Mesenchymal stem cells have the ability to renew and differentiate into various lineages of mesenchymal tissues. We used undifferentiated human mesenchymal-like stem cells from human umbilical cord vein (hUC-MSCs), a cell line which contains several mesenchymal cell markers. We characterized functional ion channels in cultured hUC-MSCs with whole-cell patch clamp and reverse transcription-polymerase chain reaction (RT-PCR). Three types of outward current were found in these cells: the Ca2+-activated K+ channel (IKCa), a transient outward K+ current (Ito), and a delayed rectifier K+ current (IKDR). IKCa and IKDR were totally suppressed by tetraethylammonium, and IKCa was sensitive to a specific blocker, iberiotoxin. Ito was inhibited by 4-aminopyridine. Another type of inward rectifier K+ current (Kir) was also detected in approximately 5% of hUC-MSCs. Elevation of external potassium ion concentration increased the Kir current amplitude and positively shifted its reversal potential. In addition, inward Na+ current (INa) was found in these cells (∼30%); the current was blocked by tetrodotoxin and verapamil. In the RT-PCR analysis, Kv1.1, Kv4.2, Kv1.4, Kir2.1, heag1, MaxiK, hNE-Na, and TWIK-1 were detected. These results suggested that multiple functional ion channel currents, IKCa, IKDR, Ito, INa, and Kir, are expressed in hUC-MSCs.
Disclosure of potential conflicts of interest is found at the end of this article.
Mesenchymal stem cells in blood or tissue can differentiate into several types of cells, including adipocytes, chondrocytes, osteocytes, cardiomyocytes, and neurons [1, , , –5]. For these reasons, MSCs have drawn considerable interest as useful materials for tissue engineering and cell-based therapy.
Human bone marrow has been recognized as one major source of MSCs for both experimental and clinical studies [1, 6, , –9]. However, the number of human bone marrow-derived MSCs (hBM-MSCs) and differential potential significantly decline with age [10, 11], which makes the urgency to search for adequate alternative sources of MSCs for autologous and allogeneic use necessary. Many scientists have also obtained MSCs from other sites in the adult, fetus , amniotic fluid , and BM. A few groups have also succeeded in isolating MSCs from umbilical cord (UC) blood [14, , , , , –20]. Bieback et al. reported that UC blood could be an additional stem cell source for experimental and clinical purposes because MSC-like cells can be isolated at high efficacy from full-term UC blood donations . The group suggested that the success rate of isolating MSCs was only 63% for UC blood. Furthermore, in a more recent report, they noted that UC blood-MSCs could be cultured longest and showed the highest proliferation capacity . However, controversy still exists over whether cord blood is a source for MSCs [21, 22].
Thus, instead of using the cord blood, a potential alternative source of MSCs became possible with the culture of cells from Wharton's jelly, the primitive connective tissue of the human UC . The fibroblast-like cells of human UC could be induced to differentiate into “neural-like” cells . Another technical approach for human UC could be feasible to an autologous cell source of myofibroblasts for cardiovascular tissue engineering [25, , –28]. There are many reports on the ability of human umbilical cord (hUC)-MSCs to differentiate into several cell types of other tissues, including adipocytes, neuronal cells, chondrocytes, and osteocytes [24, –26, 29, –31]. hUC-MSCs could be induced to differentiate into neuron-like cells (approximately 87%) . In particular, dopaminergic neurons transformed from MSCs could be transplanted into the striatum of rats previously induced to have Parkinsonism by unilateral striatal lesioning with 6-hydroxydopamine HCl . These results suggest that hUC-MSCs have the potential for treatment of Parkinson disease. Also, hUC-MSCs can be induced to form cardiomyocytes by treatment with 5′-azacytidine or by culturing them in cardiomyocyte-conditioned medium [33, 34]. Many experimental reports on hUC-MSCs support the possibility that the cells might be a new source of cells for cellular therapies. Namely, hUC-MSCs are more accessible and easier to isolate compared with hBM-MSCs, and the UC can serve as a rich source of MSCs, which may be used in experimental and clinical applications in treating central nervous system diseases and myocardial infarctions.
