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Logo of nihpaAbout Author manuscriptsSubmit a manuscriptHHS Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
 
Knee. Author manuscript; available in PMC 2012 August 1.
Published in final edited form as:
PMCID: PMC2991424
NIHMSID: NIHMS209693

Human anterior cruciate ligament fibroblasts from immature patients have a stronger in vitro response to platelet concentrates than those from mature individuals

Abstract

A number of recently published studies have established a substantial age dependence of the response of ACL fibroblasts to stimulation by platelet-rich plasma (PRP). Further in-depth research of this age dependence revealed negative effects on both histological and biomechanical results in a large animal model. However, while it has been postulated that this association could affect potential human applications negatively too it remains to be proven that the same effects occur in human cells. Thus it was the objective of this study to search for age dependence in human fibroblasts before further human experiments are done. Human fibroblasts were obtained from 10 immature and adolescent patients, based on a-priori power calculations, and culture in a collagen-PRP composite. Three parameters that are pivotal for defect remodeling and wound healing – cell migration, cell proliferation, and scaffold contraction – were chosen as endpoints. Both migration and proliferation were significantly higher in immature cells, but no differences were seen in wound contraction. The former findings suggest that immature patients respond more favorably to treatment with PRP, which consequently might translate into better results in ACL tissue engineering.

INTRODUCTION

Injury to the Anterior Cruciate Ligament (ACL) is an important clinical problem leading with two main consequences: immediate joint instability and early onset of osteoarthritis, both considerably painful and disabling 1. A growing body of evidence has recently been accumulated that consistently shows that while current treatment options alleviate instability almost entirely, the risk for premature osteoarthritis remains high even in those patients receiving the best currently available treatment, ACL reconstruction 24. Due to these poor long-term results even with the current gold standard of treatment, new methods for ACL repair are being sought 3; 5.

Ongoing research has had an increased focus on repairing ACL ruptures using tissue engineering in the form of a suture repair enhanced with implanted provisional scaffold materials (namely collagen-platelet composites) to promote regeneration and healing 3; 69. With the use of the provisional scaffolds as structural support and a platelet concentrate as a source of growth factors, a marked improvement in ligament healing can be stimulated 3; 612. A body of literature has been published on the development and testing of such an approach in large animal models 3; 59; 12. This research has produced a consistent and comprehensive picture of the in vitro and in vivo mechanisms, from the cell to the tissue and organ level, of enhanced primary ACL repair, but its human application still awaits confirmation.

One of the probably most intriguing findings in this model was clear evidence for age dependence of ACL fibroblast behavior, particularly in response to stimulation by a platelet-concentrate. This difference was mostly seen when comparing skeletally immature (open physes) with either adolescent (closing physes) or adult (closed physes) individuals 1315. While this seems biologically plausible and is consistent with conventional orthopaedic wisdom, suggesting that fractures in skeletally immature patients will heal faster than those in adolescents or adults 16; 17, the influence of age on the healing of ligaments has not been sufficiently studied or determined before. Moreover, considering that there is still a lack of clinically convincing treatment options in skeletally immature patients with ACL tears and that immature individuals have disconcertingly high failure rates for ACL reconstruction, this population could profit most from a tissue engineering repair procedure 5. Such an interpretation is supported by recent findings showing that age-dependence does not only exist on the cellular level, but translates on to the tissue level as well, thus being reflected in biomechanical outcome after tissue engineering enhanced primary repairs 15.

While research in animal models has demonstrated efficacy of this technique it is yet unknown if human cells will have similar responses. In this paper, we hypothesize that skeletally immature human ACL fibroblasts (from patients with open physes) in a collagenous biomaterial have a stronger response to a platelet concentrate than cells from older individuals. Assuming that enhanced repair will primarily target younger individuals, and given that evidence suggests on differences in the behavior of adolescent and adult cells13; 14, we chose adolescent, rather than adult, patients as controls. We chose the three parameters of cellular migration, proliferation, and scaffold contraction as endpoints for modeling the extent of wound healing and scar maturation in vitro.

