This article is mentioned in:

Introduction

Human mesenchymal stem cells (MSCs) are widely used adult stem cells which have self-renewal potential and multipotent cell differentiation capacity. In particular, human bone marrow-derived mesenchymal stem cells (hBM-MSCs) have been used experimentally in a number of cell therapies and in regenerative medicine due to their abundant and non-tumorigenic properties (1). hBM-MSCs have the ability to differentiate into various types of cells, such as fibroblasts, chondrocytes, adipocytes and osteoblasts (2). In addition, hBM-MSCs play an essential role in the repair of bone (3).

Previous studies have indicated that bone regeneration occurs following an electrical stimulation and leads to bone development (4,5). Based on this knowledge, the effect of electromagnetic fields (EMFs) on osteogenesis has been investigated. Recently, it has been reported that an extremely low frequency of EMF stimulation plays an essential role in the osteogenic differentiation and proliferation of hBM-MSCs. Tsai et al (6) demonstrated that exposure to an extremely low frequency of EMFs (7.5 Hz) played a modulatory role in the osteogenic differentiation of hBM-MSCs, with an increase in alkaline phosphatase (ALP) levels. Sun et al (7) demonstrated that a frequency of 15 Hz EMFs increased the expression of osteogenesis-related genes in hBM-MSCs.

Nanomagnetic particles (MPs) have been widely used in biomedicine. MPs may be applied to apply drug delivery, biological labels and the detection of proteins due to their controllable size and magnetic properties (8). Cartmell et al (9) reported that the mechanical stimulation of primary human osteoblasts by magnetic particle technology affected osteoblastic activity. In the present study, iron oxide (Fe3O4) MPs were encapsulated with a polyethylene glycol (PEG)-phospholipid shell for enhanced biocompatibility.

In the present study, we investigated the effects of EMF exposure and Fe3O4 MP treatment on the osteogenic differentiation of hBM-MSCs. hBM-MSCs were treated with 50 μg/ml of Fe3O4 MPs or exposed to a frequency of 45 Hz at an intensity of 1 mT EMF twice every 8 h per day for 7 days. We also examined whether treatment with Fe3O4 MPs in conjunction with exposure to EMFs is more effective in enhancing osteogenic differentiation. The osteogenic differentiation was analyzed by immunohistochemical staining, western blot analysis, quantitative reverse transcription-polymerase chain reaction (RT-qPCR) and by measuring ALP activity. Lactate dehydrogenase (LDH) activity in the 4 experimental groups was similar; this suggests that treatment did not affect LDH secretion and did not induce damage to the cell membrane.

Materials and methods

Cell culture

hBM-MSCs were purchased from Lonza (Basel, Switzerland) and maintained in culture in Dulbecco’s modified Eagle’s medium (DMEM; Welgene, Daejeon, Korea) supplemented with 10% fetal bovine serum (FBS; Lonza), 1% penicillin/streptomycin (PS; Welgene), 25 μM L-ascorbic acid 2-phosphate (Sigma-Aldrich, St. Louis, MO, USA) in a 37°C incubator in a humidified atmosphere of 5% CO2. The hBM-MSCs were used from passages 4 to 7 with similar results obtained throughout.

Osteogenic differentiation of hBM-MSCs

Osteogenic differentiation medium consisted of DMEM (Welgene) supplemented with 10% fetal bovine serum (FBS; Lonza), 1% penicillin/streptomycin (PS; Welgene), 10 mM β-glycerophosphate (Sigma-Aldrich), 50 μM L-ascorbic acid 2-phosphate (Sigma-Aldrich) and 100 nM dexamethasone (Sigma-Aldrich). The medium was changed every 2–3 days.

Exposure to EMFs

A schematic representation of the sinusoidal EMF device is presented in Fig. 1. The EMF device was placed in a 37°C incubator in a humidified atmosphere of 5% CO2.

Figure 1 Schematic representation of the sinusoidal electromagnetic field device, which was placed in a 5% CO2 and a 37°C incubator.

