Characterization of bursa subacromialis-derived mesenchymal stem cells
© Steinert et al. 2015
Received: 15 August 2014
Accepted: 21 May 2015
Published: 3 June 2015
The bursa subacromialis (BS) provides the gliding mechanism of the shoulder and regenerates itself after surgical removal. Therefore, we explored the presence of mesenchymal stem cells (MSCs) within the human adult BS tissue and characterized the BS cells compared to MSCs from bone marrow (BMSCs) on a molecular level.
BS cells were isolated by collagenase digest from BS tissues derived from patients with degenerative rotator cuff tears, and BMSCs were recovered by adherent culture from bone-marrow of patients with osteoarthritis of the hip. BS cells and BMSCs were compared upon their potential to proliferate and differentiate along chondrogenic, osteogenic and adipogenic lineages under specific culture conditions. Expression profiles of markers associated with mesenchymal phenotypes were comparatively evaluated by flow cytometry, immunohistochemistry, and whole genome array analyses.
BS cells and BMSCs appeared mainly fibroblastic and revealed almost similar surface antigen expression profiles, which was CD44+, CD73+, CD90+, CD105+, CD106+, STRO-1+, CD14−, CD31−, CD34−, CD45−, CD144−. Array analyses revealed 1969 genes upregulated and 1184 genes downregulated in BS cells vs. BMSCs, indicating a high level of transcriptome similarity. After 3 weeks of differentiation culture, BS cells and BMSCs showed a similar strong chondrogenic, adipogenic and osteogenic potential, as shown by histological, immunohistochemical and RT-PCR analyses in contrast to the respective negative controls.
Our in vitro characterizations show that BS cells fulfill all characteristics of mesenchymal stem cells, and therefore merit further attention for the development of improved therapies for various shoulder pathologies.
With an incidence of about 30 %, degenerative tears of the rotator cuff emerge as one of the most common musculoskeletal diseases in the older population [1, 2] with significant socio-economic impact [3–7]. Interestingly, it has been noted in the clinical area that localized reactions of the bursa subacromialis (BS) are evident in cases with rotator cuff tears , and that rotator cuff reconstructions reveal a lower success rate when surgical techniques are used that include radical resection of the BS . Furthermore, in revision cases we have observed that the BS tissue is restored after complete surgical resection within approximately three to six months, indicating its high regenerative potential.
The BS represents extraarticular synovialis-like tissue that is anatomically located between the rotator cuff and the acromion and provides the gliding mechanism of the shoulder [9, 10]. Unfortunately, the BS has not received much attention by the scientific community yet. The subacromial bursa was traditionally regarded as the main source of subacromial pain, adhesions and inflammatory response in rotator cuff disease. This derives mainly from the concept of Duplay in the 19th century who influenced generations of orthopedic surgeons to remove the bursa during subacromial decompression and rotator cuff repair . These ideas were supported by findings of increased levels of cytokines and nociceptors in subacromial impingement and rotator cuff tears [12–14]. Therefore, in the past most surgeons believed that the subacromial bursa acts mainly as a mediator of inflammation and tendon destruction rather than as a useful healing response for the repair of tendon lesions. Uhthoff and Sarkar first proved the healing potential of the subacromial bursa in human biopsies , and in an experimental animal model , which have been confirmed by others [17, 18]. However, the cellular mechanism of these findings has not been clarified yet, although BS cells have been recognized to express several morphogens and cytokines upon damage of the underlying rotator cuff tendon .
Mesenchymal stem cells (MSCs) have been isolated and extensively characterized from bone marrow [20, 21] and several mesenchymal tissues including bone , fat , cartilage , muscle , tendon [26, 27], ligament [28–30] and other sources [31, 32]. Given the self-regeneration capacities of the BS in vivo after surgical removal along with its localization adjacent to the rotator cuff, it was the purpose of this study to characterize the cells that reside within the BS, and secondly to explore their MSC properties compared to those of the well-characterized MSCs isolated from bone marrow (BMSCs).
