- Open Access
Pentosan polysulfate binds to STRO-1+ mesenchymal progenitor cells, is internalized, and modifies gene expression: a novel approach of pre-programing stem cells for therapeutic application requiring their chondrogenesis
Stem Cell Research & Therapy volume 8, Article number: 278 (2017)
The pharmaceutical agent pentosan polysulfate (PPS) is known to induce proliferation and chondrogenesis of mesenchymal progenitor cells (MPCs) in vitro and in vivo. However, the mechanism(s) of action of PPS in mediating these effects remains unresolved.
In the present report we address this issue by investigating the binding and uptake of PPS by MPCs and monitoring gene expression and proteoglycan biosynthesis before and after the cells had been exposed to limited concentrations of PPS and then re-established in culture in the absence of the drug (MPC priming).
Immuno-selected STRO-1+ mesenchymal progenitor stem cells (MPCs) were prepared from human bone marrow aspirates and established in culture. The kinetics of uptake, shedding, and internalization of PPS by MPCs was determined by monitoring the concentration-dependent loss of PPS media concentrations using an enzyme-linked immunosorbent assay (ELISA) and the uptake of fluorescein isothiocyanate (FITC)-labelled PPS by MPCs. The proliferation of MPCs, following pre-incubation and removal of PPS (priming), was assessed using the Wst-8 assay method, and proteoglycan synthesis was determined by the incorporation of 35SO4 into their sulphated glycosaminoglycans. The changes in expression of MPC-related cell surface antigens of non-primed and PPS-primed MPCs from three donors was determined using flow cytometry. RNA sequencing of RNA isolated from non-primed and PPS-primed MPCs from the same donors was undertaken to identify the genes altered by the PPS priming protocol.
The kinetic studies indicated that, in culture, PPS rapidly binds to MPC surface receptors, followed by internalisation and localization within the nucleus of the cells. Following PPS-priming of MPCs and a further 48 h of culture, both cell proliferation and proteoglycan synthesis were enhanced. Reduced expression of MPC-related cell surface antigen expression was promoted by the PPS priming, and RNA sequencing analysis revealed changes in the expression of 42 genes.
This study has shown that priming of MPCs with low concentrations of PPS enhanced chondrogenesis and MPC proliferation by modifying their characteristic basal gene and protein expression. These findings offer a novel approach to re-programming mesenchymal stem cells for clinical indications which require the repair or regeneration of cartilaginous tissues such as in osteoarthritis and degenerative disc disease.
Adult mesenchymal stem cells (MSCs) are an abundant source of self-renewing, multipotent undifferentiated cells that can be readily isolated from bone marrow, adipose tissue, muscle, and synovium. They can be serially expanded in culture and cryopreserved almost indefinitely without significant loss of their tissue regenerative capacity [1,2,3,4]. In-vitro studies have shown that when MSCs are exposed to the appropriate physical, chemical, or biological stimuli they will differentiate into cells of the mesodermal lineage, including osteoblasts, chondrocytes, tenocytes, myocytes, and adipocytes [3,4,5]. Moreover, when administered systemically, MSCs exhibit the capacity to migrate to the site(s) of tissue injury, where they can modulate inflammatory and immune-regulatory pathways as well as release pro-anabolic factors [6,7,8,9]. These unique activities of MSCs have led to extensive investigations into their potential applications as biological agents for the treatment of a variety of clinical applications [5,6,7]. MSCs have been considered a suitable therapy for muscular skeletal and connective tissue disorders, including degenerative disc disease, osteoarthritis, and repair of articular cartilage, owing to the high incidence of such disorders as well as their limited capacity for spontaneous repair and the limited treatment options [10,11,12,13,14,15,16].
As indicated, MSCs possess the ability to localize to sites of tissue injury, suppress inflammation, and facilitate repair. Moreover, there is considerable evidence to suggest that MSCs engraft at these sites, undergo differentiation, and synthesise an extracellular matrix consistent with the endogenous tissue [17, 18]. However, for the regeneration or repair of cartilaginous tissues it is important that the initial differentiation of MSCs to chondrocytes is not followed by further differentiation to osteoblasts, a process that has been observed in some experimental studies using these osteochondral precursors [19, 20].
In previous studies  we showed that the incubation of STRO-1+ immuno-selected mesenchymal progenitor cells (MPCs) with the pharmaceutical agent pentosan polysulfate (PPS) not only improved their viability and enhanced their chondrogenic differentiation but also suppressed osteogenesis in vitro. In subsequent in-vivo studies using ovine models, MPCs were formulated with PPS and injected directly into degenerate intervertebral discs, and were found to promote the deposition of a new disc matrix without evidence of osteogenic differentiation [22,23,24]. However, in these animal studies the MPCs and PPS were always mixed together immediately prior to administration. As such, it remained to be determined whether the positive outcomes observed represented the sum of the pharmacological activities of the individual components or whether the mechanism of action was via a reprogramming of MPC genetic expression mediated by PPS.
