NOVEL THERAPEUTIC STRATEGIES
Biodrugs 2008; 22 (6): 361-374 1173-8804/08/0006-0361/$48.00/0 © 2008 Adis Data Information BV. All rights reserved.
Embryonic Stem Cell Transplantation Promise and Progress in the Treatment of Heart Disease Feixiong Zhang and Kishore B.S. Pasumarthi Department of Pharmacology, Dalhousie University, Halifax, Nova Scotia, Canada
Contents Abstract . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 361 1. Embryonic Stem (ES) Cells . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 362 2. In Vitro Cardiac Differentiation of ES Cells . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 363 3. Electrophysiologic Properties of ES Cardiomyocytes . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 363 4. Structural and Functional Heterogeneity of ES-Derived Cardiomyocytes . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 364 5. Enrichment Methods for ES-Derived Myocardial Cells . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 365 6. ES-Cell Transplantation for Cardiac Repair . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 366 7. Conclusion and Future Perspectives . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 371
Abstract
Cardiovascular diseases remain the leading cause of death worldwide, and the burden is equally shared between men and women around the globe. Cardiomyocytes that die in response to disease processes or aging are replaced by scar tissue instead of new muscle cells. Although recent reports suggest an intrinsic capacity for the mammalian myocardium to regenerate via endogenous stem/progenitor cells, the magnitude of such a response appears to be minimal and has yet to be realized fully in cardiovascular patients. Despite the advances in pharmacotherapy and new biomedical technologies, the prognosis for patients diagnosed with end-stage heart failure appears to be grave. While heart transplantation is a viable option, this life-saving intervention suffers from an acute shortage of cardiac organ donors. In view of these existing issues, donor cell transplantation is emerging as a promising strategy to regenerate diseased myocardium. Studies from multiple laboratories have shown that transplantation of donor cells (e.g. fetal cardiomyocytes, skeletal myoblasts, smooth muscle cells, and adult stem cells) can improve the function of diseased hearts over a short period of time (1–4 weeks). While long-term follow-up studies are warranted, it is generally perceived that the beneficial effects of transplanted cells are mainly due to increased angiogenesis or favorable scar remodeling in the engrafted myocardium. Although skeletal myoblasts and bone marrow stem cells hold the highest potential for implementation of autologous therapies, initial results from phase I trials are not promising. In contrast, transplantation of fetal cardiomyocytes has been shown to confer protection against the induction of ventricular tachycardia in experimental myocardial injury models. Furthermore, results from multiple laboratories suggest that fetal cardiomyocytes can couple functionally with host myocytes, stimulate formation of new blood vessels, and improve myocardial function. While it is neither practical nor ethical to test the potential of fetal cardiomyocytes in clinical trials, embryonic stem (ES) cells serve as a novel source for generation of unlimited quantities of cardiomyocytes for myocardial repair. The initial success in the application of ES cells to partially repair and improve myocardial function in experimental models of heart disease has been quite promising. However, multiple hurdles need to be crossed before the potential benefits of ES cells can be translated to the clinic. In this review, we summarize the current knowledge of cardiomyocyte derivation and enrichment from ES-cell cultures and provide a brief survey of factors increasing cardiomyogenic induction in both mouse and human ES cultures. Subsequently, we summarize the current state of research using mouse and human ES cells for the treatment of heart disease in various experimental models. Furthermore, we discuss the challenges that need to be overcome prior to the successful clinical utilization of ES-derived cardiomyocytes for the treatment of end-stage heart disease. While we are optimistic that the researchers in this field will sail across the hurdles, we also suggest that
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a more cautious approach to the validation of ES cardiomyocytes in experimental models would certainly prevent future disappointments, as seen with skeletal myoblast studies.
Cardiomyocyte division stops in the mammalian heart during early postnatal life.[1,2] As a result, myocytes that die in response to aging as well as pathologic insults are replaced by scar tissue instead of new muscle cells. Furthermore, overactivation of compensatory signals from the sympathetic and renin-angiotensin systems can compromise myocyte viability and cardiac performance, and ultimately cause heart failure. Cardiovascular diseases (e.g. myocardial infarction (MI) and congestive heart failure) account for the death of more people than any other disease. Although recent reports suggest an intrinsic capacity for the mammalian myocardium to regenerate via endogenous stem/progenitor cells, the magnitude of such a response appears to be minimal and yet to be realized fully in the case of cardiovascular patients. According to the latest data from Statistics Canada, approximately 32% of all male deaths and 34% of all female deaths in 2002 were due to cardiovascular disease.[3] While organ transplantation may extend the life of patients diagnosed with end-stage heart failure, this approach suffers from a severe shortage of donor availability. New biomedical technologies have facilitated the development of a number of life-saving drugs and surgical interventions for patients with end-stage heart failure. However, current drug therapies can increase the life expectancy of heart failure patients by only 2–3 years.[4] Data from a large number of cardiovascular clinical trials indicate that pharmacologic therapies can reduce patient mortality by 25–30%.[5] For patients with acute MI, percutaneous coronary intervention combined with fibrinolytic drugs can reduce in-hospital mortality rates to less than 10%.[6] Similarly, life-saving devices such as defibrillators and left-ventricular assist devices can reduce mortality rates by 20–50%.[7,8] Nonetheless, given the increasing incidence of heart failure and cardiovascular-related deaths around the globe, heart disease patients may benefit from the development of new life-saving interventions. Donor cell transplantation is emerging as a promising strategy to regenerate diseased myocardium.[9] Studies from multiple laboratories have shown that transplantation of donor cells (fetal and embryonic stem [ES] cell-derived cardiomyocytes, skeletal myoblasts, smooth muscle cells. and adult stem cells) can improve the function of diseased hearts.[9] In general, paracrine factors secreted from the transplanted cells are thought to play key roles in stimulating angiogenesis and improving the function of the engrafted myocardium. Among these donor cells, skeletal myoblasts and bone marrow stem cells (BMSC) hold the highest potential for implementation of autologous therapies. Following intra-cardiac skeletal myoblast transplantation, a cohort of patients with severe heart failure showed improvement in the ejection fraction.[10] © 2008 Adis Data Information BV. All rights reserved.