The stimulation unit is designed to handle a pair of identical coils of 30 cm in diameter assembled in a Helmholtz configuration. The pair of coils operates on alternating current, generating an EMF. The current in the coil is controlled by a generator. The applied magnetic field consisted of 45 Hz frequency and an intensity of 1 mT twice every 8 h per day for 7 days. The cells were seeded into a culture plate or dish.

Preparation and characterization of Fe3O4 MPs

Water- dispersible and biocompatible Fe3O4 MPs were prepared using a method previously described with some modifications (10). The monodispersed Fe3O4 MPs were dispersed in a non-polar organic solvent and synthesized using a high-temperature organic solution phase reaction. Iron (III) acetylacetonate (Fe (acac)3, 2 mmol; 99.9%), 1,2-hexadecanediol (10 mmol; 90%), oleic acid (6 mmol; 99%), oleylamine (6 mmol; 70%) and 1-octadecene (20 ml; 90%) (all from Sigma-Aldrich) were mixed and magnetically stirred under a nitrogen atmosphere. The mixture was heated to 200°C for 2 h and then heated to reflux (~300°C) for an additional hour. The black-colored mixture was cooled down to room temperature. Ethanol (40 ml) was added to the mixture under ambient conditions, and a black material was precipitated and separated via centrifugation (12,000 rpm, 30 min). The black product was redispersed in hexane in the presence of oleic acid (~0.05 ml) and oleylamine (~0.05 ml). Centrifugation (6,000 rpm, 10 min) was applied to remove any undispersed residue. The product was then precipitated with ethanol, centrifuged (10,000 rpm, 20 min) to remove the solvent and redispersed in organic solvents, such as n-hexane and chloroform. The resulting Fe3O4 MPs dispersed in chloroform were encapsulated with a PEG-phospholipid shell to make them biocompatible. Typically, 2 ml of the organic dispersible 12 nm sized Fe3O4 MPs in chloroform (5 mg/ml) was mixed with 1 ml of chloroform solution containing 10 mg 1,2-distearoyl-sn-glycero-3-phosphoethanolamine-N-[methoxy(PEG)-2000] (mPEG-2000 PE) (Avanti Polar Lipids, Inc.) at a ratio of 5:1. After complete evaporation of the chloroform, the residue was incubated at 80°C in a vacuum for 1 h. Five milliliters of water were added, which produced a clear and dark-brown suspension containing PEG-PE micelles. As this suspension contained both empty micelles and micelles containing MPs, the empty micelles were removed by ultracentrifugation. The micelles containing MPs formed a pellet, whereas the empty micelles remained suspended. The supernatant was discarded, and the MP micelles were resuspended in phosphate-buffered saline (PBS). In the present study, 50 μg/ml of Fe3O4 MPs were added to the osteogenic differentiation medium.

Immunohistochemical staining

The cells cultured on the cover slide were fixed for 20 min at 4°C using 10% neutral-buffered formalin and subsequently washed 3 times with PBS (pH 7.2). These cover slides were then incubated with anti-osteocalcin (predilution, AM 386; BioGenex, San Ramon, CA, USA), anti-osteopontin (1:1,000 dilution) and anti-osteonectin (1:500 dilution; AB 1858, Chemicon, Carlsbad, CA, USA) antibodies for 24 h, followed by development using EnVision Plus reagent (Dako, Carpinteria, CA, USA), diaminobenzidine as a chromogen and Mayer’s hematoxylin as a counterstain.

von Kossa staining

The mineralized matrix of the cells was assessed using 5% silver nitrate (Sigma-Aldrich) under ultra-violet light for 60 min, followed by the addition of 3% sodium thiosulphate (Sigma-Aldrich) for 5 min and then counterstaining with Van Gieson (Sigma-Aldrich) for 5 min. With this staining method, the mineral matrix is stained black and the osteoid (unmineralized matrix) is stained red.