The objective of the present study was to address this question by examining the concentration-dependent binding and internalization of PPS by MPCs and determine if priming of the cells with the drug changed their genetic signature.
Preparation of human STRO-1+ immuno-selected mesenchymal progenitor stem cells
Bone marrow was collected from the posterior iliac crest of healthy volunteers (20–35 years old) following their informed consent; the procedure was approved by the Human Research Ethics Committee of the Royal Adelaide Hospital (RAH), Adelaide, South Australia. These aspirates were used to prepare immuno-selected STRO-1+ MPCs employing procedures described previously . Briefly, STRO-1+ mesenchymal precursor cells derived from the bone marrow aspirates were isolated by STRO-1 magnetic activated cell sorting and used to establish primary cultures. The primary cultures were expanded by trypsin-EDTA detachment and re-plating at a density of 4.0 × 104 cells per cm2 as previously described . Following 3–4 passages, the cells were harvested by trypsin-EDTA detachment and re-suspended in culture medium at a density of 5.0–20 × 106 cells/ml. They were then combined with ProFreeze-CDM NAO freezing medium (Lonza Australia Ltd., Blackburn Rd., Mt Waverley, Victoria 3149, Australia) (2×) containing DMSO (7.5%), they were control-rate cryopreserved and placed at –80 °C overnight, and subsequently transferred to the vapour phase of liquid nitrogen until required.
Competitive PPS enzyme-linked immunosorbent assays (ELISAs) of culture media
The concentration of PPS in culture media was determined with a competitive ELISA using a biotinylated monoclonal antibody (1B1) against polysulphated polysaccharides (kindly provided by Professor Prachya Kongtawelert, Department of Biomedical Sciences, Chiang Mei University, Thailand).
Each well of a 96-well plate was coated with 100 μl 50 μg/ml hexadimethrine bromide (Polybrene; Sigma-Aldrich, Sydney, Australia)) in phosphate-buffered saline (PBS), pH 7.4, and incubated at 37 °C for 1 h. The solution was aspirated and the plate was air-dried without washing. Wells were then blocked with 200 μl/well blocking solution (PBS + 1% bovine serum albumin (BSA)) and incubated at 37 °C for 1 h. The solution was aspirated and the wells were washed with 300 μl/well PBST (PBS + 0.05% Tween-20) three times. The plates were flicked to remove the contents of the wells and dried. The monoclonal antibody B1B1 was diluted 1:200 in Dulbecco’s modified Eagle’s medium (DMEM) and used as the primary antibody solution. The PPS compound (BenePharmachem, Munich, Germany) was used to prepare a 1 mg/ml working stock and was subsequently diluted in DMEM to create a standard curve of 0.004–4 μg/ml. The PPS standard solutions were each mixed with the 1B1 antibody solution in a 1:1 ratio and incubated at 37 °C for 1 h. Aliquots of the inhibition mixtures (100 μl) were transferred to each well and incubated at 37 °C for a further 1 h. Using the same plates, culture media samples containing PPS were mixed 1:1 with the 1B1 antibody solution in the microtitre plate wells. The samples were aspirated from each well and the plate washed with 300 μl/well PBST three times, flicked, and dried. Monoclonal anti-biotin-alkaline phosphatase (AP) antibody (Sigma-Aldrich, Sydney, Australia, cat. no. A-6561) was used as the secondary antibody and was diluted 1:5000 with blocking solution and 100 μl added to each well followed by incubation at 37 °C for 1 h. The antibody solution was aspirated and the plate was washed with 300 μl/well PBST three times, flicked, and dried. The AP substrate, para-nitrophenyl phosphate (PNP; 200 μl 1 mg/ml PNP in 0.1 M NaHCO3 buffer containing 2 mM MgCl2, pH 8.6) was added to each well and the plates incubated in the dark for 20 min. Absorbance at 405 nm was then determined with a micro-plate reader. All assays were performed in triplicate.
Kinetics of PPS uptake by MPCs in culture
Primary MPC monolayers were established in culture as described previously . Briefly, 3.0 × 105 MPCs were seeded into wells of 48-well plates and incubated with DMEM containing 10% fetal bovine serum (FBS) at 37 °C in 5% CO2 for 16 h. The media from the primary cultures was discarded and the wells were washed with DMEM (3 × 500 μl/well); media and washings were discarded and then replaced with DMEM (500 μl/well) containing gradient concentrations of PPS (0.5, 1.0, 2.5, 5, and 10 μg/ml/well). Plates were maintained at 37 °C in 95% air/CO2 and, after 0.25, 0.50, 2, 6, 20, and 24 h, media from individual wells were aspirated, cells washed (PBS, 0.5 ml/well) and media and washings pooled. The concentrations of PPS remaining in the aspirated media and washings of the cultures at each time point was determined using the PPS ELISA as described above.
