Spontaneous and evoked intracellular calcium transients in donor-derived myocytes following intracardiac myoblast transplantation (original) (raw)
Most donor-derived myocytes are functionally isolated from the host myocardium following myoblast transplantation into normal hearts. In order to monitor [Ca2+]i transients in the donor-derived myocytes, it was necessary to generate skeletal myoblasts carrying a fluorescent reporter gene compatible with the TPME imaging system. Accordingly, skeletal myoblasts were isolated from mice that express an EGFP reporter gene under the regulation of the chicken β-actin (ACT) promoter, ACT-EGFP mice (10). The transgene is expressed ubiquitously in these animals, and robust fluorescence is seen in both skeletal myoblasts and skeletal myocytes. Myoblasts prepared from ACT-EGFP mice were injected directly into the left ventricle of nontransgenic adult recipients. Myoblast transplantation into uninjured hearts typically resulted in the formation of relatively large grafts comprised of well-differentiated, aligned skeletal myocytes (Figure 1A). Cell transplantation was specifically performed in uninjured hearts so as to maximize our ability to image functional interactions between donor-derived myocytes and host cardiomyocytes.
Most engrafted donor-derived myocytes are functionally isolated from the host myocardium. (A) Fluorescence image of a typical intracardiac graft resulting from transplantation of ACT-EGFP myoblasts. Scale bar: 20 μm. (B) Full-frame TPME image of the graft/myocardium border zone of a heart following transplantation of ACT-EGFP myoblasts. Hearts were loaded with rhod-2. Host cardiomyocytes (red) and donor-derived myocytes (green/yellow) are apparent. The white bar marks the position of line-scan mode data acquisition. Scale bar: 20 μm. (C and D) Stacked line-scan images and spatially integrated traces of the changes in rhod-2 (red) and EGFP (green) fluorescence (F) during spontaneous (C) and field stimulation_evoked (D) depolarizations from the heart depicted in B at 14 days following ACT-EGFP skeletal myoblast transplantation. Field stimulation was performed at 2 Hz. Note the presence of calcium transients in the donor-derived EGFP-expressing myocyte during field stimulation of the heart, but not during sinus rhythm. a.u., arbitrary units.
To monitor donor cell function, hearts transplanted with skeletal myoblasts were harvested, loaded with rhod-2, and imaged using TPME laser scanning microscopy. To have action potential–evoked [Ca2+]i transients in the same microscopic field, initial imaging was performed at the graft/myocardium border. A representative image obtained in full-frame mode during spontaneous sinus rhythm is shown in Figure 1B. The donor-derived myocytes (which appeared yellow due to the overlay of green EGFP and red rhod-2 fluorescence) were observed to be interdigitated with the host cardiomyocytes (which appeared red due to rhod-2 fluorescence). Periodic increases in rhod-2 fluorescence resulting from action potential–evoked increases in cytosolic calcium concentration are visible as ripple-like wave fronts in host cardiomyocytes, but not in donor-derived myocytes. In order to quantitate temporal changes in [Ca2+]i, fluorescence signals were also recorded in line-scan mode during normal sinus rhythm. The scan line (Figure 1B, white bar) traversed a host cardiomyocyte and a juxtaposed donor-derived myocyte at a speed of 110 μm/ms. This line was repeatedly scanned at a rate of 32 Hz, and the resulting line scans were stacked vertically (Figure 1C, upper panel). Averaged traces of the red and green fluorescence from the host cardiomyocyte and the donor-derived myocyte were then generated from the line-scan data (Figure 1C, middle and lower panels, respectively). These traces confirmed that the host cardiomyocytes exhibited transient increases in rhod-2 fluorescence, corresponding to action potential–evoked increases in [Ca2+]i. In contrast, no [Ca2+]i transients were detected in the donor-derived skeletal myocytes.
To exclude the possibility that this observation resulted from loss of membrane excitability or malfunction of the depolarization-induced calcium release process in the donor-derived myocyte, calcium responses were also monitored during electrical field stimulation (80 V, 1 ms duration, 2 Hz). Under these conditions, [Ca2+]i transients were no longer dependent on cell-to-cell action potential propagation. Electrical field stimulation readily evoked rhod-2 transients in both the host cardiomyocyte and the donor-derived myocyte (Figure 1D, middle and lower panels, respectively). Collectively, these data indicate that the vast majority of donor-derived myocytes present at the graft/myocardium border are not functionally coupled with the host myocardium during normal cell-to-cell electrical propagation under the imaging conditions used. However, these cells are excitable and retain the ability to raise [Ca2+]i in response to membrane depolarization. Similarly, no [Ca2+]i transients were detected in the central region of the skeletal myocyte grafts during spontaneous or remote point stimulation–evoked depolarizations. A total of 585 donor-derived myocytes imaged during spontaneous sinus rhythm were observed to be electrically isolated from the host myocardium. These cells were distributed among 27 independent animals and in grafts ranging from 11 to 106 days old.
