Instruments for reproducible setting of defects in cartilage and harvesting of osteochondral plugs for standardisation of preclinical tests for articular cartilage regeneration
© Schwarz et al. 2015
Received: 20 February 2015
Accepted: 5 July 2015
Published: 28 July 2015
Standardisation is required in research, so are approval procedures for advanced therapy medical products and other procedures for articular cartilage therapies. The process of creating samples needs to be reproducible.
The aim of this study was to design, create and validate instruments (1) to create reproducible and accurate defects and (2) to isolate samples in the shape of osteochondral cylinders in a quick, reliable and sterile manner.
Adjustable instruments were created: a crown mill with a resolution of 0.05 mm and a front mill to create defects in articular cartilage and subchondral bone. The instruments were tested on knee joints of pigs from the slaughterhouse; 48 defects were created and evaluated. A punching machine was designed to harvest osteochondral plugs. These were validated in an in vivo animal study.
The instruments respect the desired depth of 0.5 and 1.5 mm when creating the defects, depending on whether the person using the instrument is highly experienced (0.451 mm; confidence interval (CI): 0.390 mm; 0.512 mm and 1.403 mm; CI: 1.305 mm; 1.502 mm) or less so (0.369 mm; CI: 0.297 mm; 0.440 mm and 1.241 mm; CI: 1.141 mm; 1.341 mm). Eighty samples were taken from knee joints of Göttingen Minipigs with this punching technique. The time needed for the harvesting of the samples was 7.52 min (±2.18 min), the parallelism of the sides of the cylinders deviated by −0.63° (CI: −1.33°; 0.08°) and the surface of the cartilage deviated from the perpendicularity by 4.86° (CI: 4.154°; 5.573°). In all assessed cases, a sterile procedure was observed.
Instruments and procedures for standardised creation and validation of defects in articular cartilage and subchondral bone were designed. Harvesting of samples in the shape of osteochondral cylinders can now be performed in a quick, reliable and sterile manner. The presented instruments and procedures can serve as helpful steps towards standardised operating procedures in the field of regenerative therapies of articular cartilage in research and for regulatory requirements.
Guidelines for the determination of therapeutic outcomes require reproducible and validated protocols to be observed. Standards would also be helpful to satisfy regulatory requirements for regeneration therapy of articular cartilage tissue in preclinical tests in vivo and in vitro [1, 2].
There are some specific challenges in preparing and isolating samples before and after the healing time regarding different types of analyses and the stated scientific hypotheses. Biomechanical tests in particular require specimens with a clear geometry. This is necessary in order to keep the specimen in place and allow free access for biomechanical testing devices such as indentation rods [3–6]. The same is true for specimens used in tribological test procedures [7–12]. Thus, the exact definition and isolation from surrounding tissue of the specimen is vital for reproducible results.
For the synthesis of regenerated articular cartilage tissue, a standardisation of the procedures is required. Most of the studies use defect models analysing regenerative concepts [13–16], but the procedures are rarely harmonised at the level of preparation. The operative procedures follow the clinical requirement that smooth defect edges, consisting of stable cartilage tissue, lie perpendicular to the bottom of the defect [17, 18]. Different procedures are described and validated for the debridement of fibrous and degenerative tissue prior to the treatment with autologous chondrocyte implantation (ACI) or Matrix-based ACI . Referring to published results and our own tests, the question arises if the frequently used curette can deliver the requested outcomes regarding the quality of the created articular defects in terms of the geometry and resection of the tissue [19, 20].
The regeneration of defects in the articular cartilage is described and investigated among others by different depths according to the hypothesis of the particular study design. One can roughly distinguish between partial and full thickness defects  which can be extended into the bone in order to open the subchondral lamella to enable stem cells to migrate into the defect  or in order to prepare osteochondral autologous transplantation .
However, the depth of the defects should be stable in dimension, homogenous in shape and conform to the same principle. The sides should be straight and the bottom of the defect should be perpendicular to the sides.
Therefore, a cutting device is required which produces smooth surfaces on the cartilage and the bone. It must be capable of working in a quick, reproducible manner and irrespective of the user’s expertise in order to guarantee standardisation in an in vivo model to produce advanced therapy medicinal product (ATMP). It also needs to be suited for scientific assessment and has to meet regulatory guidelines.