The preparation of fluorescein isothiocyanate (FITC)-labelled PPS
PPS (100 mg) was converted to the tetrabutyl ammonium (TBA) salt by incubating with tetrabutylammonium bromide (100 mg; Sigma-Aldrich, Sydney, Australia) dissolved in 10 ml de-ionized H2O for 4 h at ambient temperature. The PPS-TBA complex was dialyzed against de-ionized water for 24 h to remove excess salts and then lyophilized. The PPS-TBA complex (50 mg, dissolved in 1 ml DMSO) was mixed with 1,1-carbonyl di-imidazole (28.0 mg/0.5 ml; Sigma-Aldrich, Sydney, Australia)) and incubated at 56 °C for 1 h. After cooling to room temperature, hydrazine (47.8 mg; Sigma-Aldrich, Sydney, Australia) was added and the solution incubated with shaking for 16 h at 45 °C. The PPS carboxyhydrazide complex was then reacted with FITC (Sigma-Aldrich, Sydney, Australia) using the manufacturer’s instructions to convert the FITC-PPS derivative into a TBA salt derivative. The PPS-FITC-TBA salt was then converted to the sodium salt by mixing at 4 °C with 4.0 M NaCl (100 ml) for 16 h followed by 48 h dialysis against water with changes every 16 h, and then lyophilized. The lyophilized PPS-FITC derivative was purified by size-exclusion chromatography on a Superdex-200 column (GE Healthcare Ltd., Sydney, Australia) equilibrated in 0.25 molar NaCl. Column fractions were monitored for PPS concentration using the dimethyl-methylene blue assay  and FITC by fluorescence excitation/emission at 485/538 nm. Fractions positive for PPS and FITC fluorescence were pooled, desalted, and lyophilized. The purity of the PPS-FITC complex was established by NMR spectroscopy (by Dr. Ronald Shimmon, Department of Chemistry, University of Technology, Sydney, Australia).
PPS-FITC uptake by MPCs using fluorescence microscopy
Primary MPC monolayer cultures were established in six-well plates (2.5 × 105 cells/well) as described previously . After 16 h, DMEM (3 ml) containing various concentrations of PPS-FITC (0, 1.0, 2.5, 5.0, 10.0, and 20.0 μg/ml) were added to the wells and incubated at 37 °C in 5% CO2 for a further 24 h. The media were collected from each well, and the cells were washed 3× with PBS at room temperature. Media and washings were discarded. The washed cells were released from the plates with 250 μl 0.25% trypsin/EDTA at 37 °C for 10 min. The cells and supernatant were separated by centrifugation at 500 g for 10 min, the supernatants were discarded, and the cell pellets washed 3× with PBS (1 ml/well). The cell pellets derived from each culture well were re-suspended in 100 μl de-ionised H2O then transferred to wells of black microplates. The microplates were agitated for 1 h to lyse the cells in the absence of light, and the intensity of the fluorescence emission at 538 nm determined for all added PPS-FITC concentrations using a fluorescence microplate reader (Labsystems Fluoroskan II, ThermoFisher Scientific Australia Pty. Ltd., Scoreby, Australia) with de-ionised H2O as a blank. The levels of PPS-FITC in each well were quantified using a standard curve prepared from the purified PPS-FITC prepared above.
MPCs (6000 cells/well) were seeded on eight-well slides (Lab-Tek-II® Chamber Slide System, Permanox®, Grand Island, NY, USA) and incubated at 37 °C in a 5% CO2 atmosphere for 16 h. DMEM media (1.0 ml) containing 0, 0.5, 1.0, and 2.5 μg/ml PPS-FITC was added to each well and the slides incubated for a further 24 h at 37 °C. The media were removed and the bound cells washed 3× with 1.0 ml PBS. Media and washings were discarded and cells fixed using 300 μg/well HistoChoice MB Fixatives (Amresco, Solon, OH, USA) for 20 min at room temperature. After washing once with PBS, the cells of each slide were stained with 20 μg/ml propidium iodide (PI) for 10 min at room temperature, washed 3× with PBS, once with 70% ethanol, and 3× with absolute ethanol, and then viewed under UV light using a Nikon Eclipse 80 fluorescence microscopic (Coherent Scientific, Hilton, Australia). Cells were viewed for FITC and PI fluorescence using excitation and emission wavelengths of 485/538 nm for 2 s and 535/620 nm for 60 s, respectively. The cell images were captured using a digital camera coupled to the microscope and images analysed using the NIS-Elements software (Coherent Scientific, Hilton, Australia).
Assessment of MPC proliferation alone and after priming with PPS
Triplicate cultures of passage 4 MPCs at densities of 1 × 106 cells/ml were established in 24-well plates as described previously . High-glucose DMEM containing 5 μg/ml PPS was then added to 12 wells of the plates and an equivalent volume DMEM alone to the remaining wells. After incubation for 24 h, media were removed from all wells and cells were washed 3× with PBS and then re-established in culture. After 4, 24, and 48 h, incubations were stopped, media removed and cells washed 3× with PBS; media and washings were then discarded. Cells were released from the plates by trypsin/EDTA treatment, the harvested cells from each well were re-suspended in PBS, and aliquots were then analysed to determine MPC proliferation for each of the culture time periods using a commercial cell counting kit (Wst-8 Kit (CCK-8); Sigma-Aldrich, Sydney, Australia) according to the manufacturer’s instructions. As the non-PPS primed MPC cultures failed to demonstrate significant variation in their proliferation over the three time periods, the values obtained from each incubation period were pooled and used as the non-PPS pre-treatment control.