Materials and methods
Tissue collection and cell isolation
Human BS tissues were harvested aseptically from 10 male 42- to 58-year old patients with degenerative tears of the rotator cuff undergoing reconstruction surgery (after informed consent and as approved by the local institutional review board of the University of Würzburg). The BS tissues were then rinsed twice with serum-free Dulbecco’s modified Eagle’s medium (DMEM)/F-12 media (PAA Laboratories, Linz, Austria) containing 1 % penicillin/streptomycin (PAA Laboratories). A small part of the tissues was reserved for histology, while the rest was minced to 1-2 mm3 pieces and placed in 0.1 % collagenase 1/3 solution (Life Technologies GmbH, Darmstadt, Germany). The recovered cells from the digest solution were plated in monolayer cultures in DMEM/F-12 media containing 10 % fetal bovine serum (Life technologies GmbH) and 1 % penicillin/streptomycin.
BMSCs were isolated from surgical waste of 10 male 45- to 65-year old patients undergoing total hip arthroplasty surgery after informed consent, and as approved by the Institutional Review Board of the University of Würzburg as described previously . Briefly, bone-marrow reamings were harvested aseptically, resuspendend in DMEM/F-12 (PAA Laboratories), filtered through a 40 μm filter (BD Biosciences, Heidelberg, Germany), and plated in tissue culture flask. Non-adherent cells were removed after two days, and attached cells were washed with PBS, cultured in complete medium for 10 to 14 days to a subconfluent state, with medium changes every 3 to 4 days. Second to third passage cells were used for all experiments.
For analysis of chondrogenic differentiation, the BS and BMSC populations were expanded in the presence of 10 ng/ml fibroblast growth factor (FGF)-2 (PeproTech, Hamburg, Germany) as recommended .
Cell proliferation assay
Proliferation rates of BS cells and BMSCs were determined by luminometrical measurements of adenosine-5′-triphosphate (ATP) activity using the CellTiter-Glo® Luminescent Cell Viability Assay (Promega GmbH, Mannheim, Germany) according to the manufacturer’s instructions. In short, 1,000 first passage cells per well were seeded in 96-well plates and cultured in 100 μl of complete medium for 17 days with media changes every second day. On days 1, 3, 5, 7, 9, 12, and 17 the luminescence of ten wells per donor and cell type was determined by addition of an equal volume of Cell Titer-Glo® reagent to the cells, incubation at room temperature for five minutes, and final detection of the luminescence signal for 0.1 seconds using an Orion II Luminometer (Berthold Detection Systems, Pforzheim, Germany). A total of five donors for each cell type were included.
Flow cytometrical analyses
Expression of cell surface antigens and secreted proteins in BS cells and BMSCs
Positive cells (%)
Hematopoietic stem cell marker, cell adhesion
Osteoblast and osteoclast signal transduction
Mesenchymal, epithelial and endothelial cell marker
Fibroblast, stromal and hematopoietic stem cell marker
Mesenchymal and erythroid progenitor cells
Hematopoietic stem cell marker
Endothelial cells, cell adhesion
Mesenchymal, epithelial stem cells, fibroblasts, monocytes, cell adhesion
Fibroblast growth factor
Mesenchymal stem cell marker
Primer sequences and PCR conditions
Oligonucleotide primer sequence
Number of cycles
Annealing temp. (° C)
Product size (bp)
Verfication of array data
A: 5′— AGACGGTGAGGCAGGCCGTT—3′
S: 5′— AATGAATGGCTCAAAACTTGG —3′
A: 5′— CACTAGGTTCTCACTCGCTCAG —3′
Chondrogenic marker genes
Osteogenic marker genes
Adipogenic marker genes
Genome-wide gene expression profiling of bursa cells and BMSCs
For genome-wide gene expression profiling, hybridization experiments were performed and analyzed using Affymetrix Gene Chips HG-U133 Plus 2.0 (54,000 probesets for 47,400 transcripts and 38,500 genes, High Wycombe, UK) as described previously . Total RNA expression of three different BS and five individual BMSC preparations were analyzed using the Affymetrix Gene Chip Scanner 3000, the Affymetrix GeneChip Operating Software 1.4, and comparatively evaluated using the significance analysis of microarrays (SAM) approach .