Ion channels are widely expressed in different types of cells, and they have important roles in maintaining physiological homeostasis in many cells. In the study of stem cells, there is little information about the electrophysiological properties of ion channels of human MSCs (hMSCs), although the channels may have the role as the first intracellular signal for maintaining homeostasis and differentiation [35, , , –39]. K+ channels are found to modulate the progression through the cell cycle in proliferating cells . For therapeutic applications, we therefore have to understand not only morphological and molecular characteristics but also electrophysiological properties of ion channels in hUC-MSCs. Therefore, to begin to address this issue, we studied the population of hUC-MSCs isolated in our laboratory, and we used the whole-cell patch clamp technique to characterize the electrophysiological properties on these hUC-MSCs and reverse transcription-polymerase chain reaction (RT-PCR) to know which ion channel mRNAs are expressed.
Materials and Methods
Isolation and Culture of hUC-MSCs
All parts of this study, especially the isolation of the human UC, were performed according to the Declaration of Helsinki. Ethical approval was obtained from Hanyang University Hospital (Seoul, Korea), and written informed consent was obtained from donors of UC. The isolation and culture of hUC-MSCs (n = 21) were carried out by the method previously described [25, 41]. Briefly, each UC (approximately 5 cm) was collected and processed within 6–12 hours after normal delivery. The cord vein was washed out with phosphate-buffered saline (PBS). The vessel was filled with 0.5% collagenase and incubated for 5 hours at 37°C. After gentle massage of the cord vein, the dissociated cells were collected. The cells were centrifuged for 10 minutes at 1,000 rpm and suspended in Dulbecco's modified Eagle's medium with low glucose (DMEM-LG) supplemented with penicillin-streptomycin and 10% fetal bovine serum (FBS). The cell suspension (approximately 5 × 105 cells) was seeded in 75-cm2 culture flasks. Cultures were maintained at 37°C in a humidified atmosphere containing 5% CO2 with a change of culture medium every other day. hBM-MSCs were purchased from Cambrex (Walkersville, MD, http://www.cambrex.com).
Flow Cytometry Analysis of hUC-MSCs
The cells were analyzed by flow cytometry (FACSCalibur A; BD Biosciences, San Diego, http://www.bdbiosciences.com). To stain the hUC-MSCs, the cells were lifted with trypsin, and the trypsin was inactivated with fresh medium. Approximately 1 × 106 cells were pelleted and resuspended in PBS and fixed with 4% buffered paraformaldehyde for 5 minutes at room temperature (21°C–24°C). For staining, nonspecific binding was blocked with PBS with 2% normal serum for 5 minutes, and then the cells were incubated with primary antibody for 45 minutes at room temperature. The cells were stained with a fluorescent secondary antibody for 30 minutes. Control cells were prepared by incubation with the secondary antibody alone. In each case, the cells were gently pelleted and washed with PBS between each incubation step. For cytoplasmic antigens, the cells were permeabilized with 100% cold methanol for 5 minutes. The following cell-surface epitopes were marked with anti-human antibodies: CD29-fluorescein isothiocyanate (FITC), CD105-FITC, HLA-DR-FITC, CD34-phycoerythrin (PE), CD45-PE (Serotec Ltd., Oxford, U.K., http://www.serotec.com), CD44-FITC, CD31-PE (DakoCytomation, Glostrup, Denmark, http://www.dakocytomation.com), CD73-PE, and CD90-PE (BD Pharmingen, San Diego, http://www.bdbiosciences.com/index_us.shtml). Mouse isotype antibodies (FITC, PE) served as a control (Serotec).