However, this intervention led to an increased arrhythmic risk in several patients.[10] Similarly, the initial positive results from the BMSC clinical trials remain highly controversial.[9,11,12] In contrast, transplantation of fetal cardiomyocytes was shown to confer protection against the induction of ventricular tachycardia in experimental myocardial injury models.[13] Furthermore, results from multiple laboratories suggest that fetal cardiomyocytes can functionally couple with host myocytes, stimulate formation of new blood vessels, and improve myocardial function.[13-18] While it is neither practical nor ethical to test the potential of fetal cardiomyocytes in clinical trials, ES cells may represent a novel source of cardiomyocytes for the treatment of ischemic heart disease. In this review, we summarize the current knowledge of cardiomyocyte derivation from ES-cell cultures and provide a survey of ES-cell transplantation studies in models of experimental heart disease. Furthermore, we discuss potential challenges in the clinical realization of ES-derived cardiomyocytes for the treatment of patients with heart failure. 1. Embryonic Stem (ES) Cells ES cells were first derived in 1981 from the inner cell mass (ICM) of pre-implantation-stage mouse embryos (blastocysts) by two independent groups.[19,20] Subsequently, ES cells were derived from several other species.[21-24] In 1998, Thomson et al.[25] were the first to propagate human ES cells. Mouse ES cells can be maintained in an undifferentiated state by growing them on mitomycin-treated mouse embryonic fibroblasts (MEFs) and/or by supplementing cultures with leukemia inhibitory factor (LIF).[26,27] In contrast, human ES cells are cultured on irradiated MEFs and supplemented with basic fibroblast growth factor.[28] When maintained in an undifferentiated state, these cells can proliferate indefinitely and carry a normal karyotype. ES cells are considered as pluripotent stem cells, which can give rise to cells of all three primary germ layers.[29] In the absence of conditions that maintain them in an undifferentiated state, ES cells will spontaneously differentiate to form multicellular aggregates known as embryoid bodies (EBs). Over a period of time, aggregated cells in EBs can form elements of all three germ layers. Consistent with their in vitro pluripotent nature, injection of mouse ES cells in syngeneic or immunocompromised animals can give rise to tumors containing derivatives of all three germ layers (teratomas).[30] Existing human ES-cell lines may contain chromosomal abnormalities and are likely to form teratomas or other cell lineages after transplantation. Hence, high-fidelity methods for fractionation of differentiated cells from stem cell cultures should form the focus of future ES cell-based therapies. Biodrugs 2008; 22 (6)
ES-Cell Transplantation and Myocardial Repair
Although embryo/ICM-derived ES cells serve as a reliable source for cell-based therapies, clinical use of these stem cells for the treatment of human disease is currently prohibited because of several political, scientific, and ethical reasons (reviewed by Das et al.[31]). These concerns are mainly related to the destruction of human embryos for derivation of ES cells, immune rejection, and safety issues of human cells grown on mouse feeder cell layers (i.e. MEFs). In this regard, major efforts are being pursued to derive ES cells through alternative mechanisms. These alternative approaches include reprogramming of adult somatic cells into pluripotent stem cells using methods such as the somatic cell nuclear transfer technique (SCNT),[32,33] derivation of ES cells from single blastomeres without destruction of whole embryos,[34,35] and genetic conversion of fibroblasts into stem cells.[36-38] While all three approaches are technically challenging, the SCNT technique is yet to be realized for derivation of human ES cells. In contrast to the first two methods, genetic conversion of fibroblasts does not rely on the use of either human oocytes or fertilized embryos and hence is rapidly gaining popularity. It has been shown that the introduction of four genes, POU5F1 (Oct3/4), SOX2, MYC, and KLF4 into adult mouse or human fibroblasts can give rise to pluripotent stem cells with much higher efficiency compared with the efficiencies of SCNT and blastomere approaches.[36-39] The ES cells resulting from genetic conversion of fibroblasts are referred to as induced pluripotent stem (iPS) cells. Similar to the ICM-derived ES cells, iPS cells can give rise to cells of all three germ layers, form teratomas, and also give rise to chimeric animals when injected into blastocysts. Furthermore, the iPS approach eliminates the immune rejection associated with cell-based therapies, as it facilitates generation of patient-specific stem cells from their own somatic cells. However, the presence of MYC or random genomic integration of exogenous genes in differentiated cells derived from iPS cells is believed to increase the risk of cellular transformation.[31] Furthermore, iPS cells have been shown to exhibit some differences in DNA methylation status compared with ICM-derived ES cells.[39] Current efforts are aimed at finding alternative gene combinations for genetic conversion of adult fibroblasts into iPS cells to lower the risk of transformation.[40] Availability of new-generation iPS cells could certainly reduce some of these pending concerns. Additional studies should be conducted to fully characterize electrophysiologic features of iPS-derived cardiomyocytes, optimize methods of cardiomyocyte enrichment, and also test their potential for the regeneration of diseased myocardium similar to the ongoing validation studies performed on ICM-derived ES cells. 2. In Vitro Cardiac Differentiation of ES Cells The cardiomyogenic potential of mouse and human ES-cell lines has been well documented.[29,41-43] For cardiac differentiation of mouse cell lines, dispersed ES cells are grown in suspension © 2008 Adis Data Information BV. All rights reserved.