Stimulation-evoked [Ca2+]i transients are similar in donor-derived myocytes in situ and in vitro. The relatively long duration of [Ca2+]i transients in field-stimulated donor-derived skeletal myocytes (see Figure 1D) was surprising, given that the duration of field stimulation–induced [Ca2+]i transients in adult murine skeletal muscle fibers is typically less than 100 ms under comparable experimental conditions (12). To further address this point, the temporal profiles of field stimulation–evoked [Ca2+]i transients were quantitatively compared between donor-derived myocytes and adjacent host cardiomyocytes. Although no variability existed in the rising phase, the duration of the recovery phase differed significantly between individual donor-derived myocytes as well as between the donor-derived myocytes and their neighboring host cardiomyocytes (Figure 2A). Similar variability in recovery phase duration was seen following field stimulation of in vitro–differentiated skeletal myocytes prepared from nontransgenic mice and imaged in the absence of cytochalasin D (Figure 2B). Quantitative comparisons revealed no significant differences in [Ca2+]i transient profiles between the myoblast-derived skeletal myocytes in situ and in vitro (Figure 2C). These data also indicated that neither expression of EGFP nor the presence of cytochalasin D contributed to the heterogeneity in [Ca2+]i transient duration. Prolongation and heterogeneity in the [Ca2+]i transient recovery phase has been reported previously for skeletal myocytes following in vitro differentiation (13, 14). Importantly, the imaging conditions and the effects on recovery-phase kinetics were very similar to the in situ and in vitro results obtained here.
Donor-derived myocytes retain skeletal muscle_like functional characteristics following transplantation into the ventricular myocardium. (A) Relative changes in rhod-2 fluorescence (ΔF) as a function of time in donor-derived, EGFP-expressing myocytes (red, blue, and black traces) and a neighboring host ventricular cardiomyocyte (green trace) during electrical field stimulation (2 Hz). The relative changes in rhod-2 fluorescence were normalized such that 0 represents the pre-stimulus fluorescence intensity and 1 represents the peak fluorescence intensity. (B) Relative changes in rhod-2 fluorescence in in vitro_differentiated skeletal myocytes (red and blue traces) following field stimulation (2 Hz; data normalized as in A). (C) Quantitative comparisons of [Ca2+]i transient parameters from donor-derived, EGFP-expressing myocytes (white bars) vs. in vitro_differentiated skeletal myocytes (gray bars) following field stimulation (2 Hz). Values are mean ± SEM of 12 donor-derived, EGFP-expressing myocytes distributed among 4 hearts and from 7 in vitro_differentiated, WT skeletal myocytes after 7_10 days of culture. There were no significant differences between the groups (P > 0.05). (D) Spatially integrated traces of the changes in rhod-2 (red) and EGFP (green) fluorescence during field stimulation at incrementally increasing rates in a donor-derived, EGFP-expressing myocyte in situ (upper panel), in a neighboring host cardiomyocyte (middle panel), and in an in vitro_differentiated skeletal myocyte (lower panel). Note the development of tetanus in the donor-derived skeletal myocyte in situ and in the in vitro_differentiated skeletal myocyte, but not in the cardiomyocyte.
It is well known that rapid pacing in skeletal muscle results in the fusion of successive [Ca2+]i transients such that they cannot be distinguished from one another (i.e., tetanus), a property that sets it apart from cardiac muscle. To further characterize the [Ca2+]i signaling phenotype in the donor-derived myocytes, hearts with cellular transplants were harvested and loaded with rhod-2, and line-scan imaging was performed during field stimulation at incrementally higher frequencies. Integrated traces of the line-scan data from a rapidly paced, engrafted donor-derived myocyte revealed that the cell developed tetanus in response to rapid stimulation (Figure 2D, upper panel). The donor-derived myocyte [Ca2+]i returned to baseline levels once pacing was terminated. In contrast, [Ca2+]i transient amplitudes in the host (EGFP-negative) cardiomyocyte did not develop tetanus with increased pacing rates (Figure 2D, middle panel). As a control, in vitro–differentiated skeletal myocytes were also subjected to field stimulation at incrementally higher frequencies. As expected, the cultured skeletal myocytes developed tetanus with high-frequency stimulation (Figure 2D, lower panel). Thus, the donor-derived myocytes retained many functional properties characteristic of in vitro–differentiated cells.