RT-qPCR

Total RNA was isolated from the cells using 500 μl TRIzol reagent (Sigma-Aldrich). Subsequently, 100 μl of chloroform were added and the solution was mixed and incubated for 3 min. Following centrifugation (12,000 rpm, 4°C for 15 min), the upper phase was transferred to a new tube and 500 μl of isopropanol were added. After an incubation period of 10 min and another centrifugation step (14,000 rpm, 4°C for 10 min), the supernatant was discarded. The pellet was washed with 1 ml of 70% ethanol and centrifuged (9,500 rpm, 4°C for 5 min). The supernatant was discarded and the pellet was dried. Following the addition of 20 μl of diethylpyrocarbonate (DEPC)-treated water, the pellet was dissolved for 10 min on ice. The amount and purity of total RNA were determined using a nanodrop spectrophotometer (Hankyong National University). Reverse transcriptase (RT) reactions were used to synthesize the cDNA from 1 μg of total RNA using an Advantage RT-for-RCR kit (Clontech Laboratories, Inc., Palo Alto, CA, USA). RT-PCR was routinely performed. The sample was cooled to −20°C and stored until further analysis. For PCR, the primers were purchased from Bioneer Corp. (Deajeon, Korea). The primer sequences used for quantitative PCR are listed in Table I.

Table I Primers used for RT-qPCR.

Table I

Primers used for RT-qPCR.

Genes	Upstream primer sequence	Downstream primer sequence
GAPDH	5′-ACC ACA GTC CAT GCC ATC AC-3′	5′-TCC ACC ACC CTG TTG CTG TA-3′
Collagen I	5′-GAA AAC ATC CCA GCC AAG AA-3′	5′-CAG GTT GCC AGT CTC CTC AT-3′
Collagen III	5′-CAG GTG AAC GTG GAG CTG C-3′	5′-TGC CAC ACG TGT TTC CGT GG-3′
Osteonectin	5′-CCA GAA CCA CCA CTG CAA AC-3′	5′-GGC AGG AAG AGT CGA AGG TC-3′
Osteocalcin	5′-AGG GGA AGA GGA AAG AAG GG-3′	5′-CCA GGC GCT ACC TGT ATC AA-3′
Osteopontin	5′-TCG CAG ACC TGA CAT CCA GT-3′	5′-TCG GAA TGC TCA TTG CTC TC-3′
BMP-2	5′-GTC CAG CTG TAA GAG ACA CC-3′	5′-GTA CTA GCG ACA CCC ACA AC-3′
Runx-2	5′-CTC ACT ACC ACA CCT ACC TG-3′	5′-TCA ATA TGG TCG CCA AAC AGA TTC-3′
BSP	5′-CAC AGC CTC ATC TTC ATG G-3′	5′-GCA TCT CAT AGT GCA TCT GG-3′
CACNA1C	5′-ACA GTG ACC AGT GTG GTG GA-3′	5′-CGT AGC CTC TGG AGA ACC TG-3′
CACNA1E	5′-GTT CGG CCG CGA TCA CCT TTG T-3′	5′-GGC GGC CAA TCG ATG AGC TTC T-3′
CACNA1G	5′-CGG CAA CTAC GTG CTC TTC A-3′	5′-GTG ACT TCA TCT CGT GGG CC-3′
CACNA1I	5′-CGT TGT CAT AGC GAC CCA GTT-3′	5′-CAC AGC TCT CTT CCC CGA GTG A-3′

[i] BMP-2, bone morphogenic protein-2; Runx-2, runt-related transcription factor-2; BSP, bone sialoprotein; CACNA1C, alpha 1C subunit of the L-type voltage-gated calcium channel; CACNA1E, alpha 1E subunit of the R type voltage-dependent calcium channel; CACNA1G, alpha 1G subunit of the T-type voltage-dependent calcium channel; CACNA1I, alpha 1I subunit of T-type voltage-dependent calcium channel.