Proteoglycan synthesis by MPCs alone and after priming with PPS
Wells of six-well culture plates were seeded with passage 4 MPCs (2.8 × 105/well) and incubated with DMEM + 10% FBS at 37 °C in 5% CO2 for 16 h. High-glucose DMEM containing 5 μg/ml PPS was then added to three wells of the plates and DMEM alone to the remaining three wells. After incubation for 24 h, media were removed from all wells and cells were washed twice with PBS (3 ml/well) and then re-established in culture. The biosynthesis of proteoglycans (PGs) by these cells over 24 h was then determined as previously described . Briefly, media (3 ml) containing 2.2 μCi/ml H2 35SO4 (Perkin-Elmer Life and Analytical Science Knoxfield, Victoria, Australia) was added to each well and plates incubated for 48 h. The medium was removed and discarded. Cells were washed with 3× PBS, and then collagenase solution (Sigma Aldrich, Sydney, Australia; 500 μl, 1 mg/ml) was added to each well and the plate incubated at 37 °C for 1 h to detach the cells and matrix from the plates. The collagenase digests were transferred to 1.5-ml tubes and an equal volume of acetate-buffered papain (Sigma-Aldrich, Sydney, Australia; 1 mg/ml) added to each tube. After incubation at 65 °C for 1.5 h, aliquots (100 μl) of the digests were assayed for DNA content  and the remainder transferred to 1.5-ml tubes, and 40 μl 1 mg/ml chondroitin sulphate A (Sigma Aldrich, Sydney, Australia) and 60 μl 5% aqueous cetyl pyridinium chloride (CPC; Sigma Aldrich, Sydney, Australia) was added. The tubes were vortexed and then centrifuged at 11,000 rpm for 3 min to pellet the precipitated 35S-glycosaminoglycan (GAG)-CPC complex. The precipitates were collected by centrifugation, washed (3× PBS), and then dissolved in 1 ml scintillant (Perkin-Elmer Life and Analytical Science Knoxfield, Victoria, Australia) and transferred to a scintillation vial. The radioactivity of 35S incorporated to newly synthetized S-GAGs of the PGs was determined by scintillation counting (Perkin-Elmer Tricarb 2910TR, Perkin-Elmer Corp., Massachusetts, USA). Results were calculated as 35S-GAG-DPM/μg DNA as an index of proteoglycan synthesis per cell.
Monitoring of MPC phenotypic receptors by flow cytometry
Suspensions of passage 4 MPCs (2.5 × 105) derived from three independent healthy young donors (RAH1, RAH2, and RAH3) were seeded into each well of a six-well plate (in duplicate) and incubated with DMEM + 10% FBS at 37 °C in 5% CO2 for 16 h. The next day, DMEM containing 5 μg/ml PPS was added to three wells of both six-well plates. The remaining three wells of the same plates only received DMEM and were used as the controls (MPCs alone). After an additional 24 h, the cultures from one plate were terminated. The remaining plate was incubated for a further 24 h (i.e. a total incubation time of 48 h). At termination, all media were removed and the six wells of the plates were washed twice with PBS (3 ml/well). Media and washings were discarded, and MPCs were detached from wells by trypsin/EDTA treatment; enzyme activity was quenched and the cells were strained through a 70-μm cell strainer (Becton Dickinson Biosciences, CA, USA) to ensure preparation of single cell suspensions. The MPC suspensions were washed with 10 ml wash buffer (Hank’s buffered salt solution + 5% fetal calf serum (FCS)) and then centrifuged at 400 g for 7 min at 4 °C. Cells were re-suspended in blocking buffer (wash buffer supplemented with 1% (v/v) normal human serum + 1% v/v BSA) and counted in 0.4% Trypan Blue and left on ice in blocking buffer for 30 min. Cells were then pelleted by centrifugation (400 g for 7 min at 4 °C), and the supernatant removed and discarded. The cell pellet was re-suspended in 100 μl of one of the primary antibody listed in Table 1 at a final concentration of 20 μg/ml per tube or 100 μl neat supernatant antibody. After maintaining the tubes at 4 °C for 45–60 min, cells were washed twice with 2 ml cold wash buffer and centrifuged at 400 g for 7 min at 4 °C. Cells were re-suspended in 100 μl blocking buffer containing the appropriate secondary goat anti-mouse antibody or FITC-conjugated antibody at a 1:50 dilution (Southern Biotechnology, USA) (Table 1) and incubated for 30 min and then washed twice with 2 ml cold wash buffer at 400 g for 5 min at 4 °C. Antibody-labelled MPCs were then re-suspended in 0.5 ml FACS FIX (1% (v/v) formalin, 0.1 M d-glucose, 0.02% sodium azide, in PBS) for flow cytometric analysis using a BD FACS Canto II and Flow Data Analysis Software V10 (Becton Dickinson Biosciences, CA, USA).