To assess differentially expressed genes between BS and BMSC groups, pre-defined conditions were established: the number of “present” calls for a given gene had to be greater than 50 % in at least one of the groups and only those genes were taken into account that displayed a fold change (FC) less than 0.5 and more than 2. Probesets which showed an FC between 0.5 and 2 were stated as “not differentially expressed”. In order to obtain reliable data, the q-value, i.e. false discovery rate had to be less than 10 %. For heatmap generation and to identify significantly overrepresented gene clusters, Gene Ontology (GO) analysis and mapping was performed with all differentially expressed probesets by using the web service for microarray data analysis CARMAweb . Confirming RT-PCR analyses from five up- and five downregulated genes were performed using primers and PCR conditions as listed in Table 2.
Chondrogenic differentiation was performed in high density cultures as previously described . Briefly, 3 × 105 cells were resuspended in 0.5 ml chondrogenic medium DMEM high glucose (PAA Laboratories) supplemented with 50 μg/ml L-ascorbic acid 2-phosphate, 100 nM dexamethasone, 100 μg/mL pyruvate, 40 μg/ml L-proline, 1 % ITS+ (all Sigma Aldrich GmbH, Munich, Germany), 10 ng/ml transforming growth factor-β1 (TGF-β1) (R&D Systems) and pelleted. The generated aggregates were maintained in chondrogenic medium for three weeks with medium changes every two to three days. Control pellets were maintained without TGFβ1 supplementation. For histological and immunohistochemical analyses, aggregates were fixed in 4 % paraformaldehyde, dehydrated in a graded series of alcohols and embedded into paraffin. Thick sections (4 μm) were mounted on slides, washed with xylene, and rehydrated in a series of graded alcohols. Stainings were performed using standard protocols for matrix-associated proteoglycans using alcian blue. Immunohistochemical detection of collagen type II (COL II) was performed as described in detail previously  using a primary monoclonal COL II antibody (Acris Antibodies GmbH, Herford, Germany), while negative controls were treated with mouse serum instead. Detection of the staining was done using the Biogenex Super SensitiveTM Link-Label IHC Detection System (DCS Innovative Diagnostic Systems, Hamburg, Germany) according to the manufacturer’s instructions.
Expression of chondrogenic marker genes was performed using RT-PCR analyses with the lineage specific primers and PCR conditions summarized in Table 2. Six pellets per group were initially frozen in liquid nitrogen, ground using pellet pestles and added to 1 ml of Trizol reagent (Life Technologies GmbH), with an additional purification step using RNeasy separation columns (RNeasy kit; Qiagen, Hilden, Germany) according to the manufacturer’s instructions. Three different donors for each cell type were analyzed.
For osteogenic differentiation 1 × 105 cells per cm2 were seeded in four-well chamber slides and 25 cm2 culture flasks (both Nunc). Once the cell layers reached confluency, osteogenic differentiation was induced by cultivation in complete osteogenic DMEM high glucose medium (PAA) supplemented with 100 nM dexamethasone, 50 μg/ml L-ascorbic acid 2-phosphatase, 10 mM β-glycerophosphate (all Sigma Aldrich GmbH) as well as 25 ng/ml recombinant human BMP2 (R&D Systems GmbH). Cultures maintained in control medium (lacking the above listed supplements) served as a negative control for differentiation. Osteogenesis was conducted for three weeks with medium changes every two to three days. Histological analyses were performed by staining for alkaline phosphatase (ALP) using the Leukocyte ALP Staining Kit (Sigma Aldrich GmbH) according to the manufacturer's instructions. Matrix mineralization was evaluated by staining with alizarin red, as described previously . The parameters for expression analysis of osteogenic marker genes are listed in Table 2 and semi-quantitative RT-PCR analyses were performed as described above. Three different donors for each cell type were analyzed.
Adipogenic differentiation required the initial seeding of cells at a density of 1 × 105 cells per cm2. After the cell layer reached about 50-70 % confluency, the cells were further cultivated in adipogenic induction medium, consisting of complete DMEM high glucose supplemented with 1 μM dexamethasone, 1 μg/ml insulin, 0.5 mM 3-isobutyl-1-methylxanthine (IBMX) and 100 μM indomethacin for three weeks with media changes every two to three days. Control cells were cultivated in supplement-free adipogenic control medium. Histological analyses using oil red O staining were conducted to detect formation of lipid droplets. RT-PCR analyses were performed as stated previously using lineage specific primers and PCR conditions as summarized in Table 2. Three different donors for each cell type were analyzed.
