Many studies have reported that an electromagnetic field can promote osteogenic differentiation of mesenchymal stem cells. However, experimental results have differed depending on the experimental and environmental conditions. Optimization of electromagnetic field conditions in a single, identified system can compensate for these differences. Here we demonstrated that specific electromagnetic field conditions (that is, frequency and magnetic flux density) significantly regulate osteogenic differentiation of adipose-derived stem cells (ASCs) in vitro. Before inducing osteogenic differentiation, we determined ASC stemness and confirmed that the electromagnetic field was uniform at the solenoid coil center. Then, we selected positive (30/45 Hz, 1 mT) and negative (7.5 Hz, 1 mT) osteogenic differentiation conditions by quantifying alkaline phosphate (ALP) mRNA expression. Osteogenic marker (for example, runt-related transcription factor 2) expression was higher in the 30/45 Hz condition and lower in the 7.5 Hz condition as compared with the nonstimulated group. Both positive and negative regulation of ALP activity and mineralized nodule formation supported these responses. Our data indicate that the effects of the electromagnetic fields on osteogenic differentiation differ depending on the electromagnetic field conditions. This study provides a framework for future work on controlling stem cell differentiation.
Low-frequency, low-energy, electromagnetic fields are commonly used to promote bone fracture healing.1, 2 These electromagnetic fields enhance osteogenesis, decrease osteoporosis3, 4, 5, 6 and regulate diverse osteoblastic responses for osteogenesis in vitro. DNA synthesis can also be enhanced by electromagnetic fields.7, 8 In addition, electromagnetic fields increase osteogenic marker gene expression during differentiation9 and affect calcified matrix production during mineralization.10
Two parameters primarily characterize electromagnetic field properties: frequency and magnetic flux density. The magnetic flux density used in most previous studies to induce osteogenesis varied from 0.1 to 3 mT.6, 8, 9, 11, 12, 13 Such studies have shown that a low-frequency electromagnetic field is more effective than a static field in causing biological effects.14, 15 Frequencies used for osteogenesis varied from 7.5 to 75 Hz.5, 6, 7, 8, 11, 16, 17 Unlike bio-mimetic stimuli (for example, cyclic strain and shear stress), this time-varying electromagnetic field does not have logical cues for each stimulation parameter. Thus, studies aimed at identifying optimal parameters, at least within the ranges of previous investigations, are required.
Previous studies on osteogenesis using electromagnetic fields have been performed under various conditions,1, 2, 4, 5, 6, 7, 8, 9, 10, 12, 13, 15, 16, 17 and the results have differed depending on the experimental and environmental conditions. These differences may be attributable to different experimental systems. Moreover, authors have rarely discussed why they selected specific conditions for stimulating cells in their studies. Therefore, these conditions should be optimized in a single, identified system where the experimental and environmental conditions are fixed.
We examined the effects of various electromagnetic field conditions on the osteogenic differentiation of mesenchymal stem cells. We used adipose-derived stem cells (ASCs) because ASCs easily attach to surfaces and proliferate rapidly.18 In addition, ASCs can be derived from fat tissue, which afforded us an abundant source of cells. ASCs also have osteogenic potential, among various differentiation lineages,18, 19, 20, 21, 22 and are known to play a role in bone regeneration, including the acceleration of bone fracture healing23, 24 and promotion of bone regeneration in cases of calvarial defects without chemical induction.19
Here, we observed the effects of an electromagnetic field under various conditions on osteogenic differentiation of ASCs. A fixed electromagnetic field distribution was used to provide uniform field effects on cells. Among various combinations of frequency and magnetic flux density, we selected and investigated specific conditions that had positive (30–45 Hz, 1 mT) or negative (7.5 Hz, 1 mT) effects on ASC differentiation.
Materials and methods
This study was approved by the Institutional Review Board of Seoul St Mary’s Hospital and conformed to the principles expressed in the Declaration of Helsinki. All patients provided written informed consent for the collection of cells and subsequent analysis.
Isolation, culture and characterization of ASCs
ASCs were isolated and cultured as previously described.25 The isolated ASCs were cultured in Dulbecco’s modified Eagle’s medium (Gibco BRL, Grand Island, NY, USA) containing 10% (v/v) fetal bovine serum (Gibco BRL), 100 U ml−1 penicillin and 100 μg ml−1 streptomycin (Gibco BRL) at 37 °C in a humidified atmosphere containing 5% CO2. All experiments were performed at passage three. To induce osteogenic differentiation, the culture medium was changed to osteogenic induction medium (OM) containing 10 nM dexamethasone (Sigma-Aldrich, St Louis, MO, USA), 10 mM β-glycerol phosphate (Sigma-Aldrich) and 50 μg ml−1 ascorbic acid-2-phosphate (Sigma-Aldrich).