Extraction of RNA from MPC cultures and genomics analysis
Cells from the three donors (RH1, RH2, and RH3) were used for these studies. Each cell line was processed as described above for flow cytometric analysis but cells were detached from plates using TrypLE select (Gibco 12563-029), an animal origin-free cell dissociation reagent, which was then inactivated by diluting with Hanks buffer without FCS. Cells were pelleted by centrifugation at 400 g for 7 min at 4 °C, and the supernatant removed. Cells were re-suspended and washed again with Hanks buffer then lysed using 700 μl QIAzol (Qiagen #79306). The RNA was isolated using a MiRNeasy Mini Kit (Qiagen #217004) and the on-column DNAse treatment was performed according to the manufacturer’s instructions (RNAse free DNase set; Qiagen #79254). RNA concentrations were measured using a Nanodrop reader. The RNA samples were processed by automated RNASeq-FastQ sequencing using the NEXTflex™ Rapid Illumina Directional RNA-Sequencer (BIOO Scientific, Austin, Texas, USA); for each sample, 300 ng of total RNA was processed using the NEXTflex™ Rapid Illumina Directional RNA-Seq Library Prep Kit (BIOO Scientific, Austin, Texas, USA). Briefly, the method selects poly-adenylated mRNA with coated beads and then converts them to strand-preserved cDNA (via dUTP) before the ligation of sequencing adapters and barcodes. After PCR amplification for 15 cycles the samples were quantified by a fluorescence assay before pooling in equimolar ratios for sequencing. The sample pool was sequenced by the Illumina Nextseq 500 sequencer using a High Output v2 (2 × 75 bp) paired-end sequencing kit ((Illumina, San Diego, USA)) as per the manufacturer’s instructions except that the loading concentrations were reduced by 30% to 0.9 pM. The data were analysed with de-multiplexed reads that were aligned (human hg38) using the TopHat aligner and the differential expression of transcripts was assessed using Cufflinks in Illumina’s Base-space analysis cloud.
All data analysis and graphical representations were performed using Microsoft Excel for Mac (Microsoft version 15.33) and Prism for Mac (version 7.0b, GraphPad Software Inc.). Parametric data were analysed using one-way analysis of variance (ANOVA), with Tukey’s multiple comparison test undertaken when significant differences in means were observed. Non-parametric data were analysed using the Kruskal-Wallis test of median values followed by Dunn’s multiple comparison test. Treated/non-treated groups were compared using the two-tailed Student’s t test followed by Mann-Whitney U tests. P values < 0.05 were considered statistically significant. For the genomic cDNA sequencing, analysis of statistical differences in gene levels in cells from the 24- and 48-h primed and non-primed MPC cultures were determined using the manufacturers’ software with q values < 0.045 being accepted as significant. However, for the majority of gene changes identified, statistical significance was observed at the q = 0.017 level.
Kinetics of binding and uptake of PPS by MPCs in culture
The kinetics of binding and uptake of PPS by cultured MPCs when added to the media at concentrations of 0.5–10 μg/ml was monitored by the percentage decrease in their media levels over 24 h using the PPS ELISA. As shown in Fig. 1, all concentrations of PPS added to the culture media decreased over the first 0.5–2.0 h of incubation with MPCs. For media concentrations of 0.5 and 1.0 μg/ml PPS, this initial decline was followed by a partial release of PPS into the media over the subsequent 6–24 h (shedding period). However, for cultures spiked with 2.5, 5.0, or 10.0 μg/ml PPS, the reduced media levels were sustained over this period. Interestingly, cultures to which 5.0 μg/ml PPS had been added demonstrated the highest decline in media levels after 0.5 h and only released relatively small amounts over the subsequent 24-h period (Fig. 1). These observations suggest a rapid binding of PPS to cell surface heparin receptors, followed by a time- and concentration-dependent shedding and uptake by the MPCs over the 24 h of culture [28, 29]. Moreover, under the conditions used for these cultures, optimum uptake of PPS by MPCs was found to occur with a medium concentration of 5.0 μg/ml.
As the PPS ELISA was not sufficiently sensitive to evaluate the amounts of PPS associated with the MPCs following their removal from culture, we used the PPS-FITC preparation and a fluorometric assay to assess the amounts of PPS associated with the MPCs. This was coupled with fluorescence microscopy to identify the intra-cellular distribution of PPS over the indicated time points. The results of these studies are shown in Figs. 2 and 3. As is evident from Fig. 2, significantly higher levels of PPS-FITC were associated with the MPCs after 24 h of culture with 5.0 μg/ml than with 1.0 μg/ml (p < 0.004), 2.5 μg/ml (p < 0.012), or 20 μg/ml as a trend (p < 0.054). However, significant difference could not be demonstrated between media concentration of 5.0 and 10.0 μg/ml using the PPS-FITC fluorometric assay.
