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Several prior studies have been performed to determine the feasibility of tissue decellularization to create a non-immunogenic xenogenic tissue replacement for bladder, vasculature, heart valves, knee meniscus, temporomandibular joint disc, ligament, and tendon. However, limited work has been performed with articular cartilage, and no studies have examined the decellularization of tissue engineered constructs. The objective of this study was to assess the effects of different decellularization treatments on articular cartilage constructs, engineered using a scaffoldless approach, after 4 wks of culture, using a two-phased approach. In the first phase, five different treatments were examined: 1) 1% SDS, 2) 2% SDS, 3) 2% Tributyl phosphate, 4) 2% Triton X-100, and 5) Hypotonic followed by hypertonic solution. These treatments were applied for either 1 h or 8 h, followed by a 2 h wash in PBS. Following this wash, the constructs were assessed histologically, biochemically for cellularity, GAG, and collagen content, and biomechanically for compressive and tensile properties. In phase II, the best treatment from phase I was applied for 1, 2, 4, 6, or 8 h in order to optimize the application time. Treatment with 2% SDS for 1 h or 2 h significantly reduced the DNA content of the tissue, while maintaining the biochemical and biomechanical properties. On the other hand, 2% SDS for 6 h or 8 h resulted in complete histological decellularization, with complete elimination of cell nuclei on histological staining, although GAG content and compressive properties were significantly decreased. Overall, 2% SDS, for 1 or 2 h, appeared to be the most effective agent for cartilage decellularization, as it resulted in decellularization while maintaining the functional properties. The results of this study are exciting as they indicate the feasibility of creating engineered cartilage that may be non-immunogenic as a replacement tissue.
Injuries to articular cartilage, whether traumatic or from degeneration, generally result in the formation of mechanically inferior fibrocartilage, due to the tissue’s poor intrinsic healing response. As such, tissue engineering strategies have focused on developing replacement tissue in vitro for eventual in vivo implantation. One such strategy employs a “self-assembly process” in which chondrocytes can be used to form robust tissue engineered constructs without the use of a scaffold.
Although engineered articular cartilage tissue has recently been created with biochemical and biomechanical properties in the range of native tissue values,  there are currently two significant limitations to cartilage tissue engineering. First, human cells are scarce in number and difficult to procure, and passage of these cells leads to dedifferentiation.  These issues make the use of autologous cells for cartilage repair difficult. Additionally, the majority of cartilage tissue engineering approaches have employed bovine or other animal cells, and tissues grown from these cells are xenogenic. Thus, their use may result in a severe immune response following implantation, though this has not been fully elucidated.
It is believed that a decellularized xenogenic tissue may be a viable option as a replacement tissue, as the antigenic cellular material will be removed while preserving the relatively non-immunogenic extracellular matrix (ECM), as described in an earlier review.  Ideally, this will also preserve the biomechanical properties of the tissue. For instance, an acellular dermal matrix has seen successful use clinically as the FDA approved Alloderm product. Additionally, acellular xenogenic tissues have been created for many musculoskeletal applications, including replacements for the knee meniscus,  temporomandibular joint disc,  tendon,  and ACL,  as well as in other tissues including heart valves, [11–17] bladder,  artery,  and small intestinal submucosa.[20, 21]
However, studies demonstrating the effects of tissue decellularization on cartilage are limited,  and there are no studies demonstrating the effects of decellularization on musculoskeletal tissue engineered constructs. In the only other study examining cartilage decellularization,  a photo-oxidation approach was employed to decellularize bovine xenografts, after which they were implanted in vivo into a sheep model. It was determined that the photo-oxidation approach, which resulted in nonviable chondrocytes, resulted in a reduced monocyte and plasma cell infiltration in the implant after 6 months. In this study, the primary benefit of using an approach involving tissue engineered cartilage constructs, rather than explants, is the potential to modulate the geometry and functional properties of the construct to match those of a specific patient or joint surface. Additionally, xenograft approaches are appealing, as animal tissue provides a relatively limitless and cost-effective cell source. However, decellularization of the xenograft tissue may be required to eliminate the immunogenicity of the tissue. While the use of decellularized xenograft explants can also be considered, both approaches must be explored before determining which approach should be pursued. As such, we are also pursuing an explant-based approach.
