliably formed a flat disc with proteoglycans produced throughout the depth (Fig. 2). As a primary objective of the study was to create tissues of a flattened and uniform disc shape, only tissues generated in fibronectin-coated Transwell inserts were used for the remainder of the experiments.

FIG. 1.

(A) Schematic representing stages of self-organization of scaffold-free neocartilage beginning with cell seeding through centrifugation onto a protein-coated membrane to direct cell condensation into a restricted geometry. Over the course of culture, cells produce an extracellular matrix that starts as an immature homogeneous matrix and matures over time with signals from the culture environment. (B) Gross images of AC- and ACP-derived neocartilage show that each cell type produced a disc of uniform dimensions after 28 days of culture. AC, articular chondrocyte; ACP, articular cartilage progenitor. Color images available online at www.liebertpub.com/tea

FIG. 2.

Toluidine blue histology and gross images demonstrate that human-derived ACs and ACPs formed a large pellet when cultured in nonadherent agarose wells after seeding into a flattened disc. Only ACs retained a disc morphology when cultured on porous polyester membranes, but both cell types retained a disc morphology when cultured on a polyester membrane coated with fibronectin. Scale bars = 400 μm. Color images available online at www.liebertpub.com/tea

Physioxia promotes biochemical anabolism of ACs

Compared with culture in hyperoxia, ACs in physioxia produced significantly more total GAGs; however, this increase was not significant when normalized to DNA content (Fig. 3). In contrast, ACPs did not produce significantly more GAGs in physioxia versus hyperoxia, but produced significantly more GAGs than ACs in hyperoxia, a difference retained with normalization to DNA. DNA content was not different between cell types and oxygen levels. There was no statistically significant difference in total collagen for either cell type between oxygen levels, but ACP-derived neocartilage contained significantly more collagen in physioxia compared with AC-derived neocartilage. There were no differences in wet weight or thickness between cell types and oxygen levels.

FIG. 3.

(A) Tissue wet weight and (B) thickness were not different between cell type and oxygen level. Quantitative measurements for biochemical constituents of neocartilage discs, including (C, E) GAGs as a readout for total proteoglycan content, (D) DNA for relative cell count, and (F) hydroxyproline for total collagen content, indicating that relative to hyperoxia, culture in physioxia significantly increased total GAG content for only ACs. ACPs, however, had a significantly higher total collagen content than AC culture in physioxia. Results reported as mean + SD, and statistical significance was determined as *p < 0.05 by a paired or unpaired t-test where appropriate. GAG, glycosaminoglycan.

Physioxia enhances the bulk mechanical properties of AC neocartilage, but ACP neocartilage is mechanically superior

AC-derived neocartilage cultured at physioxia had significantly higher compressive equilibrium modulus for stress relaxation tests at 10% and 20% strain than in hyperoxia (Fig. 4). It also exhibited strain-stiffening behavior—increasing in stiffness with increasing deformational compressive strain. The compressive equilibrium modulus for ACP-derived neocartilage was not different in physioxia versus hyperoxia, but was significantly higher than that for AC-derived neocartilage at matched oxygen level for each strain ramp, and with strain-stiffening behavior in physioxia. The dynamic modulus for 1% dynamic strain at 1 Hz frequency was not different between cell types and oxygen levels.

FIG. 4.

Quantitative analysis of (A) equilibrium compressive modulus reveals that scaffold-free neocartilage demonstrated strain-stiffening behavior, physioxia significantly increased the bulk compressive equilibrium modulus for AC neocartilage, and ACP neocartilage was significantly more stiff than AC neocartilage. There were no differences in (B) dynamic compressive modulus between cell types and oxygen levels. Results reported as a box plot, representing mean, the 1st and 3rd quartiles, and SD. Statistical significance was determined as *p < 0.05, **p < 0.01, and ****p < 0.0001 by a paired t-test within a cell type between oxygen levels, an unpaired t-test between cell types within a given oxygen level. Statistical significance between consecutive strain ramps for a given group was determined as #p < 0.05 to characterize strain stiffening. Chevron box represents a range of reported values for native adult articular cartilage.^45,54,55