Qualitative studies of the interaction of PPS-FITC with MPCs using fluorescence microscopy together with co-staining of the preparations with the selective nucleus stain PI showed that, after 16 h of culture, the PPS-FITC was largely located within the nucleus of the cell (Fig. 3).
Although the kinetic and fluorometric studies on the uptake of PPS by MPCs suggested that with media concentrations of 5.0 μg/ml more than 50% of the agent was bound and internalised by the cells, the culture periods used never exceeded 24 h. A study was therefore undertaken to monitor MPC proliferation when the cells were cultured alone or after pre-incubation (priming) with 5.0 μg/ml PPS for 4, 24, and 48 h. The results of this study are shown in Fig. 4 where it is evident that MPCs primed with PPS increased proliferation after 48 h to a significantly higher extent than non-primed MPCs (p < 0.028). As an earlier study  had reported that co-cultures of MPCs with PPS promoted chondrogenic differentiation, we next investigated the biosynthesis of PGs of MPCs alone and after pre-culturing with PPS as described for the proliferation study.
The results of this experiment are shown in Fig. 5 and demonstrate that the MPCs primed with PPS increased de novo PG biosynthesis to a greater extent than when MPCs were cultured alone (p < 0.005). Since the PPS priming process was known to promote MPC proliferation (Fig. 4), we normalized the incorporation of 35SO4 into the S-GAGs of the newly synthetized PG relative to cell numbers (DNA content).
In view of these findings, we next sought to determine, using flow cytometry, if the PPS priming process also induced changes in the MPC cell surface phenotypic antigens after culturing the primed and non-primed cells for 24 and 48 h. The results of these studies are shown in Fig. 6 and Additional file 1, where the net differences between primed and non-primed MPC antigen levels were calculated for each donor and expressed as their delta change. Figure 6 depicts graphically the total delta changes that occurred in surface antigen levels for each donor over the 24- and 48-h culture periods. As is shown, donors RAH2 and RAH3 exhibited patterns of changes with marked decreases in the CD73, CD90, CD105, and CD44 surface antigens of between 15–30%. However, expression of CD146 on MPCs from donor RAH3 declined by more than 50%. MPCs from donor RAH1 were found to be less responsive to the priming procedure but still exhibited the same pattern of decline in the characteristic MPC surface phenotype receptors. Interestingly, the STRO-1 marker used to isolate the MPCs from bone marrow aspirates was not markedly affected by the priming step; only donor RAH3 exhibited a 10% decrease, with the cells from the other two donors showing minimal change in expression of this antigen following the PPS priming procedure. The low levels of the hematopoietic and monocyte cell markers CD34, CD45, and CD14 were not affected by PPS priming, suggesting preservation of the mesenchymal cell lineage (Fig. 6).
Additional evidence to support the finding that priming of MPCs with PPS mediated altered gene expression by these cells was provided by isolating the RNA extracted from MPCs of the three donors after culturing for 24 and 48 h and undertaking RNASeq-FastQ sequencing. The results of this study are shown in Tables 2 and 3, which record the mean statistically significant gene changes for the three donors that were detected between their primed and non-primed MPCs after 24 and 48 h of culture. Using internet-based gene search engines, the proteins encoded by these genes are also identified in Tables 2 and 3. These datasets show that after the initial 24 h of culture only four genes were upregulated and 16 downregulated (Table 2) by the priming process. However, after 48 h 16/42 genes were upregulated and 26 downregulated.
This study has shown that priming of MPCs with PPS results in the initial binding of the drug to the cell surface receptors accompanied by partial shedding, and then internalization and migration to the cell nucleus where it influenced gene and protein expression. The extent of changes induced in MPC cell surface markers by the PPS priming step for the three donors was found to be variable (Fig. 6). Indeed, differences in gene expression by bone marrow-derived MSCs from different donors have been previously reported as a potential problem for their routine application in clinical practice . This inter-donor variability has also been attributed to a variety of other factors, including the inherent heterogeneity of the MSC populations isolated from different individuals, the duration of their culture expansion, and the period and nature of their storage [31,32,33]. The MPCs used in the present study were all within the age range of 20–35 years, were selected on the basis of their expression of STRO-1, and were subjected to similar culture and storage conditions to minimize inter-donor cell variability. Nevertheless, the magnitude of change in MPC surface marker expression induced by the PPS priming step for these three donors was found to be quite variable, suggesting that individual genetic variations may represent a dominant role. However, apart from STRO-1, the markers CD73, CD90, CD105, CD44, and CD146 were all observed to decline following PPS priming of the cells.