Western blot analysis

After 10 days of cell culture, the cells were lysed with RIPA buffer containing 50 mM Tris-HCl, pH 8.0, 150 mM NaCl, 1% NP-40, 0.5% sodium deoxycholate, 0.1% SDS (Sigma-Aldrich), protease inhibitors (Complete™; Roche Diagnostics, Mannheim, Germany). Protein (30 μg) was then separated by SDS-polyacrylamide gel electrophoresis and blotted onto nitrocellulose membranes, which were then blocked with 5% skim milk in phosphate-buffered saline (PBS) containing 0.2% Tween-20. Western blot analysis was performed according to the manufacturer’s instructions (Abcam, Cambridge, MA, USA) with the following primary antibodies: anti-bone sialoprotein (BSP, ab52128; Abcam), anti-bone morphogenetic protein 2 (BMP-2, ab17885; Abcam), anti-osteopontin (ab63856; Abcam), anti-osteonectin (ab14174; Abcam), anti-phosphorylated extracellular signal-regulated kinase (p-ERK, #9101; Cell Signaling Technology, Danvers, MA, USA) and anti-actin (ab3280; Abcam). The blots were incubated with the primary antibodies at a dilution of 1:5,000 and then further incubated with horseradish peroxidase-conjugated secondary antibody (#7076; Cell Signaling Technology).

Cell surface antigen analysis by fluorescence-activated cell sorting (FACS)

Antibodies against the human antigens, CD73 and CD90, were purchased from BD Biosciences (San Jose, CA, USA) and the antibody against CD105 was purchased from Ancell Corp. (Bayport, MN, USA). A total of 5×105 cells were resuspended in 200 μl of PBS and incubated with fluorescein isothiocyanate (FITC)- or phycoerythrin (PE)-conjugated antibodies for 20 min at room temperature (or for 45 min at 4°C). The fluorescence intensity of the cells was evaluated using a flow cytometer (FACScan; BD Biosciences), and the data were analyzed using CellQuest software (BD Biosciences).

Proliferation and activity assay of hBM-MSCs

Cell proliferation and activity were measured using a cell counter (Scepter™; Millipore Corp., Billerica, MA, USA) and a 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyl tetrazolium bromide (MTT; Sigma) assay. For the MTT assay, the cells were cultured in a 6-well plate, and each well was supplemented with MTT (3 mg/ml) (n=4). The plates were then incubated in the dark at 37°C in an atmosphere containing 5% CO2 for 2 h and the supernatant was aspirated. Dimethylsulfoxide (DMSO) was added and the 6-well plate was shaken slowly for 5 min. The absorption was measured at 570 nm.

LDH assay

LDH activity was measured using an LDH-LQ kit (Asan Pharmaceutical Inc., Seoul, Korea). Briefly, after 7 days of culture, 20-μl aliquots of medium and 50-μl of working solution were mixed and incubated in the dark at room temperature for 30 min. The reaction was terminated by the addition of stop solution (1 N HCl) and the absorbance was measured at 570 nm.

ALP assay

ALP deposition was measured using a SensoLyte® pNPP Alkaline Phosphatase Assay kit (AnaSpec Inc., Fremont, CA, USA). Following sample preparation, the samples were mixed with pNPP substrate solution. The mixtures were incubated for 30–60 min and stop solution was added. The amount of ALP was quantified by ELISA at 405 nm.

Results and Discussion

Morphology and characterization of hBM-MSCs

The hBM-MSCs were cultured in osteogenic differentiation medium and were treated with MPs or exposed to EMFs over a period of 7 days. The morphology of the hBM-MSCs during osteogenesis under the different experimental conditions [control (no treatment), MP incorporation, EMF exposure, MP incorporation and exposure to EMF] is shown in Fig. 2. No morphological changes or necrosis of the hBM-MSCs were observed following the induction of osteogenic differentiation (Fig. 2). Therefore, MP incorporation, EMF exposure and MP incorporation in conjunction with exposure to EMF did not induce any cytotoxic effects.

Figure 2 Morphology of the hBM-MSCs following the induction of osteogenic differentiation. Cells cultured in (A) osteogenic differentiation medium, with (B) magnetic nanoparticle (MP) incorporatiohn, (C) exposure to electronic magnetic fields (EMFs) and (D) MP incorporation and exposure to EMFs (MP +EMF ) for 7 days. Original magnification, ×100.

