Cartilage Tissue Engineering Using Stem Cells and Bioprinting Technology—Barriers to Clinical Translation
Sam L. Francis
Claudia Di Bella
Gordon G. Wallace
Peter F. M. Choong- 1Department of Surgery, University of Melbourne, Melbourne, VIC, Australia
- 2Department of Orthopaedics, St Vincent's Hospital, Melbourne, VIC, Australia
- 3Biofab 3D, Aikenhead Centre for Medical Discovery, Melbourne, VIC, Australia
- 4Australian Research Council, Centre of Excellence for Electromaterials Science, Intelligent Polymer Research Institute, University of Wollongong, Wollongong, NSW, Australia
There is no long-term treatment strategy for young and active patients with cartilage defects. Early and effective joint preserving treatments in these patients are crucial in preventing the development of osteoarthritis. Tissue engineering over the past few decades has presented hope in overcoming the issues involved with current treatment strategies. Novel advances in 3D bioprinting technology have promoted more focus on efficient delivery of engineered tissue constructs. There have been promising in-vitro studies and several animal studies looking at 3D bioprinting of engineered cartilage tissue. However, to date there are still no human clinical trials using 3D printed engineered cartilage tissue. This review begins with discussion surrounding the difficulties with articular cartilage repair and the limitations of current clinical management options which have led to research in cartilage tissue engineering. Next, the major barriers in each of the 4 components of cartilage tissue engineering; cells, scaffolds, chemical, and physical stimulation will be reviewed. Strategies that may overcome these barriers will be discussed. Finally, we will discuss the barriers surrounding intraoperative delivery of engineered tissue constructs and possible solutions.
Introduction
Articular cartilage defects pose a significant burden to patients both symptomatically and functionally, leading to reduced quality of life. Younger patients particularly have no long-term treatment strategy and face multiple operations and possible complications in their lifetime due to the inevitable development of osteoarthritis (1, 2).
Several surgical options exist in current practice (Discussed in detail under the current treatment strategies section); however, they only provide short-term benefit in certain subsets of patients based on the nature of the defect and host factors. Fibrocartilage production is the major barrier in long-term viability of these methods and is detrimental to joint function (3).
Treatment strategies currently being pursued in research, focus on the development of 3D bioprinting of engineered cartilage tissue. This is a diverse field with many factors warranting optimization and integration to deliver the ultimate 3D tissue structure. However, there are several obstacles with each individual component, collectively leading to a barrier with respect to clinical use of cartilage tissue engineering and 3D bioprinting for cartilage repair. These hurdles will need to be addressed prior to any design of a human clinical trial.
Articular Cartilage: Structure and Repair
Articular cartilage is primarily composed of hyaline tissue. Hyaline cartilage is a specialized tissue found in most joints and provides low friction and shock absorption. It also provides a structural and biological barrier between two bone surfaces leading to smooth uniform range of motion (4).
Articular cartilage has unique biomechanical properties stemming from its structure (Figure 1) and composition. The lubricated surface provides low friction for articular motion. The extracellular matrix (ECM) and large water content from the effect of proteoglycans provides resistance to strong and repetitive loads of compression and shear. Variations of structure and composition in the different zones allow articular cartilage to resist complex loads and forces encountered in daily activity (4).
Figure 1. H&E stain and schematic representation of hyaline cartilage morphology and structure. SZ, superficial zone; MZ, middle zone; DZ, deep zone; CZ, calcified zone; SB, subchondral bone. Picture used with permission obtained from J Cytochem Biochem.
Damaged hyaline cartilage is unable to self-repair (5) due to its avascular nature. This characteristic of articular cartilage represents a major challenge in the field of orthopedics. Overtime, either with or without treatment the defect is filled with fibrocartilage, which represents a stiff tissue that doesn't provide the specialized properties of hyaline cartilage (3).
Current Treatment Strategies
Surgically many techniques have been developed in an attempt to repair/regenerate cartilage. These can be classified into bone marrow stimulation techniques (drilling, abrasion, and microfracture), direct chondral replacement (mosaicplasty and osteochondral allograft transplantation) and cell culture-based treatment (Autologous Chondrocyte Implantation and Matrix-induced Autologous Chondrocyte Implantation).
Microfracture is the most commonly used technique whilst Autologous Chondrocyte Implantation (ACI) and Matrix-induced Autologous Chondrocyte Implantation (MACI) are used by some surgeons in specific cases. Microfracture is an arthroscopic technique in which holes are created in the subchondral bone to allow blood and bone marrow to proximate, clot, and stimulate cartilage repair (6). ACI involves cartilage being harvested from non/low-weight bearing regions from which chondrocytes are isolated and expanded over 6–8 weeks, after which the cells are implanted back in surgically (7). MACI is a progression of the ACI technique characterized by the delivery of cells in association with a scaffold (8).
Comparison between all three methods have shown no superiority of the newer techniques compared to the less expensive microfractures. A randomized control trial comparing ACI to microfracture showed no significant improvement in cartilage repair outcomes (9), furthermore, no difference was shown comparing ACI to MACI (10). With no significant difference prevailing amongst the three techniques the general surgical inclination has been to opt for microfracture which is a simpler and cheaper option.
Studies involving microfracture show better outcome in patients <40 years old with isolated lesions averaging 2 cm2 in size, however at 36 months follow up there was significant reduction in clinical outcome (11). This technique can therefore only be provided to a small subset of patients and lacks long-term outcome data. Reasons for poor long-term outcomes include fibrocartilage production, patient age, functional level, location, and size of the defect (3, 11–13).
The Emergence of Cartilage Tissue Engineering
Poor long-term results and outcomes from bone marrow stimulation techniques like microfracture introduced the field of cartilage tissue engineering (Figure 2). The general principle of tissue engineering involves the use of cells, scaffolds, growth factors, and physical stimulation (diamond concept) to regenerate living tissue (13).
Figure 2. General components used in cartilage tissue engineering.
In the field of cartilage, the aim is to develop bio-mimetic tissue that can reliably perform, both biologically and biomechanically, as hyaline cartilage. There is a long history of cartilage tissue engineering attempts with initially engineered components resembling hyaline cartilage, however compared to native cartilage they lacked in mechanical properties (14, 15). Over time there has been additional focus on the biomechanical properties and cell-matrix/scaffold properties. The biomechanical forces being replicated in cartilage engineering include shear, tension, and compression which are endured in day to day activity within native joints (16).
