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The goal of this study is to characterize resident cardiac stem cells (CSCs) and investigate their therapeutic efficacy in myocardial infarction by molecular imaging methods.
CSCs have been isolated and characterized in vitro. These cells offer a provocative method to regenerate the damaged myocardium. However, the survival kinetics and function of transplanted CSCs have not been fully elucidated.
CSCs were isolated from L2G85 transgenic mice (FVB background) that constitutively express both firefly luciferase (Fluc) and enhanced green fluorescence protein (eGFP) reporter gene. CSCs were characterized in vitro and transplanted in vivo into murine infarction models. Multi-modality noninvasive imaging techniques were used to assess CSC survival and therapeutic efficacy for restoration of cardiac function.
CSCs can be isolated from L2G85 mice and FACS analysis showed expression of resident CSCs markers (Sca-1, c-Kit) and mesenchymal stem cell markers (CD90, CD106). Afterwards, 5×105 CSCs (n=30) or PBS control (n=15) was injected into the hearts of syngeneic FVB mice undergoing left anterior descending artery (LAD) ligation. Bioluminescence imaging (BLI) showed poor donor cell survival by week 8. Echocardiogram, invasive hemodynamic pressure-volume (PV) analysis, positron emission tomography (PET) imaging with Fluorine-18-fluorodeoxyglucose ([18F]-FDG), and cardiac magnetic resonance imaging (MRI) demonstrated no significant difference in cardiac contractility and viability between the CSC and control group. Finally, postmortem analysis confirmed transplanted CSCs integrated with host cardiomyocytes by immunohistology.
In a mouse myocardial infarction (MI) model, Sca-1 positive CSCs provide no long-term engraftment and benefit to cardiac function as determined by multi-modality imaging.
Recent years have brought stem cell therapy for heart disease to the forefront. Several clinical trials have shown beneficial effects of stem cell transplantation to improve cardiac function after myocardial infarction (1–3). However, the mechanism(s) behind this benefit is not clearly understood. Although numerous studies have suggested the cardioprotective benefits from various stem cell types, they also carry limitations including the potential of tumorigenicity with embryonic stem cells (4), arrhythmogenicity with skeletal myoblasts (5), as well as existing controversies surrounding transdifferentation of bone marrow-derived stem cells (6,7).
The identification of undifferentiated cells with stem cell-like properties derived from the myocardium has renewed the excitement to this field. A number of recent studies have confirmed the presence of cells bearing stem cell markers in the myocardium, which were successfully terminally differentiated into cell lineages that can benefit myocardial function (8–12). A recent study even used resident cardiac stem cells (CSCs) derived from human myocardial biopsy specimen and injected them into mice, showing engraftment and improved myocardial function (12).
We have previously described the L2G85 transgenic mice which constitutively express both the firefly luciferase (Fluc) and enhanced green fluorescence protein (eGFP) genes (13,14). Cells derived from these mice provide the advantage of being “trackable” over time. Using the previously described methods for CSC isolation and proliferation (10), we now provide in detail the survival kinetics of transplanted CSCs in infarcted murine hearts. In contrast to previous studies (9,10,12,15,16), our results suggest that these CSCs do not constitute long-term improvement in myocardial function. We also show definitive evidence via bioluminescence imaging that the majority of these cells are not viable by eight weeks post transplantation.