For flow cytometry, cells were harvested with trypsin/EDTA and washed in 1% bovine serum albumin (Pierce, Rockford, IL, USA). Cells were then incubated with fluorescently labeled monoclonal antibodies against CD13, CD29, CD34, CD45, CD90 and CD105 (Serotec, Oxford, UK) for 30 min at 4 °C and analyzed using a flow cytometer (Becton Dickinson, Mountain View, CA, USA).
Exposure of ASCs to the electromagnetic field
A solenoid coil was used because it could generate a uniform electromagnetic field. A custom-made solenoid coil had the wire wound 7300 times and the DC resistance was 450 Ω for 10 mT. The inner diameter and length were 180 and 400 mm, respectively. We used 3-axis magnetic field sensors (MFS-3A, Ametes, San Carlos, CA, USA) to measure the magnetic flux density inside the coil. The 24-well plates were used with a cell density of 2 × 104 cells per well. Cells were exposed to the electromagnetic field for 8 h per day in a humidified incubator at 37 °C under a 5% CO2 atmosphere. All experiments were conducted in the conditions without heat generation.
Total RNA (1 μg) extracted from cultured cells at day 7 using TRIzol reagent (Invitrogen, Groningen, The Netherlands) was used as a template for complementary DNA synthesis (Invitrogen, Eugene, OR, USA). Real-time PCR was performed using the SYBR Green PCR Master Mix assay (Applied Biosystems, Warrington, UK) and the ABI StepOnePlus system (Applied Biosystems, Foster City, CA, USA). The amplification reaction consisted of 40 cycles of 95 °C for 10 min, 95 °C for 15 s and 60 °C for 1 min. The following primers were used: GAPDH sense, 5′-IndexTermCCAGGTGGTCTCCTCTGACTTC-3′; GAPDH antisense, 5′-IndexTermGTGGTCGTTGAGGGCAATG-3′; alkaline phosphatase (ALP) sense, 5′-IndexTermATGTCATCATGTTCCTGGGAGAT-3′; ALP antisense, 5′-IndexTermTGGAGCTGACCCTTGAGGAT-3′; collagen type-I, α1 (COL-I) sense, 5′- IndexTermCAAGACAGTGATTGAATACAAAACCA-3′; COL-I antisense, 5′- IndexTermACGTCGAAGCCGAATTCCT-3′; osteocalcin (OC) sense, 5′- IndexTermAAGAGACCCAGGCGCTACCT-3′; OC antisense, 5′- IndexTermAACTCGTCACAGTCCGGATTG-3′; osterix (OSX) sense, 5′- IndexTermGGCAGCGTGCAGCAAATT-3′; OSX antisense, 5′- IndexTermCCTGCTTTGCCCAGAGTTGT-3′; runt-related transcription factor 2 (RUNX2) sense, 5′- IndexTermAACCCACGAATGCACTATCCA-3′; RUNX2 antisense, 5′- IndexTermCGGACATACCGAGGGACATG-3′. Gene expression levels of all experimental groups were expressed as fold changes relative to levels of the control group.
ALP activity and staining
After culture for 10 days, cells were washed three times with phosphate-buffered saline and then lysed in lysis buffer (RIPA buffer, Upstate, Temecula, CA, USA). Cell lysates were incubated with p-nitrophenyl phosphate (Sigma-Aldrich) at 37 °C for 30 min. The reaction was stopped by adding 2 N NaOH. Absorbances were measured at 405 nm using a microplate reader. ALP activity was normalized to the total protein content of each sample. Protein contents were measured using a BCA protein assay kit (Pierce). For ALP staining, cells were fixed with 4% paraformaldehyde (Wako Pure Chemical, Osaka, Japan). ALP was then stained using a solution containing 0.01% Naphthol AS-MX phosphate and 0.05% Fast Red Violet LB Salt (Sigma-Aldrich). Fixed cells were incubated with substrate solution at room temperature for 30 min.
Measurement of mineralization
Alizarin Red S was used to detect mineralization. Cells were fixed by incubation with 4% paraformaldehyde for 30 min at day 20. Samples were then immersed in Alizarin Red S solution at room temperature for 30 min. After washing, stained cells were observed under an optical microscope.