Physioxia promotes the stable AC phenotype

Relative to culture in hyperoxia, ACs in physioxia had a significant fold change increase in expression of many genes associated with the articular phenotype (COL2A1, COL11A2, COL9A1, ACAN, SOX9, PRG4) and a significant decrease in genes of the fibrocartilaginous (COL1A1) and hypertrophic (MMP13) phenotypes (Fig. 5). COL10A1 was also consistently decreased among replicates, but not to a significant level. There was no difference between the gene expression profile for ACPs cultured in hyperoxia versus physioxia, although COL2A1, COL1A1, and COL10A1 were each changed in the same direction, but to a smaller magnitude. Genes coding for SOX9 and L-SOX5 were decreased in ACPs. Regardless of oxygen tension, COL2A1, ACAN, and COL1A1 were highly expressed for both ACs and ACPs relative to the housekeeping gene; PRG4 was highly expressed for ACs, but very low for ACPs.

FIG. 5.

Fold change in chondrogenic gene expression for culture in physioxia relative to hyperoxia demonstrates that (A) ACs, but not (B) ACPs, were highly responsive to oxygen level and upregulated genes representative of the articular cartilage phenotype in physioxia. Results reported as mean ± SD of log2-fold change, and statistical significance for comparison of mean expression in physioxia versus hyperoxia was determined as *p < 0.05 by a paired or unpaired t-test where appropriate.

Physioxia promotes articular cartilage matrix protein production

ACP- and AC-derived neocartilage had similar collagen II distribution (Fig. 6A). Collagen I was present throughout the matrix after 28 days of culture in hyperoxia, but more localized to the outer edges in physioxia for both cell types. Collagen X was detectable for AC-derived neocartilage cultured in hyperoxia, but undetectable in physioxia. In contrast, it was undetectable in all ACP-derived neocartilage regardless of oxygen tension. ACPs expressed more collagen II than I protein and expressed significantly less collagen I than ACs, even though ACs had an improved II:I ratio in physioxia (Fig. 6B). AC-derived neocartilage produced lubricin that was primarily localized to the side contacting the well that was agitated during culture. This expression was independent of oxygen tension (Fig. 7). In contrast, lubricin was not detectable in ACP-derived neocartilage. Investigation of pericellular proteins revealed that perlecan was distributed throughout the bulk of matrix for both cell types, while collagen VI was more pericellular for only ACPs; both protein distributions were independent of oxygen level.

FIG. 6.

(A) Collagen immunohistochemistry demonstrates consistently high collagen II expression in tissues derived from both ACs and ACPs in hyperoxia and physioxia, but reduced collagen I for both AC- and ACP-derived tissues in physioxia relative to hyperoxia. AC-derived neocartilage had low collagen X expression in hyperoxia that was undetectable in physioxia, but ACP-derived neocartilage lacked collagen X at both oxygen levels. (B) Quantification of collagen by ELISA indicates that ACP-derived neocartilage contained more collagen II and I regardless of oxygen level, but AC-derived neocartilage increases the ratio of collagen II to collagen I with culture in physioxia relative to hyperoxia. Scale bars = 100 μm. Color images available online at www.liebertpub.com/tea

FIG. 7.

Immunohistochemistry of lubricin, perlecan, and collagen VI revealed that only AC-derived neocartilage produced lubricin that was localized to the surface regardless of oxygen level. In addition, independent of oxygen level, neocartilage from both cell types produced perlecan that was distributed throughout the extracellular matrix, and ACP-derived neocartilage had collagen VI localized to the pericellular matrix, while collagen VI was distributed throughout the entire extracellular matrix for AC-derived neocartilage. Scale bars = 100 μm for lubricin and perlecan, 20 μm for collagen VI. Color images available online at www.liebertpub.com/tea

Discussion

Expanded adult human chondrocytes contracted into pellets in nonadherent culture, but produced a disc-like tissue morphology when cultured on a polymer substrate, consistent with a previous report.²¹ However, ACPs needed a fibronectin substrate initially. Fibronectin is the earliest expressed extracellular matrix molecule during cell condensation^22,23 and this, plus the high binding affinity between fibronectin and ACPs during their isolation, informed our decision to employ fibronectin, as opposed to other matrix molecules previously used to guide scaffold-free self-organization.²¹ The ability to define tissue morphology in a scaffold-free approach will ultimately be necessary to develop personalized therapies for focal cartilage defect repair. To this end, other groups have recently developed sophisticated molds to guide cell condensation into large-scale cartilaginous tissues.^17,38 As a foundation for ACPs as a novel cell type in scaffold-free tissue engineering, we found that these cells generated uniform discs when simply cultured on fibronectin-coated membranes.