Animal protocols were approved by the Stanford University Animal Care and Use Committee. The L2G85 transgenic mice of FVB background with β-actin promoter driving Fluc-eGFP have been described previously (14,17). Normal adult female FVB mice were used as recipient controls. CSCs were isolated from 6 to 12 weeks old L2G85 mice as described with some modifications (10,11,16). In brief, myocardial tissue was cut into 1- to 2-mm piece, washed with Hanks’ balanced salt solution (HBSS) (Invitrogen, Carlsbad, CA), and incubated with 0.1% collagenase II for 30 minutes at 37°C with frequent shaking. Cells were then filtered through 100-μm mesh. The obtained cells were cultured in Iscove’s Modified Dulbecco’s Medium (IMDM) supplemented with 10% fetal bovine serum (FBS) (Hyclone, Logan, UT), 0.1 mM nonessential amino acids, 100 U/mL Penicillin G, 100 μg/mL streptomycin, 2 mmol/L glutamine, and 0.1 mmol/L β-mercaptoethanol. After 2 to 3 weeks, a population of phase-bright cells appeared over the adhered fibroblast-like cells. These phase-bright cells were collected by two washes with PBS, and one wash with cell dissolution buffer (Gibco, Grand Island, NY) at room temperature under microscope monitoring, and sub-cultured in poly-lysine coated plates (BD Biosciences) with the same medium.
The cells were fixed with 4% paraformaldehyde and processed for immunofluorescence with antibodies to Sca-1 (BD Pharmingen) in situ. Briefly, cells were incubated with rat anti-mouse Sca-1 for 1 hr at room temperature and incubated with goat anti-rat Alexa Fluor 594 (Invitrogen). DAPI was used for nuclear counterstaining.
FACS analysis of the bright cells and the cells sub-cultured on poly-lysine coated plates were carried out and the third passage of bone marrow-derived mesenchymal stem cells (BM-MSCs) from L2G85 mice were used as control. The isolation and culturing techniques of BM-MSCs were similar to previous report (18). Antibodies used in this study were phycoerythrin (PE) conjugated anti-CD34, CD29, CD90, CD44, CD54, Allophycocyanin (APC) conjugated anti-CD31 and c-Kit, APC conjugated anti-rat IgG2a, and rat anti-mouse CD62E, CD62P, Tie-2 (all from BD Pharmingen). The stained cells were analyzed using FACS LSR (Becton-Dickinson, MA). Dead cells stained by propidium-iodide (PI) were excluded from the analysis. Isotype-identical antibodies served as controls (BD Pharmingen). FlowJo software (Tree Star Inc, Ashland, OR) was used for followed data analysis.
For cardiac and smooth muscle differentiation, CSCs were cultured in poly-lysine coated plates in differentiation medium containing 35% IMDM with 10% FBS/65% DMEM–Ham F-12 mix containing 2% B27, 0.1 mmol/L 2-mercaptoethanol, 10 ng/mL epidermal growth factor (EGF; R&D Systems Inc., Minneapolis), 20 ng/mL basic fibroblast growth factor (bFGF; R&D), 40 nmol/L cardiotrophin-1 (R&D), 40 nmol/L thrombin (Sigma-Aldrich, St. Louis), 100 U/mL Penicillin G, 100 μg/mL streptomycin, and 2 mmol/L glutamine (10). After 1 week, the cells were fixed with 4% paraformaldehyde and processed for immunofluorescence with antibodies specific to cardiac troponin T (cTnT), myocyte enhancer factor 2C (MEF-2C), connexin 43, and α-smooth muscle actin (SMA) (all from Santa Cruz Biotech, Santa Cruz, CA) in situ. Briefly, cells were incubated with first antibody for 1 hr at room temperature and incubated with goat anti-rabbit or donkey anti-mouse Alexa Fluor 594. DAPI was used for nuclear counterstaining. For endothelial differentiation, the phase-bright cells were cultured on fibronectin coated plates with EGM-2 (Cambrex, Walkersville, MD) with an extra 20 ng/ml of VEGF. DiI-ac-LDL uptake assay and Matrigel assay were used to confirm endothelial cell phenotype differentiation. For DiI-ac-LDL uptake assay, cells were incubated with 10 μg/ml of DiI-Ac-LDL (Molecular Probes, Eugene, OR) at 37°C for 6 hours. After washing with PBS twice, the slides were fixed and detected with fluorescence microscopy as described (19,20). The formation of endothelial tubes was assessed by seeding cells in 24-well plates coated with Matrigel (BD Pharmingen) and incubating them at 37° for 12 hours as described (19,20). For adipogenic differentiation, the phase-bright cells were cultured in DMEM with 10% FBS, 100 U/mL Penicillin G, 100 μg/mL streptomycin, 2 mmol/L glutamine, 1 μM dexamethasone, 10 μg/ml insulin, 0.5 mM isobulyl-1-methylxanthione, and 200 μM indomethacin for 2 weeks and medium was changed every 3 days. The differentiated adipocytes were confirmed by oil red staining and RT-PCR analysis for peroxisome proliferator-activated receptors gamma (PPARγ) and lipoprotein lipase (LPL) expression. For osteogenic differentiation, the phase-bright cells were cultured in osteogenic differentiation medium (Cambrex, PT-3002) for 2–3 weeks and medium was changed every 3 days. The osteocytes differentiation was confirmed by Alizarin red S staining and RT-PCR analysis for osteocalcin expression as described (21).