3D bioprinting has emerged as a new technique to overcome some of the difficulties encountered in standard tissue engineering strategies, thanks to its speed, reliability, and precision (17). With respect to cartilage regeneration, the potential superiority of 3D bioprinting is in the ability to provide an efficient and tailored approach in the treatment of unique defect patterns.
Cartilage engineering-based techniques would be indicated in those with pure chondral lesions. If stem cells are used for such a repair approach, then any size of isolated chondral injury can be repaired due to the high replicative ability of these cells, meaning an abundant cell number can be obtained with expansion. With research progression osteochondral defects could theoretically be repaired by building distinct layers with cells differentiated into cartilage or bone.
Cells–Barriers
Many different cell lineages of various potencies and sources (Figure 3) have been studied; advantages and disadvantages of the types are outlined in Table 1. Mesenchymal stem cells (MSC) have emerged as a major line with respect to cartilage engineering and show excellent chondrogenic potential (18, 19).
Figure 3. Different cell types used in cartilage tissue engineering based on potency. ESC, Embryonic stem cell; iPSC, Induced pluripotent stem cell; and MSC, Mesenchymal stem cell.
Table 1. Advantages and disadvantages of different cell potencies that have been used in cartilage tissue engineering.
The optimal tissue sources for harvesting MSCs has traditionally been the bone marrow and adipose tissue, due to easier access and the amount of tissue available. Adipose derived MSCs has been shown to produce superior chondrogenic differentiation when compared to bone marrow derived MSCs (20, 21), furthermore, more MSCs can be isolated per tissue volume when using adipose compared to bone. Abdominal subcutaneous tissue and the infrapatellar fat pad (IFP) are the most commonly used adipose tissue harvest sites for MSC isolation. Although abdominal subcutaneous fat is more abundant, IFP tissue has been shown to be more superior with respect to chondrogenic potential (22).
Irrespective of final cell choice and source there are several key barriers that need to be addressed for clinical translation using cell-based cartilage engineering.
Concerns Around in-vitro Lab-Based Cell Expansion
Cell expansion systems are timely and currently require in-vitro lab-based cell culture. This opens up concerns with respect to lab sterility, ethics, and risks associated with the use of animal serum-based media products (23–26). Development of a rapid isolation approach may allow avoidance of any in-vitro lab-based cell culture if enough cells can be isolated and implanted directly in theater (27, 28), eliminating concerns surrounding sterility and limiting the exposure to animal serum-based media.
Irrespective of isolation timeframes it will be critical to establish protocols for cell culture without animal serum-based media products in view of human clinical translation. The development of animal serum-free culture media using human derived growth supplements for MSC expansion, such as human platelet lysates (29–33) presents a promising solution. Furthermore, development of animal and human serum-free culture media for the expansion of MSC toward clinical applications is another promising strategy (34–36).
How Many Cells Are Needed Based on Defect Size?
Cell-free cartilage repair techniques such as microfracture are based primarily on lesion thickness (37, 38). Current cell implantation techniques such as ACI and MACI use an expanded number of chondrocytes based on either surgeon preference or rough physiological cartilage cell counts with preference leaning toward higher than normal cell densities (39). The use of higher chondrocyte densities in-vitro can inhibit matrix synthesis leading to reduced ECM production (40, 41), whilst using lower densities will not produce enough ECM in-vitro (42, 43). Only a few in-vivo and in-vitro studies report cell densities used and the use of higher cell densities has not been shown to be superior to lower densities, therefore, no optimal clinical cell density has been identified (39).
There is no data on the desired stem cell density in the literature, with research groups tending to use cell counts based on anatomical human data which shows roughly 1 × 104 chondrocytes in 1 mm3 of tissue (44). Stem cells have a higher proliferate ability compared to chondrocytes (45), therefore, use of chondrocyte based cell numbers with stem cells will not be an accurate measure of the optimal cell density needed at time of repair. It will be imperative to investigate the optimal cell density per defect volume when using stem cells and taking into consideration other factors such as the matrix type and volumes used.
Scaffold Materials–Barriers
The vast majority of cartilage tissue engineering techniques use scaffolds, which help support and create 3D structures of the cellular matrix. Successful scaffold designs optimize certain requirements (46–48) including; biocompatibility, environment, toxicity, degradation rate, pore size, pore geometry, and scaffold stiffness.
Scaffolds can be classified as natural polymers, synthetic polymers, or a hybrid. In cartilage engineering softer polymers, which can initially fill in defects and then solidify at later stages, are the bio-scaffolds that show most promise for clinical application due to their ability to fill complex morphologies which present at the time of surgical repair (49). Soft polymers such as hydrogels have biomimetic properties similar to soft tissue (50), however, at their starting point, i.e., liquid phase, hydrogels have relatively poor mechanical stability, which represents a limitation of their use in this state (51).
Can Hydrogels Provide Biomimetic Mechanical Strength?
Normally hydrogels are printed in a liquid state, which can then solidify after a phase transformation induced by chemical or non-chemical reactions. Cross-linking can be undertaken via photo, thermal or chemical induction (52). This process allows molecules to crosslink and provides increased mechanical stability to the tissue (53, 54).
Over time tunable hydrogel composites have been formulated which can be tweaked to enhance the mechanical properties of the material (55–57) and allow vertical construction of a 3D shape which was another initial limitation of hydrogel use (57). However, each addition or modification that is made can interact and effect the biocompatibility and therefore needs to be thoroughly tested.
Can Cross-Linking of the Scaffold Be Incorporated Intraoperatively?
Cross linking can be performed prior to implantation, meaning the engineered construct is made on a bench then implanted separately. This will prevent normal human tissue from being affected directly by cross-linking reactions and the sources used. To date, most in-vivo animal models have utilized bench-based formation of cross-linked pre-formed cartilage tissue, with subsequent implantation into simple non-complex defect morphologies which are man-made at time of surgery (58–60).