Electrophysiological recording was performed in the whole-cell configuration using a patch clamp amplifier (Axopatch 200B; Axon Instruments/Molecular Devices Corp., Union City, CA, http://www.moleculardevices.com). Borosilicate glass electrodes (1.2-mm outside diameter; Warner Instruments, Hamden, CT, http://www.warneronline.com) were pulled with a vertical pipette puller (model PP-830; Narishige, Tokyo, http://www.narishige.co.jp) and had tip resistances of 2–3 MΩ when filled with pipette solution. The tip potentials were compensated before the pipette touched the cell. After a giga-seal was obtained by negative suction, the cell membrane was ruptured by gentle suction to establish the whole-cell configuration. All recordings were performed at room temperature. The recorded signal was filtered at 2 kHz and transferred to a computer using the Digidata 1322A interface (Axon Instruments). Acquired whole cell current data were analyzed with the pCLAMP program (version 9.02; Axon Instruments).
Initially, we tried to record currents of hUC-MSCs attached to glass coverslips. However, electrophysiological recording was not feasible under these conditions. We therefore detached subconfluent hUC-MSCs from small culture flasks using trypsin-EDTA. After centrifugation at 1,000 rpm for 5 minutes, cells were recovered in culture medium. For electrophysiological recordings, the cells were transferred to a small chamber and allowed to attach to the glass bottom for 15 minutes. The suspension was stored at room temperature and used within 6 hours.
The normal Tyrode solution contained 143 mM NaCl, 5.4 mM KCl, 0.5 mM MgCl2, 1.8 mM CaCl2, 0.5 mM NaH2PO4, 10 mM glucose, and 5 mM HEPES; the pH was adjusted to 7.4 with NaOH. The pipette solution contained 150 mM KCl, 1.0 mM MgCl2, 10 mM HEPES, 5.0 mM EGTA, 2.0 mM Mg-ATP; the pH was adjusted to 7.2 with KOH. External solution was replaced by equimolar N-methyl-d-glucamine (NMDG+) when Na+-free conditions were applied for test of Na+ current (INa).
Cell Culture Media, Plastics, and Chemicals
DMEM-LG, PBS, penicillin-streptomycin, trypsin-EDTA, FBS, and collagenase were obtained from Invitrogen (Carlsbad, CA, http://www.invitrogen.com). Verapamil, 4-aminopyridine (4-AP), and tetraethylammonium (TEA) were ordered from Sigma-Aldrich (St. Louis, http://www.sigmaaldrich.com), and tetrodotoxin (TTX) and iberiotoxin were from Tocris (Ellisville, MO, http://www.tocris.com).
Reverse Transcription-Polymerase Chain Reaction
Total RNA in the hUC-MSCs (after the fourth passage) was extracted using TRIzol (Invitrogen). The RNAs from hUC-MSCs were reverse transcribed to cDNA with SuperScript reverse transcriptase (Invitrogen). We resuspended 1 μg of total RNA in 25 mM deoxynucleotide triphosphate (dNTP), 1 μl of oligo(dT) (0.5 μg/ml), and 3 μl of diethylpyrocarbonate-treated water, and the suspension was subsequently heated to 65°C for 5 minutes. After cooling to 4°C, that solution was added to a mixture of 4 μl of 5X First-Strand Buffer, 2 μl of 0.1 M dithiothreitol, and 1 μl of RNase inhibitor and incubated at 42°C for 2 minutes. Then, 1 μl of SuperScript (50 units/μl) was added to the RNA solution. This was followed by incubation at 42°C for 50 minutes. Each cDNA was subjected to polymerase chain reaction (PCR) amplification using gene-specific primers. PCR was performed with 2X PCR PreMix (SolGent, Daejeon, Korea, http://www.solgent.co.kr). PCR was performed using a Promega (Madison, WI, http://www.promega.com) PCR system with Taq DNA polymerase and accompanying buffers. The cDNA at 2-μl aliquots was amplified by a DNA thermal cycler (Bio-Rad, Hercules, CA, http://www.bio-rad.com) in a 25-μl reaction mixture containing 1.0× thermophilic DNA polymerase reaction buffer, 1.25 mM MgCl2, 0.2 mM each dNTP, 0.6 μM each forward and reverse primer, and 1.0 U of Taq DNA polymerase under the following conditions: the mixture was annealed at 50°C–61°C (1 minute), extended at 72°C (2 minutes), and denatured at 95°C (45 seconds) for 30–35 cycles. This was followed by a final extension at 72°C (10 minutes) to ensure complete product extension. The PCR products were electrophoresed through an agarose gel, and amplified cDNA bands were visualized by ethidium bromide staining. The bands were imaged by the Gel Doc EQ System (Bio-Rad).