All surgical procedures were performed on 8–10 week old female FVB mice (Charles River Laboratories, Inc.) by a single experienced micro-surgeon (GH). FVB mice were anesthetized with inhaled isoflurane (2% to 3%). Mice were intubated, ventilated, and anesthesia was maintained with inhaled isoflurane (1% to 2.5%). A left thoracotomy was performed and the pericardium was opened. The left anterior descending (LAD) artery was permanently ligated with a 9-0 Ethilon suture just distal to the level of the left atrium. Infarction was visually confirmed by blanching of the anterolateral region of the left ventricle along with dyskinesis. After 30 minutes, 5×105 CSCs were injected intramyocardially into the peri-infarct zone at two different sites with a total volume of 20 μl in each animal (n=30). Control animals received PBS injection instead (n=15). For sham operated animals (n=5), open thoracotomy was performed without suturing of the LAD and without injection of CSCs or PBS. A thoracotomy tube was placed and lungs were re-expanded using positive pressure ventilation. The chest cavity was closed in layers with 5-0 Vicryl suture, and the animal was gradually weaned from the respirator. Once spontaneous respiration resumed, the endotracheal and thoracotomy tubes were removed, and the animals were placed in a temperature-controlled chamber until they resumed full alertness and mobility.
BLI was performed on all animals (n=30 CSC, n=15 PBS, and n=5 sham) using the Xenogen IVIS 200 system by a blinded investigator (MH). A majority of the animals were scanned on days 2, 7, 14, 21, 28, 49, and 56. After intraperitoneal injection of the reporter probe D-Luciferin (150 mg/kg), animals were imaged for 1–10 minutes. The same mice were imaged longitudinally for up to 8 weeks. Bioluminescence signal was quantified in units of maximum photons per second per cm square per steridian (photons/sec/cm2/sr) as described (19).
Small animal microPET imaging (Vista system, GE Healthcare) was performed in a subset of the animals (n=14 CSC and n=8 PBS) on baseline (day -7) and days 2, 28, and 56 post-operatively. Mice were fasted for 3 hours prior to radioisotope injection. Animals were then injected with 139±23 μCi [18F]-FDG via the tail vein. At 45 to 60 minutes after injection, animals were anesthetized with inhaled 2% isoflurane. Images were performed, reconstructed by filtered back projection (FBP), and analyzed using image software Amide (http://amide.sourceforge.net/index.html) by blinded investigator (AL). Three-dimensional regions of interest (ROIs) were drawn encompassing the heart. For each ROI, counts/ml/min were then converted to counts/gram/min and divided by the injected dose to obtain the image ROI derived [18F]-FDG percentage injected dose per gram of heart (% ID/g) as described (22). To measure the myocardium infarction size, [18F]-FDG PET images were assembled into polar maps (23). The size of perfusion defects was measured as the myocardium with 50% of maximum activity and expressed as percent total myocardium polar map by GE Healthcare Advantage Workstation (GE Healthcare, UK).