However, as mentioned earlier implanting pre-formed tissue will be difficult due to the complexity associated with cartilage defect morphology and therefore if at time surgical printing is preferred then the ability to cross link needs to be performed during surgery also leading to the issue of safe intraoperative cross-linking.
A recent pilot study (61) showed an intraoperative direct hand-held repair technique in a sheep model where tissue was formed and cross-linked directly into a defect at time of repair, thus avoiding any pre-printed bench-based tissue engineering techniques. In this study an ultraviolet light was used to cross link the hydrogel material which was preloaded with a photo initiating material, the light source was used as a separate component to the hand-held bioprinter. Macroscopically the use of the light source didn't affect surrounding healthy tissue. This study also used simple man-made defects and therefore doesn't confirm the ability to directly bio-print engineered cartilage into complex morphologies, however, if validated with more complex lesion patterns provides a more suitable option compared to implanting pre-formed cartilage tissue.
In future studies it will be ideal to directly add such a source to a hand-held printing device limiting the need for additional components and complexity to the surgical approach.
Chondrogenic Stimulation–Barriers
Molecules including growth factors and soluble non-protein chemical compounds chemically regulate cell behavior. Molecules bind to surface receptors on stem cells to activate intracellular signal pathways controlling cellular proliferation, differentiation, and synthesis. Mesenchymal stem cells have an important paracrine effect on cartilage formation and promoting an anti-inflammatory environment (62, 63).
Many combinations such as transforming growth factor (TGF) beta-3 with bone morphogenetic protein (BMP) 2 have induced chondrogenesis in adult stem cell use (64). Irrespective of the combination used, during in-vitro experimentation chemical stimulants can be provided (via culture media) periodically, producing consistent chondrogenic differentiation.
However, regular delivery and monitoring of stimulation can't be translated into an in-vivo setting as the native knee synovium must take over nutritional control. The native synovium in an adult is not catered to newly growing cartilage, meaning the desired growth factors and respective concentrations provided in in-vitro studies will not be present in-vivo, therefore, synovial take-over of nutritional regulation becomes an unknown obstacle in the way of human clinical trials.
Can Engineered Cartilage Tissue Be Maintained in the Body in the Long Term?
With a view of translating tissue engineered cartilage into the human knee, a major barrier will be with the formation of reliable and consistent chondrogenic tissue over time. Human blood supply will have growth factors and chemical stimulants that can assist with chondrogenic stimulation, however, highest activity is during fetal/young stages of life with increasing age associated with less stimulation and organization of chondrocytes and extracellular matrix (65). Therefore, theoretically if engineered tissue (composed of newly forming cartilage cells from a stem cell base) is used in adolescent cartilage repair we have no certainty of cellular control and regulation in-vivo.
Short term results are promising with respect to the use of cartilage tissue engineering methods in an in-vivo animal model (58, 59, 61). However, no mid/long-term (>12 weeks) in-vivo animal studies using cartilage tissue engineering and 3D bioprinting methods have been performed, therefore, no superiority compared to current clinical techniques such as microfracture and ACI can be ascertained. Mid/long-term in-vivo animal studies using tissue engineering techniques will be crucial in validating the ability of the native synovium in nourishing and maintaining engineered cartilage over large periods of time, this data will be pivotal to obtain prior to any progression to human clinical trials.
Physical/Environmental Stimulation–Barriers
With respect to mechanical and environmental stimulation, if tissue is to be printed directly in-vivo then native forces encountered by the knee in conjunction with synovial nourishment should directly take over adequate stimulation. Therefore, with an approach avoiding lab-based tissue growth there is no major concern with the ability to mimic the environment of the human knee.
The replication and delivery of such an environment is only important when trying to maintain a bench based in-vitro model of repair research where a bio-printed piece of tissue is maintained in a lab for in-vitro investigation or for in-vivo models using pre-formed tissue which is maintained in a lab then implanted at a later date. In these studies, tissue will need to be maintained as close to the native in-vivo environment as possible whilst in the lab. Therefore, ideally these cartilage constructs should be exposed to the different types of mechanical forces encountered by the native knee, such as shear stress, perfusion, hydrostatic pressure, and compression (16, 66).
Recreating the Properties of the Human Knee in a 3D Culture Environment–3D Bioreactors
Well-designed bioreactor systems can provide stimulation in one consistent and regular setting therefore providing a culture environment that promotes cartilage growth (67).
Single stimulation bioreactor environments
Induction of shear force to promote cartilage growth has been demonstrated using rotating vessels (68–70), spinner flasks (71, 72), and stirred double chambers (73). Induction of perfusion to promote cartilage growth has been demonstrated using fluid perfusion bioreactor systems either using a unidirectional (74) or a bidirectional (75) bioreactor. Induction of hydrostatic pressure to promote cartilage growth has been demonstrated using fluid filled chambers with water pumps (76, 77). Induction of compression to promote cartilage growth has been widely demonstrated (78).
Bioreactors for inducing multiple/combined mechanical force
Bioreactors applying multiple mechanical properties are currently being developed. One study combining intermittent unconfined shear and compressive loading for 2.5 weeks showed increase in glycosaminoglycan and collagen type II production in human chondrocytes by 5.3- and 10-fold, respectively, after simultaneous stimulation (74).
More development is warranted into the application of multiple mechanical forces within bioreactor systems with respect to in-vitro cartilage tissue engineering.
Construct Delivery—Barriers
Modern advancement in 3D bioprinting technology opens up novel techniques with respect to the delivery of engineered human tissue. As mentioned earlier with respect to cartilage tissue engineering the ideal materials for printing are hydrogels given their ability to accommodate complex morphologies (49). With respect to 3D bioprinting of engineered cartilage tissue the ideal printing device would need to be small, portable, and operator friendly to allow for direct intraoperative printing into defects.
Bioprinting has largely come about to combat the limitations of past tissue engineering methods and allows for accurate control of cell distribution, production of biomimetic geometry, and rapid production of construct (79, 80). With respect to cartilage tissue repair, it is impossible to accurately characterize defects even with current advances in medical imaging, therefore bioprinting techniques in this field need to be focused more on flexibility rather than computer aided precision. Several different types of bioprinters have been developed (Figure 4), characteristics and disadvantages of each type are shown in Table 2. Hand-held bioprinting used in conjunction with hydrogels are best suited to achieve this as they can plug defects of any nature easily like using a glue stick/gel, avoiding the need for large and heavy machinery in the operating theater (81).