In the field of research of tissue engineering of articular cartilage, osteochondral blocks or plugs are often used with the subchondral bone as a fixation and the cartilage layer on top as protruding tissue to be examined. Thus, the isolation of samples can become a challenge when new tissue has to be isolated for testing. The time for preparation should be as short as possible to avoid changes arising after opening the joint.
Samples for biomechanical and other tests have to be of a specific size, depending on the test procedure. Several biomechanical tests require samples of a size varying between 4 mm  and 6 mm  in diameter. Therefore, large animal models have an advantage over small ones in this context also for measuring the outcome in osteoarthritis (OA) research . Sheep, goats, dogs, horses, pigs and also rabbits are mainly used in studies dealing with regenerative therapies for articular cartilage [26, 13, 27–30].
The aim of the study was to establish a reproducible design to create and isolate regenerative articular cartilage samples in large animals applicable in and ex vivo and in vitro.
In particular, instruments had to be designed and constructed allowing (1) the creation of defects and (2) the isolation of the area of the regenerated tissue after healing. The operating sequence can also be applied to other species, either in vitro, in vivo and ex vivo.
Material and methods
Tool for creating defects
We constructed and built tools for the creation of reproducible chondral or osteochondral defects in vivo and in vitro in joints of animals.
The outer sleeve of the front mill is placed in the groove and the inner section is turned clockwise, until the inbuilt stop respects the depth defined by the crown mill (Fig. 3c, d). Residual tissue at the bottom of the defect can be removed with the front mill or a curette. A curette (Uteruskürette 4.5 ml, Aesculap, Tuttlingen, Germany) was sharpened by the toolmaker for this purpose.
Validation of the defect tool
The hypothesis for the validation of the newly created instrument was twofold:
Firstly, we wanted to investigate if the tool could deliver the expected depth of a defect in articular cartilage or bone after the desired dimension was preset at the instrument. Secondly, differences between an experienced and a less experienced practised operator were to be addressed.
To validate the tool for creating defects with defined depths, we used trochleae of the knee joints of pigs (age approximately 5 months) from the local slaughterhouse. Defects with 0.5 mm (n = 12) and 1.5 mm (n = 12) in depth, respectively, were placed at random in each trochlea.
Two operators created a total of 48 defects in 12 trochleae, using the same tool.
One operator was a highly experienced operator (toolmaker DS); the other one was a scientist (biologist GR) with an assumed lower skill level in using tools.
The measurement algorithm was based on the idea that the first groove made by the crown mill represents the point of reference. Thus, the area in the middle of the defect that was created by the front mill and the untouched cartilage surface can be calculated as the difference in height according to the point of reference. The defects were measured in four positions (12, 3, 6 and 9 o’clock) at the three levels (circular groove, untouched articular surface and middle of the defect) three times. Taking the means of the triplicates, the average depth of one defect was calculated with regard to the depth of the groove created by the crown mill and the area created by the front mill. The measurements of the twelve defects with the same defined depth provided the average depth and the corresponding statistical deviation.
The depths were calculated by Excel 2010 (Microsoft® Corporation, Redmond, USA) in terms of differences, and the values of the results are shown graphically by box blots created by the Origin 8.6G software (OriginLab Corporation, Northampton, USA). Differences in the results of both operators were tested by the t test procedure in the SAS 9.3 program (SAS® Institute, Cary, USA). The level of significance was α = 0.05.
Harvesting the samples after healing
There are some issues to be considered and overcome when osteochondral samples have to be taken out of the joint, in particular from the bone after a longer healing period.