Echocardiography was performed in all animals (n=30 CSC, n=15 PBS, and n=5 sham). A majority of the animals were scanned on baseline (day -7) and days 2, 28, and 56 post-operatively by a blinded investigator (MH) using the Siemens-Acuson Sequoia C512 system equipped with a multi-frequency (8–14 MHz) 15L8 transducer. Animals were anesthetized with inhaled 2% isoflurane. Analysis of M-mode images was performed. Left ventricular end diastolic diameter (LVEDd) and end-systolic diameter (LVESd) were measured and used to calculate fractional shortening (FS) by the following formula: FS= [LVEDd-LVESd]/LVEDd. At the end of the study (week 8), invasive hemodynamic measurements were performed in a subset of the animals (n=5/group for CSC, PBS, and sham) as described (24). Briefly, after midline neck incision, a conductance 1.4 conductance catheter (Millar Instruments, Houston, TX, USA) was introduced into the left ventricle through the right carotid artery. After stabilization, the signals were continuously recorded at a sampling rate of 1000/s using pressure-volume conductance system coupled to a PowerLab/4SP analog to digital converter (ADInstruments). Data were analyzed by using a cardiac pressure-volume analysis program (PVAN 3.4; Millar Instruments, Houston, TX, USA) and Chart/Scope Software (AD Instruments, Colorado Springs, CO, USA).
Please see Supplemental Methods.
After completion of the imaging protocols, all animals were sacrificed at week 8. For immunostaining, explanted hearts (n=10 for CSC, n=5 for PBS, and n=2 for sham) were embedded into OCT compound (Miles Scientific), snap frozen in liquid nitrogen, and cut into transverse sections at 5 μm thickness. To track GFP positive CSC-derived cells and cardiomyocytes differentiation in hearts, anti-GFP antibody (Invitrogen) and anti-α-sarcomeric actin (α-SA) antibody (Sigma) were used. Alexa Fluor 488 and Alexa Fluor 594-conjugated secondary antibodies were applied appropriately. DAPI was used for nuclear counterstaining. To detect microvascular density (MVD) in the peri-infarct area, a rat anti-mouse CD31 (BD Pharmingen) and Alexa Fluor 647-conjugated secondary antibody were used. The number of capillary vessels was counted by a blinded investigator (HC) in ten randomly selected areas using a fluorescence microscope (200x magnification). To detect fibrosis in cardiac muscles, explanted hearts (n=10 for CSC, n=5 for PBS, and n=2 for sham) were fixed in 4% paraformaldehyde, cut transversely, embedded in paraffin, and stained with Masson’s trichome (25). Five to six sections from apex to base were subjected to staining. Images of each section were taken to calculate the fibrotic and nonfibrotic areas as well as ventricular and septal wall thickness. The thinning index is a ratio of the amount of wall thinning in the infarct normalized to the thickness of the septum and is calculated by dividing the minimal infarct wall thickness with maximal septal wall thickness. The measurement of area of fibrosis and thinning index were determined by Image J software (NIH) performed on 3 separate sections, and the averages were used for statistical analysis.
Comparison of fractional shortening (FS), ejection fraction (EF), cardiac viability, and infarction size between CSC and sham/PBS groups over time was done by two-way repeated measures ANOVA with group and day as factors, using a Greenhouse-Geisser correction for lack of sphericity. Comparison of end systolic and diastolic volume and pressure between CSC and sham/PBS groups was done by two-way repeated measures ANOVA with group and cardiac phase as factors, using a Greenhouse-Geisser correction for lack of sphericity. Comparison of histological infarct size and microvascular density between PBS and CSC groups was done by two-tailed t-test. Statistics were calculated using SPSS 14.0 (SPSS Inc., Chicago, IL, USA). Descriptive statistics included mean and standard error. Differences were considered significant at P values of <0.05.
The authors had full access to and take full responsibility for the integrity of the data. All authors have read and accept the manuscript as written.