Figure 4. Different types of 3D Bioprinting methods. (A) Inkjet bioprinter, (B) Micro-extrusion bioprinter, (C) Laser-assisted bioprinter, and (D) Stereolithography bioprinter.
Table 2. Characteristics and disadvantages of the different 3D Bioprinting methods.
The most suitable mechanism to fit a portable hand-held type device would be extrusion printing given the compactable nature of the mechanism, an example of this is the “bio pen” which uses pneumatic extrusion-based technology to allow printing of hydrogels (82), Figure 5 shows the intraoperative use of the bio pen in an sheep model. This device can be loaded with two cartridges allowing for a co-axial based printing method (Figures 6A–D) which can concentrate cells in the middle core with an outer hydrogel shell layer that can be crosslinked and protect the inner cellular tissue (83).
Figure 5. Intra-operative photograph of the Biopen in action in a sheep model. [Modified from and used with permission from Di Bella et al. (81), under CC BL].
Figure 6. Core/Shell 3D printing by co-axial extrusion. (A) Schematic representation of the 3D co-axial handheld printer. (B) Schematic representation of the co-axial nozzle. (C) Picture of the cartridges dedicated to Core and Shell loading in the printer, with relative magnification of the nozzle during co-axial deposition. (D) Representative 3D rendered confocal images of Core/Shell printed sample labeled with fluorescent beads. The hydrogel shell is shown in red channel, while the cellular/hydrogel core is shown in green channel. The panel shows the same image representative of 3D rendered of superimposed green and red channels in three different orientations. [Modified from and used with permission from Duchi et al. (83) under CC BL].
Engineered tissue using a portable hand-held device can be printed directly during surgery on the spot with the top of the construct being immediately crosslinked using methods mentioned earlier. This approach allows for implant stability within the lesion (61). However, when using non-portable printers and non-hydrogel-based scaffolds/materials the formed implant will need to be manually positioned (requires precise geometry when initially created) into the lesion and then anchored with either sutures or a flap approach.
In-vivo animal delivery of engineered cartilage tissue has been performed to-date using large incisions over the knee, similar to those made in conventional knee replacement surgeries (61, 84). Larger incisions, however, increase the risk of wound complications (e.g., infection and wound dehiscence) and reduce cosmetic satisfaction, both of which are important factors to consider in treatment of a young-middle aged population.
Can Engineered Cartilage Tissue Be Provided Using Less Risk Adverse Minimally Invasive Techniques?
Arthroscopic knee surgery (85) (key-hole surgery) can provide such a solution and is performed in a day surgery setting allowing patients to return to daily activity almost immediately. Technically speaking the desired bioprinting device would therefore be incorporated as an attachment into an arthroscopic kit, once again the most suited to this would be a small hand-held bioprinter. This microsurgical kit/device will need adequate valdiation and training prior to use.
If as mentioned earlier a rapid stem cell isolation can be established to fit within a surgical time frame (28) then this will open up the ability to harvest tissue, isolate stem cells then directly re-implant a cell/scaffold interface into knee joint in one single operation. Furthermore, if stem cells can be harvested from a source like the infrapatellar fat pad (IFP) (86) which is in close proximity to the knee joint (Figure 7) the operation can be performed using one surgical site. Arthroscopic harvest of the IFP for adipose-derived mesenchymal stem cells isolation has been performed successfully in a rabbit model (22).
Figure 7. Infrapatellar fat pad (IFP) location and harvested tissue. Sagittal magnetic resonance imaging scan of the knee showing the relationship of the IFP (arrow) to the articular cartilage (double arrow). [Modified from and used with permission from Hindle et al. (22) under CC BL].
Will the Delivered Construct Integrate Effectively With Host Tissue?
Another uncertainty is the ability of engineered cartilage tissue to integrate with healthy tissue. It is evident that superior cartilage repair can be achieved using a hand-held printing method, however both hand-held and bench-based printing methods can produce the development of voids (Figure 8) between the edges of the implanted tissue and health native tissue (61).
Figure 8. Histology (Safranin/Fast green staining) showing better new cartilage formation in the HH group compared to the other groups. Subchondral cysts and collapse are seen in the BB and MF group, with fibrocartilage formation. Voids at the implanted/native tissue interfaces are seen in the HH and BB groups indicated by the yellow stars. HH, Hand held Biopen printed scaffold; BB, Bench Based 3D printed scaffold; MF, Microfractures; C, Negative Control (defect left empty). Voids at the implanted/native tissue interfaces are seen in the HH and BB groups. [Modified from and used with permission from Di Bella et al. (81), under CC BL].
A possible solution to overcome this would be to apply an initial coat of biocompatible adhesive (87) into the defect prior to implantation allowing better proximation of tissue. Subsequently it will be pivotal to investigate if such a method then allows interaction of the implanted tissue with the healthy tissue, this could be investigated adding tracking materials/dyes to the constructed tissue, and then assessing movement/integration at different time points (88, 89).
Conclusion–Human Clinical Translation
Cartilage repair techniques using stem cells and 3D bioprinting technology still remains elusive with respect to human clinical translation. Many challenges remain to be addressed and overcome as described in this review. More focus on in-vivo animal studies will be essential to investigate many of these barriers. Whilst continued progress is made on such issues it is important to begin setting up larger scale in-vivo animal trials which will be the next step toward human clinical translation.
Author Contributions
SF completed a literature search, contributed to the preparation of the manuscript, and critically revised the manuscript. CD, GW, and PC contributed ideas, content to the manuscript, and critically revised the manuscript.
Conflict of Interest Statement
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
Acknowledgments
The cartilage research group is currently supported by funding from the Royal Australian College of Surgeons (RACS), The Australian Research Council Industrial Transformation Training Centre (ARC-ITTC) in Additive Biomanufacturing and the Medical Technologies and Pharmaceuticals (MTPConnect) BioMedTech Horizons program.