Histology and immunohistochemistry of BS cells and tissue
Following fixation with 4 % paraformaldehyde, paraffin embedding, sectioning to 4 μm and rehydration of BS tissues was performed as described previously . A general histological assessment of the sections was given using hematoxylin and eosin (H&E) staining, whereas mucines were stained using periodic acid-Schiff (PAS) staining and collagenous structures were detected by Azan, Masson-Goldner trichrome (MG), or van Gieson (VG) staining as described in detail earlier . Immunohistochemical detection of surface antigens was performed as described above making use of antibody dilutions specific for CD44 (1:200), CD90 (1:25), CD105 (1:50) and the Stro1 (1:20) antigen (all Dako Deutschland GmbH, Hamburg, Germany) after tissue processing. For more detailed analyses of the intracellular distribution of positive Stro1 staining we also employed a fluorescein isothiocyanate (FITC) labeled Stro1 antibody with counterstaining of the nuclei using 4, 6-diamidino-2-phenylindole (DAPI) and phase contrast (bright field) and fluorescence microscopy (1:10; Santa Cruz Biotechnology Inc., Heidelberg, Germany).
The numerical data are expressed as means +/- standard error (SEM). Determination of the statistical significance between groups was performed using student’s t-test, or the Mann-Whitney U test as indicated.
Cell morphology, proliferation and surface antigen expressions of BS cells and BMSCs
Immunohistochemical detection of the MSC-associated surface markers CD44, CD90 and CD105 was strongly and equally positive for BS cells and BMSCs (Fig. 1c). Staining for the Stro1 antigen in contrast resulted in weak but positive signals for both cell types (Fig. 1c). Control cells incubated with mouse serum instead of the respective primary antibodies showed no staining and therefore validated the immunohistochemical investigations. Additionally PAS staining for the histological detection of mucines showed positive signals for BS cells, while BMSC monolayer cells remained unstained (Fig. 1c). For a more detailed analysis of the distribution of STRO1+ areas in BS cells and BMSCs, immunostaining with a FITC-labeled STRO1 antibody and DAPI counterstain of the nuclei was performed, revealing positive staining at similar levels for both cell types in the respective phase contrast (bright field) and corresponding fluorescence microscopy images (Fig. 1d).
Further in-depth analyses of cell surface markers using flow cytometry revealed that expression of the antigens CD73, CD90 and CD105 was strongly positive on BS cells and BMSCs (Table 1). Furthermore, CD166 is highly expressed on BMSCs while BS cells have a small subset of cells, which are negative for the respective antigen. In contrast, CD53, CD133, CD144 as well as the Stro1 antigen were not, or almost not, detectable on both cell types. Heterogeneous cell distributions were found for FGF, which is expressed by half of the BS cells and BMSCs. Further differences were found concerning the secretion of ALP: while about half of the BMSCs were positive, only a quarter of the BS cells showed positive signals. The expression of CD34 was negative in BMSCs, while a small subset of BS cells (7.69 %) expressed the respective antigen. On the other hand, BS cells showed no expression of CD106, which is in contrast to the moderate expression (55.55 %) of this marker in BMSCs.
Microchip hybridization of RNA from BS cells and BMSCs
Chondrogenic differentiation of BS cells and BMSCs
Immunohistochemical detection of COL II was positive for both cell types after chondrogenic induction, and negative for the control pellets (Fig. 3a). The staining was very prominent in the inner areas of the aggregates. Analysis of RNA expression validates the staining with COL II being exclusively expressed by chondrogenic differentiated pellets and not by the related controls (Fig. 3b). Furthermore, maintenance of BS cells and BMSCs in chondrogenic medium instead of control medium resulted in higher expression of the chondrogenic SRY transcription factor box9 (SOX9), and the prehypertrophy-related marker gene indian hedgehog (IHH), while both mRNAs were not expressed in the corresponding controls (Fig. 3b).