Explanted hearts were subjected to enzymatic digestion, cultured, and are composed of Sca-1 positive cells (Figure 1A). Phase bright spherical cells that spontaneously separated from the myocardium samples were identified after 2–3 weeks. These cells demonstrated a high nucleus to cytoplasm ratio and expressed robust GFP (Figure 1B). Importantly, assessment of Fluc expression showed a linear correlation (r2=0.98) between the total cell numbers and the bioluminescence signals (Figure 1C), which is needed for accurate tracking of cell fate in subsequent in vivo imaging studies. The cells also demonstrated linear growth with population doubling time of approximately 5 days (Figure 1D), similar to previous studies (10,12,16).
Previous studies have shown that Sca-1 expressing cells possess the potential to differentiate into cardiomyocytes (10,11). Our results showed that ~35.0±5.5% of the phase-bright cells were Sca-1 positive. After subculturing for 1–2 weeks, Sca-1 expression on CSCs was up-regulated close to 95% (Figure 2A). In order to further characterize their cellular phenotypes, detailed flow cytometry analysis was performed. Overall, the subcultured group had higher expression of mesenchymal stem cell markers (CD29, CD90, CD44, CD106), but endothelial (CD31, CD34, CD44) and c-Kit markers were both down-regulated (Figure 2B). Interestingly, compared to BM-MSCs, sub-cultured CSCs have similar expression pattern but express higher CD29 and CD90 and lower CD54. CSCs isolated from normal syngeneic FVB mice also showed similar results (data not shown), suggesting no significant effects on cellular characteristics from the stable expression of Fluc-eGFP reporter gene. Overall, the expression of these markers in our CSCs are similar to previously published data (12,26).
We next examined the differentiation of CSCs into various cell types. Similar to other studies (10,21,27,28), these cells can differentiate into cardiomyocytes and smooth muscle cells, as documented by positive staining for cardiac troponin T (cTnT), connexin 43, MEF-2C, and α-smooth muscle actin (Figure 3A). After seven days in differentiation medium, the cells developed into clusters, and after two weeks they formed into spherical collection of cells, some of which showed spontaneous contractility (Supplementary Video). In addition, these cells were capable of differentiating into endothelial cells as demonstrated by DiI-ac-LDL uptake and Matrigel angiogenesis assays (Figure 3B), into adipocytes as demonstrated by oil red staining and RT-PCR analysis (Figure 3C), and into osteoblasts as demonstrated by Alizarin Red S staining and RT-PCR analysis (Figure 3D).
Several groups have reported that CSCs can proliferate indefinitely in vitro (10,21,27,28). This begs the question whether CSCs can have similar growth properties in vivo, and if so, whether this could lead to potential tumorigenesis. In order to address this question, adult FVB mice were subjected to LAD artery ligation followed by injection with either 5×105 cultured CSCs (n=30) or PBS (n=15). Injection of CSCs into infarcted myocardium resulted in a robust bioluminescence signal at day 2. However, serial imaging of the same animals out to 8 weeks demonstrated a significant decay in the bioluminescence signal. When normalized to results from day 2, the percent bioluminescence signals were 6.7±0.5 at day 7, 3.9±0.8 at day 14, 1.7±0.2 at day 21, 1.4±0.1 at day 28, and 0.4±0.1 at day 56 (Figure 4). Control animals injected with PBS showed no imaging signals as expected.
To date, only a few studies have demonstrated that CSC can improve cardiac function (10,21,27,28). In order to confirm these results, echocardiograms were performed at baseline, day 2, day 28, and day 56 post surgery (Figure 5A, B). At day 2 following infarction, there was a significant decrease in the fractional shortening (FS) in both the CSC group and PBS group compared to the baseline, consistent with successful induction of myocardial infarction. At day 28 and day 56, there was trend toward slight improvement in the FS for both groups, but the difference was not statistically significant. These results were also confirmed in a subset of the animals that underwent cardiac MRI which showed no functional change in ejection fraction (EF) (Supplemental Figure 1). In addition, invasive hemodynamic parameters showed decrease in EF for both CSC and control groups compared to sham group (Supplemental Figure 2). This was associated with higher left ventricular end diastolic volume (EDV) and left ventricular end systolic volume (ESV) in both groups compared to sham. Finally, as highlighted in Supplemental Table 2, there was no significant difference in other functional parameters (e.g., cardiac output, stroke volume) between CSC transplanted mice and PBS control mice.