METHODS

Institutional Review Board approval was obtained prior to beginning the study. Consistent with earlier published data 1315, a sample size was calculated to allow for testing for an effect size of at least 2 with 80% at an alpha of 5%. Thus, with parental consent, ACL tissue was obtained from the tibial stump from 5 skeletally immature (11.0 ± 0.9 years, male) and 5 adolescent patients (15.0 ± 0 years, 4 female 1 male) undergoing surgical treatment for complete, midsubstance ACL tears within 6 months after the initial injury. Age grouping was based on physeal status about the knee, again in consistency with both methods and findings from said earlier studies. All tissues were obtained from patients undergoing ACL reconstruction surgery Children’s Hospital Boston, MA, and Children’s Hospital, Waltham, MA.

Cell Culture

ACL tissue was harvested intra-operatively using sterile technique. After harvest, explants were washed three times in 1% Antibiotic-Antimycotic solution (AB/AM) (Mediatech Inc., Herndon, VA.) followed by three washes with sterile 1X Phosphate Buffer Saline (PBS) (EMD Chemicals, Gibbstown, NJ), cut to approx 1mm3 and transferred onto six-well plates. The explants were allowed to adhere to the plates, and then media (DMEM (Mediatech, Herndon, VA.) 10% FBS (HyClone Inc., South Logan, UT), 10% Fetal Bovine Serum (FBS) and 1% AB/AM) was added. The explants were maintained in culture, and the media was changed two times per week. When the primary outgrowth cells were 80% confluent, they were trypsinized using a standard trypsin EDTA protocol and either reseeded in T-75 culture flasks or frozen and stored at −80°C until all groups had been collected for the experiment. All cells used for this experiment were first or second passage.

Migration Assay

Cell migration was measured using a modified Boyden chamber assay (Chemicon International Inc. Kit: QCM 24-well colorimetric cell migration assay). The upper and lower chambers are separated by an 8μm polycarbonate membrane and their migration through this membrane from the upper to lower chamber is measured using a cell stain solution. For each time point (4 and 24 hours) eight wells were analyzed per patient per age group. In addition, four negative control wells without cells (empty controls) were analyzed at each time point to control and adjust for potential interaction between the used scaffold and the test reagents. The results of these negative controls were subtracted from the actual samples.

Serum-free quenching medium was added to each T-75 flask (Serum-free DMEM containing 10% FBS) and incubated for 24 hours prior to assay. After 24 hours, cells were washed with sterile Phosphate Buffer Saline (EMD Chemicals, Gibbstown, NJ). Five milliliters of harvesting buffer (0.05% trypsin in Hanks Balanced Salt Solution (HBSS) containing 25mM HEPES, Cellgro, Mediatech, Inc, Herndon, VA) was added to the cells and incubated at 37°C for 15 minutes. After 15 minutes, cells were gently pipetted off the dish and 15mL of quenching medium (Serum-free DMEM containing 10% FBS) was added. Cells were centrifuged for 5 minutes at 1200rpm until pellets were formed. Pellets were resuspended in 5mL of quenching medium [serum-free DMEM containing 5% Bovine Serum Albumin (BSA)]. 300 μL of cell suspension (0.5–1.0 × 106 cells/mL in chemoattractant-free media (serum-free DMEM containing 5% BSA) and 500μL of serum free media (serum-free DMEM) were added to each insert. Inserts were handled with forceps sterilized with 70% ethanol. Plates were covered and incubated for 4 to 24 hours (37°, 5% CO2). At the designated time points, cells were removed from the top side of the insert by pipetting out remaining cell suspension and placed into a clean well containing 400μL of cell stain. New wells were incubated for 20 minutes at room temperature. Inserts were dipped into a clean well with water to rinse. Promptly after rinsing, the cells were removed from the interior of the insert using cotton-tipped swabs. Inserts air dried for 20 minutes and then transferred into a clean well containing 200μL of extraction buffer (part no. 90145) for 15 minutes at room temperature. Stain was extracted by tilting insert back and forth several times during incubation. Inserts were removed from the well mixture was transferred onto a 96-well microtiter plate from which the optical density was read at 562nm.