For quantitative calcium measurement, cells were decalcified in 0.6 N HCL at day 20 followed by shaking for 24 h at room temperature. Then, their calcium content was measured using a QuantiChrom Calcium Assay kit (BioAssay Systems, Hayward, CA, USA), as previously reported.26 Briefly, 5 μl of lysate was mixed with 200 μl of working solution from the kit and incubated for 20 min. Absorbances were measured at 612 nm using a microplate reader.
After culture with OM for 4 days, cells were fixed with 4% paraformaldehyde for 30 min, permeabilized with 0.1% Triton X-100 and blocked with 0.2% bovine serum albumin for 15 min. They were then incubated with anti-RUNX2 (Santa Cruz, Heidelberg, Germany) (primary antibody). After washing with phosphate-buffered saline, secondary antibody (Alexa 488 anti-rabbit, diluted 1:200) was added and incubated for 1 h at room temperature. Samples were mounted with antifade reagent (Invitrogen) and observed using a FluoView 1000 confocal microscope (Olympus, Melville, NY, USA). All images were captured without changing the camera settings.
All experiments were performed in triplicate. Data are presented as the mean±s.d. Statistical significance was determined by a one-way analysis of variance (n=3). Differences were considered to be statistically significant at *(or #) P<0.05.
Electromagnetic field identification
Before evaluating the effects of the electromagnetic field on ASCs, we characterized the electromagnetic field generated by the solenoid coil (Figure 1a). The magnetic flux density was predicted using three-dimensional finite element analysis before development of the coil. The distribution of the magnetic flux density in the cross-section of the coil was described in Figure 1b when we set the magnetic flux density to 1 mT. The magnetic flux density varied throughout the cross-section and was highest at the center along the y axis (axial direction). In contrast, it decreased from both sides (walls) to the center point along the x axis (radial direction).
The magnetic flux density inside the solenoid coil was measured using a three-axis sensor. As described in Figure 1c, the sinusoidal magnetic flux density generated by the coil was controllable. All measured data along the cross-section of the solenoid coil when it was set to 1 mT are described in a three-dimensional graph (Figure 1d). The magnetic flux density at the central area along the axial direction was higher than in the other sections.
This measured magnetic flux density corresponded to predicted values from Figure 1b, as shown in Figure 2. These data were predicted and measured under identical conditions when cells were exposed to the electromagnetic field with an average magnetic flux density of 1 mT. We established a nearly uniform area (based on these results) as the experimental section where cells were positioned. This experimental area was at the center along both the axial and radial directions with the dimensions of a commercialized well-plate (128 × 86 mm). The average magnetic flux density in this area had a 5% margin of error.
Before inducing osteogenic differentiation, ASCs were characterized using flow cytometry (Figure 3a). ASCs showed negative expression of hematopoietic markers CD34 and CD45. In contrast, ASCs were positive for the cell adhesion molecules CD29 (integrin β1) and CD90 (Thy-1), the metalloproteinase CD13 (aminopeptidase N) and the receptor molecule CD105 (endoglin).
Next, we evaluated the osteogenic potential of ASCs under both the electromagnetic field and OM (Figure 3b). Both the electromagnetic field (electromagnetic field-normal growth medium (NM)) and OM (Control-OM) increased ALP expression and matrix mineralization as compared with the control-NM group. ALP was most strongly activated and mineralized nodules were most heavily formed if ASCs were treated with both the electromagnetic field and OM simultaneously.
Relative ALP expression was evaluated using real-time PCR for condition optimization. The magnetic flux density varied from 0.1 to 3 mT, and the frequency ranged from 7.5 to 75 Hz. All groups were composed of subgroups (that is, NM; Figure 4a and OM; Figure 4b) to evaluate the synergistic effects of the induction medium and electromagnetic field. ALP expression increased in the frequency range of 30 to 50 Hz and a magnetic flux density of 0.8 to 2.4 mT. The area in red represents the most highly expressed conditions. Frequencies and magnetic flux densities outside of these ranges made no change of ALP expression (blue and violet colors). As shown in Figure 4b, 30 and 45 Hz (1 mT) increased ALP expression. In contrast, ALP expression was not increased (compared with the control treated with OM; 2.38) at 7.5 Hz (1 and 2 mT). Overall, we selected three groups to further examine osteogenic differentiation of ASCs; namely, two groups with increased ALP expression (30 Hz (1 mT), 45 Hz (1 mT)) and one with decreased ALP expression (7.5 Hz (1 mT)).