Abbreviations
3D, Three dimensional; ACI, Autologous Chondrocyte Implantation; MACI, Matrix-induced Autologous Chondrocyte Implantation; MSC, Mesenchymal Stem Cell; TGF, Transforming Growth Factor; BMP, Bone Morphogenetic Protein.
References
1. Robertsson O, Stefánsdóttir A, Lidgren L, Ranstam J. Increased long-term mortality in patients less than 55 years old who have undergone knee replacement for osteoarthritis: results from the swedish knee arthroplasty register. J Bone Joint Surg. (2007) 89:599–603. doi: 10.1302/0301-620X.89B5.18355
2. Julin J, Jämsen E, Puolakka T, Konttinen YT, Moilanen T. Younger age increases the risk of early prosthesis failure following primary total knee replacement for osteoarthritis: a follow-up study of 32,019 total knee replacements in the Finnish Arthroplasty Register. Acta Ortho Scand. (2010) 81:413–9. doi: 10.3109/17453674.2010.501747
3. Redman SN, Oldfield SF, Archer CW. Current strategies for articular cartilage repair. Eur Cell Mater. (2005) 9:23–32. doi: 10.22203/eCM.v009a04
4. Fox SA, Bedi A, Rodeo SA. The basic science of articular cartilage: structure, composition, and function. Sports Health (2009) 1:461–8. doi: 10.1177/1941738109350438
5. Hunter W. On the structure and diseases of articulating cartilage. Phil Trans R Soc. (1743) 42B:514–21.
6. Steadman Jr, Briggs KK, Rodrigo JJ. The microfracture technic in the management of complete cartilage defects in the knee joint. Orthopade (1999) 28:26–32.
7. Brittberg M, Lindahl A, Nilsson A, Ohlsson C, Isaksson O, Peterson L. Treatment of deep cartilage defects in the knee with autologous chondrocyte transplantation. N Engl J Med. (1994) 331:889–95. doi: 10.1056/NEJM199410063311401
8. Franceschi F, Longo UG, Ruzzini L, Marinozzi A, Maffulli N, Denaro V. Simultaneous arthroscopic implantation of autologous chondrocytes and high tibial osteotomy for tibial chondral defects in the varus knee. Knee (2008) 15:309–13. doi: 10.1016/j.knee.2008.04.007
9. Knutsen G, Drogset JO, Engebretsen L, Grontvedt T, Isaksen V, Ludvigsen TC, et al. A randomized trial comparing autologous chondrocyte implantation with microfracture. Findings at five years. J Bone Joint Surg Am. (2007) 89:2105–12. doi: 10.2106/JBJS.G.00003
10. Bartlett W, Skinner JA, Gooding CR, Carrington RW, Flanagan AM, Briggs TW, et al. Autologous chondrocyte implantation versus matrix-induced autologous chondrocyte implantation for osteochondral defects of the knee: a prospective, randomised study. J Bone Joint Surg Br. (2005) 87:640–5. doi: 10.1302/0301-620X.87B5.15905
11. Kreuz PCSMR, Erggelet C, Krause SJ, Konrad G, Uhl M, Südkamp N. Results after microfracture of full-thickness chondral defects in different compartments in the knee. Osteoarthritis Cartilage (2006) 14:119–25. doi: 10.1016/j.joca.2006.05.003
12. Steadman JR, Briggs KK, Rodrigo JJ, Rodkey WG. Outcomes of microfracture for traumatic chondral defects of the knee: average 11-year follow-up. Arthroscopy. J Arthroscopic Relat Surg. (2003) 19:477–84. doi: 10.1053/jars.2003.50112
13. Giannoudis PV, Einhorn TA, Marsh D. Fracture healing: the diamond conceptt. Injury (2007) 38(Suppl. 4):S3–6. doi: 10.1016/S0020-1383(08)70003-2
14. Grad S, Eglin D, Alini M, Stoddart MJ. Physical stimulation of chondrogenic cells in vitro: a review. Clin Orthop Relat Res. (2011) 469:2764–72. doi: 10.1007/s11999-011-1819-9
15. Schulz RM, Bader A. Cartilage tissue engineering and bioreactor systems for the cultivation and stimulation of chondrocytes. Eur Biophys J. (2007) 36:539–68. doi: 10.1007/s00249-007-0139-1
16. Lai JH Levenston ME. Meniscus and cartilage exhibit distinct intra-tissue strain distributions under unconfined compression. Osteoarthritis Cartilage (2010) 18:1291–9. doi: 10.1016/j.joca.2010.05.020
17. Mandrycky C, Wang Z, Kim K, Kim DH. 3D bioprinting for engineering complex tissues. Biotechnol Adv. (2016) 34:422–34. doi: 10.1016/j.biotechadv.2015.12.011
18. Ronziere MC, Perrier E, Mallein-Gerin F, Freyria AM. Chondrogenic potential of bone marrow- and adipose tissue-derived adult human mesenchymal stem cells. Biomed Mater Eng. (2010) 20:145–58. doi: 10.3233/BME-2010-0626
19. Rada T, Reis RL, Gomes ME. Adipose tissue-derived stem cells and their application in bone and cartilage tissue engineering. Tissue Eng. (2009) 15:113–25. doi: 10.1089/ten.teb.2008.0423
20. Strioga M, Viswanathan S, Darinskas A, Slaby O, Michalek J. Same or not the same? comparison of adipose tissue-derived versus bone marrow-derived mesenchymal stem and stromal cells. Stem Cells Dev. (2012) 21:2724–52. doi: 10.1089/scd.2011.0722
21. Jang Y Koh YG, Choi YJ, Kim SH, Yoon DS, Lee M, et al. Characterization of adipose tissue-derived stromal vascular fraction for clinical application to cartilage regeneration. In Vitro Cell Dev Biol Anim. (2015) 51:142–50. doi: 10.1007/s11626-014-9814-6
