Calcium (Ca2+) signalling plays an indispensable role in dental pulp and dentin regeneration, but the Ca2+ responses of human dental pulp stem cells (hDPSCs) stimulated with tricalcium silicate-based (TCS-based) dental biomaterials remains largely unexplored. The objective of the present study was to identify and correlate extracellular Ca2+ concentration, intracellular Ca2+ dynamics, pH, cytotoxicity, gene expression and mineralization ability of human dental pulp stem cells (hDPSCs) stimulated with two different TCS-based biomaterials: Biodentine and ProRoot white MTA. The hDPSCs were exposed to the biomaterials, brought in contact with the overlaying medium, with subsequent measurements of extracellular Ca2+ and pH, and intracellular Ca2+ changes. Messenger RNA expression (BGLAP, TGF-β, MMP1 and BMP2), cytotoxicity (MTT and TUNEL) and mineralization potential (Alizarin red and Von Kossa staining) were then evaluated. Biodentine released significantly more Ca2+ in the α-MEM medium than ProRoot WMTA but this had no cytotoxic impact on hDPSCs. The larger Biodentine-linked Ca2+ release resulted in altered intracellular Ca2+ dynamics, which attained a higher maximum amplitude, faster rise time and increased area under the curve of the Ca2+ changes compared to ProRoot WMTA. Experiments with intracellular Ca2+ chelation, demonstrated that the biomaterial-triggered Ca2+ dynamics affected stem cell-related gene expression, cellular differentiation and mineralization potential. In conclusion, biomaterial-specific Ca2+ dynamics in hDPSCs determine differentiation and mineralization outcomes, with increased Ca2+ dynamics enhancing mineralization.
Tricalcium silicate-based (TCS-based) cements are hydraulic bioactive materials widely used as endodontic cements in dentistry and as bone substitutes in orthopedics1. Several commercial TCS-based cements with subtle modifications in the manufacturing process and composition are available. ProRoot White MTA (WMTA) (Dentsply, Tulsa Dental, OK, USA) and Biodentine (Septodont, Saint-Maur-des-Fossés, France) are two representative TCS-based cements with superior clinical success in dentistry. The widespread clinical indications of TCS-based cements are primarily based on their ability to form calcium hydroxide as a by-product of hydration2. The subsequent dissolution of calcium hydroxide to release hydroxide (OH-)and calcium ions (Ca2+) creates a desirable environment to promote healing and repair of soft and hard tissues3,4. While hydroxide ions create an alkaline environment responsible for antibacterial and anti-inflammatory activity, Ca2+ ions play a comprehensive role as a vital intracellular second messenger that governs diverse cellular processes such as gene transcription, protein expression, cell proliferation, differentiation, apoptosis, and activation of excitatory cell types5,6.
TCS-based cements release Ca2+ in the microenvironment causing elevated extracellular Ca2+ concentration and as a consequence transiently increase the intracellular Ca2+ concentration due to calcium-sensing receptor (CaSR) activation7,8. The dynamic Ca2+ dependent signalling system can affect numerous Ca2+ sensitive enzymes that convert changes in extracellular Ca2+ concentration and intracellular Ca2+ dynamics into well-defined cell actions9. Analysis of the molecular cues embedded in the intracellular Ca2+ dynamics will lead to better understanding of the intracellular signalling mechanisms involved in regulating the bioactivities of cells10. Intracellular Ca2+ dynamics play a dual role by acting both as an initiator and mediator of stem cell differentiation. Thorough knowledge on the role of Ca2+ dynamics in the differentiation of stem cells into a tissue-specific lineage may offer an alternative biotechnological approach to exploit the unique properties of stem cells10.
Calcium signalling is multifaceted and depends on the cell type9. Although Ca2+ signalling plays an indispensable role in dental pulp and dentin regeneration, there is a lack of information on the Ca2+ dynamics of human dental pulp stem cells (hDPSCs). The aim of the present study was to identify and correlate extracellular Ca2+ concentration, intracellular Ca2+ dynamics, pH, cytotoxicity, gene expression and mineralization ability of human dental pulp stem cells (hDPSCs) stimulated with two different TCS-based biomaterials; ProRoot WMTA and Biodentine. Our work shows significant differences in extracellular and intracellular Ca2+ changes that link to distinct patterns of hDPSCs gene expression, cellular differentiation and mineralization potential.
