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. 2019 Mar 15;42(3):200–209. doi: 10.14348/molcells.2019.2439

Directed Differentiation of Pluripotent Stem Cells by Transcription Factors

Yujeong Oh 1, Jiwon Jang 1,2,*
PMCID: PMC6449710  PMID: 30884942

Abstract

Embryonic stem cells (ESCs) and induced pluripotent stem cells (iPSCs) have been used as promising tools for regenerative medicine, disease modeling, and drug screening. Traditional and common strategies for pluripotent stem cell (PSC) differentiation toward disease-relevant cell types depend on sequential treatment of signaling molecules identified based on knowledge of developmental biology. However, these strategies suffer from low purity, inefficiency, and time-consuming culture conditions. A growing body of recent research has shown efficient cell fate reprogramming by forced expression of single or multiple transcription factors. Here, we review transcription factor-directed differentiation methods of PSCs toward neural, muscle, liver, and pancreatic endocrine cells. Potential applications and limitations are also discussed in order to establish future directions of this technique for therapeutic purposes.

Keywords: differentiation, embryonic stem cell, pluripotent stem cell, transcription factor

INTRODUCTION

Pluripotent stem cells (PSCs), including embryonic stem cells (ESCs) and induced pluripotent stem cells (iPSCs), hold great promise in many biomedical fields. Indefinite proliferation of PSCs provides an unlimited cell source. Pluripotent differentiation potential enables PSCs to generate any desired cell type in vitro. PSC-derived cells such as neurons are particularly valuable for human due to the lack of alternative sources. Therefore, generation of functional and fully differentiated cells from PSCs has been an active field of stem cell research. Common strategies rely on a vast knowledge of developmental biology learned from animal studies. Small molecules and recombinant signaling proteins have been applied to PSC differentiation in order to derive specific lineage cells. Despite the attempt to faithfully mimic in vivo development, these approaches suffer from several major limitations. The first limitation is that procedures are time-consuming. Neural differentiation, for example, usually takes 4~6 weeks and functional maturation requires a few more months depending on neuronal subtypes (Tao and Zhang, 2016; Xie et al., 2013). The second limitation is variability with low purity. Dramatic difference in differentiation potentials across particular PSC lines has been well documented in recent studies (Bock et al., 2011; Hu et al., 2010; Kajiwara et al., 2012; Kim et al., 2011; Koyanagi-Aoi et al., 2013; Osafune et al., 2008; Wu et al., 2007). This variability influences the response of PSCs to signaling molecules, resulting in different purity of desired cell types. Furthermore, difficulty in quality control of small molecules and recombinant proteins adds more variability to protocols. Given that large scale production of mature cells with high purity is necessary for clinical applications, alternative strategies might shed light on how to produce disease-relevant cell types from PSCs.

During embryonic development, cell fates are determined by a network of transcription factors. Consistently, successful reprogramming of cell fates by forced induction of single or a combination of transcription factors has been reported. Most strikingly, overexpression of four transcription factors (OCT4, SOX2, KLF4, c-MYC) can reprogram fibroblasts to PSCs (Takahashi et al., 2006). In some cases, single transcription factor is sufficient for direct reprogramming of fibroblasts to other cell types such as neurons and myoblasts (Chanda et al., 2014; Davis et al., 1987). These examples are very striking because cell fate acquisition relies on sequential requirement of multiple transcription factors over the course of development according to traditional views. To test the feasibility of transcription factor-directed PSC differentiation, systemic induction of transcription factors has been performed in mouse ESCs (mESCs)(Correa-Cerro et al., 2011; Nishiyama et al., 2009). Interestingly, 63 out of 137 transcription factors were able to initiate and direct specific differentiation programs when they were induced individually, suggesting that transcription factor induction could be an efficient strategy to direct PSC differentiation. In this review, we present PSC differentiation methods based on transcription factor induction. Potential limitations of this approach and possible solutions are also discussed.