Preparation of collagen-PRP provisional scaffold

Acid -soluble, Type I collagen slurry was made by solubilizing bovine patellar tendon tissue. In brief, bovine tissue was sterilely harvested and solubilized in an acid solution as previously described11. Collagen content within the slurry was adjusted to greater than 5 mg/ml and neutralized with 0.1M HEPES (Cellgro, Mediatech, Inc, Herndon, VA), 5X PBS (HyClone Logan, Utah)to obtain a final pH of 7.4.

Platelet rich plasma (PRP) was prepared from human whole blood. Human platelets were prepared from six hundred milliliters of whole blood drawn from one hematologically normal individual. Blood was collected in a bag with 10% by volume acid-citrate dextrose. The blood was centrifuged for 6 minutes at 150g (GH 3.8 rotor, Beckman GS-6 Centrifuge, Fullerton, CA). The supernatant was aspirated and collected as platelet-rich plasma in a 50 ml tube. The platelet-rich plasma was then centrifuged again (GH 3.8 rotor, Beckman GS-6 Centrifuge, Fullerton, CA) and the platelet poor plasma supernatant was aspirated off. Complete blood counts (CBC’s) were performed on the whole blood, platelet poor and platelet rich solutions. The resulting platelet pellet was resuspended in enough platelet poor plasma to bring the platelet concentration of the solution to approximately 3× that of the whole blood. A second CBC was performed on the platelet rich plasma to ensure the desired concentration was achieved.

The collagen-platelet composites were made by combining the cell-seeded platelet solution and cold, neutralized collagen solution. Each 0.5 ml CPC contained 0.19 ml cell-seeded PRP and 0.31 ml collagen-buffer solution and 7.5×105 cells per gel. The collagen solution was transferred into silicone semitubular molds with polyethylene mesh at each end to anchor the gels within six well plates using a repeat pipettor. This was done to ensure uniform volume across all scaffolds. The scaffolds were incubated at 37°C for one hour, to ensure complete gelation. Negative control scaffolds were created in the exact same fashion using PRP without cells. After gelation, six milliliters of complete media was added to each well to cover the composites. Samples were cultured in a 37°C CO2 humidified incubator and the complete media was changed twice per week.

MTT Assay

Fibroblast number in the CPCs at day 2, 7, and day 14 was determined by using the MTT [3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide] assay; MTT powder (USB Corporation, Cleveland, OH) was mixed with PBS at a ration of 1mg/ml for this assay. A total of eight cell-seeded scaffolds analyzed at each time point (2, 7, and 14 days) for each patient per age group. In addition, four cell-free, negative controls of collagen-PRP were analyzed at each time point and all samples were normalized using these empty controls.

At the designated time point, the media was aspirated from each well, and the scaffolds were removed from the silicone semitubular molds and placed into individual wells of twelve well plates. One milliliter of the 1 mg/ml MTT solution was added to each well. Each gel was fully immersed in the MTT solution. After the MTT was added, the plates were incubated for 3 hours at 37 C and 5% CO2. Subsequently, the excess MTT solution was removed and 1 ml of sterile 1X PBS was added to each well. The plates were then placed on a horizontal agitator (Fisher Scientific Clinical Rotator, 100 rpm) and left to rinse at room temperature for 30 minutes. Rinses were repeated until absorbencies of the wash were less than 0.100 at 562 nm. All PBS was then removed and each gel transferred with a sterile spatula into a sterile 5.0 ml centrifuge tube. The gels were then placed in 1 ml of a detergent containing 20% aqueous Sodium dodecyl sulfate/formamide (1:1 volume ratio) in each tube and incubated overnight in at 37° C. Finally, the tubes were vortexed on high for 5 seconds and then centrifuged for 5 minutes at 1500rpm. Two hundred microliter aliquots of the supernatant from each tube were then transferred onto a sterile 96-well plate. The absorbencies were measured and 650nm, and the relative numbers of fibroblasts were determined.