In addition, we performed [18F]-FDG PET scans of the mice at baseline, day 2, day 28, and day 56 post surgery. This technique can be used to detect changes in cardiac viability following interventions in small animal models (29). At day 2 following infarction, there was a significant reduction in cardiac viability for both groups (20.2±4.9 %ID/g for PBS and 20.8±4.2 %ID/g for CSCs; P<0.001), consistent with successful induction of myocardial infarction. However, at day 28 and day 56, there was no significant difference between the treatment arm and control group (Figure 6A,B). Moreover, analysis of the [18F]-FDG PET images using polar-map reconstruction revealed no significant difference of infarction size between the CSC transplantation group and the PBS group (Figure 6C,D).
Histologic analysis of the myocardium was performed by both looking at thin sections of the gross specimen and via immunofluorescent microscopic examination. Microscopic examination showed the presence of GFP positive cells within myocardium at day 3 (Figure 7A–B). At day 14, CSCs could differentiate into cardiomyocytes as confirmed by α-SMA and GFP double stainings (Figure 7C). However, this population became significantly decreased when the tissues were examined at day 28 (Figure 7D), which is also consistent with the decrease in bioluminescence signals over this period of time (Figure 4). Finally, examination of the explanted hearts showed no significant difference in the infarct size and microvascular density (MVD) between the two groups (Supplemental Figure 3).
In this study, we isolated cardiac resident stem cells from L2G85 transgenic mice that constitutively expressed Fluc-eGFP, enabling us to track stem cell by both noninvasive imaging and invasive histopathology. Upon culturing, we demonstrated that these phase-bright cells upregulated Sca-1 and expressed surface markers resembling mesenchymal stem cells. We also present evidence that molecular imaging can be used to track CSCs survival in a murine model of myocardial infarction. When injected directly into the infarcted heart, these cells initially demonstrated viability by bioluminescence imaging. But after a period of eight weeks, the majority of the imaging signals were no longer present, suggesting elimination from the myocardium. Consequently, we found no significant physiologic benefit from CSC therapy as determined from multiple parameters, including fractional shortening by echocardiogram, myocardial glucose uptake by [18F]-FDG PET scan, ejection fraction by MRI, invasive PV loop analysis, and infarct size by histopathologic assessment.
Recent works have documented the presence of a reservoir of stem and progenitor cells in the myocardium (8,10,16,21,30–32). These cells have been successfully isolated and expanded ex vivo, and have been differentiated into cardiomyocytes, smooth muscle cells, and endothelial cells (10,16,21,26,30–32). Previous works using CSCs have also demonstrated significant improvement in cardiac function after CSC injection, which was in part attributed to the persistent engraftment of the injected CSCs into the infarct zone (9,12,16,33). Higher percentage of viable myocardium within the infarct zone and improved ejection fraction were demonstrated up to five weeks after cell transplantation (9). In contrast, bioluminescence imaging data from our study suggests that by week 8, <0.5% of the transplanted CSCS are still alive. By echocardiography and PET imaging, no significant changes were observed at day 28 and day 56 in cardiac contractility and viability.