Calcium release and pH
Ca2+ measurements in the cell medium, in response to exposure to TCS-based cements in the absence as well as presence of hDPSCs were performed (Fig. 8). In the absence of cells, Biodentine released significantly more Ca2+ in the α-MEM medium than ProRoot WMTA (p < 0.001) (Fig. 1); no significant difference in pH was found between the groups (Supplementary Fig. 1). Interestingly, in the presence of hDPSCs in the culture dishes, the larger Biodentine-linked Ca2+ release in the medium was reduced to the level observed with ProRoot WMTA (p < 0.001), indicating that the cells take up the extra Ca2+ load provided by Biodentine (Fig. 1).
Ca2+ imaging experiments to determine the cellular responses to biomaterial exposure and its associated changes in extracellular Ca2+ were performed. Cells with acetylcholine (1 µM) were challenged to verify their responsiveness. Oscillatory changes in intracellular Ca2+ that are typical for hDPSCs were found (Supplementary Fig. 2). Subsequently, cells were exposed to TCS-based cements placed in an insert, which after baseline Ca2+ recording, was lowered to contact the bathing solution under continuous Ca2+ imaging (Fig. 2). Gross analysis of the intracellular Ca2+ signal averaged over all cells in view, demonstrated a Ca2+ increase characterized by a peak followed by recovery (Fig. 2).
Finer grained analysis of the Ca2+ dynamics in individual cells, in response to TCS challenging with the two biomaterials were performed. This showed **that Biodentine produced a significantly higher maximum amplitude of the Ca2+ transients (p < 0.0001) (Fig. 3A), a reduced time to reach the maximum (p < 0.0001) (Fig. 3B) and an increased area under the curve (p < 0.01) (Fig. 3C) as compared to ProRoot WMTA. The number of cellular Ca2+ transients per cell dish did not differ significantly between the groups (Fig. 3D). On average, the number of Ca2+ transients per cell after biomaterial challenging was low, amounting to 0.92 transients per 10 min for Biodentine and 1.12 for ProRoot WMTA (~ 3 transients over 30 min for both).
Control experiments under conditions of cell pre-loading with the intracellular Ca2+ chelator BAPTA-AM were performed. Complete absence of intracellular Ca2+ dynamics upon exposure to the two biomaterials were found (Supplementary Fig. 3).
Elevations in extracellular Ca2+ concentrations11 as well as intracellular Ca2+ changes are well known to influence gene expression12. The response of four specific gene markers were tested: BGLAP, TGF-β, MMP1 and BMP2 to the two TCS-based biomaterials. Biodentine exposure for 1 day resulted in upregulation of BGLAP and TGF-β that was more than twice as large compared to ProRoot WMTA (Fig. 4A,B); only small differences were observed for MMP-1 (Fig. 4C). BMP2 was upregulated by Biodentine but ProRoot WMTA downregulated the gene (Fig. 4D), demonstrating again a pronounced difference between the two TCS-based cements. These experiments were repeated under conditions of intracellular Ca2+ chelation by loading the cells with 1 µM BAPTA-AM which also present during the 1 day exposure to the TCS-based cements. Such treatment clearly suppressed the BGLAP and TGF-β responses observed with both biomaterials. By contrast, the small changes observed for MMP1 became more pronounced in BAPTA-AM treated cells. For BMP2, the effects were intermediate, with a reduction by one third of the Biodentine induced upregulation and a one third increased downregulation in response to ProRoot WMTA (Fig. 4D).
Experiments on cell death
Subsequently, it was verified whether cell survival/cell death was affected by any of the treatments used in the experiments on gene expression. Viability as measured with the MTT assay demonstrated that 1 day exposure to the TCS-based cements did not result in significant differences compared to control (Fig. 5A). However, BAPTA-AM treatment (as applied in the gene studies) significantly decreased the MTT signal (p < 0.01) (Fig. 5A). Further investigations with the TUNEL assay (Fig. 5B) and live/dead staining (Supplementary Fig. 4) did not reveal any difference in terms of cell death, suggesting that the BAPTA-AM induced decrease in MTT signal is most likely caused by suppression of mitochondrial metabolic activity resulting from the dampening effect of BAPTA-AM on intracellular Ca2+ dynamics and not resulting from cell death13.