Apparent functional coupling of a limited number of donor-derived myocytes at the graft/myocardium border. Quite unexpectedly, a small fraction of the donor-derived myocytes exhibited [Ca2+]i transients in synchrony with host cardiomyocytes during spontaneous sinus rhythm. These cells were localized exclusively along the graft periphery (Figure 3, A–C). Fluorescence signals were recorded in line-scan mode to quantitate temporal changes in [Ca2+]i; the scan line (Figure 3, A–C; white bars) traversed at least one host cardiomyocyte (red cell) and the juxtaposed EGFP-expressing donor-derived myocyte (which appeared yellow due to the overlay of EGFP and rhod-2 fluorescence). The resulting stacked line-scan images (Figure 3, D–F) showed that rhod-2 fluorescence increased simultaneously in the EGFP-expressing donor-derived myocytes and their neighboring host cardiomyocytes (within the temporal resolution of the imaging system). The presence of synchronous [Ca2+]i transients in the donor-derived myocytes and juxtaposed host cardiomyocytes strongly suggested that these cells were functionally coupled.
A small fraction of donor-derived myocytes are functionally coupled to the host myocardium. (A_C) Full frame_mode images of rhod-2_loaded hearts after transplantation of ACT-EGFP myoblasts; rhod-2 (red) and EGFP (green) signals were superimposed. White bars mark the position of the line-scan mode data acquisitions. Scale bars: 10 μm. (D_F) Stacked line-scan images depicting spontaneous [Ca2+]i transients in the indicated regions in panels A, B, and C, respectively. (G_I) Superimposed tracings of spontaneous changes in rhod-2 fluorescence as a function of time from the donor-derived EGFP-positive myocyte and host EGFP-negative cardiomyocytes in A, B, and C, respectively. For each cell, spatially averaged changes in rhod-2 fluorescence were obtained and subsequently normalized such that 0 represents the fluorescence intensity before the [Ca2+]i transient and 1 represents the peak fluorescence intensity.
Spatially averaged traces from coupled donor-derived myocytes and the host cardiomyocytes along the scan lines were generated, and changes in fluorescence were normalized such that 0 represented the fluorescence value prior to [Ca2+]i transient onset and 1 represented the peak fluorescence value. Superimposition of normalized [Ca2+]i transients (Figures 3, G–I) demonstrated that both the coupled donor-derived myocytes and the host cardiomyocytes exhibited rapidly rising [Ca2+]i transients. In contrast, the time course of the recovery phase of the [Ca2+]i transients was heterogeneous in the coupled donor-derived myocytes. While some cells exhibited recovery phases of similar duration to those in the neighboring host cardiomyocytes (Figure 3G), others were markedly shorter (Figure 3H) or longer (Figure 3I) in duration.
On average, the values for [Ca2+]i transient duration (_CaT_50%, _CaT_90%) and decay times (_t_90–50%, _t_50–10%) were similar in the coupled donor-derived myocytes and the host cardiomyocytes during spontaneous sinus rhythm. However, given the marked heterogeneity in transient duration, the variances for many of the parameters measured were significantly greater in the skeletal myocytes (Table 1). Interestingly, the variability of the [Ca2+]i transient recovery phase in the coupled donor-derived myocytes was very similar to that seen for uncoupled donor-derived myocytes during field stimulation: values for _t_90–50%, _t_50–10%, _CaT_50%, and _CaT_90% were 79 ± 8.9, 123 ± 7.6, 141 ± 11.3, and 264 ± 17.6 ms, respectively (stimulation at 2 Hz; 12 cells, distributed among four recipient hearts, were analyzed). The heterogeneity in [Ca2+]i transient duration observed during spontaneous depolarization (about 2 Hz) persisted during point stimulation at 4 Hz (data not shown). A total of 177 donor-derived myocytes exhibiting [Ca2+]i transients synchronous with those in neighboring cardiomyocytes during spontaneous sinus rhythm have been imaged. These cells were distributed among 27 different animals and in grafts ranging from 11 to 106 days old. Thus, on average fewer than seven coupled donor-derived myocytes per heart were detected in the areas amenable to image analysis.