NEURONS

Producing functionally mature neurons from human PSCs (hPSCs) is important to understand normal physiology of human neurons and pathology of neurological diseases. Conventional methods follow the developmental path of neuronal derivation. First, PSCs are differentiated into neural progenitor cells (NPCs) by embryoid body formation or dual SMAD inhibition (Chambers et al., 2009). After that, NPCs are directed into specific neurons by a combination of signaling molecules (Tabar and Studer, 2014; Tao and Zhang, 2016). Based on the finding that forced expression of three transcription factors (BRN2, ASCL1, and MYT1L) can reprogram mouse fibroblasts into functional neurons (Vierbuchen et al., 2010), whether the same combination of transcription factors could bypass the long developmental path from hPSCs to neurons has been tested (Pang et al., 2011). Surprisingly, hPSCs expressing these three transcription factors showed bipolar neuron-like morphologies as early as day 3. They expressed neuronal markers such as β-III-tubulin (also known as Tuj1) and MAP2 by day 8. Electrophysiological analysis showed that these hPSC-derived neurons generated action potentials as early as day 6. The rapid induction of neuronal fate implicates that transcription factor induction can bypass sequential developmental stages and drive direct differentiation of hPSCs into neurons. More strikingly, a single transcription factor, ASCL1, was sufficient to drive direct neuronal differentiation of both human and mouse PSCs (Chanda et al., 2014; Pang et al., 2011; Yamamizu et al., 2013). BRN2 and MYT1L likely contribute to neuronal maturation by increasing morphological complexity. ASCL1 induction during mESC differentiation increased the percentage of neural cells (PSA-NCAM+) from less than 5% (no ASCL1 induction) to almost 50%, highlighting the robustness of transcription factor-directed differentiation (Yamamizu et al., 2013). Other transcription factors previously known to play important roles in neurogenesis were also tested. Ectopic expression of NEUROG2 can efficiently drive mouse and human PSCs into pure excitatory neurons in less than two weeks (Thoma et al., 2012; Zhang et al., 2013). These NEUROG2-directed neurons showed neuronal transcription profiles, formed synapses, and produced robust action potentials. Furthermore, when these human neurons were transplanted into mouse brain, functional integration and active electrophysiological properties were observed (Zhang et al., 2013), suggesting potential applications of these neurons for cell replacement therapy. Forced induction of another proneural transcription factor, NEUROD1, also drove rapid differentiation of hPSCs into excitatory neurons (Zhang et al., 2013).

GABAergic interneurons are inhibitory neurons that balance neuronal excitation in the brain. Given that the majority of cortical interneurons are originated from the medial ganglionic eminence (MGE)(Wonders and Anderson, 2005), four transcription factors (ASCL1, DLX2, NKX2.1, and LHX6) have been chosen based on their expression in the MGE (Sun et al., 2016). Through extensive comparison, a combination of three transcription factors (ASCL1, DLX2, and LHX6) has been found to be able to drive hPSCs into GABA and MAP2 double-positive neurons within 10 days (Sun et al., 2016). Co-expression of miR-9/9* and miR-124 further increased the efficiency of interneuron derivation. These GABAergic interneurons exhibited electrophysiological properties within 6~8 weeks and functionally integrated into the host’s neural circuit upon transplantation to mouse brain (Sun et al., 2016). In another study, co-expression of ASCL1 and DLX2 was sufficient to differentiate hPSCs into GA-BAergic interneurons with ~90% efficiency (Yang et al., 2017). These interneurons showed electrophysiological properties at five weeks after transcription factor induction and survived well in the transplanted mouse brain. Interestingly, ASCL1 also contributed to the conversion of hPSCs into dopaminergic neurons when it was co-expressed with NURR1 and LMX1A (Theka et al., 2013). This combination of transcription factors produced mature and functional dopaminergic neurons within 21 days.

Motor neurons are typically produced from PSC-derived NPCs that are caudalized and ventralized by retinoic acid and sonic hedgehog, respectively (Li et al., 2005; Wichterle et al., 2002). These methods suffer from a long and inefficient differentiation process. To overcome such problem, motor neuron-specifying transcription factors have been identified based on temporal gene expression analysis upon retinoic acid/sonic hedgehog treatment (Hester et al., 2011). Forced expression of three transcription factors, NEUROG2, ISL1, and LHX3, in hPSC-derived NPCs accelerated motor neuron differentiation (Hester et al., 2011). At day 11 post transcription factor induction, cells expressed motor neuron markers HB9 and CHAT, formed neuromuscular junctions, and exhibited electrophysiological properties. Given that conventional methods using retinoic acid and sonic hedgehog take ~45 days to acquire mature motor neurons, transcription factor-directed motor neuron derivation could be a faster and more efficient alternative method. ISL1–LHX3 fusion proteins can also drive mESCs into mature motor neurons in the absence of sonic hedgehog by suppressing a spinal interneuron fate (Lee et al., 2012).