Further, the mineralization potential of TCS-based cements was verified. Therefore, hDPSCs cultured in the presence of TCS-based biomaterials were evaluated for 7, 14, 21 and 28 days. Our results show that Biodentine induced faster mineralization (14 days) compared to ProRoot WMTA (21 days). At 21 days, Biodentine showed extensive mineralization while ProRoot WMTA displayed scattered presence of mineral nodules comparable to that seen in the Biodentine group at 14 days (Fig. 6).
TCS-based cements are primarily used in dentistry and their interaction with hDPSCs are of great interest14. Potential use of hDPSCs in tissue regeneration by virtue of their ability to differentiate into fibroblasts, osteoblasts, odontoblasts, adipocytes, neurogenic and myogenic tissues in vitro make them a favorable model system for studying Ca2+ signals15. hDPSC derived odontoblasts play an active role in the transport and accumulation of Ca2+ which leads to regeneration of the dentin-pulp complex16. In this study, custom prepared hDPSCs with 96% purity, extracted by an enzyme digestion method from healthy unerupted human third molars were used. Transwell membranes with a pore diameter of 0.4 µm were used to mimic the absence of direct contact between the biomaterial and hDPSCs while allowing for soluble compounds from the biomaterials to reach the cells, similar to clinical conditions17.
TCS-based cements are known to release Ca2+ in varying concentration, depending on the cement composition. In this study, Biodentine released significantly more Ca2+ than ProRoot WMTA after 30 min in α-MEM medium (p < 0.001). This could be explained by the fact that despite both ProRoot WMTA and Biodentine contain TCS as their main ingredient, the structure and composition of the two TCS-based cements reveal certain differences that could contribute either directly or indirectly to the difference in Ca2+ release. Compared to ProRoot WMTA, Biodentine has a smaller particle size, which is known to increase the Ca2+ release18. In addition to TCS as the major ingredient, ProRoot WMTA contains dicalcium silicate and tricalcium aluminate19. These additional ingredients form minimal or no calcium hydroxide upon hydration leading to a lesser degree of Ca2+ release. The fact that the Ca2+ release was not accompanied by a corresponding rise in pH suggests that the source of this Ca2+ is not only from the formation and dissolution of calcium hydroxide but possibly also from other calcium compounds being present. Biodentine uses calcium chloride as the liquid medium for hydration while ProRoot WMTA uses water. The use of calcium chloride could enhance the Ca2+ release by accelerating the setting reaction, increasing calcium hydroxide formation and by Ca2+ release from unreacted calcium chloride20.
The larger Ca2+ release from Biodentine was not detectable in the presence of hDPSCs, indicating that Ca2+ is taken-up by the cells. Cellular Ca2+ uptake involves subsequent Ca2+ binding to proteins and uptake into organelles like the endoplasmic reticulum (ER) and mitochondria9,21. This organelle-based Ca2+ load may affect gene expression and viability/cell death. In fact, the ER-mitochondrial Ca2+ axis is a major player and determinant of cell survival/cell death22 and is also known to affect gene expression23.
Our results obtained from intracellular Ca2+ measurements closely reflect the differences observed between the two TCS-based cements on extracellular Ca2+. The significantly larger Ca2+ release from Biodentine correlates well with the significantly larger area under the curve of intracellular Ca2+ changes (p < 0.01), the significantly higher maximum amplitude (p < 0.0001) and the significantly shorter time to maximum change (p < 0.0001) observed in Biodentine as compared to ProRoot WMTA (see Fig. 3). The larger Ca2+ load associated with Biodentine may act through increased Ca2+ entry into the cell, possibly via Cav1.2 L-type Ca2+ channels24,25, ORAI1, an essential pore subunit of store-operated Ca2+ entry (SOCE) channels in stem cells26 or TRPM4 channels27. Increased Ca2+ entry is followed by intracellular cycling between the cytoplasm, ER Ca2+ stores and mitochondria in mesenchymal stem cells, thus leading to the observed Ca2+ dynamics28,29.