Immunohistochemical staining

To evaluate the protein expression levels of osteogenic markers and mineralization, immunohistochemical staining was performed. Osteocalcin protein is specifically synthesized by osteoblasts and is a marker of osteoblast differentiation during the later stages of bone formation (11). Osteonectin is a glycoprotein in the bones which binds sodium. It is secreted by osteoblasts during bone formation, initiating mineralization and promoting mineral crystal formation (12). Osteopontin is a highly phosphorylated sialoprotein, which is a prominent component of the mineralized extracellular matrices of bones (13). The osteogenic markers (osteocalcin, osteopontin and osteonectin) were strongly expressed in the cells treated with MPs, in those exposed to EMFs and in the cells treated with MPs and exposed to EMFs compared to the control group (Fig. 3A–L). The results from immunohistochemical staining of the expression levels of the osteogenic markers are presented in Table II.

Figure 3 Immunocytochemical and von Kossa staining of the BM-MSCs following the induction of osteogenic differentiation for 7 days. (A–D) Ostoecalcin; (E–H) osteonectin; (I–L) osteopontin; and (M–P) von Kossa staining.

Table II Staining results of the osteogenic markers.

Table II

Staining results of the osteogenic markers.

	Control	MP	EMF	MP + EMF
Osteocalcin	−	+	++	++
Osteonectin	+	++	+++	+++
Osteopontin	+	+++	++	+++
von Kossa	−	++	+	++

[i] −, no or weak staining; +, low intensity; ++, moderate intensity; and +++, strong intensity.

von Kossa staining is widely used to quantify mineralization (14–16). It is generally believed that, in von Kossa’s technique, silver cations react with phosphates and carbonates in calcium deposits (17). We used von Kossa staining for the investigation of the mineralization of hBM-MSCs during osteogenesis (Fig. 3M–P). The untreated hBM-MSCs (control) or those exposed to EMFs growing in osteogenic medium exhibited a small amount of matrix mineralization; however, the hBM-MSCs treated with MPs and those treated with MPs and exposed to EMFs exhibited a stronger matrix mineralization compared to the untreated controls on day 7. The amount of mineralization in each treatment group is shown in Table II.

RT-qPCR

The mRNA expression levels of osteogenesis-related genes from the hBM-MSCs following the induction of osteogenic differentiation for 3 days is shown in Fig. 4A. The osteoblast markers, osteocalcin, osteopontin and osteonectin were highly expressed in the hBM-MSCs treated with MPs and exposed to EMFs. We also examined the expression levels of major bone matrix protein genes, such as collagen I, collagen III, BMP-2 and BSP. BMP-2 induces osteoblastic differentiation by acting directly on MSCs and is clinically used to induce bone formation although high doses are required (18). BSP is a highly post-translationally modified acidic phosphorus protein normally expressed in mineralized tissue, such as bone and dentin (19). The representative osteogenesis-related genes were highly expressed in the hBM-MSCs treated with MPs, those exposed to EMFs and in those treated with MPs and exposed to EMFs. The results of our experiments indicated that the expression levels of BSP, OPN, OCN, and collagen I were significantly increased in the EMF with MP exposure group. Osteogenic gene expression can be used as an early index during osteogenesis. BSP is a late stage marker of osteoblast differentiation and an early stage marker of matrix mineralization. OPN is expressed throughout matrix maturation, followed first by BSP and finally by OCN, which characterizes the post-proliferate phase. The OCN protein is specifically synthesized by osteoblasts and is a marker of osteoblast differentiation during the later stages of bone formation. Collagen I is the most abundant protein in the bone matrix and is an early marker of osteoblastic differentiation and the major organic component of the mineralized bone matrix. Additionally, the mRNA expression of the transcription factor Runx-2 was measured by RT-qPCR. Runx-2 is involved in the production of bone matrix proteins as it is able to upregulate the expression of major bone matrix protein genes leading to an increase in immature osteoblasts from pluripotent stem cells; the immature osteoblasts form immature bone (20–25). Runx-2 was strongly expressed in the hBM-MSCs treated with MPs, those exposed to EMFs and in those treated with MPs and exposed to EMFs compared to the untreated control.

Figure 4 Determinatino of gene expression levels by RT-qPCR in the hBM-MSCs following the induction of osteogenic differentiation for 3 days. Electrophoretic RT-qPCR analysis of (A) osteogenesis-related genes and (B) calcium channel-related genes.