The articular cartilage layer is supported by the subchondral bone lamella which can develop into a rigid structure [31–33] during OA. This structure can occur in an in vivo experiment after a healing time of up to 1 year or even less. In preliminary tests, we experienced that the preparation with hammer and chisel or punches could result in specimen with uneven geometry regarding the sides and the shape of the desired cylinders (plugs). We noticed that the specimen cannot be stabilised enough and the tool (punch) cannot be kept in position relative to the specimen, as the specimen have to be kept moist to prevent exsiccation. The use of a saw for the separation of specimen causes damage, and the sawdust created by the sawing process can pollute the adjacent surface. Furthermore, the width of the saw has to be taken into account as it needs a layer of tissue between two desired samples, or valuable tissue may be lost in the process. The more defects are created close to one another in one anatomical structure like the facets of the trochlea, the more the distance between them and the surrounding tissue becomes critical. For biomechanical tests, osteochondral plugs are required with isolated regenerated cartilage tissue on the top, to enable e.g. unconfined compression  or tribological tests . Thus, the osteochondral plug had to be taken out of the middle of the defect area and frayed edges had to be avoided. A cylindrical shape of the sample guarantees a correct and reproducible way of fixating the plug in fixing devices used for mechanical tests. The plane with the layer (cartilage or cartilage like tissue) on top should be perpendicular to the middle axis of the cylindrical plug. In particular, regarding tribological tests, the surface of the regenerated or cartilage tissue has to be protected against touching or any other outside influence. This has to be taken into account when handling (e. g. while harvesting) the samples. Several types of analyses make the samples sensitive for tissue defects like drying or degradation of proteins. The frictional properties change as well . An important requirement in this context seems to be a quick and safe preparation technique. This is even more important when the analysis requires sterile samples for e.g. cell culture.
The isolation of the samples has to be easy and reliable despite all critical situations described above.
The presented construction for harvesting samples of articular cartilage after healing in vivo is based on a solid frame. A bench vise is mounted which is movable below and allows the adjustment of the fixed sample under the vertically mounted punch in a correct, perpendicular position in relation to the articular surface.
In some cases, the osteochondral plug remains in the punch when retracting it. The punch (Fig. 5a) is equipped with a kind of window through which the plug can be taken out with tweezers. A rod is inserted at the bony end of the plug and driven out by gentle blows with a hammer; thus, the surface of the cartilage remains untouched.
Validation of the harvesting tool
We applied the harvesting tools in a study using a large animal model with artificial articular defects in both facets of the trochlea at both sides according to Gotterbarm et al. . The study was approved by the ethical committee number 35-9185.81/G-6/11 (Regierungspräsidium Karlsruhe, Germany).
We determined (1) the time needed to create an osteochondral plug, (2) the parallelism of the sides of the plug, (3) the deviation of its surface from its symmetric axis that should be 0° regarding the addressed 90°, and (4) the sterility of the procedure if sterile samples are needed.
We started timing when the adjustment of the defect to the punch above began after the separated trochlea was fixated in the bench clamp and stopped the time when the osteochondral plug was positioned under the camera taking pictures (body: Canon EOS 7D; lens: Canon EF 100 mm/2.8 L; Canon, Tokyo, Japan) for analysing the shape and geometry of the plug. The camera was mounted on a frame (camera stand RSX, arm RTX and lightning device RB5000; Kaiser Fototechnik GmbH und Co.KG, Buchen, Germany) parallel to the base where the plug was placed on its side. Thus, the optical-parallaxes were avoided, and a contactless measurement became possible.
The geometry of the osteochondral plugs was analysed through the pictures taken after harvesting. For this purpose, pictures were taken from four different angles, and a particular view of the side of the plug that seemed the least straight was taken for evaluation. The geometry of the plug was analysed with the OpenOffice 3.4 Draw program (Apache Software Foundation, Forest Hill MD, USA).
Both sides of the plug form a positive angle towards the cartilage at the top if the tangents at the sides converge, a negative angle vice versa.
Eighty plugs, harvested from both trochleae of 10 Göttingen Minipigs, were analysed. Sterility was checked by swabs (Copan Diagnostics Inc. Murrieta CA, US or Nerbeplus, Winsen/Luhe, Germany) at the surfaces of the remaining trochlea and analysed. The swabs were incubated according to the microbiological and infectiological quality standards (Mikrobiologisch-infektiologische Qualitätsstandarts (MiQ)) of the German Society for Hygiene and Microbiology (Deutsche Gesellschaft für Hygiene und Mikrobiologie (DGHM)) between 2 and 10 days both in an anaerobic and aerobic environment . Positive results were not detected.
The time needed for harvesting the plugs was calculated in Excel for the mean and standard deviation. We calculated the means and 95 % confidence intervals (CI) by SAS 9.3 for the parallelism of the sides of the plug and the deviation of the edge of the surface of the plugs from their centreline.