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culture with no LIF and allowed to form EBs. After 3–4 days, EBs are transferred to plastic culture dishes and allowed to attach. Regions of cardiogenesis can be readily identified by the presence of spontaneous contractile activity 8–10 days after EB attachment.[26,43] The procedure for in vitro cardiac differentiation of human ES cell lines is identical to that of mouse ES cells, but the time schedule for each step is a little longer (i.e. 5–6 days for EB aggregation and 10–14 days for beating).[41] Under normal culture conditions, about 15–20% of mouse EBs can spontaneously differentiate into cardiomyocytes. In contrast, the cardiomyogenic differentiation rates of existing human ES-cell lines are relatively low and account for only 5–20%.[26,41,44] In order to increase cardiomyogenic induction, different factors were used during the differentiation process of both mouse and human ES cells (see tables I and II). These agents include growth factors/hormones (e.g. transforming growth factor-β, vascular endothelial growth factor, insulin growth factor-1, bone morphogenetic protein-2, oxytocin) and chemical reagents (e.g. H2O2, dimethyl sulfoxide, nitric oxide, 5-azacytidine). A number of studies confirmed that the expression profiles of transcription factors, ion channels, and myocyte-specific proteins during ES cardiogenesis are similar to the stage-dependent changes observed during embryonic and neonatal development.[45-47] The ability of ES cells to differentiate into atrial,[46,48,49] ventricular,[46,49-51] and pacemaker cells[52-54] was documented by monitoring marker gene expression via immunostaining or reverse transcription-PCR, as well as action potential (AP) recordings. In addition to the conventional suspension culture of EBs in culture dishes, efforts are underway to facilitate large-scale propagation of ES cardiomyocytes using engineered heart tissue constructs,[55,56] rotary cell culture systems,[57] and bioreactor technologies.[58-60] Although preliminary studies are encouraging, further studies are required, particularly with human ES cells, to optimize conditions and growth factor combinations for maximal yield of cardiomyocytes using these new technologies. 3. Electrophysiologic Properties of ES Cardiomyocytes ES-derived cardiomyocytes can be classified as pacemaker, atrial, ventricular, nodal, His, and Purkinje-like cells based on their AP characteristics. In mouse ES cultures, cells with pacemaker-like AP were found only at the early and intermediate stages, whereas cells with atrial, ventricular, or nodal types of APs were identified primarily in the later stages of differentiation in ES-cell cultures.[46,51] Pacemaker-like cells were identified by a relatively depolarized and short-lasting AP of smaller amplitude.[46,51] Cells with a relatively stable resting potential and a characteristic notch and plateau phase were designated as Purkinje-like cells.[46,51] In contrast, ES-derived atrial cells exhibited a stable resting potential and a short-lasting AP. Ventricular Biodrugs 2008; 22 (6)
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Table I. Factors increasing cardiomyogenesis of mouse embryonic stem (ES) cells ES-cell line (mouse)
Factor
Reference
D3
RA
50
D3
H2O2, menadione
61
CGR 8
BMP2
62
CGR 8
TGFβ
62
D3
VEGF
63
J1
FGFR1
64
ht7
RA
65
D3
PDGF-BB, SPP
66
R1
Avian precardiac endoderm/mesoderm
67
D3
IGF1
68
D3
Nitric oxide
69
ht7
TSA
70
E14
RXR agonist, BMP4, and serum-free condition
71
CGR 8
BMP2
72
CGR 8
TGFβ2
73
D3
RGD oligopeptides (inhibitor of β1 integrin), lithium, exoenzyme C3
74
D3, ATCC CRL 1934
Small signaling molecules (ryanodine, methoxyverapamil, and cyclosporine [ciclosporin] A)
75
D3
Icariin, icaritin, desmethylicartin
76
D3
BMP2 combined with visceral endoderm-like cells
77
D3
cAMP
78
D3
Ascorbic acid
79
D3
PPARα
80
CGR 8, R1
Chibby
81
Royan B1
Oxytocin
82
Royan B1
bFGF
83
Royan B1
BMP4
84
AB2.2
Desmin
85
D3
HGF
86
R1
RA
87
CGR 8
TGFβ1, BMP2, BMP4, activin-A, FGF2, FGF4, IL-6, IGF1, IGF2, VEGF-A, EGF
88
NA
HRG-β1
89
D3
Oxytocin
90
bFGF = basic fibroblast growth factor; BMP = bone morphogenetic protein; cAMP = cyclic adenosine 3′,5′-monophosphate; EGF = epidermal growth factor; FGF = fibroblast growth factor; FGFR = FGF receptor; HGF = hepatocyte growth factor; HRG-β1 = heregulin-β1; IGF = insulin-like growth factor; IL = interleukin; NA = not available; PDGF-BB = platelet-derived growth factor-BB; PPARα = peroxisome proliferator-activated receptor α; RA = retinoic acid; RGD = arginine, glycine, aspartic acid tripeptide; RXR = retinoid X receptor; SPP = sphingosine-1-phosphate; TGF = transforming growth factor; TSA = trichostatin A; VEGF = vascular endothelial growth factor.
cells exhibited a relatively stable, negative resting potential and a [46,51]
long plateau phase.