Many studies described above used a lentiviral vector for transcription factor delivery because this viral vector could infect PSCs in a highly efficient manner and drive stable expression of transgenes by host genome integration. However, host genome modifications could be a potential problem in terms of using transcription factor-directed differentiation methods in a clinical setting. To circumvent this issue, researchers have exploited alternative gene deliver tools such as protein transduction, synthetic mRNAs, and non-integrating viral vectors. For example, a cocktail of synthetic mRNAs encoding five transcription factors (NEUROG1, NEUROG2, NEUROG3, NEUROD1, and NEUROD2) induced rapid differentiation of hPSCs toward neurons (Goparaju et al., 2017). Synthetic mRNA-directed neurons showed electrophysiological properties as early as 7 days after mRNA transfection. A combination of synthetic mRNAs encoding ATOH1 and NEUROG2 was also tested to differentiate hiP-SCs into mature dopaminergic neurons (Xue et al., 2018). Delivery of three transcription factors, LHX3, NEUROG2, and ISL1, by non-integrating Sendai virus vectors efficiently drove hPSCs into HB9-positive and ChAT-positive motor neurons within two weeks after transduction (Goto et al., 2017). These examples suggest that transcription factor-directed differentiation methods can be further improved for clinical applications. The methods described above are summarized in Table 1.

Table 1.

Transcription factor-directed PSC differentiation toward neurons

Cell Line Final Cell Type Transcription Factor Delivery Method Time to Functional Cell Differentiation Efficiency Functional Test Therapeutic Effect Reference
mESC Excitatory neuron NEUROG2 Stable transfection ~10 days 40% (TuJ1+) Electrophysiology
Coculture with primary neurons		 ND Thoma et al., 2012
mESC Excitatory neuron ASCL1 Lentiviral vector ~5 days ND Electrophysiology ND Chanda et al., 2014
hESC ~28 days
hESC, hiPSC Excitatory neuron Either NEUROG2 or NEUROD1 Lentiviral vector ~2 weeks ~100% (MAP2+), ~100% (NeuN+) Electrophysiology
Calcium imaging
Transplantation into mouse brain		 ND Zhang et al., 2013
hESC Excitatory neuron NEUROG2, SATB2, FEZF2 Lentiviral vector ~35 days NEUROG2: 83% (MAP2+)
NEUROG2+FEZF2: 64% (MAP2+)
NEUROG2+SATB2: 49% (MAP2+)		 Electrophysiology
Transplantion into organotypic slice cultures of adult human cortex.		 ND Miskinyte et al., 2018
hESC GABAergic neuron ASCL1a, DLX2, LHX6, miR-9/9*, miR-124 Lentiviral vector ~6 weeks 81.3% (MAP2+)
84.5% (GABA+/MAP2+)		 Electrophysiology
Transplantation into mouse brain		 ND Sun et al., 2016
hESC GABAergic neuron ASCL1, DLX2 Lentiviral vector ~5 weeks 89.1% (GABA+/MAP2+) Electrophysiology
Transplantation into mouse brain		 ND Yang et al., 2017
hiPSC Dopaminergic neuron ASCL1, NURR1, LMX1A Lentiviral vector ~21 days 51% (TuJ1+) Electrophysiology
Dapamine release
Transplantation into mouse brain		 ND Theka et al., 2013
hiPSC Dopaminergic neuron ATOH1, NEUROG2 Synthetic mRNA 36–49 days >90% (TuJ1+)
>97% (TH+/TuJ1+)		 Electrophysiology
Dopamine release		 ND Xue et al., 2018
hESC, hiPSC Motor neuron NEUROG2, ISL1, LHX3 Adenoviral vector ~21 days 49~72% (HB9+CHAT+) Electrophysiology
Coculture with C2C12-derived myotubes		 ND Hester et al, 2011
hESC, hiPSC Motor neuron NEUROG1, NEUROG2, NEUROG3, NEUROD1, NEUROD2 Synthetic mRNA ~7 days 98.2% (TuJ1+)
83.2% (MAP2+/TuJ1+)
94.3% (HB9+/TuJ1+)
97.7% (ChAT+/TuJ1+)
100% (ISL1+/TuJ1+)		 Electrophysiology
Calcium imaging		 ND Goparaju et al., 2017
hiPSC Motor neuron LHX3, NEUROG2, ISL1 Sendai virus vector ~14 days >90% (TuJ1+), >90% (HB9+) Electrophysiology
Coculture with human myocytes		 ND Goto et al., 2017
mESC Motor neuron ISL1–LHX3 fusion protein Genetic recombination ~6 days 77% (HB9+/TuJ1+) Coculture with C2C12-derived myotubes ND Lee et al., 2012
hESC, hiPSC Neuron BRN2, ASCL1, MYT1L Lentiviral vector ~6 days ND Electrophysiology ND Pang et al., 2011
hESC Neuron Either NEUROG1, NEUROG2, NEUROG3, NEUROD1, or NEUROD2. PiggyBac vector ~7 days 40~90% (HuC/D+) Electrophysiology
Calcium imaging		 ND Matsushita et al., 2017
hiPSC Neuron NEUROG1, NEUROG2 Lentiviral vector ~14 days >90% (MAP2+), >90% (SYN1+) Electrophysiology ND Busskamp et al., 2014
mESC Neuron Ascl1 Genetic recombination ~11 days 8.3% (TH+/TuJ1+)
37.6% (ISL1+/TuJ1+)
27.2% (GABA+/TuJ1+)		 Electrophysiology ND Yamamizu et al., 2013
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a