Confirmation of the selected conditions
We measured RUNX2 expression using immunostaining to compare positive and negative groups with the control group (Figure 5). RUNX2 expression was increased by OM, as shown in the control group. At 45 Hz, the electromagnetic field strongly induced RUNX2 expression compared with the other groups. At 30 Hz, the electromagnetic field also increased RUNX2 expression compared with the control group. However, RUNX2 expression was reduced compared with the control groups when cells were exposed to a 7.5-Hz electromagnetic field.
We checked RUNX2, COL-I, OSX and OC expression levels using real-time PCR (Figure 6). Expression levels of all genes were increased under the electromagnetic field at 30 and 45 Hz compared with the control groups. RUNX2 and COL-I levels at 30 Hz were higher than those at 45 Hz, whereas OSX and OC levels at 30 Hz were lower than those at 45 Hz. Genes were upregulated by the electromagnetic field at both 30 and 45 Hz even without OM. Gene expression was not significantly increased at 7.5 Hz compared with the control with NM.
To evaluate the positive and negative effects of the electromagnetic field on the osteogenic differentiation we measured ALP activity (Figure 7a). We found that OM increased ALP activity compared with NM groups, regardless of the electromagnetic field. The ALP activity was higher in the 30/45 Hz groups when ASCs were treated with both NM and OM as compared with the control group cultured with identical medium. The activity levels of the 30/45 Hz groups with NM were lower than the control with OM. In contrast, lower ALP activity was detected at 7.5 Hz as compared with the control group. Although ASCs were treated with OM, the ALP activity at 7.5 Hz was lower than the control group treated with NM. Matrix production of differentiated osteoblasts was evaluated using a calcium content assay (Figure 7b). Similar to ALP activity, increased amounts of mineralized nodules were detected when ASCs were exposed to 30/45 Hz electromagnetic fields compared with the control group. The calcium levels of the 7.5 Hz electromagnetic field were lower than the control group. These results suggest that the 30/45 Hz electromagnetic fields stimulated ASC osteogenic differentiation, whereas the 7.5 Hz electromagnetic field inhibited ASC osteogenic differentiation.
Here, we demonstrated that osteogenic differentiation of ASCs could be regulated by controlling the conditions of an electromagnetic field in vitro. After characterizing the electromagnetic field generated by a solenoid coil, we verified the effects of both positive and negative conditions of the electromagnetic field on osteogenic differentiation of ASCs based on screening results using real-time PCR.
Before screening conditions, it was important to establish the experimental ranges of each parameter based on an osteogenesis literature review.1, 2, 4, 5, 6, 7, 8, 9, 10, 12, 13, 15, 16, 17 Panagopoulos et al.14 proposed the use of a weak electromagnetic field with low frequency based on a biophysical model for the action of oscillating magnetic fields on cells. Additionally, it is known that an electromagnetic field with a frequency below 100 Hz induces physiological effects as a result of ionic interactions.27, 28 Thus, based on this information and other previous studies, we established the experimental ranges of the two parameters.
To provide a uniform stimulus to the cells, we first characterized the generated stimulus before evaluating its effects on cells. We estimated the uniform magnetic flux density area of the solenoid coil using finite element analysis to determine dimensions of the solenoid coil with an effective stimulation area. The central area of the coil was reasonably uniform, which is the location of the commercial well plate. Based on these results, an electromagnetic field generator was developed, as described in Figure 1a. When the electromagnetic field was generated inside the solenoid coil, the distributions of the measured data were in good agreement with the estimated values (Figure 2). We established the uniform area with a 5% margin of error where cells could be exposed to the uniform electromagnetic field.
Before inducing the osteogenic differentiation of ASCs, we confirmed that the ASCs used in this study had typical properties of mesenchymal stem cells, that is, the ASCs expressed negative hematopoietic markers and positive adhesion/receptor molecules.29, 30, 31 These ASCs were osteogenically differentiated in the presence of permissive induction medium and electromagnetic field treatment, as illustrated in Figure 3b,32 which indicates that the ASCs used in this study had osteogenic potential that can be accelerated using induction medium and electromagnetic field treatment.