Similar AP recordings characteristic of
atrial, ventricular, and nodal-like cardiomyocytes were also documented in human ES cultures.[104,105] In addition to the AP recordings, several investigators used a microelectrode array technique to measure changes in field potentials (extracellular recordings) of ES-derived cardiomyocytes in response to pharmacologic treatments as well as during differentiation.[52,105,106] © 2008 Adis Data Information BV. All rights reserved.
4. Structural and Functional Heterogeneity of ES-Derived Cardiomyocytes As cardiomyogenesis in ES cultures is a fairly random process, it is likely that EBs from a given culture stage would contain cardiomyocytes at different stages of development. Although ESderived cardiomyocytes have been shown to express a number of cardiomyocyte-restricted markers and respond to β-adrenergic and muscarinic agonists, it was suggested that the phenotypes of cardiomyocytes in differentiating mouse EBs are reminiscent of Biodrugs 2008; 22 (6)
ES-Cell Transplantation and Myocardial Repair
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cardiomyocytes from mouse hearts at embryonic day 8.75–9 (E8.75–9), where chamber formation has just started.[107,108] This notion is consistent with other studies that documented major differences in Ca2+-induced Ca2+ release (CICR) between human ES-derived cardiomyoctyes and adult ventricular cardiomyocytes.[109,110] It was shown that the [Ca2+]i transients and contraction of human ES-derived cardiomyocytes depended on transsarcolemmal Ca2+ influx but not on the classical CICR mechanism.[109,110] Furthermore, human ES-derived cardiomyocytes did not express regulatory proteins involved in Ca2+ homeostasis such as phospholamban, junctin, triadin, and calsequestrin, which are normally expressed in mature adult cardiomyocytes.[109,111] Collectively, these studies suggest that ES-derived cardiomyocytes harbor an immature sarcoplasmic reticulum (SR) and lack a well developed CICR mechanism, which is a prerequisite for functional coupling with the host myocardium. However, it is not clear from these studies whether the immature human ES cardiomyocytes could develop functionally competent SR and CICR over a longer culture period (i.e. >3 weeks). Indeed, electrophysiologic studies on mouse ES cardiomyocytes suggest that these cells develop a functional SR and CICR mechanism in the late stages of differentiation.[112,113] In another study, 35–70% of mouse ES-derived cardiomyocytes demonstrated early afterdepolarizations (EADs) and delayed afterdepolarizations (DADs) in response to pharmacologic treatments that are known to prolong APs.[114] Both EADs and DADs are considered as underlying mechanisms for arrhythmias associated with myocardial disease. During embryonic mouse heart development (E10.5–11.5), it was shown that dual autonomic modulation of both the sympathetic and parasympathetic systems can trigger re-entry arrhythmias in the cells of the primitive
atrioventricular ring (AVR) region.[115] In contrast, both ventricular and atrial myocytes from E10.5–11.5 hearts were not susceptible to re-entry arrhythmias. Furthermore, it was suggested that the existence of such primitive AVR cells in the perinodal tissue of some adult hearts could contribute to re-entrant arrhythmia.[115] It is possible that differentiation conditions favoring development of such primitive AVR cells from ES cultures may partly explain the EADs and DADs observed by Zhang et al.[114] At present, it is not clear whether this induced arrhythmogenic potential of mouse ESderived cardiomyocytes would persist during the later stages of differentiation (i.e. >3 weeks). Taken together, these studies clearly underscore the need for the identification of mechanisms regulating proper maturation of ES-derived cardiomyocytes and also for monitoring the extent of cardiomyogenic differentiation in individual EBs. The latter part is technically challenging and perhaps can be achieved by the use of multiple, lineage-restricted, fluorescent reporters combined with live-cell imaging techniques. 5. Enrichment Methods for ES-Derived Myocardial Cells As discussed in section 1, use of undifferentiated ES cells for transplantation therapies is associated with a potential risk of teratoma development. Furthermore, the presence of undifferentiated cells in the engrafted tissue would also give rise to several undesirable cell lineages (e.g. bone, cartilage, skin). To this end, enrichment of ES-derived myocardial cells prior to transplantation is highly desirable. Enrichment strategies to date have been mainly focused on isolation of differentiated cardiomyocyte populations. Field and colleagues[42] were the first group to describe an elegant genetic selection technique for the enrichment of ES-derived
Table II. Factors increasing cardiomyogenesis of human embryonic stem (ES) cells ES-cell line (human)
Factor
Reference
H9
NGF, HGF, EGF, FGF, RA, TGFβ, activin-A
91
H1, H7, H9, H9.1, H9.2
RA, 5-aza-2′-deoxycytidine
92
HES2, HES3, HES4
Visceral endoderm-like cells
93
HES2, HES3, HES4
Serum-free medium
94
H7 and H1
IGF/PI-3-kinase/Akt signaling pathway
95
H7
Serum-free medium + CCTI
96
Miz-hES2 and HSF-6
5-azacytidine
97
H-9
Nitric oxide
98
BG01V and ReliCellhES1
BMP2 with low serum concentration
99
HUES-1 and I6
BMP2 with SU5402 (FGF receptor inhibitor)
100
H1
FBS
101
HES2, HES3, HES4
SB203580 (p38 MAP kinase inhibitor)
102
H7
Activin A, BMP4
103
BMP = bone morphogenetic protein; CCTI = creatine, carnitine, taurine, and insulin; EGF = epidermal growth factor; FBS = fetal bovine serum; FGF = fibroblast growth factor; HGF = hepatocyte growth factor; IGF = insulin-like growth factor; MAP = mitogen activated protein; NGF = nerve growth factor; PI-3-kinase = phosphatidylinositol-3-kinase; RA = retinoic acid; TGF = transforming growth factor. © 2008 Adis Data Information BV. All rights reserved.