Scaffold Contraction

Images of the gels were captured at Days 0, 2, 7 and 14 using a Canon, Rebel XT, EOS digital camera. The area of each scaffold was measured at each day using NIH Image J 1.37V. For each group, the scaffold areas were averaged and the mean and standard deviation reported. In addition, the percent of Day 0 size was calculated at each subsequent day. Again, 4 unseeded collagen-PRP scaffolds were used as negative controls.

Statistical analysis

Data analysis was done using intercooled Stata 10 (StataCorp, College Station, Tx). Repeated measure ANOVA or two-tailed t-tests were used; the Bonferroni method was employed to adjust p-values in case of multiple testing. All results are given as means±SD. A p-value of less than 0.05 was considered significant.

RESULTS

Platelet Solution Preparation

Platelet (PLT) count, Red Blood Cell (RBC) count, and White Blood Cell (WBC) count of the whole blood, platelet rich plasma, and platelet poor plasma can be found in Table 1. The enrichment factor for the platelet rich plasma was 3.39× of the whole blood platelet concentration.

Table 1
shows the cell counts for whole blood and PRP.

Migration Assay

No significant differences were seen between age groups at 4 hours (p=0.8605). However, at 24h the immature cells had a 14% greater increase in migration than the adolescent cells (327%±99% vs 287%±117%, p=0.0377, Figure 1).

Figure 1
Migration of Immature and Adolescent ACL Fibroblasts at 4 and 24 hours showed no differences initially, but a significantly higher rate of migration in immature cells after 24h. Error Bars represent standard deviation. (repeated measure ANOVA with post-hoc ...

MTT Assay

At day 2 there were no significant differences between groups. At days 7 and 14, the immature cells had significantly higher MTT results (p=0.0004 at 7d, p=0.004 at 14d, Figure 2)

Figure 2
Shows the results form the MTT assay representing cell proliferation. Error Bars represent standard deviation. Equal results at day 2 suggest equivalent seeding efficiency in both groups. There was a trend for a decrease in cell numbers in adolescent ...

Scaffold Contraction

There was no difference in scaffold contraction rates between the immature and adolescent groups. At day 0 there were no significant differences in scaffold size between any age group or control scaffolds (p > 0.019 for all comparisons). At day 2, immature scaffolds were 46% smaller, adolescent 48%, than their day 0 size, differences that were significantly greater than the change in size of control scaffolds (61%, p = 0.0062). At day 7, adolescent scaffolds were 47% smaller, and immature scaffolds were 46% smaller than their day 0 size, differences that were significantly greater than the change in size of control scaffolds which had shrunk to 39% of their initial size and stay at this size until day 14 (62%, p = 0.0041 for adolescent scaffolds, and p = 0.0038 for immature scaffolds), but not significantly different across age groups. (Figure 3)

Figure 3
Scaffold size as a percentage of Day 0 size at Day 2, 7, and 14. Both groups showed almost identical rates of scaffold contraction. That fact the rate of contraction was similar to the unseeded scaffolds in the control group suggest that reasons other ...

DISCUSSION

Tissue engineering enhanced ACL repair holds some promise as a new technique for the management of ACL tears. A body of literature that supports this claim has also consistently shown that the outcome of such a procedure depends on the age of the patient 13; 14. These findings are not only biologically and empirically plausible, but also clinically important since it is young and immature patients, who otherwise lack treatment options and thus often perform badly after ACL injury, that would probably benefit most from tissue engineering a repair of the ACL. However, this age-dependence has only been shown in large animal models so far, and while validity of these findings in human could be assumed, proof of their reproducibility in a human model was still missing. In this study we looked at age-dependence in three surrogate parameters of tissue healing and repair tissue maturation – cell proliferation, cell migration, and wound contraction and found a significant difference in cell proliferation and migration, but no difference in scaffold contraction, suggesting some age-dependence in humans, but maybe to a lesser extent that seen in large animal studies.