Validation of the defect tool
Validation of the harvesting tool
The plugs were isolated after 7.42 ± 2.28 min in the mean.
The sides showed a mean deviation of −0.63° (CI: −1.33°; 0.08°) in 80 cases with a value of 0° for parallelism; thus, the punch and the whole apparatus worked consistently for all examined specimens. A critical geometry is the relation of the slope of the articular surface to the axis of the cylindrically shaped plug, which should be 90° in the best case. Deviations were calculated with 4.86° (CI: 4.154°; 5.573°) from the rectangularity (Fig. 5c).
Sterility was given in all cases (n = 80).
Reproducibility and standardisation of procedures in experimental surgery has more limitations the smaller the animals are, especially when articular cartilage is examined. But experiments with large animals are expensive in comparison to smaller ones like rodents or rabbits. A harmonisation of surgical procedures could deliver comparability between various experiments published in literature, leading to fewer animals needed in the end. Mainly regulatory requirements can be met if tools for standardisation are provided for surgeons, experimenters and lab personnel. But the quality of the particular scientific study will also benefit from tools that enable secure and quick work with animals and samples, respectively.
Information on tools used for creating defects in cartilage layer is given in publications of studies in the field [14, 15], and some authors describe the surgical technique in particular for validation [19, 20]. Frequently, the curettage is the recommended tool for creating the defects in combination with knives or circular cutting devices to determine the edges of the defect [19, 20]. The curette seems to be appropriate for removing tissue of the inner part of the defect. But its use is limited on the edges as its diameter has to be smaller than the diameter of an intended circular defect leading to irregular edges of the defect when looked at from above . Seen from the side, the required perpendicularity between the sides and the bottom of the defect is not always possible. This is also the case if the curette has an offset (15°)  and bits of tissue may be found at the bottom depending on the technique used [19, 20]. If tissue remains in the “corners”, thus creating an inclined plane, it is a possibility that the implant slips out through the shear forces arising from the joint while moving. Bits of tissue are also found in the inner part of the defects after the use of a curette if e.g. the applied force was not strong enough . However, the correct geometry of the defect is crucial for the stability of the construct. It is either glued, sutured or covered with a periosteal flap [26, 15], because the construct has to be protected through stable flanks for shouldering , and sutures need to find anchorage. Thus, primary stability of the implant can be supported by an appropriate quality of the defect avoiding a dislocation of the implanted construct. Punches or trephines are also used to create the defects as described [14, 15] to deliver well-shaped defects with regard to the defect edges. But controlling the depth is not always possible in situ during surgery due to the parallax of view in deeper levels. The removal of the core of the defect cylinder can be difficult if the bottom of the defect core stays in contact with the substrate. Chondral defects are prepared by custom-made instruments like an angulated raspatorium . However, circular punches or trephines provide no centring components like drilling tools and depth control in high resolution. Both specifications are implemented in the presented instrument: a precise and reproducible centring and adjustment of the depth in 0.05-mm steps.
The crucial issue in creating the defect is the depth. From the biological point of view, the anatomical edges are important like subchondral lamella or the tidemark. Both are hard to detect in the situs of operation, and surrogate criteria are used like the sound (“metal on stone” ) or training the surgeon to handle the curette properly . However, experienced surgeons are in demand to create the defects. But the results show that the intended depths are not always reached depending on the applied technique [19, 20].
The presented instruments work independently of the force applied  as they are adjusted via positioning before use. Thus, reproducibility is given for experts and less experienced users as the data show in the validation experiment (Fig. 6). Hence, the disadvantage of this procedure may be seen in the fact that the depth of the defect has to be determined before creating it. But information on the height of the articular cartilage can be achieved by imaging or species-specific data [36, 37]. In addition, one can proceed stepwise respecting the expected depth as the cutting behaviour will change depending on the tissue while using the crown mill; also, isolated bleeding indicates a partial opening of the bone marrow. Thus, the advantage is that the crown mill is determining the final depth and can also be used as pilot instrument. The front mill will finish the defect while respecting the previously identified depth.