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cardiomyocytes. In this method, undifferentiated ES cells are transfected with a dual drug resistance vector and transfected cells are selected using a hygromycin resistance gene under the control of a phosphoglycerate kinase promoter. Subsequently, the neomycin resistance gene under the control of a lineage-restricted, α cardiac myosin heavy chain (MYH6) promoter is used to select differentiated cardiomyocytes.[26,42] Similar genetic selection schemes harboring drug resistance/fluorescent reporters have been developed by other investigators to facilitate identification of cardiac progenitor cells, ventricular cells, atrial cells, and pacemaker cells.[44] Some investigators also used physical enrichment via dissection of beating areas[116] as well as percoll gradient density centrifugation[92] to enrich ES-derived cardiomyocytes. However, enrichment levels obtained by such physical methods are often less efficient than those of genetic selection methods.[42] Indeed, genetic selection via MYH6-promoted neomycin or puromycin resistance genes yielded cardiomyocyte purities of >90%.[42,117] Although initial gene transfer efforts in human ES cells appeared technically challenging (see Mummery[44]), two groups have successfully developed efficient genetic selection methods for the enrichment of human ES-derived cardiomyocytes.[105,118] Of all the enrichment methods tested to date, selection using an α cardiac MHC promoter appears to yield the highest level of myocyte purification (>90%). However, the α cardiac MYH6 promoter is active in differentiated atrial and ventricular myocytes as well as transiently active in primitive cardiomyocytes during development.[119-122] Because of this, genetic selection using this promoter was shown to enrich a heterogeneous population of cardiomyocytes.[42] In contrast, use of a myosin light chain-2v (MLC-2v) promoter for the enrichment of ES-derived cardiomyocytes was proposed to yield a homogeneous population of ventricular cardiomyocytes.[123] Given the fact that both α MYH6 and MYL2 promoters are also active in the primitive cells of the developing heart,[119-122] further refinements in selection schemes should be developed to rule out the enrichment of primitive myocardial cells with arrhythmogenic potential from ES cultures. While these genetic selection schemes are most suited to laboratory studies, it may be difficult to exploit such strategies for clinical applications. This is mainly due to the quality control issues over a long-term selection process as well as the risk of random integration of reporter genes in genetic loci controlling the vital functions of cardiomyocytes. Perhaps an ideal enrichment strategy for ES-derived myocardial cells would be screening for lineage-specific cell surface receptor expression via fluorescenceactivated cell sorting-based methodologies. Unfortunately, no unique cell-surface markers for cardiomyocytes or their progenitors have been identified. Nonetheless, recent studies have employed innovative fractionation schemes using a combination of intracellular transgene expression (e.g. NKX2-5 and ISL1) and © 2008 Adis Data Information BV. All rights reserved.
Zhang & Pasumarthi
extracellular receptors (FLK1 [KDR] and KIT) for successful enrichment of cardiac progenitor cells from mouse ES cultures.[124-126] These progenitor cells were shown to differentiate into cardiomyocytes, smooth muscle cells, and endothelial cells in vitro.[124-126] Identification of additional cell surface markers, as well as refinement of existing techniques, should facilitate further enrichment of myocardial lineage-specific fractions from ES-cell cultures in the near future. Given the structural and functional heterogeneity reported for ES-derived myocardial cells, it is important to assess whether such immature cells would fully differentiate in vivo after transplantation into diseased hearts. 6. ES-Cell Transplantation for Cardiac Repair In 1996, Field’s group[42] provided the first evidence that genetically selected mouse ES cardiomyocytes could form viable grafts when injected into the uninjured myocardium of dystrophic mice. Subsequently, multiple laboratories transplanted both undifferentiated mouse ES cells and enriched cardiomyocytes in normal as well as MI models (see table III). In some of these studies, mouse cells were injected into rat hearts with minimal or no rejection. Although some studies showed that undifferentiated ES cells could improve cardiac function with no risk of tumors (see table III), other studies clearly documented the ability of unselected ES cells to form teratomas as well as many undesired cell lineages in the heart.[30,117] The observed discrepancy between these studies could be due to the number of cells transplanted and/or differences in the analysis timepoints. Nonetheless, these studies clearly underscore the need for refinement of myocardial cell enrichment techniques from ES cultures. In 2004, Kehat et al.[54] reported the first human ES cardiomyocyte transplantation into the uninjured swine myocardium. Following this report, other investigators injected human ES cells or differentiated cardiomyocytes into the injured myocardium of different species (e.g. rat, mouse, and swine; see table IV). While some groups rationalized the use of immunocompromised nude or severe combined immunodeficiency animals for xenotransplantation studies, the absence of immune rejection in the immunocompetent recipient animals was attributed in part to the low expression or weak immunogenicity of major histocompatibility antigens in ES cells and their derivatives.[142,143] With few exceptions, the majority of ES transplantation studies in the heart utilized reporter genes such as enhanced green fluorescent protein and lacZ for tracking donor cells in the engrafted myocardium. The cardiomyocyte nature of the transplanted cells was confirmed using expression of markers such as cardiac troponin I, sarcomeric α-actin, smooth muscle α-actin, NKX2-5, NPPA (ANF), MYL7 (MLC2a), and MYL2 (MLC2v), in the engrafted areas (see tables III and IV). Consistent with the previous reports on other donor cells, transplantation of ES cardiomyocytes into normal and injured myocardium was shown to improve global myocardial function Biodrugs 2008; 22 (6)
© 2008 Adis Data Information BV. All rights reserved.