22. Hindle P, Khan N, Biant L, Péault B. The infrapatellar fat pad as a source of perivascular stem cells with increased chondrogenic potential for regenerative medicine. Stem Cells Transl Med. (2017) 6:77–87. doi: 10.5966/sctm.2016-0040
23. Herberts CA Kwa MSG, Hermsen HP. Risk factors in the development of stem cell therapy. J Transl Med. (2011) 9:29. doi: 10.1186/1479-5876-9-29
24. Halme DG, Kessler DA. FDA regulation of stem-cell-based therapies. N Engl J Med. (2006) 355:1730–5. doi: 10.1056/NEJMhpr063086
25. Heiskanen A, Satomaa T, Tiitinen S, Laitinen A, Mannelin S, Impola U, et al. N-glycolylneuraminic acid xenoantigen contamination of human embryonic and mesenchymal stem cells is substantially reversible. Stem Cells (2007) 25:197–202. doi: 10.1634/stemcells.2006-0444
26. Shih DT, Burnouf T. Preparation, quality criteria, and properties of human blood platelet lysate supplements for ex vivo stem cell expansion. N Biotechnol. (2015) 32:199–211. doi: 10.1016/j.nbt.2014.06.001
27. Francis MP, Sachs PC, Elmore LW, Holt SE. Isolating adipose-derived mesenchymal stem cells from lipoaspirate blood and saline fraction. Organogenesis (2010) 6:11–4. doi: 10.4161/org.6.1.10019
28. Francis SL, Duchi S, Onofrillo C, Di Bella C, Choong PFM. Adipose-derived mesenchymal stem cells in the use of cartilage tissue engineering: the need for a rapid isolation procedure. Stem Cells Int. (2018) 2018:8947548. doi: 10.1155/2018/8947548
29. Hemeda H, Giebel B, Wagner W. Evaluation of human platelet lysate versus fetal bovine serum for culture of mesenchymal stromal cells. Cytotherapy (2014) 16:170–80. doi: 10.1016/j.jcyt.2013.11.004
30. Bieback K, Hecker A, Kocaömer A, Lannert H, Schallmoser K, Strunk D, et al. Human alternatives to fetal bovine serum for the expansion of mesenchymal stromal cells from bone marrow. Stem Cells (2009) 27:2331–41. doi: 10.1002/stem.139
31. Crespo-Diaz R, Behfar A, Butler GW, Padley DJ, Sarr MG, Bartunek J, et al. Platelet lysate consisting of a natural repair proteome supports human mesenchymal stem cell proliferation and chromosomal stability. Cell Trans. (2011) 20:797–812. doi: 10.3727/096368910X543376
32. Schallmoser K, Strunk D. Preparation of pooled human platelet lysate (pHPL) as an efficient supplement for animal serum-free human stem cell cultures. J Vis Exp. (2009) 32:1523. doi: 10.3791/1523
33. Walenda G, Hemeda H, Schneider RK, Merkel R, Hoffmann B, Wagner W. Human platelet lysate gel provides a novel three dimensional-matrix for enhanced culture expansion of mesenchymal stromal cells. Tissue Eng Part C (2012) 18:924–34. doi: 10.1089/ten.tec.2011.0541
34. Chase LG, Lakshmipathy U, Solchaga LA, Rao MS, Vemuri MC. A novel serum-free medium for the expansion of human mesenchymal stem cells. Stem Cell Res Ther. (2010) 1:8. doi: 10.1186/scrt8
35. Lindroos B, Boucher S, Chase L, Kuokkanen H, Huhtala H, Haataja R., et al. Serum-free, xeno-free culture media maintain the proliferation rate and multipotentiality of adipose stem cells in vitro. Cytotherapy (2009) 11:958–72. doi: 10.3109/14653240903233081
36. Patrikoski M, Juntunen M, Boucher S, Campbell A, Vemuri MC, Mannerström B, et al. Development of fully defined xeno-free culture system for the preparation and propagation of cell therapy-compliant human adipose stem cells. Stem Cell Res Ther. (2013) 4:27. doi: 10.1186/scrt175
37. Steadman JR, Rodkey WG, Briggs KK, (eds.). Microfracture: its history and experience of the developing surgeon. Cartilage (2010) 1:78–86. doi: 10.1177/1947603510365533
38. Williams RJ, Harnly HW III. Microfracture: indications, technique, and results. Instr Course Lect. Am. Acad. Orthop. Surg. (2007) 56:419–28.
39. Foldager CB, Gomoll AH, Lind M, Spector M. Cell seeding densities in autologous chondrocyte implantation techniques for cartilage repair. Cartilage (2012) 3:108–17. doi: 10.1177/1947603511435522
40. Abbott J, Holtzer H. The loss of phenotypic traits by differentiated cells. 3. The reversible behavior of chondrocytes in primary cultures. J Cell Biol. (1966) 28:473–87. doi: 10.1083/jcb.28.3.473
41. Bernstein P, Dong M, Graupner S, Corbeil D, Gelinsky M, Günther KP, et al. Sox9 expression of alginate-encapsulated chondrocytes is stimulated by low cell density. J Biomed Mater Res A (2009) 91A:910–9. doi: 10.1002/jbm.a.32308
42. Handley CJ, Bateman JF, Oakes BW, Lowther DA. Characterization of the collagen synthesized by cultured cartilage cells. Biochim Biophys Acta (1975) 386:444–50. doi: 10.1016/0005-2795(75)90287-1
43. Francioli SE, Candrian C, Martin K, Heberer M, Martin I, Barbero A. Effect of three-dimensional expansion and cell seeding density on the cartilage-forming capacity of human articular chondrocytes in type II collagen sponges. J Biomed Mater Res A (2010) 95A:924–31. doi: 10.1002/jbm.a.32917