Recent studies have suggested that calcium activation affects bone formation. Klar et al (26) reported that the spontaneous induction of bone formation is initiated by a local peak of calcium-activating stem cell differentiation and the induction of bone formation. Moreover, Wen et al (27) mentioned that the inhibition of the L-type voltage-dependent calcium channel (VDCCL) downregulates the proliferation and osteogenic differentiation of rat MSCs (rMSCs), but promotes apoptosis. These results suggest that VDCCL plays a crucial role in the proliferation and osteogenic differentiation of rMSCs. Based on this knowledge, we investigated the effects of MPs and EMF exposure on the expression of calcium channel-related genes in the hBM MSCs during osteogenesis. After 3 days of osteogenesis and treatment with MPs and EMF exposure, the mRNA expression levels of CACNA1C and CACNA1I in the cells treated with MPs, those exposed to EMFs and in those treated with MPs and exposed to EMFs were slightly higher compared to the control group (Fig. 4B). In addition, the expression levels of CACNA1E and CACNA1G were significantly higher in the cells treated with MPs and exposed to EMFs (Fig. 4B). This suggested that the hBM-MSC calcium channel was activated during osteogenic differentiation.

Western blot analysis

To examine osteogenic differentiation, osteogenesis-related proteins were detected by western blot analysis at day 7 of induction. As shown in Fig. 5, the expression levels of osteogenesis-related proteins (BSP, BMP-2, osteopontin and osteonectin) were increased in the cells treated with MPs, those exposed to EMFs and in those treated with MPs and exposed to EMFs compared to the control group.

Figure 5 Western blot analysis of hBM-MSCs following the induction of osteogenic differentiation for 7 days. Whole cell lysates were immunoblotted with antibody of osteogenesis-related proteins (bone sialoprotein, BMP-2, osteopontin, osteonectin), p-ERK and β-actin.

To examine the potential p-ERK activation during osteogenesis, western blot analysis was performed. Several studies have reported that p-ERK activation is an essential mediator of growth factor-induced cell proliferation and differentiation in various cell types, including osteoblasts (28–31). Kapur et al (32) demonstrated that the activation of ERK1/2 by mechanical stimuli is involved in collagen synthesis and osteopontin production. In the present study, after 7 days of osteogenesis with MP incorporation and EMF exposure, the expression of p-ERK was increased and it was highly expressed in the cells treated with MPs and exposed to EMFs (Fig. 5).

FACS analysis

Several antigens are known as MSC surface markers. The antibodies against CD73 (membrane-bound ecto-5′-nucleotisidase), CD90 (Thy-1), CD105 (endoglin) have been reported to react with undifferentiated MSCs (33–35).

To investigate whether MP incorporation and exposure to EMFs affects hBM-MSC differentiation, FACS analysis was performed for the hBM-MSC markers, CD73, CD90 and CD105 (Fig. 6). The expression level of CD73 was 91% in the control group, 76% in the MP incorporation group, 88% in the EMF-exposed group and 77% in the MP incorporation with exposure to EMF group after 7 days. The expression level of CD90 was 100% in the control group, 94% in the MP incorporation group, 96% in the EMF-exposed group and 77% in the MP incorporation with exposure to EMF group. The expression of CD105 was 95% in the control group, 80% in the MP incorporation group, 92% in the EMF-exposed group and 77% in the MP incorporation with exposure to EMF group. The expression levels of hBM-MSC surface antigens were decreased in the cells treated with MPs, those exposed to EMFs and in those treated with MPs and exposed to EMFs compared to the control group. In conclusion, our data indicate that MP incorporation and EMF exposure alter MSC surface antigen expression, suggesting that the hBM-MSCs differentiate into a specific cell type, thus changing their cell fate.

Figure 6 Fluorescence-activated cell sorting (FACS) analysis of hBM-MSC surface markers following the induction of osteogenic differentiation for 7 days.

Cell proliferation and activity assay

The cell number was determined to be approximately 3.4×105 cells in the control group, 3.7×105 cells in the MP incorporation group, 3.1×105 cells in the EMF-exposed group and 3.9×105 cells in the MP incorporation with exposure to EMF group after 7 days (Fig. 7A).