Therefore, the objective of this study was to determine the effects of multiple decellularization treatments on tissue engineered construct cellularity, biochemical, and biomechanical properties. A two-phased approach was used in which an appropriate agent for decellularization was selected in phase I, and an appropriate treatment time was selected in phase II. It was hypothesized that cells could be removed from self-assembled constructs while preserving the biochemical and biomechanical properties. To test this hypothesis, self-assembled articular cartilage constructs were cultured for 4 wks, and then treated with 1% sodium dodecyl sulfate (SDS), 2% SDS, 2% Tributyl Phosphate (TnBP), 2% Triton X-100, or a hypotonic/hypertonic solution, for either 1 or 8 h. These treatments were selected from prior literature, [7–17, 20, 21] as well as from pilot experiments in our lab. Next, the treatment selected in phase I was applied for 1, 2, 4, 6, or 8 h in phase II. The effects of the decellularization treatments were assessed on construct cellularity and functional properties.
Cartilage was harvested from the distal femur of wk-old male calves[24–26] (Research 87, Boston, MA) shortly after slaughter, and chondrocytes were isolated following digestion with collagenase type 2 (Worthington, Lakewood, NJ). To normalize variability among animals, each leg came from a different animal, and cells from all legs were combined together to create a mixture of chondrocytes; a mixture of cells from five legs was used in the study. Cell number was determined on a hemocytometer, and a trypan blue exclusion test indicated that viability remained >90%. Chondrocytes were frozen in culture medium supplemented with 20% FBS (Biowhittaker, Walkersville, MD) and 10% DMSO at −80°C for 1 day prior to use. After thawing, viability was greater than 90%. To construct each agarose well, sterile, molten 2% agarose was added to wells of a 48-well plate, and a stainless steel mold consisting of 5 mm dia. × 10 mm long cylindrical prongs was placed into a row of the plate to construct the cylindrical molds. The agarose solidified at room temperature for 60 min, after which the mold was removed from the agarose. Two changes of culture medium were used to completely saturate the agarose well by the time of cell seeding. The medium was DMEM with 4.5 g/L-glucose and L-glutamine (Biowhittaker), 100 nM dexamethasone (Sigma, St. Louis, MO), 1% Penicillin/Streptomycin/Fungizone (P/S/F) (Biowhittaker), 1% ITS+ (BD Scientific, Franklin Lakes, NJ), 50 μg/mL ascorbate-2-phosphate, 40 μg/mL L-proline, and 100 μg/mL sodium pyruvate (Fisher Scientific, Pittsburgh, PA). To seed each construct, 5.5 × 106 cells were added in 100 μl of culture medium. Constructs formed within 24 h in the agarose wells and were cultured in the same well until t=10 days, after which they were unconfined for the remainder of the study, as described previously; t=0 was defined as 24 h after seeding. Throughout the studies, constructs were cultured in an incubator at 37°C and 10% CO2.
At t=4 wks, self-assembled constructs (n=6/group) were removed from culture and exposed to one of five decellularization treatments, for either 1 h or 8 h. The decellularization treatments included:
All treatments included 0.5 mg/ml DNase Type I, 50 μg/ml RNase, 0.02% EDTA, and 1% P/S/F, in PBS. Both 1 h control and 8 h control groups were exposed to this same solution without detergent treatments. These treatments were applied at 37°C with agitation. Following the 1 h or 8 h treatment, the constructs were washed for 2 h in PBS at 37°C with agitation. Additionally, an untreated control was assessed immediately following construct removal from culture, without the treatment or wash steps.
At t=4 wks, self-assembled constructs (n=6/group) were removed from culture and exposed to 2% SDS for 1, 2, 4, 6, or 8 h. As in phase I, all treatments included 0.5 mg/ml DNase Type I, 50 μg/ml RNase, 0.02% EDTA, and 1% P/S/F, in PBS. These treatments were applied at 37°C with agitation. Following the SDS treatment, the constructs were washed for 2 h in PBS at 37°C with agitation. Additionally, an untreated control was assessed immediately following construct removal from culture, without the treatment or wash steps.
After freezing, samples were sectioned at 14 μm. To determine construct cellularity, a hematoxylin & eosin (H&E) stain was used. A Safranin-O/fast green stain was used to examine GAG distribution, [28, 29] and picrosirius-red was employed for collagen content.