44. Hunziker EB, Quinn TM, Häuselmann HJ. Quantitative structural organization of normal adult human articular cartilage. Osteoarthritis Cartilage (2002) 10:564–72. doi: 10.1053/joca.2002.0814
45. Mobasheri A, Kalamegam G, Musumeci G, Batt ME. Chondrocyte and mesenchymal stem cell-based therapies for cartilage repair in osteoarthritis and related orthopaedic conditions. Maturitas (2014) 78:188–98. doi: 10.1016/j.maturitas.2014.04.017
46. Stoop R. Smart biomaterials for tissue engineering of cartilage. Injury (2008) 39:S77–87. doi: 10.1016/j.injury.2008.01.036
47. Nava MM, Draghi L, Giordano C, Pietrabissa R. The effect of scaffold pore size in cartilage tissue engineering. J Appl Biomater Funct Mater. (2016) 14:e223–9. doi: 10.5301/jabfm.5000302
48. Arora A, Kothari A, Katti DS. Pore orientation mediated control of mechanical behavior of scaffolds and its application in cartilage-mimetic scaffold design. J Mech Behav Biomed Mater. (2015) 51:169–83. doi: 10.1016/j.jmbbm.2015.06.033
49. Kim IL, Mauck RL, Burdick JA. Hydrogel design for cartilage tissue engineering: a case study with hyaluronic acid. Biomaterials (2011) 32:8771–82. doi: 10.1016/j.biomaterials.2011.08.073
50. Peppas NA, Kavimandan NJ. Nanoscale analysis of protein and peptide absorption: insulin absorption using complexation and pH-sensitive hydrogels as delivery vehicles. Eur J Pharm Sci. (2005) 29:183–97. doi: 10.1016/j.ejps.2006.04.014
51. Drury JL, Mooney DJ. Hydrogels for tissue engineering: scaffold design variables and applications. Biomaterials (2003) 24:4337–51. doi: 10.1016/S0142-9612(03)00340-5
52. Drury JL, Mooney DJ. The effects of crosslinking of scaffolds engineered from cartilage ECM on the chondrogenic differentiation of MSCs. Biomaterials (2013) 34:5802–12. doi: 10.1016/j.biomaterials.2013.04.027
53. Chen YC, Chen M, Gaffney EA, Brown CP. Effect of crosslinking in cartilage-like collagen microstructures. J Mech Behav Biomed Mater. (2017) 66:138–43. doi: 10.1016/j.jmbbm.2016.10.006
54. D'Este M, Eglin D. Hydrogels in calcium phosphate moldable and injectable bone substitutes: sticky excipients or advanced 3-D carriers. Acta Biomater. (2013) 9:5421–30. doi: 10.1016/j.actbio.2012.11.022
55. Huang CC, Ravindran S, Yin Z, George A. 3-D self-assembling leucine zipper hydrogel with tunable properties for tissue engineering. Biomaterials (2014) 35:5316–26. doi: 10.1016/j.biomaterials.2014.03.035
56. Fathi A, Mithieux SM, Wei H, Chrzanowski W, Valtchev P, Weiss AS, et al. Elastin based cell-laden injectable hydrogels with tunable gelation, mechanical and biodegradation properties. Elastin based cell-laden injectable hydrogels with tunable gelation, mechanical and biodegradation properties. Biomaterials (2014) 35:5425–35. doi: 10.1016/j.biomaterials.2014.03.026
57. Discher DE, Janmey P, Wang Y-L. Tissue cells feel and respond to the stiffness of their substrate. Science (2005) 310:1139–43. doi: 10.1126/science.1116995
58. Guo X, Park H, Young S, Kretlow JD, van den Beucken JJ, Baggett LS, et al. Repair of osteochondral defects with biodegradable hydrogel composites encapsulating marrow mesenchymal stem cells in a rabbit model. Acta Biomater. (2010) 6:39–47. doi: 10.1016/j.actbio.2009.07.041
59. Nehrer S, Breinan HA, Ramappa A, Hsu HP, Minas T, Shortkroff S, et al. Chondrocyte-seeded collagen matrices implanted in a chondral defect in a canine model. Biomaterials (1998) 19:2313–28. doi: 10.1016/S0142-9612(98)00143-4
60. Nehrer S, Breinan HA, Ramappa A, Hsu HP, Minas T, Shortkroff S, et al. Evaluation of a hybrid scaffold/cell construct in repair of high-load-bearing osteochondral defects in rabbits. Biomaterials (2006) 27:1071–80. doi: 10.1016/j.biomaterials.2005.07.040
61. Di Bella C, Duchi S, O'Connell CD, Blanchard R, Augustine C, Yue Z, et al. In situ handheld three-dimensional bioprinting for cartilage regeneration. J Tissue Eng Regen Med. (2018) 12:611–21. doi: 10.1002/term.2476
62. van Buul GM, Villafuertes E, Bos PK, Waarsing JH, Kops N, Narcisi R, et al. Mesenchymal stem cells secrete factors that inhibit inflammatory processes in short-term osteoarthritic synovium and cartilage explant culture. Osteoarthritis Cartilage (2012) 20:1186–96. doi: 10.1016/j.joca.2012.06.003
63. Linero I, Chaparro O. Paracrine effect of mesenchymal stem cells derived from human adipose tissue in bone regeneration. PLoS ONE (2014) 9:e107001. doi: 10.1371/journal.pone.0107001
64. Sekiya I, Larson BL, Vuoristo JT, Reger RL, Prockop DJ. Comparison of effect of BMP-2,−4, and−6 on in vitro cartilage formation of human adult stem cells from bone marrow stroma. Cell Tissue Res. (2005) 320:269–76. doi: 10.1007/s00441-004-1075-3
65. Hardingham T, Bayliss M. Proteoglycans of articular cartilage: changes in aging and in joint disease. Semin Arthritis Rheum. (1990) 20(3 Suppl. 1):12–33.