Figure 7 Effect of magnetic nanoparticle (MPs) and electronic magnetic fields (EMFs) on the proliferation of hBM-MSCs during osteogenic differentiation. (A) hBM-MSCs were cultured for 7 days, and their proliferation was measured by counting cell numbers. (B) MTT assay was performed for the assessment of the viability of hBM-MSCs under the different culture conditions (control, MP, EMF and MP + EMF) after 7 days.

As shown by the cell counting results, the cells treated with MPs and those treated with MPs and exposed to EMFs exhibited slightly accelerated cell growth compared to the control group, while the group exposed to EMFs showed a more decelerated cell growth compared to the control group (Fig. 7A).

In addition, cell viability and toxicity to hBM-MSCs were measured by MTT assay 7 days after osteogenesis. MTT assay provides valuable information as to the potential cell viability and cytotoxic effects. Although the cell numbers were decreased following exposure to EMFs and increased following treatment with MPs and treatment with MPs in conjunction with EMF exposure, the cell mitochondrial activity of the 4 experimental groups was similar (Fig. 7B). Morevoer, these results demonstrated that no cytotoxic effects were detected in the hBM-MSCs treated with MPs and in those exposed to EMFs during osteogenesis.

LDH and ALP activity

LDH is a cytoplasmic catalytic enzyme related to the reversible conversion between pyruvic and lactic acid. LDH is released through the cell membrane when it is damaged (36). Therefore, less LDH release means less cellular damage. Thus, the media were collected and analyzed after 7 days in order to examine cellular damage.

In the cells treated with MPs and in those treated with MPs and exposed to EMFs there was a decrease in LDH secretion (Fig. 8A). The LDH activity of the 4 experimental groups was similar, which suggests that treatment with MPs and exposrue to EMFs did not affect LDH secretion and did not induce damage to the cell membrane.

Figure 8 Effect of different culture conditions on cytotoxicity and alkaline phosphatase (ALP) activity of hBM-MSCs during osteogenic differentiation for 7 days. (A) Cytotoxicity was measured by a lactate dehydrogenase (LDH) assay kit. (B) ALP assay was performed for the determination of ALP activity. (*P<0.05, **P<0.05).

ALP is an early mineralization-related protein marker for the osteogenesis of osteoblasts (37). The effects of MP incorporation and exposure to EMFs on cellular ALP activity during osteogenesis were examined by measuring the ALP reaction products in the untreated cells (control), the cells treated with MPs, those exposed to EMFs, and in those treated with MPs and exposed to EMFs over time. Several ALP-positive cells were observed in the cells exposed to EMFs and in those treated with MPs and exposed to EMFs (Fig. 8B). These results suggest that MP incorporation in conjunction with exposure to EMFs increases ALP activity in hBM-MSCs during osteogenesis.

In conclusion, in the present study, the effects of treatment with MPs in conjunction with exposure to EMFs on cell differentiation were investigated. We treated hBM-MSCs with 50 μg/ml of Fe3O4 MPs or exposed them to a frequency of 45 Hz and an intensity of 1 mT EMF twice every 8 h per day for 7 days. No morphological changes and no cytotoxic effects were observed during osteogenesis. The expression of osteogenic markers was detected by immunohistochemical staining, RT-qPCR and western blot analysis, demonstrating an increase in expression. FACS analysis indicated that treatment with MPs and EMF exposure reduced the expression of MSC surface markers; this suggests the possibility of hBM-MSC differentiation. The mineralization of hBM-MSCs in the MP incorporation group or EMF-exposed group was observed by ALP assay. Taken together, these results suggest that the treatment of hBM-MSCs with MP or their exposure to EMFs increases osteogenic differentiation, and that MP incorporation in conjunction with EMF exposure is more effective in enhancing osteogenic differentiation. The results of our study demonstrate that MPs may be potentially used for medical instruments or scaffold materials, and that EMFs can be used for the rehabilitation of osteogenic wounds.

Acknowledgements

The present study was supported by the Pioneer Research Center Program through the National Research Foundation of Korea funded by the Ministry of Science, ICT and Future Planning, Republic of Korea (grant number 2009-0082941).

References