Samples were frozen overnight and lyophilized for 48 h, followed by re-suspension in 0.8 mL of 0.05 M acetic acid with 0.5 M NaCl and 0.1 mL of a 10 mg/mL pepsin solution (Sigma) at 4°C for 72 h. Next, 0.1 mL of 10x TBS was added along with 0.1 mL pancreatic elastase and mixed at 4°C overnight. A Picogreen® Cell Proliferation Assay Kit (Molecular Probes, Eugene, OR) was used to assess total DNA content. GAG content was quantified using the Blyscan Glycosaminoglycan Assay kit (Biocolor), based on 1,9-dimethylmethylene blue binding. [30, 31] After hydrolysis with 2 N NaOH for 20 min at 110°C, total collagen content was determined using a chloramine-T hydroxyproline assay.
Samples were assessed with an indentation apparatus, as described previously.  A 0.7 g (0.007 N) mass was applied with a 1 mm flat-ended, porous indenter tip, and specimens crept until equilibrium, as described elsewhere.  For the constructs treated for 1 h with the hypotonic/hypertonic solution and 8 h with 1% SDS, 2% TnBP, or 2% Triton X-100, a 0.27 g (0.0027 N) mass was applied instead such that all constructs would experience a similar strain during indentation testing. Examined over the entire study, strains from 3–9% were recorded. The thickness was measured using digital calipers with accuracy to 0.01 mm. Preliminary estimations of the aggregate modulus of the samples were obtained using the analytical solution for the axisymmetric Boussinesq problem with Papkovich potential functions. [34, 35] The sample biomechanical properties, including aggregate modulus, Poisson’s ratio, and permeability were then calculated using the linear biphasic theory. 
A uniaxial materials testing system (Instron Model 5565, Canton, MA) was employed to determine tensile properties with a 50 N load cell, as described previously. Briefly, samples were cut into a dog-bone shape with a 1-mm-long gauge length. Samples were glued to paper tabs with cyanoacrylate glue outside of the gauge length. The 1-mm-long sections were pulled at a 1% constant strain rate. All samples broke within the gauge length. The gauge length, thickness, and initial cross-sectional area were measured using digital calipers. For each construct, a stress-strain curve was created from the load-displacement curve and the Young’s modulus was calculated from each stress-strain curve using the initial cross-sectional area.
All biomechanical and biochemical assessments were made using n=6. In phase I, the three control groups were compared using a single factor ANOVA. As no difference was noted, only the culture control was used in the final analysis. To compare treatment groups in both phases, a single factor ANOVA was used, and a Tukey HSD post hoc test was used when warranted. Significance was defined as p< 0.05.
In all groups, the construct diameter was approximately 6 mm at 4 wks. In phase I, treatment for 8 h with either 1% SDS or the hypotonic/hypertonic solution resulted in a significant decrease in construct thickness (Table I). Additionally, treatment for 8 h with 1% SDS, 2% SDS, 2% Triton X-100, or the hypotonic/hypertonic solution resulted in a significant decrease in construct wet weight (Table I). In phase II, treatment with 2% SDS for 6 h or 8h resulted in a significant decrease in construct thickness and wet weight (Table II).
Figure 1 displays the histological results of phase I. Extensive staining for cell nuclei was observed in the H&E staining of the control group. Treatment with 1% SDS for 1 h reduced the number of cell nuclei, while treatment for 8 h eliminated all nuclei from the construct. The 2% SDS treatment had similar results. However, treatment with 2% TnBP or 2% Triton X-100, for either timepoint, had no effect on the number of nuclei. Both hypotonic/hypertonic treatments resulted in a slight reduction in number of cell nuclei. All decellularization treatments for 8 h resulted in a significant reduction or complete elimination of staining for GAGs. Additionally, 1 h treatment with the hypotonic/hypertonic solution reduced the GAG content. However, there were no apparent differences in GAG staining among the 1 h treatments with 1% SDS, 2% SDS, 2% TnBP, 2% Triton X-100, and the control. Finally, all constructs demonstrated extensive staining for collagen.
Figure 2 displays the histological results of phase II. Extensive staining for cell nuclei was observed in the H&E staining of the control group. Increasing decellularization was observed with 2% SDS treatment from 1–4 h, while 6 or 8 h application times were required for complete histological decellularization. Treatment for 1 and 2 h resulted in maintenance of GAG and collagen staining, while the 4 h treatment resulted in decreased staining. However, treatment for 6 and 8 h resulted in no GAG staining and poor collagen staining.