This is the first report of scaffold-free tissue engineering utilizing ACPs. Few studies have extensively investigated scaffold-free tissue engineering from adult human-derived cells; the only study to directly compare scaffold-free tissues generated from adult human chondrocytes and MSCs used a single biologic donor for each.³⁹ Studies of scalable scaffold-free techniques indicate that neonatal mammalian primary chondrocytes build tissues with characteristics of articular cartilage following self-assembly^6,9 or self-organization.¹⁸ However, it was not clear whether these were viable strategies to generate tissues with adult human-derived cells, which are limited in metabolism and expansion potential in comparison with neonatal or juvenile mammalian cells.^40,41

One study suggested that low oxygen is detrimental to the development of scaffold-free neocartilage,²⁰ but we posit that the central voids found were the result of tissue anoxia from nutrient deprivation, previously characterized by both diffusion modeling and oxygen delivery experiments.^42,43 We generated tissues without a central void through optimization of cell seeding density and medium volume. In accordance with our previous data from redifferentiating expanded human chondrocytes in pellet culture,^34,35 physioxia promoted the stable chondrocyte phenotype in scaffold-free discs. Lowering oxygen stabilizes hypoxia-inducible factors (HIFs), which are targeted for proteasomal degradation in the presence of oxygen. HIFs, in turn, regulate genes with hypoxia-responsive elements (HREs), drive chondrogenesis toward the AC phenotype, and modulate extracellular matrix metabolism.⁴⁴ In physioxia, ACs significantly upregulated genes with HREs, including SOX9 and PRG4, which also led to a downstream increase in SOX-9 targets—COL2A1 and ACAN. Although all ACP clones upregulated COL2A1 in physioxia, the response was not statistically significant. We have previously shown that the response of postnatal human stem cells to lowered oxygen depends on the intrinsic chondrogenic differentiation capacity, and highly chondrogenic ACP clones were less responsive at the gene level than poorly chondrogenic clones. We therefore did not expect significant differences in the ACP gene expression based on our prior results with these same cells in pellet culture.³⁵ The only significant difference in gene expression between hyperoxia versus physioxia for ACPs was decreased SOX9, possibly a consequence of examining gene expression after 28 days of culture—a time point much later than the induction of differentiation by TGF-β and physioxia when SOX9 is promoted. Both cell types consistently downregulated COL10A1 of the hypertrophic chondrocyte phenotype, and ACs significantly downregulated COL1A1 and MMP13; results were consistent with our previous work exploring the role of physioxia in regulating hypertrophy.^34,35 However, it is important to point out that ACP expression of these genes/proteins is minimal even in hyperoxia for the highly chondrogenic clones selected for this work based on our prior studies.³⁵

Culture in physioxia significantly increased the bulk equilibrium modulus for AC-derived neocartilage, concomitant with increased total GAG production. Consistent with our prior results,³⁵ the highly chondrogenic ACP clones used in this study were less responsive to lowered oxygen tension with respect to GAG synthesis in comparison with ACs. These cells, however, produced significantly more GAGs in hyperoxia than ACs and had likely reached a maximum rate of proteoglycan synthesis regardless of oxygen tension. While compressive stiffness directly correlates with proteoglycan content in native tissue,⁴⁵ a >10-fold higher equilibrium modulus of ACP- relative to AC-derived tissue was not attributable only to proteoglycan content based on equivalent GAG levels in physioxia. These differences in compressive stiffness that are not attributable to proteoglycan content likely involve other constituents of the extracellular matrix, including collagen. There were not only differences in the total collagen content but also in the collagen types between AC- and ACP-derived tissues, with more collagen II in ACP-derived neocartilage. Increased collagen may be complemented by greater collagen crosslinking in physioxia through lysyl oxidase, which has an HRE, to drive a further increase in compressive modulus similar to mechanisms of postnatal native tissue maturation.⁴⁶ Previous studies have shown that lowered oxygen increases collagen crosslinking in scaffold-free tissues generated from primary bovine chondrocytes.⁸ In physioxia, both AC- and ACP-derived neocartilage exhibited strain-stiffening behavior—a property of the collagen network of mature articular cartilage that immature postnatal tissues lack⁴⁶—possibly due to enhanced collagen crosslinking. Unlike the compressive equilibrium modulus, the dynamic modulus was not different between tissue types and oxygen levels. In native tissue, dynamic modulus is proportional to collagen content;⁴⁵ however, ACP-derived neocartilage did not have a significantly higher dynamic modulus despite increased collagen content in physioxia. This may be a consequence of the relatively low total collagen content and dynamic stiffness in all neocartilage discs in comparison with native tissues.