Our study has some limitations. First of all, while we calculated power a-priori, a point could be made that the lack of a significant difference in cell migration or contraction is due to a lack of power. However, while a large sample might have shown a statistically significant result, the absolute difference between groups would still have been too small to be clinically meaningful. Secondly, we based our categorization on biological age and skeletal maturity assessed by physeal closure about the knee, which might have left some room for error given the natural variability of maturation. A recently published study on the role of growth-factor receptors in the age-dependence of ACL fibroblast behavior showed that this dependence is rather based on absolute age than age groups18. Thirdly, cells obtained from human individuals should be considered more heterogeneous than those obtained from research animals, since samples cannot be take immediately after rupture/transection, but only during surgery, which is staged some time after the initial injury and not all time points are the same for all patients. However, these problems would also be encountered in a clinical scenario and might be appreciated as a shortcoming from a biological perspective, but an asset from a clinical one. Lastly, we were not able to obtain autologous PRP for all patients, because it is difficult to draw large volumes of blood from immature patients. Hence, we did not use autologous PRP, which limits the generalizablity of our findings for future clinical application.

For healing to occur following ACL injury, population by ACL fibroblasts of the wound site and the biomaterial spanning it is pivotal, which happens intitally by cell migration into the scaffold. These cells are critical to scar tissue formation in the joint, and have been found to migrate in the direction of the wound19; 20. However, after 24 hours, there is a statistically significant and likely clinically meaningful, by absolute numbers, superior migration in immature cells. Previous in vitro studies of porcine and ovine ACL cells have support this finding of greater migration potential in immature cells than adolescent or adult cells21. It is important to note, however, that these cells were taken from intact ACL tissue, whereas those used in this study of human cells were from patients undergoing surgery following a marked ACL tear, thus there is potential for even larger differences.

After repopulation of the wound site by cell migration, proliferation of these cells is the next crucial step in wound healing. Here, evidence for a significant difference between age groups was seen suggesting that immature cells grow faster and migrate faster than adolescent cells. These findings corroborate earlier findings in porcine and ovine cells 13; 14.

Finally, scaffold contraction should be seen as surrogate for wound contraction, which is a characteristic of wound maturation. The initial decrease in scaffold size, which occurred in both seeded slurries and negative controls, might be interpreted partially as shrinkage due to fluid flowing from the slurry to the osmotic denser cell culture medium and partially due to contraction by PRP clotting. From day 2 to day 7 and day 14 there are only marginal changes in scaffold size. This fact can be interpreted in two ways. First of all, this suggests that the cell-collagen construct is stable, which is an important finding for future clinical applications. Secondly, it suggests that our wound model is not fully mature yet, following the generally accepted fact that cell differentiation and contraction occur as final stages of wound healing subsequent to an earlier stage of cell migration and proliferation.

In conclusion, our findings show that cellular migration and proliferation are affected by age of human ACL fibroblasts, in a similar way as it has been described for large animal models. These findings indicate that immature individuals would benefit from tissue engineering ACL repair greater than adolescent individuals, or adults. Future research focusing on the reasons for such differences might allow bridging this rift.

Acknowledgments

The authors would like to thank Eduardo Abreu, Sophia L Harrison, and Ashley N Mastrangelo for their assistance with this project. Funding was received from NIH Grant AR054099 and AR052772 (MMM). Martha M. Murray is a founder and shareholder of Connective Orthopaedics.