At present, we can only speculate that the discrepancy in findings may be attributed to differences in isolation techniques (cardiosphere, side population), stem cell marker expression (c-Kit, Sca-1), donor cell sources (human, mice), particular strains of mice used, or host animal models (non-reperfused LAD ligation, ischemia-reperfusion) (34). From the procedural standpoint, we can not exclude that the possibility that our mice may have been oversedated (2% isoflurane) given the lower baseline fractional shortening values (35–40%) observed compared to previous studies (35). This could have undermined the chances of detecting a small but significant change between the two groups. From the transgenic model standpoint, it is possible that Fluc reporter gene silencing may have occurred and limited our ability to detect surviving CSCs at late time points. However, a previous study using hematopoietic stem cells isolated from these mice was able to demonstrate complete reconstitution of the irradiated bone marrow at late time points as detected by BLI, which argues against significant transgene silencing (17). From the technical standpoint, BLI is limited to small animal imaging as the low energy photons (2–3 eV) can become attenuated within deeper tissues (e.g., heart) compared with more superficial locations (e.g., skeletal muscles). At present, a conservative estimate of minimal detectable cell number by BLI is ~1,000 in the heart vs. ~100 in the leg (14). Finally, from the instrumentation standpoint, it is plausible that the image resolution (~1.5 mm3) and detection sensitivity (10−9 to 10−12 molar) of the small animal microPET scanner is still insufficient to distinguish subtle but significant differences in [18F]-FDG uptake between the two groups. Thus, additional studies will be needed in the future to further examine each of these variables separately.
Just as the mechanism of stem cells exerting benefit on myocardial function remains to be fully elucidated, the mechanism of their elimination over time also remains poorly understood. The pattern of acute donor cell death seen in our CSC transplantation is also consistent with previous studies showing poor donor cell survival after transplantation of neonatal cardiomyocytes (36), mesenchymal stem cells (37), bone marrow mononuclear cells (14), and human embryonic stem cell-derived cardiomyocytes (38). A number of culprits may be involved, including inflammation, ischemia, apoptosis, anoikis, and autophagy may all play contributory roles. Furthermore, the myocardial milieu in vivo is a stark contrast to the rich nutrients and oxygen concentration that have been optimized for their cell culturing, growth, and expansions in vitro. It is interesting to note historically that myoblast transplantation as a potential cell-based therapy for patients with Duchenne muscular dystrophy (DMD) met with disappointing failures in the 1990s (39). One of the main reasons was acute donor cell death following transplantation. Future clinical studies aimed at transplanting CSCs in patients will likely need to first understand the mechanism of acute donor cell death.
Despite the limitation of acute donor stem cell death, both animal and clinical studies have suggested beneficial effects following transplantation of various stem cell types (40), perhaps acting through paracrine pathways (41). Thus, strategies aimed at prolonging cell survival (and hence prolonging paracrine activation) may lead to even more favorable results. To that extent, the application of bioengineering methods (42) or pro-survival cocktails (43) or genetic modification (44), rather than direct stem cell injection, may prove to be a more viable approach for achieving long-term engraftment in the future. Encouragingly, recent study by Tillmanns et al. showed that CSCs activated with insulin-like growth factor 1 and hepatocyte growth factor before their injection into infarcted sites had significantly improved cell survival rate and was able to form conductive arterioles and capillaries in the host myocardium (45).
In summary, our study demonstrates that imaging can be used to monitor CSC fate noninvasively in living animals and that CSC transplantation provides no significant benefits to cardiac function in a mouse myocardial infarction model. As the field of cardiac stem cell therapy continues to mature, it is critical to better understand the underlying mechanism of the treatment modality, and to identify the potential pitfalls of the therapy prior to its incorporation into the clinical realm (1). Although a stem cell source from the heart is of tremendous potential, cautious optimism is necessary prior to full clinical use of these cells.
Videos 1-2: After 1-2 week culture, some phase-bright cells formed cardiospheres and started beating. Images are shown in bright field (video 1) and immunofluorescence views (video 2).
This work was supported in part by grants from the NIH HL089027 (JCW), Burroughs Wellcome Foundation Career Award for Medicine Scientists (JCW), and Society of Nuclear Medicine Pilot Research Award (ZL).
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