66. Zhao J, Griffin M, Cai J, Li S, Bulter PEM, Kalaskar DM. Bioreactors for tissue engineering: an update. Biochem Eng J. (2016) 109:268–81. doi: 10.1016/j.bej.2016.01.018
67. Griffin DJ, Vicari J, Buckley MR, Silverberg JL, Cohen I, Bonassar LJ. Effects of enzymatic treatments on the depth-dependent Viscoelastic shear properties of articular cartilage. J Orthop Res. (2014) 32:1652–7. doi: 10.1002/jor.22713
68. Takebe T, Kobayashi S, Kan H, Suzuki H, Yabuki Y, Mizuno M, et al. Human elastic cartilage engineering from cartilage progenitor cells using rotating wall vessel bioreactor. Transplant Proc. (2012) 44:1158–61. doi: 10.1016/j.transproceed.2012.03.038
69. Marlovits S, Tichy B, Truppe M, Gruber D, Schlegel W. Collagen expression in tissue engineered cartilage of aged human articular chondrocytes in a rotating bioreactor. Int J Artif Organs (2003) 26:319–30. doi: 10.1177/039139880302600407
70. Ohyabu Y, Kida N, Kojima H, Taguchi T, Tanaka J, Uemura T. Cartilaginous tissue formation from bone marrow cells using rotating wall vessel (RWV) bioreactor. Biotechnol Bioeng. (2006) 95:1003–8. doi: 10.1002/bit.20892
71. Liu L, Wu W, Tuo X, Geng W, Zhao J, Wei J, et al. Novel strategy to engineer trachea cartilage graft with marrow mesenchymal stem cell macroaggregate and hydrolyzable scaffold. Artif Organs (2010) 34:426–33. doi: 10.1111/j.1525-1594.2009.00884.x
72. Klionsky DJ, Abdelmohsen K, Abe A, Abedin MJ, Abeliovich H, Acevedo Arozena A, et al. Enhanced cartilage formation via three-dimensional cell engineering of human adipose-derived stem cells. Tissue Eng A (2012) 18:1949–56. doi: 10.1089/ten.TEA.2011.0647
73. Chang C-H, Lin F-H, Lin CC, Chou C-H, Liu H-C. Cartilage tissue engineering on the surface of a novel gelatin–calcium–phosphate biphasic scaffold in a double-chamber bioreactor. Biomed Mater Res B Appl Biomater. (2004) 71B:313–21. doi: 10.1002/jbm.b.30090
74. Santoro R, Olivares AL, Brans G, Wirz D, Longinotti C, Lacroix D, et al. Bioreactor based engineering of large-scale human cartilage grafts for joint resurfacing. Biomaterials (2010) 31:8946–52. doi: 10.1016/j.biomaterials.2010.08.009
75. Wendt D, Marsano A, Jakob M, Heberer M, Martin I. Oscillating perfusion of cell suspensions through three-dimensional scaffolds enhances cell seeding efficiency and uniformity. Biotechnol Bioeng. (2003) 84:205–14. doi: 10.1002/bit.10759
76. Candiani G, Raimondi MT, Aurora R, Lagana' K, Dubini G. Chondrocyte response to high regimens of cyclic hydrostatic pressure in 3-dimensional engineered constructs. Int J Artif Organs (2008) 31:490–9. doi: 10.1177/039139880803100604
77. Correia C, Pereira AL, Duarte AR, Frias AM, Pedro AJ, Oliveira JT. Dynamic culturing of cartilage tissue: the significance of hydrostatic pressure. Tissue Eng Part A (2012) 18:1979–91. doi: 10.1089/ten.TEA.2012.0083
78. Hoenig E, Winkler T, Mielke G, Paetzold H, Schuettler D, Goepfert C, et al. High amplitude direct compressive strain enhances mechanical properties of scaffold-free tissue-engineered cartilage. Tissue Eng Part A (2011) 17:1401–10. doi: 10.1089/ten.TEA.2010.0395
79. Murphy SV, Atala A. 3D bioprinting of tissues and organs. Nat Biotechnol. (2014) 32:773–85. doi: 10.1038/nbt.2958
80. Collins SF. Bioprinting is changing regenerative medicine forever. Stem Cells Dev. (2014) 23(Suppl. 1):79–82. doi: 10.1089/scd.2014.0322
81. Di Bella C, Fosang A, Donati DM, Wallace GG, Choong PF. 3D bioprinting of cartilage for orthopedic surgeons: reading between the lines. Front Surg. (2015) 2:39. doi: 10.3389/fsurg.2015.00039
82. O'Connell CD, Di Bella C, Thompson F, Augustine C, Beirne S, Cornock R, et al. Development of the Biopen: a handheld device for surgical printing of adipose stem cells at a chondral wound site. Biofabrication (2016) 8:015019. doi: 10.1088/1758-5090/8/1/015019
83. Duchi S, Onofrillo C, O'Connell CD, Blanchard R, Augustine C, Quigley AF, et al. Handheld co-axial bioprinting: application to in situ surgical cartilage repair. Sci Rep. (2017) 7:5837. doi: 10.1038/s41598-017-05699-x
84. Holland TA, Bodde EW, Cuijpers VM, Baggett LS, Tabata Y, Mikos AG, et al. Degradable hydrogel scaffolds for in vivo delivery of single and dual growth factors in cartilage repair. Osteoarthritis Cartilage (2007) 15:187–97. doi: 10.1016/j.joca.2006.07.006
85. Watanabe M. Memories of the early days of arthroscopy. Arthroscopy (1986) 2:209–14. doi: 10.1016/S0749-8063(86)80073-1
86. Dragoo JL, Samimi B, Zhu M, Hame SL, Thomas BJ, Lieberman JR, et al. Tissue-engineered cartilage and bone using stem cells from human infrapatellar fat pads. J Bone Joint Surg Br. (2003) 85:740–7. doi: 10.1302/0301-620X.85B5.13587
87. Bhagat V, Becker ML. Degradable adhesives for surgery and tissue engineering. Biomacromolecules (2017) 18:3009–39. doi: 10.1021/acs.biomac.7b00969
88. Allen AB, Gazit Z, Su S, Stevens HY, Guldberg RE. In vivo bioluminescent tracking of mesenchymal stem cells within large hydrogel constructs. (2014) 20:806–16. doi: 10.1089/ten.TEC.2013.0587
Keywords: cartilage, stem cells, scaffolds, hydrogels, tissue engineering, bioprinting, bio fabrication
Citation: Francis SL, Di Bella C, Wallace GG and Choong PFM (2018) Cartilage Tissue Engineering Using Stem Cells and Bioprinting Technology—Barriers to Clinical Translation. Front. Surg. 5:70. doi: 10.3389/fsurg.2018.00070
Received: 31 August 2018; Accepted: 08 November 2018;
Published: 27 November 2018.
Edited by:
Zsolt J. Balogh, University of Newcastle, AustraliaReviewed by:
Konstantinos Markatos, Biomedical Research Foundation of the Academy of Athens, GreeceHolly Tyler-Paris Pilson, Wake Forest Baptist Medical Center, Winston-Salem, United States
Copyright © 2018 Francis, Di Bella, Wallace and Choong. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Sam L. Francis, sfrancis1@student.unimelb.edu.au