Properties of [Ca2+]i transients in functionally coupled, donor-derived myocytes and bordering host cardiomyocytes
Functionally coupled donor-derived myocytes retain characteristics of skeletal muscle cells. The [Ca2+]i transient shape and recovery-phase heterogeneity suggested that coupled donor-derived myocytes retain functional attributes characteristic of skeletal muscle. To further explore this point, the [Ca2+]i response to incremental increases in stimulation rate was monitored in the coupled donor-derived myocytes and neighboring host cardiomyocytes using line-scan analysis. The line scan traversed three juxtaposed myocytes (Figure 4A, white line); cell 1 was a coupled donor-derived myocyte (EGFP positive), and cells 2 and 3 were host cardiomyocytes (EGFP negative). The cells were subjected to field stimulation at frequencies ranging from 2 Hz to 7 Hz. Examination of the resulting stacked line scans (Figure 4B) and the integrated traces (Figure 4C) revealed that the coupled donor-derived myocyte developed tetanus. In contrast, tetanus did not develop with increased pacing rates in the neighboring host cardiomyocytes (rather, a 2:1 stimulus-response block eventually occurred). These observations suggested that coupled donor-derived myocytes retain functional characteristics of skeletal muscle cells. It is well documented that sustained rapid pacing of isolated mouse skeletal muscle fibers induced fatigue, which was manifest by marked decreases in both developed tension and [Ca2+]i transient amplitude (15, 16). Fatigue was also readily induced in myoblast-derived skeletal myocytes during sustained pacing at 10 Hz (Figure 4D).
Incremental increases in the frequency of field stimulation cause development of [Ca2+]i transients (tetanus) in a coupled donor-derived, EGFP-expressing myocyte but not in neighboring cardiomyocytes. (A) Full frame_mode image of a spontaneous [Ca2+]i transient in a rhod-2_loaded heart at 16 days after transplantation of ACT-EGFP skeletal myoblasts; rhod-2 (red) and EGFP (green) signals were superimposed. The white bar marks the position of the line scan_mode data acquisition. Scale bar: 10 μm. (B) Stacked line-scan images of the regions in A indicated by the white line for cells numbered 1 (a coupled, donor-derived myocyte), 2, and 3 (cardiomyocytes). The pacing rate is indicated. (C) Spatially integrated traces of the changes in rhod-2 (red) and EGFP (green) fluorescence for cells 1, 2, and 3. Note that tetanus develops in the coupled donor-derived myocyte, but not in the cardiomyocytes. Identical results were observed when an additional 9 coupled EGFP-expressing myocytes were analyzed. *Ca2+ waves; #dual-peak elevations of [Ca2+]i transients due to superimposition of spontaneous and field stimulation_induced transients. (D) Sustained rapid stimulation induced a decline of [Ca2+]i in in vitro_differentiated skeletal myocytes. Line-scan images from two skeletal myocytes during rest and during continuous field stimulation at 10 Hz for 5 minutes were obtained, and spatially averaged rhod-2 intensities were plotted as function of time. Rapid stimulation causes an initial elevation of [Ca2+]i followed by a slow decay.
Low levels of cellular fusion between donor skeletal myoblasts and host cardiomyocytes. Recent studies have demonstrated that a number of multipotent stem cells can fuse with host cardiomyocytes following systemic delivery (17, 18). To determine whether skeletal myoblasts could fuse with host cardiomyocytes, myoblasts prepared from ACT-EGFP mice were injected into the hearts of myosin heavy chain–nLAC (MHC-nLAC) transgenic mice. The MHC-nLAC reporter gene targets expression of a nLAC reporter exclusively to cardiomyocytes (11, 19); consequently, cardiomyocyte nuclei stain blue when histologic sections from MHC-nLAC mice are incubated with 5-bromo-4-chloro-3-indolyl-β-D-galactoside (X-GAL, a chromogenic substrate for β-gal). Fusion events between donor EGFP-expressing myoblasts and host nLAC-expressing cardiomyocytes can thus easily be identified by the presence of blue nuclei in cells with green fluorescent cytoplasm following X-GAL staining.