Calcium dynamics can activate signalling pathways in both the nucleus and cytoplasm to induce gene expression by different pathways, that can function both as an inhibitor or activator of gene expression30. The frequency, duration and amplitude of Ca2+ transients are essential for increasing the efficiency and specificity of gene expression21. There is a nonlinear relationship between gene transcription and intracellular Ca2+ dynamics, that periodically exceeds the threshold for activation of gene transcription31. The Ca2+ oscillation frequency hereby differentially controls the activation of different genes and direct cells to specific developmental pathways32. The present experiments did not reveal prominent oscillatory activity, with only 3 elevations occurring per cell over the 30 min recording period for both biomaterials. This makes it possible that amplitude rather than frequency is most important in the observed effects, as is the case in the slow oscillatory activity leading to oocyte activation33,34. In any case, the results revealed that Biodentine promoted mRNA expression of BGLAP, TGF-β, and BMP2 indicating that the increased Ca2+ load and intracellular dynamics can enhance the expression of genes associated with odonto-/osteogenic differentiation necessary for successful regeneration of the dentine-pulp complex35,36. Intracellular buffering with BAPTA-AM treatment inhibited the expression of BGLAP and TGF-β, thereby supporting an underlying role of Ca2+ signalling in the upregulation of these genes. Furthermore, addition of BAPTA-AM reduced the upregulation of BMP2 but resulted in overexpression of MMP1. It is well known that an increase in extracellular Ca2+ enhances the expression of BMP2 by activation of the Ca2+ sensing receptor, elevation of intracellular Ca2+ and stimulation of Ca2+/calmodulin-dependent nuclear factor of activated T cells (NFAT) signalling pathways7.
Calcium plays a significant role in molecular processes responsible for mediating cell survival and death, including defence and programmed cell death mechanisms, such as cell cycle, apoptosis, and autophagy37,38. In the present study, combined MTT and TUNEL assays revealed absence of cytotoxicity after 1 day exposure to the biomaterials. Moreover, BAPTA-AM treatment caused suppression of mitochondrial metabolic activity causing a decrease in the MTT signal in all the groups. Inconsistent results regarding cell death were seen in the literature where Biodentine performed better39, similar40,41,42,43 or worse44 than MTA. Such contradictory results may be related to the type of target cells, method of cytotoxicity assessment, direct contact of cells with the materials and concentration of materials. Three-dimensional culture of dental pulp stem cells in direct contact to Biodentine and MTA revealed higher cell viability compared to ProRoot MTA after 1, 3 5 and 7 days45. In the study by Daltoe et al., serial dilutions (1:1, 1:10 and 1.100) of extracts from Biodentine and ProRoot MTA showed no significant differences in cell viability after 1 and 2 days in any of the concentrations tested46. The cytotoxic effect of Biodentine and ProRoot MTA on hDPSCs were concentration dependent as cell viability was higher at 1:100 concentration compared to 1:10 or 1:1 concentration. Similar results were obtained when hDPSCs were cultured in medium conditioned with Biodentine or ProRoot MTA47. When transwell membrane was used to avoid direct contact between the biomaterials and hDPSCs, there was no significant difference in cell viability and cell migration between ProRoot MTA and Biodentine48.
Further, the effects of TCS-based cements on the mineralization potential of hDPSCs were investigated using the Alizarin red and Von Kossa staining technique. Biodentine induced faster and increased mineralized nodule formation compared with the other groups, consistent with previous literature42,49,50. The increased mineralization potential of Biodentine is in conformity with its larger material-linked Ca2+ discharge, the larger intracellular Ca2+ response and the upregulation of BMP2, BGLAP and TGF-β observed in our study. As Ca2+ is deposited by osteoblasts and/or odontoblasts, the present results also highlight the osteogenic and/or odontogenic differentiation potential of hDPSCs in the presence of Biodentine and ProRoot WMTA. In agreement with the findings of the present study, previous literature suggests that in comparison to ProRoot MTA, Biodentine demonstrated significantly better cell survival and proliferation of osteoblasts and periodontal ligament cells39,51.