Footnotes

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References

1. Von Porat A, Roos EM, Roos H. High prevalence of osteoarthritis 14 years after an anterior cruciate ligament tear in male soccer players: a study of radiographic and patient relevant outcomes. Br J Sports Med. 2004;38:263. [PMC free article] [PubMed]
2. Louboutin H, Debarge R, Richou J, Selmi TA, Donell ST, Neyret P, et al. Osteoarthritis in patients with anterior cruciate ligament rupture: a review of risk factors. Knee. 2009;16:239–244. [PubMed]
3. Murray MM. Current status and potential of primary ACL repair. Clin Sports Med. 2009;28:51–61. [PMC free article] [PubMed]
4. Oiestad BE, Engebretsen L, Storheim K, Risberg MA. Knee osteoarthritis after anterior cruciate ligament injury: a systematic review. Am J Sports Med. 2009;37:1434–1443. [PubMed]
5. Vavken P, Murray MM. Translational Studies in ACL repair. Tissue Eng Part A. 2009
6. Murray MM, Palmer M, Abreu E, Spindler KP, Zurakowski D, Fleming BC. Platelet-rich plasma alone is not sufficient to enhance suture repair of the ACL in skeletally immature animals: an in vivo study. J Orthop Res. 2009;27:639–645. [PMC free article] [PubMed]
7. Murray MM, Spindler KP, Abreu E, Muller JA, Nedder A, Kelly M, et al. Collagen-platelet rich plasma hydrogel enhances primary repair of the porcine anterior cruciate ligament. J Orthop Res. 2007;25:81–91. [PubMed]
8. Murray MM, Spindler KP, Ballard P, Welch TP, Zurakowski D, Nanney LB. Enhanced histologic repair in a central wound in the anterior cruciate ligament with a collagen-platelet-rich plasma scaffold. J Orthop Res. 2007;25:1007–1017. [PubMed]
9. Murray MM, Spindler KP, Devin C, Snyder BS, Muller J, Takahashi M, et al. Use of a collagen-platelet rich plasma scaffold to stimulate healing of a central defect in the canine ACL. J Orthop Res. 2006;24:820–830. [PubMed]
10. Fleming BC, Magarian E, Harrison S, Murray MM. Collagen scaffold supplementation does not improve fuctional properties of the repaired anterior cruciate ligament. J Orthop Res. 2009 submitted. [PMC free article] [PubMed]
11. Fleming BC, Spindler KP, Palmer M, Magarian E, Murray MM. Collagen-platelet composites improve the biomechanical properties of healing ACL grafts in a porcine model. AJSM. 2009 in press. [PMC free article] [PubMed]
12. Spindler KP, Murray MM, Carey JL, Zurakowski D, Fleming BC. The use of platelets to affect functional healing of an anterior cruciate ligament (ACL) autograft in a caprine ACL reconstruction model. J Orthop Res. 2009;27:631–638. [PMC free article] [PubMed]
13. Mastrangelo A, Haus B, Vavken P, Palmer M, Murray MM. Immature animals have denser anterior cruciate ligament wound site cell repopulation than adolescent or adult animals. J Orthop Res. 2009 [Epub ahead of print] [PMC free article] [PubMed]
14. Mastrangelo A, Magarian E, Palmer M, Vavken P, Murray M. The effect of skeletal maturity on the regenerative function of intrinsic ACL cells. J Orthop Res. 2009 [Epub ahead of print] [PMC free article] [PubMed]
15. Murray MM, Magarian EM, Harrison SL, Zurakowski D, Fleming BC. Skeletal maturity signficantly affects functional healing of the anterior cruciate ligament. J Bone Joint Surg, Am. 2009 submitted. [PubMed]
16. Cullen MC, Roy DR, Crawford AH, Assenmacher J, Levy MS, Wen D. Open fracture of the tibia in children. J Bone Joint Surg Am. 1996;78:1039–1047. [PubMed]
17. Bales CP, Guettler JH, Moorman CT., 3rd Anterior cruciate ligament injuries in children with open physes: evolving strategies of treatment. Am J Sports Med. 2004;32:1978–1985. [PubMed]
18. Vavken P, Saad F, Murray M. Age-dependence of expression of growth factor receptors in porcine ACL fibroblasts. J Orthop Res. 2009 [Epub ahead of print] [PMC free article] [PubMed]
19. Murray MM, Bennett R, Zhang X, Spector M. Cell outgrowth from the human ACL in vitro: regional variation and response to TGF-beta1. J Orthop Res. 2002;20:875–880. [PubMed]
20. Murray MM, Martin SD, Spector M. Migration of cells from human anterior cruciate ligament explants into collagen-glycosaminoglycan scaffolds. J Orthop Res. 2000;18:557–564. [PubMed]
21. Mastrangelo A, Magarian E, Palmer M, Murray M. The Effect of Skeletal Maturity on the Regenerative Function of Intrinsic ACL Cells. J Ortho Research. 2008 In review. [PMC free article] [PubMed]