Mouse (MI)
Rat (normal)
Mouse (MI)
Mouse (normal)
Mouse (normal)
Mouse (normal)
Mouse (MI)
Mouse (MI)
Mouse (MI)
D3
D3
D3
D3
D3
D3
R1 and HM1
D3
R1
Mouse (MI)
D3
Rat (normal)
Rat (normal and MI)
D3
Sheep (MI)
Mouse (MI)
NA
CGR 8
Rat (MI)
CGR 8
NA
Mouse (MI)
Rat (MI)
CGR 8
Rat (MI)
Rat (MI)
D3
D3
Mouse (normal)
D3
D3
Host (normal or injured)
ES-cell line
Undiff
CM
Undiff
CM
Undiff
CM
Undiff
CM
Undiff
CM
CM
Undiff
Undiff
Undiff
CM
CM
CM
Undiff
CM
CM
Donor ES-cell status 7 wk 6 wk 4 wk
1 × 104 3 × 104 5 × 105
CMV-GFP α Ca. actin, MLC2v-ECFP 2 wk 3 wk 24 h to 5 wk 2 wk 2 wk 1 wk 1 mo 1, 2, 4, 8 wk 6 wk 2 wk
3 × 105 3 × 105
2 × 106 2.5 × 105 1 × 106 30 × 106 1 × 106
1 × 106 106
α Ca. actin
90 d 4 wk 2 wk
3–4 wk 8–9 wk
1.5 × 106 1.5 × 107/(ECT) 3 × 104
3 × 104–105 5 × 104
RNF4-β-Gal, CMV-EGFP α-MHC-pacIRES-EGFP A-MHC-lacZ, EF-lacZ
ND
CMV-IE-GFP
7–30 d
ND
ND
pEF1-EGFP
ND
ND
Nkx2.5-lacZ, α-actin-EYFP
ND
ND
pEF1-EGFP
ES cells labeled with SPIO
1×
6 wk
3 × 105 3 × 105
hCMVIE-GFP CMV-EGFP
ND
Analysis timepoint
No. of cells used
Reporter for cell tracking
Table III. Survey of mouse embryonic stem (ES)-cell transplantation studies
lacZ
Sarcomeric α-actin, CD45, PECAM, vWF
LacZ, GFP, sarcomeric α-actin, smooth muscle α-actin, vWF
CTnT, CTnI
GFP
CTnI, pan-cadherin, ANP, BNP
GFP
GFP, CTnI
CD3, CD4, CD8, CD45R/B220, CD11c, Mac-1, Gr-1
β-MHC, lacZ, Nkx2.5, Ki 67
EGFP, sarcomeric myosin
Sarcomeric α-actin, CD3, CD11c, MHC I, GFP
Sarcomeric α-actin, smooth muscle actin, GFP
ND
ND
α-MHC, CTnI
Troponin-1, α-MHC, GFP
MLC-2v
Sarcomeric α-actin, α-MHC, GFP, CTnI
Dystrophin
Markers used for analysis
ND
+
ND
ND
ND
+
+
ND
ND
+
ND
+
+
ND
ND
ND
+
+
ND
ND
ND
ND
ND
+
ND
ND
ND
+
ND
ND
ND
ND
ND
ND
ND
+
+
ND
ND
ND
Cx43 Angiogenesis expression
Echo
139
117
138
55
137
136
135
134
133
72
132
68
131
130
129
128
63
62
127
42
Reference
Continued next page
EP, MEA
ND
ND
Hemodyn
ND
Echo
Hemodyn
ND
Echo
ND
Echo
Echo
MRI
ECG, Echo
Hemodyn, echo
Echo
Echo
Hemodyn, echo
ND
Assay used to measure functional improvement
ES-Cell Transplantation and Myocardial Repair 367
Biodrugs 2008; 22 (6)
© 2008 Adis Data Information BV. All rights reserved.
α Ca. actin = α cardiac actin; α-MHC = α-myosin heavy chain; ANP = atrial natriuretic peptide; BNP = B-type natriuretic peptide; CFP = cyan fluorescent protein; CM = cardiomyocytes (in some cases enrichment was not performed); CMV = cytomegalovirus; CMV-IE = cytomegalovirus immediate early enhancer; CTnI = cardiac troponin I; CTnT = cardiac troponin T; Cx43 = connexin 43; echo = echocardiography; ECFP = enhanced cyan flourescent protein; ECT = engineered cardiac tissue; EF1a = elongation factor 1a promoter; EGFP = enhanced green fluorescent protein; EP = electrophysiology; EYFP = enhanced yellow fluorescent protein; GFP = green fluorescent protein; hemodyn = hemodynamics; IRES = internal ribosomal entering site; MEA = micro-electrode arrays; MHC I = major histocompatibility complex class I; MI = myocardial infarction; MLC-2v = myosin light chain-2v; MRI = magnetic resonance imaging; NA = not available; ND = not determined; PECAM = platelet/endothelial cell adhesion molecule; RNF4 = ring finger protein 4; SPIO = paramagnetic iron oxide particles; undiff = undifferentiated; vWF = Von Willebrand factor.