Human MSC monolayer cultures incubated with transforming growth factor (TGF)-beta for 7 days have been reported to undergo a similar downregulation of the surface antigens CD44, CD90, and CD105, a finding that was interpreted to signal an early phase of their de-differentiation to the chondrogenic phenotype . We also observed a strong decline in CD146 antigen presentation on PPS priming, particularly for MPCs isolated from donor RAH3. The transmembrane protein CD146 is receptor highly expressed by endothelial cells  and on the surface of perivascular cells, which have recently been proposed as the source of MSCs within the perivascular niche of bone marrow . Moreover, a recent study has provided compelling evidence that CD146 is a high-affinity netrin-1 receptor on endothelial cells . Netrin-1 is a neuronal guidance molecule that promotes angiogenesis and vascular development of the endothelium following interaction with CD146 [36, 37]. In addition, expression of CD146 is associated with populations of human MPCs that promote the establishment of bone marrow elements, and enhance osteogenic differentiation and bone deposition when these cells are implanted subcutaneously into immune-deficient mice . The present observation that CD146 expression by MPCs was markedly downregulated by PPS priming would therefore be consistent with our previous observations of reduced osteogenesis of MPCs when cultured or co-formulated with this agent in vitro  and in vivo [22,23,24].
Although many of the functions of the proteins encoded by the genes identified by RNA sequencing analysis could not be obviously assigned, the changes in the genes encoding the aggrecan core protein, IGF2, alpha chain type V collagen, FosB transgene, COMP, the proteinase ADAMTS4, and type II collagen alpha chains provided are consistent with increased chondrogenic differentiation of MPCs. For example, aggrecan core protein is necessary for the biosynthesis of PGs  and its upregulation is consistent with the known elevation of their biosynthesis by MPCs after PPS priming. The down regulation of the ADAMTSL4 gene could also be considered as beneficial for the deposition of a cartilaginous matrix as the protein it encodes is responsible for the degradation of PGs . In addition, the upregulation of type V collagen could be significant as this protein is a contributor to the assembly of collagen fibres during cell growth and matrix assembly . On the other hand, the downregulation of the COMP genes was unexpected since this protein is an abundant component of the cartilage extracellular matrix. However, studies with human MSCs have shown that enhancement of COMP gene expression did not increase the transcript levels of the chondrogenic markers Sox9 or aggrecan, suggesting that the role of COMP in matrix formation occurs at the post-transcriptional level . Notably, the IGF2 gene was found to be strongly upregulated. As the proteins encoded by this gene play significant roles in the growth, differentiation, and survival of connective tissue cells, including articular cartilage , its elevation is consistent with the present study and our previous report on MPC chondrogenesis mediated by PPS . The RNASeq-FastQ sequencing data also indicated that the FosB transgene was strongly upregulated by the priming process. Numerous studies have shown that the Fos genes are involved in the formation of heterodimeric complexes with members of the jun family of proto-oncogenes (c-jun, junB, jun D) to form the AP-I promotor complex required for gene transcription . Following binding to consensus sequences in the regulatory regions of DNA, the Fos-Jun/AP1 complex mediates transcription pathways responsible for critical cell functions, including differentiation and turnover of the extracellular matrix .
A related sulphated glycosaminoglycan, heparin, is known to bind and interact with a variety of cells where it also localizes in the nucleus and modifies gene expression [31, 32, 45,46,47,48]. Moreover, heparin has been used at low concentrations (<200 ng/ml) as a supplement for the culture expansion of embryonic stem cells [49, 50] and MSCs . However, in a recent study which used human bone marrow-derived MSCs , it was demonstrated that when serial cultures of these cells were supplemented with heparin at a concentration equivalent to that used in the present study (500 μg/ml), cell growth was strongly retarded and MSC morphology and genetic expression modified to a senescent phenotype. These conflicting findings may be explained by the structural differences between these two polymers.
Like heparin, PPS is a poly-anion, but is not a glycosaminoglycan since it has a backbone structure consisting of repeating beta-d-xylanopyranose units to which a methyl glucopyranosyluronic acid ring is attached laterally every 9–10 xylanopyranoses units (Fig. 7). The xylanopyranose backbone required for the synthesis of PPS is extracted from Beech wood (Fagus sylvatica) hemi-cellulose, is first sulphate-esterified, and then fractionated to obtain the required molecular size. This semi-synthetic process affords a water-soluble poly-dispersed pharmaceutical preparation with a weight average molecular weight (MW) of 5700 Da and a high negative charge conferred by the large number of sulphate ester groups localised along its xylanopyranose backbone .
In contrast, native heparin is a structurally heterogeneous biopolymer that consists essentially of variably spaced repeating units of either 2-O-sulphated iduronic acid and 6-O-sulphated and N-sulphated glucosamine sugar rings linked glycosidically . Commercially available heparin is more poly-dispersed than PPS with an averaged molecular weight ranging between 3000 to 30,000 Da  but is the most highly sulphated naturally occurring glycosaminoglycan with 2.7 sulphate groups/disaccharide unit . However, its charge density is less than that of PPS which on average contains 3–4 sulphate groups/disaccharide unit (Fig. 7).