In phase I, several decellularization treatments resulted in a significant reduction in construct DNA (Fig. 3). Treatment for 1 h with 2% SDS or the hypotonic/hypertonic solution, as well as 8 h treatment with 1 or 2% SDS or the hypotonic/hypertonic solution all resulted in a significant reduction of the DNA in the constructs. However, treatment with 2% TnBP or 2% Triton X-100 for either amount of time had no effect on construct DNA. In phase II, all application times resulted in a significant decrease in DNA content, although treatment for 8 h resulted in the greatest decrease (Fig. 4).
For phase I, the effects of the decellularization agents on construct GAG content are found in Fig. 5a. Treatment with 1% or 2% SDS for 1 h had no effect on GAG content, while all other treatments significantly reduced the GAG content of the constructs. Additionally, all 8 h treatments resulted in complete or nearly complete removal of GAG from the constructs. Finally, there were no significant changes in total collagen content following treatment with the decellularization agents (Fig. 5b). For phase II, the effects of the decellularization agents on construct GAG content are found in Fig. 5c. Treatment with 2% SDS for 1 or 2 h maintained GAG content, while 4 h treatment resulted in a significant decrease in GAG content. However, treatment for 6 or 8 h resulted in complete elimination of GAG. Treatment for 1, 2, 4, or 6 h did not significantly alter the collagen content, while treatment for 8 h resulted in a slight decrease in collagen content, as shown in Fig. 5d.
For phase I, the effects of the various decellularization treatments on construct aggregate modulus are displayed in Fig. 6a. Treatment for 1 h with 1% or 2% SDS as well as with 2% TnBP maintained the aggregate modulus. However, treatment for 8 h with 1% SDS, 2% TnBP, and 2% Triton X-100 significantly reduced the aggregate modulus. The groups treated for 8 h with either 2% SDS or the hypotonic/hypertonic solutions were too weak to be mechanically tested with creep indentation. Additionally, the effects of the various decellularization treatments on Poisson’s ratio and permeability are displayed in Table III. A significant decrease in Poisson’s ratio was noted for the groups treated for 8 h with 1% SDS, 2% TnBP, and 2% Triton X-100. Finally, only treatment for 8 h with 1% SDS resulted in a significantly decreased permeability. Figure 6b indicates the tensile properties of the constructs treated with the various agents in phase I. Treatment for 1 h with 1% SDS, 2% TnBP, or 2% Triton X-100 maintained the Young’s modulus. A 1 h treatment with 2% SDS actually increased the Young’s modulus. However, 8 h treatments with 2% SDS, 2% TnBP, and 2% Triton X-100 significantly decreased the Young’s modulus.
For phase II, the effects of the various application times on construct aggregate modulus are displayed in Fig. 6c. There was no significant difference in aggregate modulus with treatment for 1 and 2 h, while the 4 h treatment significantly reduced the stiffness. Additionally, the 6 and 8 h treatment resulted in constructs that were untestable in compression. As shown in Table IV, the 1, 2, and 4 h treatments did not result in significant changes in permeability and Poisson’s ratio. Figure 6d displays the tensile properties of the constructs treated in phase II. Treatment with 2% SDS for 1 h resulted in a slight increase in tensile properties, although this was not significant. Treatment for 2 and 4 h maintained the Young’s modulus while treatment for 6 h resulted in a reduced Young’s modulus. Constructs treated for 8 h were untestable in tension.
The objective of this study was to assess the effectiveness of multiple decellularization protocols on self-assembled articular cartilage constructs, and to determine an appropriate application time for the treatment. A two-phased approach was used. In phase I, a two-factor approach was employed, in which five different treatments were examined at two application times each. In phase II, the effects of multiple treatment times were examined.
The results of this study indicated that SDS, at concentrations of either 1% or 2%, is an effective treatment for tissue decellularization, thus confirming our hypothesis that the number of cells could be significantly reduced from engineered constructs. An ionic detergent, SDS typically is able to solubilize the nuclear and cytoplasmic cell membranes. Although all SDS treatments led to cell removal, treatment with 2% SDS appeared the most promising, although application time also had significant effects. For instance, treatment with 2% SDS for 1 h resulted in a 33% decrease in DNA content, while maintaining both GAG and collagen content, as well as maintaining the aggregate modulus. This treatment even resulted in an increase in Young’s modulus; a similar increase in tensile properties was observed in a study of ACL decellularization. On the other hand, treatment with 2% SDS for 8 h led to complete histological decellularization, with complete elimination of all cell nuclei on histological staining, as well as a 46% decrease in DNA content. However, this treatment also resulted in loss of all GAG and significant reduction in aggregate modulus, as well as a decrease in Young’s modulus. Treatment with 2% SDS for 8 h also resulted in a significant decrease in construct wet weight, presumably as a result of the GAG loss, which would also decrease the tissue hydration. As 2% SDS for 8 h resulted in the greatest decrease in DNA content, and treatment for 1 h maintained or increased biomechanical and biochemical properties, 2% SDS was selected for use in phase II.