Data Analysis and Statistics
Nonlinear-fitting programs (OriginLab Corporation, Northampton, MA, http://www.originlab.com) were used. Results are presented as mean ± SEM. Paired and unpaired Student's t tests were used as appropriate to evaluate the statistical significance of differences between two group means. Values of p < .05 were considered to indicate statistical significance.
Characterization of Human Umbilical Cord Vein-Derived MSC Population
Human umbilical cord vein-derived mesenchymal stem cells were isolated by the previously reported procedure of Romanov et al . With this approach, we regularly obtained a cell population in which we observed a spindle-shaped morphology in confluent wave-like layers in culture that was repeated 20 (or more) times. Images of cells from hUC-MSCs on the fourth passage are shown in Figure 1A. A characteristic growth pattern of a homogeneous cell phenotype was demonstrated during normal culture (data not shown). These attributes remained constant during repeated subcultivation up to the last ∼10th passage. Electrophysiological recordings were performed using ball-shaped cells obtained after trypsin-EDTA treatment of the cultures shown in the inset of Figure 1A. We performed an RT-PCR analysis for various genes, including markers of the undifferentiated state (LIFR, ABCG2), mesoderm markers (CXCR4, CD44, COL10A1), and extracellular matrix molecules (COL1A1) (Fig. 1B). The hUC-MSCs were obtained from different donors (lanes I–IV) and the hBM-MSCs was purchased from Cambrex. The expression levels of OPN, ABCG2, CD44, LIFR, and COL1A1 genes determined by RT-PCR were similar in the hUC-MSCs and hBM-MSCs. These cells were positive for adhesion molecules (CD44), integrin markers (CD29), and extracellular matrix protein (CD90) and MSC markers (CD105, CD73) and were negative for hematopoietic (CD34, CD45), endothelial (CD31), and major histocompatibility antigen (HLA-DR) in flow cytometry analysis (Fig. 1C).
The differentiation potential of hUC-MSCs was tested by culturing under multidifferentiation conditions. Supplemental online Figure 1A–1C shows the differentiation capacity to adipocytes, osteoblasts, and chondrocytes of hUC-MSCs, respectively.
Families of Ion Channel Currents in hUC-MSCs
Membrane currents were elicited by 300-millisecond (ms) voltage steps between −120 and +100 mV from a holding potential of −80 mV in hUC-MSCs, as illustrated in Figure 2. Two types of ionic currents activated by voltage steps in hUC-MSCs are displayed in Figure 2A. One component showed a gradually activating current at potentials between +20 and +100 mV, a delayed rectifier K+ current (IKDR). Another component showed rapid activation with noisy oscillation between +60 and +120 mV. This rapidly activating component with noisy oscillation was similar to a Ca2+-activated K+ current (IKCa). We also found another type of current named a transient outward current (Ito) (Fig. 2B). The current was similar to the Ito observed in cardiac and neuronal cells, coexisting with the IKCa in other hUC-MSCs. In another experiment, we identified an inward current, followed by IKDR, IKCa, and Ito (Fig. 2C). Most of the hUC-MSCs investigated (116 out of 125 cells, 92.8%) demonstrated IKDR and IKCa currents activated by the given voltage protocols (mostly IKCa showing at over +60 mV), and Ito was found in more than 50% (65 out of 125 cells) of hUC-MSCs. The inward current was coexistent with outward currents in ∼30% of the hUC-MSCs (36 out of 125 cells). No differences in channel type expression or ion current density were observed in the cells from different passages (ranging from third to sixth).