Limitations to simulate the complex biological conditions of the clinical situation exist and hence the results obtained from the present study must be observed with caution for direct correlation with clinical scenarios. Calcium sensitive dyes are widely used for evaluating Ca2+ signalling, but their applications have certain drawbacks. Special conditions are required for loading of the cells, bleaching may occur because of extended imaging periods and intracellular dye accumulation may increase cytoplasmic Ca2+ buffering52.
It is essential to expand our knowledge on the numerous pathways by which Ca2+ regulates cellular functions9. A typical characteristic of Ca2+ signalling is the manner by which different Ca2+ signals can be translated into specific cell functions depending on the type of signal6. The wide range of functions executed by Ca2+ is attributed to the versatility in speed, amplitude, duration and spatiotemporal pattern of Ca2+ signals as well as by interactions between Ca2+ and other signalling pathways most likely mediated by different cellular processes53. Further research on the versatile patterns of Ca2+ signals is essential for studying the mechanisms lying beyond the cellular functions5.
Our work demonstrates that hDPSCs take up the Ca2+ released from TCS-based biomaterials without provoking cell death. The larger Biodentine-linked Ca2+ load was reflected in altered intracellular Ca2+ dynamics, which consequently resulted in differential gene expression, cellular differentiation and mineralization potential of hDPSCs stimulated with TCS-based cements.
Materials and methods
Isolation of stem cells
Human Dental Pulp Stem Cells (hDPSCs) were extracted from unerupted human third molars by enzyme digestion54. Written informed consent was collected from all patients and ethical approval was obtained from the Ethical Committee of University hospital, Ghent, Belgium according to laws of ICH Good Clinical Practice (GE11-LM-go-2006/57). The tooth crown was cleaned with iodine and 70% ethanol. The tooth was then cut with a bone cutter at the cemento-enamel junction to remove the pulp tissue and digested with type 1 collagenase and dispase. Cell suspension was cultured in a 25cm2 flask in Alpha modified Eagles medium (α-MEM, Sigma-Aldrich, Overijse, Belgium) with 10% fetal bovine serum and antibiotics (100U/ml Pencillin and 100 mg/ml streptomycin) at 37 °C and 5% CO2. Flow cytometry analysis was performed to identify the purity of the stem cell culture obtained. Purity of the custom prepared stem cells were determined by mesenchymal stem cell markers CD90, and CD105. Custom prepared hDPSCs were grown to subconfluence and attained a purity of 96% (Fig. 7).
For the experiments, hDPSCs were seeded in a 24 well plate at a density of 40,000 cells/well (for Ca2+ release, pH, cytotoxicity and mineralization assay), in a 6 well plate at a density of 5 × 105 cells/well (for qRT-PCR), or in 35 mm glass bottom dishes (MatTek Corporation, Massachusetts, USA) at a density of 1 × 105 (for live Ca2+ fluorescence imaging). For intracellular buffering 1 µM of BAPTA-AM (Life technologies, California, USA) was added to α-MEM medium. All groups were maintained at 37 °C and 5% CO2 for 1 day.
Biodentine (Septodont, Saint-Maur-des-Fossés, France) and ProRoot White MTA (WMTA) (Dentsply, Tulsa Dental, OK, USA) were mixed according to manufacturer’s instructions and condensed in teflon moulds of height 1 mm and diameter 5 mm (for Ca2+ release, pH, live Ca2+ fluorescence imaging and cytotoxicity) or height 2 mm and diameter 8 mm (for qRT-PCR). Although the size of samples was different, the ratio of the exposed surface area of the sample to the volume of the surrounding medium (mm2/ml) was maintained as a constant in all experiments. The samples were allowed to set for 3 h in 100% relative humidity at 37 °C and sterilized by ultraviolet radiation for one hour. Samples were placed in transwell inserts of 0.4 µm pore size (Greiner bio-one, Kremsmünster, Austria) to avoid direct contact of the biomaterial with hDPSCs (Fig. 8). Positive control (without biomaterial), Biodentine and ProRoot WMTA groups were evaluated with/without BAPTA-AM loading. For cytotoxicity assay, qRT-PCR and mineralization assay, a sample size of n = 3/group were used while n = 6/group were used for Ca2+ release, pH and live Ca2+ fluorescence imaging experiments.