The assessed histological, biochemical and biomechanical properties of the untreated tissue engineered constructs are in the range of the starting immature bovine cartilage, although the tensile properties are only about 10–15% of native tissue. For instance, the aggregate modulus of immature bovine cartilage is 252±31, the Young’s modulus is 7.2±4.6 MPa, the GAG/WW is 0.04±0.03 mg/mg, and the collagen/WW is 0.13±0.01 mg/mg. Additionally, the constructs treated for 1 h with 1% SDS, 2% SDS, and 2% TnBP had an aggregate modulus, GAG/WW, and collagen/WW in the range of native tissue. However, the tensile properties of the tissue are lacking compared to those of native tissue. Therefore, 2% SDS treatment for 1 h, with a significant increase in Young’s modulus, results in a value closer to that of native tissue. Additionally, it is important to note that ‘control’ constructs from our prior tissue engineering studies were used as the starting point in this study, due to ease of use; however, with the use of growth factor application and mechanical stimulation such as hydrostatic pressure, we have achieved an aggregate modulus, GAG/WW, and collagen/WW matching those of native tissue, and a Young’s modulus approaching 50% of that of native tissue.[3, 38, 39] It is believed that the aggregate modulus and Young’s modulus likely will be the most important properties to match to native tissue in future tissue engineering approaches. Similar biomechanical properties between the implanted construct and the surrounding native tissue will prevent added stress at the interface site. The Poisson ratio, a measure of the tissue’s apparent compressibility, and the permeability, a measure of the resistance to fluid flow, should also approach native tissue values in order to achieve similar deformations and fluid movement under joint loading.
Treatment with 2% SDS for 1 h resulted in tissue decellularization while maintaining construct functional properties. Although SDS at all application times led to decellularization, 6 or 8 h was required for complete histological decellularization. However, these timepoints resulted in complete removal of GAG as well as an extremely poor aggregate modulus. However, the reduction in collagen content and tensile properties was less pronounced. On the other hand, as in phase I, treatment for 1 h resulted in a significant reduction in DNA content, while maintaining all biochemical and biomechanical properties, and even increasing Young’s modulus. The observed increase in Young’s modulus with a 1 h application of SDS suggests an effect of the detergent on collagen fibers within the engineered construct. SDS is known to have a propensity to disrupt non-covalent bonds in proteins and confer negative charges on proteins that have been denatured. The application of SDS for 1 h followed by a wash step may have had a transient effect on collagen architecture, wherein collagen fibers unfold as described previously,  and then return to their native conformations, reforming non-covalent bonds and strengthening interactions in the process. The putative mechanism may have led to the observed increased Young’s modulus at 1 h. With greater time in SDS, the effect is not observed, suggesting that any recovery undergone by collagen is counterbalanced by the detergent’s aggregate effect on the rest of the tissue architecture.
It must be noted that although treatment with 2% SDS for 6 or 8 h resulted in complete histological decellularization, it did not result in complete elimination of DNA, which would be defined as ‘complete decellularization.’ It appeared that SDS treatment was effective at achieving complete lysis of cell membranes and nuclear membranes, as H&E staining did not reveal any indication of the presence of cell nuclei, while the DNase treatment was not completely effective in degrading the DNA following membrane lysis. It is possible that a higher DNase concentration is required to achieve more complete elimination of DNA. Additionally, as nucleases were only added during detergent treatment, it is possible that adding a nuclease during the wash step would enable the nucleases to more effectively destroy the remaining DNA.