However, we have not compared our results to the results achieved through conventional techniques, neither before nor after healing processes. But we assume that the new technique we developed is less prone to influences such as the expertise of the surgeon executing the operation. We also believe that the new technique is likely to be a lot faster. Another disadvantage of the new technique could be that only defects of one predetermined diameter can be created during any one operation. Changing the diameter is thus not possible while operating. As the instruments were designed for the use in preclinical studies, where the size of the defect is determined before the operation, this is not a disadvantage. As our previous tests have shown, so far the diameter cannot be smaller than 4 mm. However, it is possible to create a crown mill and corresponding front mill of a larger diameter than the 6 mm we used.
Histopathological examination is indicated as the predominant outcome measurement tool in OA [26, 38, 39, 25, 16] and for regenerative therapeutic procedures, analysing the cartilage layer or regenerative tissue, the subchondral plate and the combination of both with other aspects . Thus, the suitable harvesting of osteochondral samples is crucial for the preparation of histological sections. Proper sampling protocols need to respect comparable anatomical locations, or one has to focus on the most severe lesions [40, 25, 41, 42]. There are up to 12 regions requested for examination in a medial tibial condyle if a complex analysis is required, including several issues like biochemistry, biomechanics, gene expression, etc. . The presented tool for the harvesting of osteochondral samples allows the isolation of several specimens even if they lie close together (Fig. 5). While sawing or grinding creates debris in the process, punching separates the tissue without leaving any debris. More importantly, it seems that the fact that the edges of the samples are smooth and defined, frayed and destroyed texture and cells can be avoided. Thermal alterations of the tissue can also be excluded as punching is executed under the application of PBS which, in addition, avoids drying out of the sample.
The presented punching procedure allows the exact harvesting of regenerated tissue or tissue originating from other locations, as the used apparatus allows the individual adjustment of the punch as desired. In combination with a 6-mm defect in diameter, a 5-mm sample in diameter can be extracted exactly as shown (Fig. 5). Further preparations of the articular layer on top are possible, as contamination is excluded by the used of “no touch” technique. Thus, a good starting point is also given for gene expression analysis or cell culture. The latter is possible as sterile preparation can be guaranteed.
In conclusion, we can provide new instruments and procedures for standardisation of creating defects in vitro and in vivo and for exact harvesting of samples in a quick, secure and sterile manner.
Collagen I scaffold without cells, provided by Amedrix, Esslingen, Germany.
The study was supported by the Federal Ministry of Education and Research; Grant number: 1315577G and PTJ 031577I (“Funktionelle Qualitätssicherung von regenerativen Gewebeersatzmaterialien für Knorpel und Meniskus (QuReGe)”).
Thanks to the Institute for Medical Microbiology and Hygiene, University Clinic Mannheim, Germany for support.
We acknowledge financial support by Deutsche Forschungsgemeinschaft and Ruprecht-Karls-Universität Heidelberg within the funding programme Open Access Publishing.
Thanks to Fa. Amedrix, Esslingen, Germany, for providing the Collagen1 scaffolds.
Thanks to Ms. Renate Cluever for her assistance with the English language.
Parts of this project were accepted for a poster presentation at the annual conference of the DGBM in Dresden, Germany (November, 6–8 2014).
Abstract: Reisig G., Schneider-Wald B., Schütte A., Brade J., Schleich D., Schwarz ML.
Instrumentarien zur reproduzierbaren Erstellung von Defekten im Gelenkknorpel und Gewinnung von Proben daraus im präklinischen Versuch. In: BioNanoMat. 2014; 15 (S1), 143.
- ASTM F2451-05(2010), Standard Guide for in vivo Assessment of Implantable Devices Intended to Repair or Regenerate Articular Cartilage. ASTM International, West Conshohocken, PA, 2010, http://www.astm.org; access July 13th 2015.
- EMEA/CHMP/410869/2006, Guideline on human cell-based medicinal products. European Medicines Agency, Canary Wharf, London, UK, 2008, http://www.emea.europa.eu; access July 13th 2015.