88 ND Mouse (normal and MI) CGR 8
Undiff or CM
ND
3 × 105–106
ND ND CFP, α-actinin
Echo
141 ND 2 wk Mouse (MI) R1 and HM1
Undiff
RNF4-lacZ, EGFP
3 × 104
ND ND ANP, sarcomeric cardiac α-actin
ND 3 wk Mouse (normal and MI) R1; CGR 8; C57
Undiff
pCX (β-actin)EGFP
5 × 105
ND ND GFP; α-fetoprotein, sarcomeric α-actin, smooth muscle α-actin, neurofilament, MY-32, CD45
Assay used to measure functional improvement Cx43 Angiogenesis expression Markers used for analysis Analysis timepoint No. of cells used Reporter for cell tracking Donor ES-cell status Host (normal or injured) ES-cell line
Table III. Contd
140
Zhang & Pasumarthi
Reference
368
using a wide range of techniques such as echocardiography, ECG, MRI, millar pressure-volume catheters, and microelectrode arrays. Analysis timepoints varied anywhere between 24 hours and 3 months post cell transplantation (tables III and IV). One obvious hurdle in this field is the sustained viability of donor cells in the engrafted myocardium.[151] A recent study from Murry and colleagues[103] found that pre-treatment of human ES cardiomyocytes with prosurvival agents increased cell survival in the infarcts as well as improving myocardial function 4 weeks after transplantation. Although a similar result was obtained by Mummery’s group using untreated human ES cardiomyocytes, the functional improvement observed at the 4-week timepoint was not apparent 12 weeks after transplantation.[148] In this regard, a number of scenarios have been discussed in the accompanying editorials, including the possibility of differences in cardiomyocyte content of the starting cell preparations.[152,153] To circumvent a possible decrease in the graft size over time, use of ES-derived cardiac precursor cells,[124-126] which may have a higher proliferative potential, has been proposed.[9,153] Given the potential of ES-derived cardiac progenitors to yield a heterogeneous group of cells, caution should be exercised in the assessment of their differentiation potential and Ca2+ handling status following intra-cardiac transplantation. Although a mechanistic basis for functional improvement following cell transplantation studies is not well understood, multiple possibilities have been proposed. Some possible mechanisms include donor cell-mediated increases in cell-to-cell coupling, angiogenesis, or paracrine pathways triggering a favorable remodeling process.[9,153] With regard to ES cardiomyocyte transplantation, some studies documented increases in angiogenesis of the engrafted myocardium. Furthermore, expression of connexin 43 (Cx43) was also observed in the membrane junctions between adjacent donor and host cardiomyocytes, indicating a potential for functional coupling (see tables III and IV). Indeed, intra-cardiac transplantation of Cx43-expressing embryonic cardiomyocytes (E14.5–16.5) was shown to prevent post-infarct arrhythmias in experimental models.[13] While it is tempting to speculate that ESderived cardiomyocytes may also suppress the arrhythmogenic risk of infarcted myocardium in vivo, caution should be exercised given the documentation of abnormal electrophysiologic behavior and immature Ca2+ handling properties of ES cardiomyocytes in vitro.[45,114] Further studies are required to confirm functional coupling between transplanted ES-derived cardiomyocytes and the host myocardium using well established techniques such as three-dimensional electrophysiologic mapping and multiphotonand Ca2+ indicator-based imaging techniques in situ or invivo.[13,16,54] Biodrugs 2008; 22 (6)
© 2008 Adis Data Information BV. All rights reserved.
Rat (MI)
Rat (MI)
HUSE-1; I6
H 9.2; I6
(normal)
Mouse
H1
Analysis timepoint
HLA-DR, slow/fast
muscle α-actin
troponin smooth
3–4 wk
EBs, CM
0.5–1 × 106
MHC, actinin,
ND
4–8 d
Undiff;
A/C, ANP
beating
Anti-human β-MHC,
3 × 106
2 mo
+
+
+
+
ND
+
ND
ND
ND
ND
ND
+
ND
Cx43 Angiogenesis expression
CTnI, Pan-cadherin, +
α-actin
GFP, sarcomeric
ANP, PCNA
7–28 d
3 wk
EBs
100 beating
106
GFP
fast skeletal MHC
S-100 protein,
β-III-tubulin,
anti-human lamin
ND
ND
ND
48–72 h
pan-cytokeratins,
targets
ND
ANP, MLC-2v,
pancentromeric
Lenti-CAG-GFP
α-actin, N-cadherin,
Alu repeat,
α-fetoprotein,
smooth muscle
Sarcomeric α-actin, β-MHC, α-MHC,
4 wk
α-actin
CTnI, sarcomeric
mitochondria Ab,
Anti-human
Markers used for analysis
Y-chromosome,
0.5–10 × 106
EBs
40–150 beating 1–3 wk
No. of cells used
human probes:
ISH with
ND
Reporter for cell tracking
(EBs), no
Undiff
CM
CM
CM
(normal)
Mouse (MI)
Pacemaker
CM
Guinea pig
H7
H1
(normal)
Rat
EBs
(normal)
H1 and H7
Beating
Swine
H9.2
Donor ES-cell status
Host (normal or injured)
ES-cell line
Table IV. Survey of human embryonic stem (ES)-cell transplantation studies
Echo
ND
ND
MRI
147
100
53
146
145
144
54
Reference
Continued next page
in vitro MEA
AP mapping,
In vivo optical
ND
mapping
Electroanatomic
Assay used to measure functional improvement
ES-Cell Transplantation and Myocardial Repair 369
Biodrugs 2008; 22 (6)
© 2008 Adis Data Information BV. All rights reserved.