However, the exact level of tissue decellularization requisite to eliminate an immune response, as well as the proper assessment of decellularization, is currently unclear. For instance, a recent study by Gilbert et al. demonstrated that several commercially available ECM scaffold materials contained measurable amounts of DNA; some even demonstrated histological staining for nuclear material. Most of these products have been used successfully clinically, so it is possible that having some remnant DNA and nuclear material in engineered cartilage constructs may result in a limited host response, though of course this needs to be demonstrated in in vivo studies. Additionally, as it is believed that the joint space is relatively immune privileged, as reviewed previously,  it is possible that complete decellularization of the tissue is not required. Furthermore, it is unclear if decellularization should be assessed histologically merely as elimination of cell nuclei, or if a more complete assessment involves quantifying the tissue’s DNA content, as prior studies have utilized differing approaches. For example, Lumpkins et al. found that 1% SDS treatment for 24 h resulted in complete removal of cell nuclei, although they did not assess the DNA content of the tissue. On the other hand, Dahl et al. examined the effects of a hypotonic/hypertonic treatment and found that there was complete removal of cell nuclei, but no decrease in DNA content. To study this issue further, in vivo studies are warranted to determine if there is threshold of decellularization at which an immune response is eliminated.
A drawback of using a decellularized xenograft is that it lacks chondrocytes, which are essential for the homeostasis of cartilage tissue. Eliminating the cells from the tissue leaves the ECM, which is responsible for the biomechanical properties of the tissue. Additionally, it has previously been demonstrated that decellularized bovine cartilage remained intact when implanted in a sheep for up to 6 months, and that there was cell infiltration, possibly from surrounding bone marrow MSCs. Therefore, it is possible that bone marrow infiltration of the decellularized constructs after implantation will allow for long term viability.
Although it was less effective than the 2% concentration, 1% SDS displayed similar effects. For example, treatment for 1 h resulted in a 15% decrease in DNA content, while maintaining GAG and collagen content, as well as maintaining biomechanical properties. Additionally, treatment for 8 h resulted in a 37% decrease in DNA content, loss of all GAG and aggregate modulus, as well as a decrease in Young’s modulus.
On the other hand, treatment with Triton X-100 and TnBP did not appear promising, as they had a minimal effect on tissue decellularization, and resulted in a slight decrease in GAG content. Several prior studies have indicated the ineffectiveness of Triton X-100, although it was used in this study as it is believed to have minimal effects on protein-protein interactions. For example, Dahl et al. examined the effects of 1% Triton X-100 on porcine carotid arteries, and found that this treatment resulted in similar cellularity to control and no decrease in DNA content. In another study on tendon decellularization, Cartmell and Dunn examined the effect of 1% Triton X-100 for 24 h, and found that cell density remained similar to control. Contrary to our results, this study also demonstrated complete histological decellularization with 1% TnBP, although a 48 h treatment was required. Therefore, it is possible that TnBP treatment may result in decellularization of self-assembled constructs at longer application times, although the GAG loss after as little as 8 h prevents the use of longer application times.
Finally, although a hypotonic/hypertonic treatment has been an effective decellularization agent in this study as well as prior studies, [10, 19] it did not appear to be a viable treatment for self-assembled cartilage constructs, as it had severely detrimental effects on construct functional properties. For instance, treatment for as little as 1 h resulted in nearly complete loss of compressive and Young’s modulus, while constructs treated for 8 h were untestable mechanically. Additionally, treatment at both application times resulted in nearly complete elimination of GAG content.
Based on these results, treatment with 2% SDS appears to be the most promising and should be examined further in future studies. Once complete SDS removal has been ensured, in vivo studies should be performed to determine the immune response to the decellularized tissue. Additionally, the effects of different decellularization treatments on complement activation should be addressed in future in vitro studies. Furthermore, as this study aimed to reduce the cellularity, additional studies are needed to investigate the elimination of the Galα1,3 epitope, which plays a significant role in hyperacute rejection of xenografts.
Treatment with 2% SDS appears to be the most promising method for decellularization. Treatment for 1 or 2 h maintained biomechanical and biochemical properties, while simultaneously significantly reducing the DNA content of the tissue. Additionally, treatment for 6 or 8 h resulted in complete histological decellularization, but also resulted in elimination of GAG and decreased aggregate modulus. Although the results of this study did not result in a completely decellularized construct with maintenance of biochemical and biomechanical properties, the results are promising and indicate the potential of a decellularized articular cartilage construct that could be used to treat damaged cartilage tissue without eliciting an immune response.
The authors would like to acknowledge funding from NIH NIAMS AR 053286.
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Benjamin D. Elder, Department of Bioengineering, Rice University.
Sriram V. Eleswarapu, Department of Bioengineering, Rice University.
Kyriacos A. Athanasiou, Department of Bioengineering, Rice University.