- Abedian R, Willbold E, Becher C, Hurschler C. In vitro electro-mechanical characterization of human knee articular cartilage of different degeneration levels: a comparison with ICRS and Mankin scores. J Biomech. 2013;46(7):1328–34. doi:10.1016/j.jbiomech.2013.02.004.PubMedView ArticleGoogle Scholar
- Fohr P, Hautmann V, Prodinger P, Pohlig F, Kaddick C, Burgkart R. Design of a high-dynamic closed-loop controlled cartilage test system. Orthopade. 2012;41(10):820–6. doi:10.1007/s00132-012-1953-4.PubMedView ArticleGoogle Scholar
- Katta J, Stapleton T, Ingham E, Jin ZM, Fisher J. The effect of glycosaminoglycan depletion on the friction and deformation of articular cartilage. Proc Inst Mech Eng H. 2008;222(1):1–11.PubMedView ArticleGoogle Scholar
- Stoffel M, Yi JH, Weichert D, Zhou B, Nebelung S, Muller-Rath R, et al. Bioreactor cultivation and remodelling simulation for cartilage replacement material. Med Eng Phys. 2012;34(1):56–63. doi:10.1016/j.medengphy.2011.06.018.PubMedView ArticleGoogle Scholar
- Bell CJ, Ingham E, Fisher J. Influence of hyaluronic acid on the time-dependent friction response of articular cartilage under different conditions. Proc Inst Mech Eng H. 2006;220(1):23–31.PubMedView ArticleGoogle Scholar
- Forster H, Fisher J. The influence of loading time and lubricant on the friction of articular cartilage. Proc Inst Mech Eng H. 1996;210(2):109–19.PubMedView ArticleGoogle Scholar
- Gleghorn JP, Doty SB, Warren RF, Wright TM, Maher SA, Bonassar LJ. Analysis of frictional behavior and changes in morphology resulting from cartilage articulation with porous polyurethane foams. J Orthop Res. 2010;28(10):1292–9. doi:10.1002/jor.21136.PubMedView ArticleGoogle Scholar
- Katta J, Jin Z, Ingham E, Fisher J. Effect of nominal stress on the long term friction, deformation and wear of native and glycosaminoglycan deficient articular cartilage. Osteoarthritis Cartilage. 2009;17(5):662–8. doi:10.1016/j.joca.2008.10.008.PubMedView ArticleGoogle Scholar
- Schwarz ML, Schneider-Wald B, Krase A, Richter W, Reisig G, Kreinest M, et al. Tribological assessment of articular cartilage. A system for the analysis of the friction coefficient of cartilage, regenerates and tissue engineering constructs; initial results. Orthopade. 2012;41(10):827–36. doi:10.1007/s00132-012-1951-6.PubMedView ArticleGoogle Scholar
- Wimmer MA, Grad S, Kaup T, Hanni M, Schneider E, Gogolewski S, et al. Tribology approach to the engineering and study of articular cartilage. Tissue Eng. 2004;10(9-10):1436–45. doi:10.1089/ten.2004.10.1436.PubMedView ArticleGoogle Scholar
- Chu CR, Szczodry M, Bruno S. Animal models for cartilage regeneration and repair. Tissue Eng Part B Rev. 2010;16(1):105–15. doi:10.1089/ten.TEB.2009.0452.PubMed CentralPubMedView ArticleGoogle Scholar
- Gotterbarm T, Breusch SJ, Schneider U, Jung M. The minipig model for experimental chondral and osteochondral defect repair in tissue engineering: retrospective analysis of 180 defects. Lab Anim. 2008;42(1):71–82. doi:10.1258/la.2007.06029e.PubMedView ArticleGoogle Scholar
- Jubel A, Andermahr J, Schiffer G, Fischer J, Rehm KE, Stoddart MJ, et al. Transplantation of de novo scaffold-free cartilage implants into sheep knee chondral defects. Am J Sports Med. 2008;36(8):1555–64. doi:10.1177/0363546508321474.PubMedView ArticleGoogle Scholar
- Schneider-Wald B, von Thaden AK, Schwarz ML. Defect models for the regeneration of articular cartilage in large animals. Orthopade. 2013;42(4):242–53. doi:10.1007/s00132-012-2044-2.PubMedView ArticleGoogle Scholar