Calcium release and pH
Calcium release was measured by use of a Ca2+ ion selective combination electrode (Hanna HI 4004, Hanna Instruments, Temse, Belgium). To reduce interferences and the formation of refractory oxides, 40 µl ionic strength adjuster (1 M KCl ISA buffer, HI 4004–00, Hanna Instruments, Temse, Belgium) was added to 1 ml of all sample solutions. The electrode was calibrated using a standard calibration line. The pH of the solutions was measured with a pH glass electrode (Primatrode, Metrohm, Switzerland). Calcium release from the biomaterial and pH were measured both in the presence and absence of hDPSCs.
Live cell Ca2+ imaging
For live cell Ca2+ imaging, hDPSCs were loaded with 5 µM of Fluo-3-AM (Invitrogen, California, USA) and 0.01% pluronic F127 (Invitrogen, California, USA) at room temperature in the dark and incubated for 1 h. The cells were then washed and de-esterified for 15 min in HBSS (Hanks Balanced Salt Solution) – HEPES (4-(2-hydroxyethyl)-1-piperazineethanesulfonic acid) buffer (0.14 g/l cacl2.2H2O (1.8 mM) containing 0.2 g/l MgSO4.7H2O (0.81 mM), 0.032 g/l Na2HPO4.2H2O (0.18 mM), 0.4 g/l KCl (5.36 mM), 0.06 g/l KH2PO4 (0.44 mM), 1.0 g/l D-glucose (5.55 mM), 5.95 g/l HEPES (25 mM) with PH 7.4) with a Ca2+ concentration of 1.8 mM similar to α-MEM. Cells were superfused with HBSS-HEPES buffer for 2 min and were then challenged with acetylcholine (ACh) 1 µM for 8 min. After recording the ACh induced Ca2+ oscillatory activity, superfusion was switched back to HBSS-HEPES for 1 min. The biomaterials were inserted with transwell inserts (0.4 µm) using a special holder after 1 min and recorded for 30 min. Calcium imaging was performed on an inverted fluorescence microscope with an EM-CCD camera and FluoFrame imaging Software. Peak amplitude, time to maximum amplitude, number of Ca2+ transients of individual cells and area under the curve of the Ca2+ dynamics were calculated with Matlab 8.0 (The Mathworks Inc., Natick, MA, USA) software.
qRT-PCR analyses were done after 1 day. cDNA was produced and amplified using the Reverse Transcriptome kit (QuantiTect Reverse Transcription kit, Qiagen, Hilden, Germany). Target cDNA was amplified using specific primer pairs. qRT-PCR was performed using Sensimix SYBR No-ROX Kit (Bioline, London, UK) on Light cycler 480 System (Roche Life Science, Penzberg, Germany). Samples were normalized using qBasePlus (Biogazelle NV, Zwijnaarde, Belgium) against at least three of the following genes: Rpl13a, Eif4b, B2m, Actb, or Gapdh as described previously55. Details of specific primers used for gene expression analysis are provided in Table 1.
Live/dead staining was performed using calcein acetoxymethyl (AM) ester (Tebu-Bio, Boechout, Belgium) / propidium iodide (PI; Sigma-Aldrich, Overijse, Belgium). The samples were rinsed with 500 µL phosphate buffered saline (PBS). 500 µL PBS, 1 µL PI and 1µL calcein AM (Sigma-Aldrich, Overijse, Belgium) was added to each well and after 10 min incubation in a dark room, samples were evaluated with a fluorescence microscope (Type U-RFL-T, Olympus, Antwerpen, Belgium).
To quantify cell viability, the colorimetric 3-(4,5-dimethyl-2-thiazolyl)- 2,5-diphenyl-2H-tetrazolium bromide (methyl thiazolyl tetrazolium; MTT) assay was performed. The cell culture medium was replaced by 0.5 mg/ml MTT reagent and cells were incubated for 4 h at 37 °C. After removal of the MTT reagent, lysis buffer (1% Triton X-100 in isopropanol/0.04 N HCl) was added and incubated for 30 min at 37 °C on a gyratory shaker (70 rpm). The dissolved formazan solution was transferred into a 96-well plate and the optical densities (OD) were measured spectrophotometrically at 580 nm (Universal Microplate Reader EL 800, Biotek Instruments, Vermont, USA). Cell viability was calculated according to the following equation56:
TUNEL assay kit (Roche, Basel, Switzerland) was used for staining TUNEL positive cells and DAPI nuclear stain was used for staining viable cells. The TUNEL positive and DAPI cells were visualized in fluorescence microscope (BD Pathway 435, BD Biosciences, New Jersey, USA) and images were analysed using Fiji Image J software57.