Osteogenic differentiation of BS cells and BMSCs
Expression of ALP mRNA is upregulated in osteogenic differentiated cells compared to cells maintained in osteogenic control medium for both cell types (Fig. 4b). Other osteogenic markers such as collagen type I (COL I) and Cbfa1 were also upregulated following differentiation along the osteogenic lineage, with Cbfa1 being exclusively expressed in differentiated cells of both cell types and not in the related controls (Fig. 4b).
Adipogenic differentiation of BS cells and BMSCs
Histological and immunohistochemical characterization of tissue sections from bursa subacromialis
Bursae are saclike cavities situated in places in the body where friction would otherwise strongly occur, facilitating the gliding of tendons over solid surfaces . Bursae in shoulder joints retain the ability to regrow after partial or total surgical removal according to our own clinical observations. The subacromial bursa (BS) vividly responds to rotator cuff injuries  and degeneration  and successfully augments rotator cuff repair surgery . Therefore the purpose of the current study was to characterize the phenotype of BC cells compared to the well-characterized BMSCs. Our results provide evidence for the existence of a rich population of multipotent MSCs within the BS with similar fibroblastic appearance and almost similar proliferation profile compared with BMSCs (Fig. 1). This is consistent with findings of different MSC populations in the literature with differences in cell proliferation being attributed to different tissue sources and disease pathologies [38–40].
Characterization of cell surface markers of BS cells and BMSCs revealed the markers CD44, CD90, and CD105 positive by immunohistochemistry (Fig. 1c) and flow cytometry (Table 1) which is consistent with the abundant literature in the MSC field [28, 41, 42]. In contrast, the Stro1 antibody showed only a slight staining in immunohistochemistry and was not detectable at marked levels in either cell type using flow cytometrical methods. This might be an antibody-related effect  and corresponds with previous findings in ligament MSCs . Marked differences between cell types could be seen in the expression of CD34, CD106 and ALP (Table 1), indicating that a subset of cells identified in BS could be CD34+ endothelial progenitors, while a larger amount of ALP+ bone progenitors is present in BMSCs [44–46]. Additionally, PAS staining of mucopolysaccharides could be detected in BS cells but not in BMSCs illustrating a major difference between the donor sources of the two mesenchymal cell types used, which did not impair the multilineage potential of the BS cells (Figs. 3, 4 and 5). This finding was supported by a strong expression of mucin marker MUC1 in BS cells (Fig. 2e). As this marker, however, was also present in BMSCs, we can speculated on the role of secretory pathway activation in stem cells of mesenchymal origin.
Not only did the immunohistochemical staining of monolayer cells show a strong correlation of BS cells and BMSCs, but detection of the same MSC markers, CD44, CD90, and CD105, showed that positive areas for these markers could be located on the fibrous as well as the mucinous portions of the BS tissue, indicating the presence of MSCs within different parts of the BS (Figs. 1c and 6). Notably, variability in staining intensity may reflect different stages of vascularity rather than different staining intensities in the stromal matrix of the bursa tissue. This corresponds to the finding of MSCs in the palatine tonsil, where stem cell niches could also be located in mucinous and fibrous regions of this gland . Therefore, it remains to be seen in future experiments, whether the PAS+ subset of exocrine cells within the BS population exhibits a different multipotency profile compared to the PAS- fraction of the BS population (Fig. 6), and also to explore the regenerative capacities of these cell types.
Differences between BS cells and BMSCs could be further resolved on a molecular level using analyses of the respective transcriptomes, indicating 7.29 % up- and 4.38 % downregulated probesets in BS cells compared to BMSCs (Fig. 2a). Interestingly, further examinations revealed that several cartilage and bone-associated genes (e.g. BSP, WISP3, COL X) were exclusively upregulated in BMSCs but not in BS cells, indicating the relevance of the tissue source in the evaluation of transcriptional profiles [34, 47]. This is in agreement with the finding of FGF9 and FGF18 expression in BS cells and not in BMSCs, with FGF9 being an inverse regulator of BMP2 , and FGF18 responsible for dedifferentiation of chondrocytes and fibroblast proliferation . CD200, a regulator of macrophage activation and novel MSC marker [49, 50], was only confirmed for BMSCs but not for BS cells, holding the advantage to distinguish between both cell types. While microchip array analyzes are powerful screening tools, significant variation and room for interpretation of results has to be considered.