Characteristics of Na+ Currents of hUC-MSCs
It is well known that an inward current such as Na + current or Ca2+ current is conducted by electrochemical driving forces in physiological solutions. Here, we found that an inward current was present in 36 out of 125 cells (∼30%) in our experimental voltage protocols applied for recording outward currents (Fig. 2C). To study the nature of the inward current, we applied typical pharmacological agents such as the Na+ channel blocker TTX and the L-type Ca2+ channel blocker verapamil in hUC-MSCs with inward currents. The current traces were recorded with K+ pipette solution and normal Tyrode's bath solution with voltage steps as shown in the inset in the absence and presence of TTX (Fig. 3A). The typical inward current-voltage relationships (I-V relationships) were shown to be bell-shaped, and the current peaks were shown at 0 mV (Fig. 3A-1).
Interestingly, the inward current was blocked not only by TTX but also by verapamil (Fig. 3B). Thus, we investigated the sensitivity of two drugs on the inward current. The inward current was entirely abolished by application of TTX (100 nM) and verapamil (100 μM) in bath solution. The blocking effect on the current by TTX was recovered after a drug washout for 5 minutes, but the effect by verapamil was not fully eliminated. Half-block concentrations of TTX and verapamil on the current were 4.5 nM and 15.7 μM, respectively. To establish which ions carry the inward current, the external (bath solution) Na+ ions were replaced by NMDG+. The inward current was abolished under Na+-free conditions in the same cell that showed effects from TTX and verapamil treatment. As shown in Figure 3B, the TTX- and verapamil-sensitive current was clearly absent in a Na+-free bath solution (1.8 mM CaCl2 remained in the bath solution). Indeed, nifedipine, L-type Ca2+ channel blocker, had no effect on this current (data not shown). These findings suggested that the inward current may be a TTX-sensitive INa with verapamil sensitivity.
The Existence of Inward Rectifying K+ Currents of hUC-MSCs
We found another type of inward current in hUC-MSCs (Fig. 3C). Representative inward rectifying current traces in hUC-MSCs were evoked by a ramp voltage from −150 to +60 mV for 400 ms at 0 mV of holding potential. I-V relationships were plotted by ramp voltage-induced inward currents against membrane potentials in the bath solutions containing 5, 15, 30, 75, and 150 mM K+ as indicated, respectively. Elevation of the external (bath solution) K+ concentration increased the inward current amplitude and positively shifted its reversal potential after the K+ equilibrium potential and the linear slope conductance of the inward current increased, suggesting that K+ carries this current. I-V relationship exhibited strong inward rectification with a reversal potential of −85 mV. The currents were dose-dependently blocked by Ba2+ (data not shown). These properties are very similar to inward rectifier K+ currents (Kir). We conclude that Kir channels are present in hUC-MSCs, where they contribute to its resting membrane potential.
Outward K+ Currents of hUC-MSCs
All hUC-MSCs investigated demonstrated outward currents (125 out of 125 cells). We found that three types of outward current were present in hUC-MSCs, including IKCa, IKDR, and Ito.
The most abundant outward current rapidly activated at positive voltages. As shown in Figure 4, current traces were recorded in a representative cell with the voltage protocol shown in the inset. The noisy oscillation current was remarkably reduced by application of 100 nM iberiotoxin (Fig. 4A). This current was identified as a Ca2+-activated K+ current, conducted by big conductance K+ (MaxiK or BKCa) channels, due to its high sensitivity to iberiotoxin, which is known as a MaxiK channel-specific blocker. The remaining current detected with the voltage protocol shown in the inset was inhibited by TEA in a dose-dependent manner (Fig. 4B), suggesting that IKCa was coexistent with IKDR in hUC-MSCs.