Further investigation of the extracellular matrix revealed that the collagen expression profile was improved with culture in physioxia relative to hyperoxia for neocartilage from both ACs and ACPs—maintaining global collagen II expression, but apparently decreasing collagens I and X throughout the tissues. These results are consistent with those for pellet culture of each cell type.^34,35 In comparison with ACPs, ACs produced significantly more collagen I in hyperoxia—results that are consistent with known collagen profiles following expansion and dedifferentiation of chondrogenic cells.^47,48 Consistent with gene expression data, ACs responded favorably to lowered oxygen with a reduction in collagen I toward the level of ACPs, resulting in an increase in the ratio of collagen II to collagen I more similar to the phenotype of native articular cartilage. Regardless of oxygen tension, AC-derived neocartilage did not show evidence of pericellular matrix localization of collagen VI or perlecan, with these proteins expressed throughout the bulk of the matrix. In contrast, ACP-derived neocartilage had collagen VI localized to the pericellular matrix after 28 days. Since these proteins are distributed throughout the matrix in neonatal cartilage and subsequently localized to the pericellular matrix with maturation,^49,50 this result suggests greater matrix maturity for ACP-derived neocartilage.

Independent of oxygen level, ACs produced lubricin, localized primarily to one surface of the disc. In contrast, ACPs did not produce detectible amounts of lubricin. Chondroprogenitors have recently been identified by PRG4 expression²⁶ or lubricin production^51,52 in vivo, but this is the first study to investigate lubricin and PRG4 expression during in vitro differentiation of ACPs. Lack of PRG4 and lubricin expression may indicate that these cells are subject to phenotypic modification when isolated, cloned, expanded, and/or differentiated in vitro. Alternatively, ACPs may represent a progenitor population up- or downstream from the PRG4-expressing lineage identified in vivo^26,53 or the cell populations may be entirely distinct; these remain future topics for investigation.

Our results indicate that physioxic culture is beneficial for neocartilage development toward the articular cartilage phenotype. Highly chondrogenic ACP clones produced a tissue that was mechanically superior and more mature than tissues derived from ACs. Unlike ACs, ACP discs were derived from a single cell following clonal isolation and expansion. The ability to produce large-scale scaffold-free constructs of a defined geometry from this adult human cell source may eventually allow us to generate tissues that satisfy the structural and functional demands required for articular cartilage repair and thus be able to offer personalized and autologous therapies for focal articular cartilage injuries.

Footnotes

Author's Contributions

D.A. contributed to study conception, experimental design, cell and tissue culture, biochemical analyses, statistical analyses, and manuscript preparation. B.M. contributed to study conception, experimental design, and manuscript revision. K.W. contributed to histological analyses and manuscript revision. H.M. contributed to cell and tissue culture and manuscript revision. B.J. contributed to study conception, experimental design, result analyses, and manuscript revision. All authors have read and approved the manuscript.

Acknowledgments

The authors thank the following surgeons for providing human tissue: Dr. Dennis Crawford at Oregon Health and Science University (OHSU) and Dr. Paul Rooney at the NHS Blood and Tissue bank (Liverpool, United Kingdom) for providing healthy human articular cartilage. The authors would like to thank Ms. Teresa Pizzuto at Case Western Reserve University for technical assistance in histologic specimen processing. Finally, the authors would like to thank Dr. Robert Mauck and Breanna Seiber at the University of Pennsylvania for providing tools and assistance in characterization of mechanical properties of neocartilage. This work was supported by funding from NIH/NIAMS (1R21AR064431) and the OHSU Foundation.

Disclosure Statement

No competing financial interests exist.

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