Notwithstanding these significant molecular, charge, and conformational differences, PPS, because of its poly-anionic structure, does exhibit some heparin-like pharmacological activities. Although it is a weaker anti-coagulant than heparin, PPS is a strong fibrinolytic and lipolytic agent [52, 54]. These pharmacological activities resulted in its original clinical applications in the 1950s for the treatment of thrombotic and arteriosclerotic vascular disease . However, over the intervening years, PPS has been shown to be effective for the management of more diverse medical indications, including interstitial cystitis , soft tissue inflammation , osteoarthritis [58,59,60], and Ross River Virus-related arthropathies .
In our earlier in-vitro studies, MPCs were cultured with PPS at various concentrations including 5.0 μg/ml, but for up to 10 days . With the longer incubation periods, gene expression of Sox-9 and Aggrecan by MPCs was not significantly elevated relative to MPCs alone until day 7. In addition, expression of type II collagen was not significantly increased until day 10, when type X collagen, RUNX2, and Noggin gene expression was also suppressed . These earlier RNA studies suggest that the present protocol of 24-h priming of MPC with PPS followed by maintaining cultures for up to 48 h prior to determination of gene expression may have been too short to establish the lifetime of genetic modifications. We therefore acknowledge that the maintenance of our PPS-primed MPC cultures for only 48 h represents a limitation of the present study. However, using an ovine model of disc degeneration induced by lumbar microdiscectomy we have demonstrated that PPS-primed MPCs when embedded in biodegradable collagen sponges implanted into the degenerate discs promoted the deposition of higher levels of proteoglycans and tissue repair after 6 months, compared with the injured disc injected with non-primed MPCs . We consider that this in-vivo study supports our proposition that PPS-primed MPCs retained their modifying effects on gene and protein expression beyond the 48-h experimental period used in the present study.
These studies have shown that pre-incubation of MPCs with 5.0 μg/ml PPS for only 24 or 48 h was sufficient to invoke significant changes in their gene signature and protein expression consistent with enhanced proliferation and differentiation to the chondrogenic phenotype. The PPS priming step was undertaken at the penultimate phase of MPC culture expansion, a procedure that eliminated the necessity of combining the required quantities of the two agents at the time of clinical application and thereby eliminating the possibility that ‘free’ PPS was co-administered with the progenitor stem cells. Furthermore, from the results of the present study, together with the positive outcome of our animal model study , we conclude that pre-culturing of MSCs with agents such as PPS could provide an alternative method for reprogramming these cells to promote their differentiation towards a targeted phenotype that may be required for a specific medical indication, rather than their co-administration with agents that may independently be associated with undesirable side effects.
A disintegrin-like metalloproteinase with thrombospondin motifs
Bovine serum albumin
Cartilage oligomeric matrix protein
Cetyl pyridinium chloride
Dulbecco’s modified Eagle’s media
Enzyme-linked immunosorbent assay
Fetal bovine serum
Fetal calf serum
Insulin-like growth factor
Mesenchymal progenitor cell
Mesenchymal stem cell
Transforming growth factor
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The authors gratefully acknowledge the contribution of Mark Van der Hoek of the David R. Gunn Genomics Suite, South Australia Health and Medical Research Institute, Adelaide South Australia, for subjecting the RNA isolated from the PPS primed and non-primed MPCs to NEXTflex™ Rapid Illumina Directional RNA-Sequencing and providing data analysis of the results. We also thank Professor Silviu Itescu CEO of Mesoblast Ltd for permission to use the immune-selected human STRO-1+ MPC for this study and acknowledge that Mesoblast Ltd have been granted international patent rights for the commercial application of these cells.
This project was partially funded with a research grant provided by Proteobioactives Pty. Ltd.
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All the data and material not included in this report are available from the authors on request. However, some material is presently archived by Proteobioactives Pty. Ltd. but would be made available on written request.
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Ethics approval and consent to participate was obtained from the Human Research Ethics Committee of the Adelaide Hospital.
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PG is a Director of Proteobioactives Pty. Ltd. but does not hold shares in the company. JW and SS were employees of Proteobioactives Pty. Ltd. but do not hold shares in the Company. The remaining authors declare that they have no competing interests.
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(A–E) Surface antigen expression of MPCs derived from three donors (RAH1, RAH2, and RAH) when cultured for 24 and 48 h with and without priming with 5.0 μg/ml PPS. Delta change represents the percentage change in antigen levels mediated by the PPS priming step. (DOCX 18 kb)
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Wu, J., Shimmon, S., Paton, S. et al. Pentosan polysulfate binds to STRO-1+ mesenchymal progenitor cells, is internalized, and modifies gene expression: a novel approach of pre-programing stem cells for therapeutic application requiring their chondrogenesis. Stem Cell Res Ther 8, 278 (2017). https://doi.org/10.1186/s13287-017-0723-y
- Mesenchymal progenitor cells
- Pentosan polysulfate
- Gene expression