Ito traces recorded in representative hUC-MSCs under control conditions and after the application of 4-AP and TEA are shown in Figure 5A. Ito was substantially inhibited by 300 μM 4-AP, whereas TEA had no effect on it. Ito at +60 mV was inhibited to 8.8 ± 4.2 picoampere (pA)/picofarad (pF) from 26.4 ± 4.7 pA/pF of the control (n = 6). I-V relationships of Ito mean values in the absence and presence of 4-AP are displayed in Figure 5A-1. The inhibition was relieved after washout of the drug for less than 5 minutes.
The percentages of hUC-MSCs expressing ion channel patterns are summarized in Figure 5C. Because almost all patch samples showed the TEA-sensitive current (IKTEA), we set the expression rate of IKTEA to 100% and then measured the expression rate of Ito, INa, and Kir comparatively. Ion channel expression rates were 52% (65 of 125), 28.8% (63 of 125), and 4.8% (6 of 125) in Ito, INa, and Kir, respectively.
mRNA Expression of Functional Ion Channels in hUC-MSCs
To study the molecular identity of the functional ionic currents observed, we investigated the expression pattern in hUC-MSCs with RT-PCR using specific primers (Fig. 6B). Figure 6A displays the mRNA expression (mRNA) for ion channel α-subunits related to functional outward and inward ionic currents. High mRNA levels of MaxiK (responsible for IKCa), Kv1.4 and Kv4.2 (responsible for Ito), Kv1.1 and heag1 (responsible for IKDR), hNE-Na (responsible for INa), and Kir2.1 (responsible for Kir) were detected in hUC-MSCs. We used β-actin for the control. These results provide the molecular basis for the functional ionic currents observed in hUC-MSCs.
In this report, we have demonstrated that several specialized K+ channels and Na+ channels at the mRNA and functional levels were present in undifferentiated human MSCs from the umbilical cord vein. The direct comparison reported here showed that hUC-MSCs and hBM-MSCs express the same gene markers (Fig. 1B) and share common cell surface antigens (Fig. 1C). Also, hUC-MSCs have an ability to undergo multilineage mesenchymal differentiation (supplemental online Fig. 1). Ca2+-activated K+ channel, delayed rectifying K+ current, and transient outward K+ current were present mainly in hUC-MSCs, although inward rectifying K+ current and Na+ current were present in a small portion of the population. Also, we demonstrated characteristics of hUC-MSCs with morphological and immunophenotypical methods. To our knowledge, this is the first time that hUC-MSCs have been extensively characterized from an electrophysiological viewpoint, not just in hBM-MSCs as studied until now [8, 9, 42].
Characteristics and Functional Role of Ion Channels in hUC-MSCs
Electrophysiologically isolated IKDR and Ito from hUC-MSCs were confirmed as Kv1.1, heag1, Kv4.2, and Kv1.4 by RT-PCR. The Kv1.1 subfamily is expressed in the embryonic nervous system [43, 44], and mutations in Kv1.1 are associated with human episodic ataxia type 1 syndrome, which is characterized by movement disorders and epilepsy [45, 46]. Mammalian ether a go-go (EAG) subfamily K+ channels have been studied in several species including rat , mouse , bovine , and human . Human EAG (heag) K+ channels were found to participate in cell proliferation in human breast cancer cells, and inhibition of heag K+ channels arrested cells in the early G1 phase .