- Behrens P, Bosch U, Bruns J, Erggelet C, Esenwein SA, Gaissmaier C, et al. Indications and implementation of recommendations of the working group “Tissue Regeneration and Tissue Substitutes” for autologous chondrocyte transplantation (ACT). Z Orthop Ihre Grenzgeb. 2004;142(5):529–39. doi:10.1055/s-2004-832353.PubMedView ArticleGoogle Scholar
- Steinwachs MR, Erggelet C, Lahm A, Guhlke-Steinwachs U. Clinical and cell biology aspects of autologous chondrocytes transplantation. Unfallchirurg. 1999;102(11):855–60.PubMedView ArticleGoogle Scholar
- Drobnic M, Radosavljevic D, Cor A, Brittberg M, Strazar K. Debridement of cartilage lesions before autologous chondrocyte implantation by open or transarthroscopic techniques: a comparative study using post-mortem materials. J Bone Joint Surg Br. 2010;92(4):602–8. doi:10.1302/0301-620X.92B3.22558.PubMedView ArticleGoogle Scholar
- Mika J, Clanton TO, Pretzel D, Schneider G, Ambrose CG, Kinne RW. Surgical preparation for articular cartilage regeneration without penetration of the subchondral bone plate: in vitro and in vivo studies in humans and sheep. Am J Sports Med. 2011;39(3):624–31. doi:10.1177/0363546510388876.PubMedView ArticleGoogle Scholar
- Redman SN, Oldfield SF, Archer CW. Current strategies for articular cartilage repair. Eur Cell Mater. 2005;9:23–32. discussion 23-32.PubMedGoogle Scholar
- Richter W, Diederichs S. Regenerative medicine in orthopaedics. Cell therapy—tissue engineering—in situ regeneration. Orthopade. 2009;38(9):859–67. doi:10.1007/s00132-009-1459-x. quiz 68-9.PubMedView ArticleGoogle Scholar
- Gudas R, Kalesinskas RJ, Kimtys V, Stankevicius E, Toliusis V, Bernotavicius G, et al. A prospective randomized clinical study of mosaic osteochondral autologous transplantation versus microfracture for the treatment of osteochondral defects in the knee joint in young athletes. Arthroscopy. 2005;21(9):1066–75. doi:10.1016/j.arthro.2005.06.018.PubMedView ArticleGoogle Scholar
- Schneider U, Schmidt-Rohlfing B, Gavenis K, Maus U, Mueller-Rath R, Andereya S. A comparative study of 3 different cartilage repair techniques. Knee Surg Sports Traumatol Arthrosc. 2011;19(12):2145–52. doi:10.1007/s00167-011-1460-x.PubMedView ArticleGoogle Scholar
- Little CB, Smith MM, Cake MA, Read RA, Murphy MJ, Barry FP. The OARSI histopathology initiative—recommendations for histological assessments of osteoarthritis in sheep and goats. Osteoarthritis Cartilage. 2010;18 Suppl 3:S80–92. doi:10.1016/j.joca.2010.04.016.PubMedView ArticleGoogle Scholar
- Brehm W, Aklin B, Yamashita T, Rieser F, Trub T, Jakob RP, et al. Repair of superficial osteochondral defects with an autologous scaffold-free cartilage construct in a caprine model: implantation method and short-term results. Osteoarthritis Cartilage. 2006;14(12):1214–26. doi:10.1016/j.joca.2006.05.002.PubMedView ArticleGoogle Scholar
- Gavenis K, Schneider U, Maus U, Mumme T, Muller-Rath R, Schmidt-Rohlfing B, et al. Cell-free repair of small cartilage defects in the Goettinger minipig: which defect size is possible? Knee Surg Sports Traumatol Arthrosc. 2012;20(11):2307–14. doi:10.1007/s00167-011-1847-8.PubMedView ArticleGoogle Scholar
- Gille J, Kunow J, Boisch L, Behrerns P, Bos I, Hoffmann C, et al. Cell-laden and cell-free matrix-induced chondrogenesis versus microfracture for the treatment of articular defects: a histological and biomechanical study in sheep. Cartilage. 2010;1(1):29–42.PubMed CentralPubMedView ArticleGoogle Scholar
- Goodrich LR, Hidaka C, Robbins PD, Evans CH, Nixon AJ. Genetic modification of chondrocytes with insulin-like growth factor-1 enhances cartilage healing in an equine model. J Bone Joint Surg Br. 2007;89(5):672–85. doi:10.1302/0301-620X.89B5.18343.PubMedView ArticleGoogle Scholar