Rat (MI)
Mouse (MI)
Rat (MI)
Mouse
H7
HES3-GFP
HES3-GFP
H1
Analysis timepoint
2–3 d
actin, MLC-2a,
timepoints
desmoplakin 1 and
Pan-cadherin,
MF20, cytokeratin
α-actinin, α-MHC,
tropomyosin,
GFP, sarcomeric
Various
laminin
desmoplakin,
muscle α-actin,
Ki 67, smooth
MLC-2a, MLC-2v,
troma 1, PECAM-1,
tropomyosin,
GFP, α-actinin,
mitochondrial Ab,
ND
+
ND
ND
ND
ND
measurement
Force
ND
MRI
Echo, MRI
Assay used to measure functional improvement
150
149
148
103
Reference
nuclear antigen; PECAM-1 = platelet/endothelial cell adhesion molecule-1; undiff = undifferentiated; + indicates positive.
myocardial infarction; MLC-2a = myosin light chain-2a; MLC-2v = myosin light chain-2v; MRI = magnetic resonance imaging; ND = not determined; PCNA = proliferating cell
troponin I; Cx43 = connexin 43; EBs = embryoid bodies; echo = echocardiography; GFP = green fluorescent protein; ISH = in situ hybridization; MHC = myosin heavy chain; MI =
Ab = antibody; Alu repeat = short repetitive elements defined by Alu enzyme; ANP = atrial natriuretic peptide; AP = action potential; CM = cardiomyocytes; CTnI = cardiac
mitochondria
α-actinin, human
clusters
3–10 beating
2 × 106
ND
Cx43 Angiogenesis expression
Anti-human nuclear/ +
Nkx 2.5, MLC-2v
CTnI, human
pan-cadherin,
MHC, β-MHC,
Sarcomeric
Markers used for analysis
slices)
ND
ND
probe
12 wk
pancentromeric
2 d, 1 wk, 3 wk, 10 wk,
0.2–1 × 106
3.9 ± 0.8 × 107 4 wk
No. of cells used
human-specific
ISH with a
ND
Reporter for cell tracking
2, vimentin, cardiac
CM
CM
CM
CM
Donor ES-cell status
ventricular
(ischemic
Host (normal or injured)
ES-cell line
Table IV. Contd
370 Zhang & Pasumarthi
Biodrugs 2008; 22 (6)
ES-Cell Transplantation and Myocardial Repair
7. Conclusion and Future Perspectives Recent studies suggest that transplantation of donor cells in diseased myocardium can improve myocardial function over a short period of time (1–4 weeks). While long-term follow-up studies are warranted, it is generally perceived that the beneficial effects of transplanted cells are mainly due to increased angiogenesis or favorable scar remodeling in the engrafted myocardium. With the exception of fetal cardiomyocytes, other donor cells are incapable of electrical coupling with the host myocardium. In this regard, ES cells serve as an attractive source for the generation of unlimited quantities of cardiomyocytes for myocardial repair. The initial success in the application of ES cells to partially repair and improve myocardial function in experimental models of heart disease has been quite promising. However, multiple hurdles need to be crossed before the potential benefits of ES cells can be translated to the clinic. Given the heterogeneity of Ca2+ handling proteins and the electrophysiologic properties of ES-derived cardiomyocytes, current enrichment methods should be further refined to derive a homogenous population of ES cardiomyocytes. In addition, electrical coupling of ES-derived cardiomyocytes with the host myocardium is yet to be confirmed at the cellular level. This is particularly important in view of the increased arrhythmogenic risk seen with skeletal myoblast transplantation in phase I clinical trials. An urgent requirement in this field is to perform long-term monitoring for the incidence of arrhythmias and teratomas in animals transplanted with ES cardiomyocyte preparations. A more cautious approach to the validation of ES cardiomyocytes in experimental models would certainly prevent future disappointments as seen with skeletal myoblast studies. In addition, future studies should focus on optimizing the yield of cardiomyocytes from ES-cell cultures as well as developing ethically approved methods for derivation of patient-specific ES-cell lines. In view of our initial progress in the validation of ES-derived cardiomycoytes as a potential donor cell type, we should have an optimistic mindset to sail across the hurdles toward an ultimate clinical realization. Acknowledgments We apologize to those whose work could not be cited because of space limitations. We thank the Canadian Institutes of Health Research and the Heart and Stroke Foundation of Canada for support. Dr Pasumarthi is a New Investigator of the Heart and Stroke Foundation of Canada. We thank Karim Wafa, Sarah Remley, and Adam Hotchkiss (members of the Pasumarthi laboratory) for their helpful comments on this manuscript. The authors have no conflicts of interest that are directly relevant to the content of this review.
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Correspondence: Dr Kishore B.S. Pasumarthi, Department of Pharmacology, Dalhousie University, Sir Charles Tupper Building, 5850 College Street, Halifax, B3H 1X5, Canada. E-mail:
[email protected]
Biodrugs 2008; 22 (6)