Apparently, the BS is often a site of pathology in impingement of the shoulder . In this study, all BS cells were obtained from patients undergoing rotator cuff repair surgery as a result of degenerative full-thickness tears. It is known that the size of the tear has a direct influence on the inflammatory status of the adjacent bursa , as evidenced by the increasing levels of inflammatory cytokines, such as interleukin 1 (IL1), IL6, metalloproteases, tumor necrosis factor α [14, 51] and myofibroblast invasion . Therefore, we cannot rule out that myofibroblasts from the underlying rotator cuff might have entered the bursa and added to the BS cell population examined, as BS tissues from healthy donors could not be retrieved, which is a limitation of this study. Indeed, it is not possible to know where these inflammatory bursal cells may have migrated from, or whether they existed in the bursa to start. Thus, future studies are necessary to understand better the impact of the inflammatory microenvironment on MSCs for their application in therapeutic protocols.
Only recently, the BS has been identified by others as a novel source of MSCs within the shoulder, confirming their differentiation potential into the chondrogenic, osteogenic and adipogenic lineage and expression of the surface antigens CD73 and 90 . Furthermore BS cells were also found to express the surface markers CD29 and platelet-derived growth factor receptor-beta (PDGFRB) , which have not been tested in this study. Additionally, we are able to provide detailed insight into the expression of a series of commonly used surface antigen markers of BS cells compared to BMSCs (Table 1) and give insights into the comparative transcriptome characteristics between these two cell types (Fig. 2). Interestingly, BS cells have also been shown to be able to undergo neurogenic  and tendogenic differentiation  underlining their potential impact for the treatment of subacromial pathology. Because of the similarities between both cell types, as shown in this work, it is also conceivable that BMSCs, which can be easily obtained from bone marrow, might be harnessed to augment reconstitution of the subacromial bursa after surgical removal, providing potential support for the restoration of the gliding mechanism after such treatments.
The present study shows that cells isolated from the subacromial bursa of the shoulder meet the minimal criteria for their classification as MSCs . Although in certain areas, marked differences between BS cells and BMSCs could be resolved on molecular levels (e.g. ALP expression, transcriptome), both cell types could be expanded using plastic adherence, are capable of multilineage differentiation, and showed a similar expression of several MSC surface markers, indicating the MSC potential of the BS cells. Such multipotent BS cells can be located at high density in the fibrous, as well as the mucinous parts of the BS tissue. Thus, we conclude that BS tissues can be regarded as a reservoir rich in MSCs within the shoulder, and it remains to be seen in further investigations, whether this knowledge might be harnessed for the development of improved treatments for subacromial pathologies.
Bone marrow-derived MSC
Core binding factor alpha 1
Cluster of differentiation
- COL I:
Collagen type I
- COL II:
Collagen type II
Elongation factor 1α
Fibroblast growth factor
Forkhead box P2
Mesenchyme homeobox 2
Mesenchymal stem cell
Peroxisome proliferator-activated receptor gamma 2
SRY (sex determining region Y)-box 9
WNT1 inducible signalling pathway protein 3
We are grateful to Viola Monz, Martina Regensburger and Beate Geyer for their excellent technical assistance. We thank Mr. Thomas Peter and Mrs. Andrea Heymer, PhD (Fraunhofer IGB, Stuttgart, Germany) for their expertise and help with the FACS analyses. This work was financed in part by a grant from the Bayerische Forschung (FORZEBRA, TP2WP5, to AFS and UN) and by an intramural start-up grant from the König-Ludwig-Haus, Bezirk Unterfranken, Würzburg, Germany. This manuscript received the Perthes Prize awarded by the Deutsche Gesellschaft für Schulter- und Ellenbogenchirurgie (DVSE) 2014. This publication was funded by the German Research Foundation (DFG) and the University of Wuerzburg in the funding programme Open Access Publishing.
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