- Shortkroff S, Barone L, Hsu HP, Wrenn C, Gagne T, Chi T, et al. Healing of chondral and osteochondral defects in a canine model: the role of cultured chondrocytes in regeneration of articular cartilage. Biomaterials. 1996;17(2):147–54.PubMedView ArticleGoogle Scholar
- Lahm A, Kreuz PC, Oberst M, Haberstroh J, Uhl M, Maier D. Subchondral and trabecular bone remodeling in canine experimental osteoarthritis. Arch Orthop Trauma Surg. 2006;126(9):582–7. doi:10.1007/s00402-005-0077-2.PubMedView ArticleGoogle Scholar
- Pastoureau P, Leduc S, Chomel A, De Ceuninck F. Quantitative assessment of articular cartilage and subchondral bone histology in the meniscectomized guinea pig model of osteoarthritis. Osteoarthritis Cartilage. 2003;11(6):412–23.PubMedView ArticleGoogle Scholar
- Orth P, Cucchiarini M, Kohn D, Madry H. Alterations of the subchondral bone in osteochondral repair—translational data and clinical evidence. Eur Cell Mater. 2013;25:299–316. discussion 4–6.PubMedGoogle Scholar
- Pickard JE, Fisher J, Ingham E, Egan J. Investigation into the effects of proteins and lipids on the frictional properties of articular cartilage. Biomaterials. 1998;19(19):1807–12.PubMedView ArticleGoogle Scholar
- (DGHM) DGfHuM, Podbielski AH, Herrmann MH, Kniehl EH, Mauch HH, Rüssmann HH. MiQ: Qualitätsstandards in der mikrobiologisch-infektiologischen Diagnostik. München: Urban & Fischer Verlag/Elsevier GmbH; 2007.Google Scholar
- Frisbie DD, Cross MW, McIlwraith CW. A comparative study of articular cartilage thickness in the stifle of animal species used in human pre-clinical studies compared to articular cartilage thickness in the human knee. Vet Comp Orthop Traumatol. 2006;19(3):142–6.PubMedGoogle Scholar
- Koff MF, le Chong R, Virtue P, Chen D, Wang X, Wright T, et al. Validation of cartilage thickness calculations using indentation analysis. J Biomech Eng. 2010;132(4):041007. doi:10.1115/1.4000989.PubMedView ArticleGoogle Scholar
- Custers RJ, Saris DB, Dhert WJ, Verbout AJ, van Rijen MH, Mastbergen SC, et al. Articular cartilage degeneration following the treatment of focal cartilage defects with ceramic metal implants and compared with microfracture. J Bone Joint Surg Am. 2009;91(4):900–10. doi:10.2106/JBJS.H.00668.PubMedView ArticleGoogle Scholar
- Jung M, Kaszap B, Redohl A, Steck E, Breusch S, Richter W, et al. Enhanced early tissue regeneration after matrix-assisted autologous mesenchymal stem cell transplantation in full thickness chondral defects in a minipig model. Cell Transplant. 2009;18(8):923–32. doi:10.3727/096368909X471297.PubMedView ArticleGoogle Scholar
- Appleyard RC, Burkhardt D, Ghosh P, Read R, Cake M, Swain MV, et al. Topographical analysis of the structural, biochemical and dynamic biomechanical properties of cartilage in an ovine model of osteoarthritis. Osteoarthritis Cartilage. 2003;11(1):65–77.PubMedView ArticleGoogle Scholar
- Young AA, Appleyard RC, Smith MM, Melrose J, Little CB. Dynamic biomechanics correlate with histopathology in human tibial cartilage: a preliminary study. Clin Orthop Relat Res. 2007;462:212–20. doi:10.1097/BLO.0b013e318076b431.PubMedView ArticleGoogle Scholar
- Young AA, McLennan S, Smith MM, Smith SM, Cake MA, Read RA, et al. Proteoglycan 4 downregulation in a sheep meniscectomy model of early osteoarthritis. Arthritis Res Ther. 2006;8(2):R41. doi:10.1186/ar1898.PubMed CentralPubMedView ArticleGoogle Scholar
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