Ito was first observed in hMSCs through mRNA expression analysis by Heubach et al. , and then it was detected in a small population of hMSCs (∼8%) by another group . However, in our group, surprisingly, Ito was recorded in over 50% of hUC-MSCs. During development of embryonic stem cell-derived cardiomyocytes, inhibition of Ito by 4-AP changed the duration and frequency of action potentials in the early stage but not in the late stage, suggesting that the Ito of early-stage cardiomyocytes plays an important role in controlling electrical activity . These reports suggest that K+ currents may modulate progression through the cell cycle in proliferating cells and in early embryonic development as well as at later stages of differentiation [37, 38, 40, 52].
IKCa usually coexists with IKDR, and the channel was proven to have a MaxiK channel by pharmacological and molecular biological approaches (Figs. 4, 6). MaxiK channels are usually believed to be sensors of intracellular Ca2+ and are found to regulate membrane potential in an intracellular Ca2+-dependent manner in hMSCs . These results suggest that MaxiK current could, therefore, be an effector of trophic factors within the body fluids or cell culture medium.
Voltage-gated Na+ channels are responsible for action potential initiation and propagation in excitable cells, including nerve, muscle, and neuroendocrine cells. We recorded INa in about 30% of hUC-MSCs and found that the current was highly sensitive to blockage by TTX (Fig. 3A). NaV1.7 (SCN9A or hNE-Na) is highly TTX sensitive and is broadly expressed in neurons, whereas NaV1.5 (SCN5A) is TTX resistant . Electrophysiological properties and mRNA expression pattern of Na+ channel of hUC-MSCs are consistent with the report by Li et al . Unexpectedly, TTX-sensitive Na+ current in hUC-MSCs was also inhibited by verapamil, known as an L-type Ca2+ channel-specific blocker. Furthermore, the current was not eliminated in the absence of Ca2+, and Ca2+ channel transcripts (1αC, 1αD, 1αG, 1αH, and 1αS) were not detected by RT-PCR analysis (data not shown). However, some groups observed the L-type Ca2+ channel in hBM-MSCs using patch clamp and RT-PCR analysis [8, 9]. These results suggest that the variety of ion channel distribution in MSCs may depend on the species or source of MSCs. Na+ channel may play important physiological roles during differentiation of hUC-MSCs into cardiac cells and neuronal cells. Therefore, further studies on the late passages or differentiated cells are needed because these characteristics of the channel may disappear during differentiation of hMSCs. In our view, undifferentiated cells may have undifferentiated channels.
We also demonstrated the presence of an inwardly rectifying K+ current in a small population of hUC-MSCs. Kir2.1 (classic Kir channel or IRK1) transcript was detected by RT-PCR. To our knowledge, this is the first electrophysiological recording of Kir in human MSCs, not in rodent MSCs [42, 54]. Usually Kir likely plays a dominant role in the maintenance of resting membrane potential, in regulating the action potential duration, and thus in controlling the excitability of a variety of cells. It has been reported that Kir is distributed in hemopoietic progenitor cells and neural stem cells [55, 56], raising the possibility that the presence of Kir might be a physiological marker for the pluripotent neural stem cells or neural progenitor cells.
Functional Implications and Conclusions
The present observations focused on the functional expression of ion channels, and we demonstrated that various ion channels are present in hUC-MSCs. An understanding of the regulation of ion channels in undifferentiated hUC-MSCs will be helpful to investigate possible biological solutions, such as gene and/or cell therapy, to medical challenges such as teratogenicity, infection, and immune rejection. Our results provide strong support for the study of the physiological roles of these ionic currents in the proliferation and differentiation of hMSCs in the future, in order to gather more information on human stem cell biology.
Disclosure of Potential Conflicts of Interest
The authors indicate no potential conflicts of interest.
This work was supported by a Grant (034475) from the BioGreen 21 Program, Rural Development Administration, a Grant (KOSEF-2006-04670) from the Basic Research Program of the Korea Science & Engineering Foundation (KOSEF), and a Grant from Korea Research Foundation (R05-2004-000-11589-0). K.S.P. and K.H.J. equally contributed as first author.