The cells were seeded on plastic coverslips of 13 mm diameter (Nunc Thermanox, ThermoFisher, Massachusetts, USA) in an adhesive 24 well plate. Osteogenic medium was prepared by supplementing standard culture medium with 10 mM β-glycerophosphate (Sigma-Aldrich), 100 µM L-ascorbic acid 2-phosphate (Sigma-Aldrich) and 100 nM dexamethasone (Sigma-Aldrich). Sample extracts were prepared at a non-toxic dilution as determined by MTT assay. For both Alizarin Red and Von Kossa staining, either pure extract with standard culture medium or extract supplemented with osteogenic medium was added to the cells. At 7, 14, 21 and 28 days, Alizarin Red (Alizarin red dye 1 g in 40 ml ultra-pure water, VWR, Oud Heverlee, Belgium) and Von Kossa (silver nitrate 1 g in 20 ml ultra-pure water, VWR, Oud Heverlee, Belgium) staining were performed. After rinsing with PBS, the cells were fixed with neutral buffered formaldehyde. The reaction was accelerated by adding formaldehyde-sodium carbonate solution (1 g in 15 ml ultra-pure water, VWR, Oud Heverlee, Belgium). Unreduced silver ions were removed by Farmer’s solution (Sigma-Aldrich, Overijse, Belgium) containing 10% potassium ferrocyanide and 90% sodium thiosulfate. All images were captured with a microscope (Olympus BX51, Olympus, Tokyo, Japan) equipped with Xcellence software (Olympus, Tokyo, Japan).
All data were subjected to statistical analysis by unpaired t-test with Welch's correction, analysis of variance (ANOVA) and individual comparisons were performed by Tukey post-hoc at a significance level of p < 0.05 using Statistical Package for Social Sciences (SPSS) v25.0 (IBM Corp., Armonk, NY, USA) and GraphPad Prism (version 6, GraphPad Software Inc., San Diego, CA, USA).
Parts of this study has been presented at the 6th Belgian Symposium on Tissue Engineering, 2018.
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The authors would like to thank Diego De Baere for his technical support in live calcium imaging experiments. We also thank Dr. Ellen Cocquyt and Elke Decrock for their help with TUNEL assay experiments. We thank Chris Vercruysse and Leen Pieters for their assistance with the MTT and mineralization assay. We also thank Dr. Jayaprakash Rajasekharan for the analysis of results with Matlab.
The research was supported by grants from the Fund for Scientific Research –Flanders (Dr. Leybaert, Dr. Elewaut) and Group-ID Multidisciplinary Platform (MRP) of Ghent University (Dr. Elewaut). Dr. Rajasekharan holds a post-doctoral fellowship from the Fund for Scientific Research –Flanders (FWO). Dr. Govindarajan holds a post-doctoral fellowship from the Fund for Scientific Research –Flanders (FWO).
Dr. Martens reports research grants and non-financial support (i.e. cement materials free of charge) from Septodont, Saint-Maur-des-Fossés, France negotiated with the Ghent University. Outside of the submitted work, Dr. Martens and Dr. Rajasekharan report personal fees (honoraria / lecture fees / educational courses). Ms. Rathinam, Dr. Govindarajan, Dr. Declercq, Prof. Elewaut, Dr. De Coster and Prof. Leybaert report no competing interests. All authors assert and confirm that the funders had no role in the design of the study; in the collection, analyses, or interpretation of data; in the writing of the manuscript, or in the decision to publish the results.
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Rathinam, E., Govindarajan, S., Rajasekharan, S. et al. The calcium dynamics of human dental pulp stem cells stimulated with tricalcium silicate-based cements determine their differentiation and mineralization outcome. Sci Rep 11, 645 (2021). https://doi.org/10.1038/s41598-020-80096-5
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