To screen for cell fusion events, hearts from MHC-nLAC mice that received ACT-EGFP myoblast transplants were harvested, sectioned, stained with X-GAL, and visualized under bright field illumination. Cardiomyocyte nuclei at the graft/myocardium border were readily identified by the presence of blue nuclear staining (Figure 5, A–C). Examination of the same microscopic fields under fluorescence illumination (Figure 5, D–F, respectively) revealed that some myocytes with nuclear β-gal activity also exhibited cytoplasmic EGFP fluorescence (arrows). The presence of cells with green cytoplasm and blue nuclei is indicative of fusion events between donor skeletal myoblasts and host cardiomyocytes. Given the typical dimensions of adult cardiomyocytes and myoblast-derived skeletal myocytes, and given that the sections analyzed were 10 μm thick, the presence of a blue nucleus within a green cytoplasm cannot result from simple overlay of two individual cells. Cell fusion events were detected only at the graft/myocardium border. A total of 83 fusion events were found in six hearts harvested between 27 and 50 days following transplantation. This represents on average less than one myoblast-cardiomyocyte fusion event per graft-containing section.
Donor skeletal myoblasts can fuse with host cardiomyocytes. (A_C) Bright field photomicrographs of 10-μm sections from MHC-nLAC hearts transplanted with ACT-EGFP skeletal myoblasts. β-Gal_positive cardiomyocyte nuclei at the graft/myocardium border are readily seen. Hearts were harvested between 46 and 49 days after transplantation. (B_F) Fluorescent photomicrographs from the same fields depicted in A_C. Arrows identify the myocytes with blue nuclear staining and green fluorescent cytoplasm.
To further characterize the fused cells, sections prepared from MHC-nLAC hearts that received ACT-EGFP skeletal myoblast grafts were processed for anti-connexin43 immune histologic analyses. Connexin43 immune reactivity was readily detected between neighboring host cardiomyocytes, as evidenced by punctate red signal at the junctional borders between myocytes with blue nuclei and nonfluorescent cytoplasm (Figure 6, A–C). In contrast, no connexin43 immune reactivity was detected between donor-derived myocytes within the center of the graft, as evidenced by the absence of punctate red signal at the junctional borders of myocytes with green fluorescent cytoplasm and nonblue nuclei (Figure 6, D–F; diffuse red autofluorescence was frequently observed in the donor-derived myocyte grafts). This result was expected, given the absence of functional coupling between these cells (see above). Examination of cells arising from fusion events (cells with blue nuclei and green fluorescent cytoplasm) revealed the presence of connexin43 immune reactivity (punctate red signal) at the junctional borders of neighboring host cardiomyocytes (cells with blue nuclei and nonfluorescent cytoplasm; see Figure 6, G–L). Thus, cells arising from fusion events between the donor skeletal myoblasts and host cardiomyocytes retained molecular attributes required for electrical communication with the host myocardium.
Connexin43 immune reactivity between cells arising from myoblast-cardiomyocyte fusion events and host cardiomyocytes. Ten-micron sections prepared from MHC-nLAC hearts transplanted with ACT-EGFP skeletal myoblasts were stained with X-GAL and reacted with an anti-connexin43 Ab, followed by a rhodamine-conjugated secondary Ab. (A_C) Connexin43 is present at the junction of host cardiomyocytes. Host cardiomyocytes are identified by blue nuclear staining (A) and the absence of EGFP fluorescence (B). (C) A higher-magnification image of connexin43 immune reactivity in the boxed region is shown (red signal). (D_F) Connexin43 is absent between donor-derived skeletal myoblasts. Donor-derived myocytes are identified by the absence of blue nuclear staining (D) and the presence of green fluorescence (E). (F) A higher-magnification image of the boxed region after staining for connexin43 immune reactivity. Note the absence of punctate red signal. (G_I) Connexin43 is present at the junction between cells derived from myocyte-cardiomyocyte fusion events and host cardiomyocytes. Cells arising from myocyte-cardiomyocyte fusion events are identified by the presence of blue nuclear staining (G) and EGFP fluorescence (H). Host cardiomyocytes are identified by the presence of nuclear β-gal activity and the absence of EGFP fluorescence. (I) A higher-magnification image of connexin43 immune reactivity in the boxed region. Arrows mark punctate red signal, indicative of the presence of connexin43 (and hence, the presence of gap junctions). (J_L) Additional example of connexin43; arrows indicate the position of the gap junctions. Scale bars: 10 μm.