Relative ALP mRNA expression was evaluated using real-time PCR on day 7 to optimize conditions for osteogenic differentiation of ASCs. Two parameters, that is, magnetic flux density and frequency, were controlled independently during the electromagnetic field treatment. When ASCs were stimulated with an electromagnetic field (NM), ALP expression levels were dependent on a combination of magnetic flux density and frequency (Figure 4a). In Figure 4b, ALP was significantly upregulated at a magnetic flux density between 1 and 2 mT and a frequency from 30 to 45 Hz. In contrast, the electromagnetic field did not show positive effects on ALP expression at 7.5 Hz, regardless of the medium type. Taken together, we selected 30/45 Hz (1 mT) and 7.5 Hz (1 mT) as positive and negative conditions for osteogenic differentiation of ASCs, respectively.
The effect of the selected three conditions on osteogenic differentiation was evaluated using the gene expression of other osteogenic markers. Similar to ALP, RUNX2 is an important early osteogenic marker.33 Both the 30 and 45 Hz groups had increased RUNX2 expression compared with the nonstimulated group, whereas the electromagnetic field at 7.5 Hz did not increase RUNX2 expression even though cells were treated with OM (Figure 5). Other osteogenic markers were upregulated with the electromagnetic field at both 30 and 45 Hz compared with the nonstimulated (control) group. However, it was difficult to conclude which frequency had stronger potential to osteogenic differentiation (Figure 6).
ALP activity and calcium content results corroborated the RUNX2 expression data. Although the positive conditions of the electromagnetic field generated synergistic effects with OM on ALP activity and mineralization (Figure 7), the individual effects of OM on osteogenic differentiation appear stronger than the electromagnetic field. This synergistic effect with the electromagnetic field can be highly induced by other growth factors such as bone morphogenetic protein 2.16 Without OM, ALP activities and calcium content in the positive groups were not higher than the control with OM.
The 7.5 Hz electromagnetic field seemed to inhibit osteogenic differentiation of ASCs. ALP activity at 7.5 Hz was lower than the control group regardless of the medium type. Calcium content was not increased at this frequency compared with the control groups under the identical medium. Moreover, lower expression levels of other osteogenic markers showed that specific conditions had negative potential to osteogenic differentiation, even though all markers were not inhibited significantly. This inhibitory effect (7.5 Hz) did not seem to be as strong as the positive effect (30/45 Hz). Based on these data, we conclude that osteogenic differentiation of ASCs can be regulated by controlling the electromagnetic conditions.
Previous papers reported that osteogenic activities can be affected by different frequencies such as 15 or 60 Hz.12, 16, 17 Similarly, we observed that the electromagnetic field at these frequencies increased ALP expression (Figure 4b). However, our results suggested that frequencies from 30 to 45 Hz can provide stronger osteogenic effects than either 15 or 60 Hz. This is meaningful because these results were obtained in a single identified system among various conditions to avoid differences caused by experimental and environmental conditions.
Although many questions remain unclear, our study provides a framework for future work to control differentiation lineages of stem cells using biophysical stimulation. Several general mechanisms regarding how electromagnetic fields influence cells have been introduced; analyses suffer from lack of proof on how specific conditions affect osteogenic differentiation.14, 27, 28, 34, 35 We guess that our finding might be related to moving ions with specific frequencies, for example, calcium ions. The ratio of the efflux of Ca2+ through the membrane can be increased at the frequency from 30 to 50 Hz.36 Higher efflux of Ca2+ might influence osteoblastic viability and function because the released ions play a structural role of extracellular matrix formation.36, 37, 38
Treatment using the electromagnetic field could be an auxiliary approach to enhancing cellular activities for tissue regeneration. Stimulation of cells with both electromagnetic field and proper chemical signals will promote the cellular reaction synergistically. Additionally, this inherently noninvasive and noncontact treatment method is easy to be applied to tissue regeneration using three-dimensional scaffolds.39, 40, 41, 42, 43 Exposure of the electromagnetic field to cells on scaffolds with specific electromagnetic conditions will accelerate tissue formation in vitro.
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This work was supported by the National Research Foundation of Korea (NRF) grant funded by the Korea government (MEST) (No. 2012-0001235) and World Class University (WCU) program through the National Research Foundation of Korea funded by the Ministry of Education, Science and Technology (Project No. R31-2008-000-10105-0).
The authors declare no conflict of interest.
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Cite this article
Kang, K., Hong, J., Kang, J. et al. Regulation of osteogenic differentiation of human adipose-derived stem cells by controlling electromagnetic field conditions. Exp Mol Med 45, e6 (2013). https://doi.org/10.1038/emm.2013.11
- adipose-derived stem cells
- electromagnetic field
- magnetic flux density
- osteogenic differentiation
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