ASCL1: mutant form of ASCL1 in which five serine residues are substituted with alanine

ND: Not Determined

PANCREATIC β-CELLS

β-cells are a type of endocrine cells in the pancreas that can produce insulins to control blood glucose levels. Because transplantation of β-cells is a promising approach to treat diabetes patients, many researchers have been working on generating functional β-cells from PSCs. Common and conventional methods for β-cell derivation follow the developmental process of pancreas (Van et al., 2009). PSCs are first induced into definitive endoderm which is further specified into pancreatic lineage cells. To facilitate β-cell differentiation, PAX4, an essential transcription factor for β-cell development, is overexpressed in mESCs (Blyszczuk et al., 2003). Constitutive expression of PAX4 increased the formation of insulin-producing cells from 10~20% to 60~80%. Furthermore, transplantation of PAX4-directed insulin-producing cells maintained normal blood glucose levels in streptozotocin-induced diabetic mice.

Other studies have also confirmed that forced induction of PAX4 could be an efficient method to derive insulin-producing β-cells from mouse and human PSCs (Liew et al., 2008; Lin et al., 2007). Other transcription factors that play key roles in pancreatic development have also been tested in PSCs. Forced expression of PDX1 could facilitate mESC differentiation toward insulin-producing cells although these cells lacked mature properties such as high insulin secretion and glucose-responsiveness (Miyazaki et al., 2004). It has been reported that biphasic induction of PDX1 that mimic the normal development of pancreatic β-cells had better effects on mouse and human ESC differentiation than constitutive expression (Bernardo et al., 2009). The ESC-derived β-cells secreted insulins and C-peptides. However, they failed to respond to glucose stimulation, suggesting that PDX1 alone might not be sufficient for mature β-cell derivation from PSCs. However, a later study reported that mESC-derived insulin-producing cells by PDX1 overexpression were glucose-responsive. They reduced hyperglycemia when they were transplanted into streptozotocin-induced diabetic mice (Raikwar and Zavazava, 2012). Such discrepancy could be due to different differentiation media conditions used to differentiate PDX1-expressing ESCs into insulin-producing cells. PDX1 induction has also been proven to be useful for β-cell derivation when it is combined with other transcription factors such as NKX6.1 and NEUROG3 (Ida et al., 2018; Kubo et al., 2011; Walczak et al., 2016). Moreover, it has been reported that induction of NKX2.2 alone can result in appearance of insulin-producing cells (stained by Dithizone) as early as 14 days in mESC-derived embryoid bodies although glucose-dependent secretion is not observed (Shiroi et al., 2005). Overall, forced induction of pancreatic transcription factors tested so far can drive a pancreatic β-cell fate from PSCs, although functional maturation might require other transcription factor networks.

Transcription factor-directed methods for pancreatic β-cell differentiation are summarized in Table 2.

Table 2.

Transcription factor-directed PSC differentiation toward pancreatic β-cells

Cell Line Final Cell Type Transcription Factor Delivery Method Time to Functional Cell Differentiation Efficiency Functional Test Therapeutic Effect Reference
mESC Insulin-producing cell PAX4 Stable transfection ~36 days 80% (Insulin+) Insulin release
Transplantation to diabetic mice		 Reduce blood glucose levels in diabetic mice Blyszczuk et al., 2003
mESC Insulin-producing cell PAX4 Plasmid transfection ~18 days 55% (Insulin+) Insulin release
Transplantation to diabetic mice		 Reduce blood glucose levels in diabetic mice Lin et al., 2007
hESC Pancreatic β-cell PAX4 Stable transfection ~28 days ND Proinsulin synthesis
C-peptide release		 ND Liew et al., 2008
hESC Pancreatic β-cell PDX1-VP16a Stable transfection ~17 days ND Insulin expression ND Bernardo et al., 2009
mESC ~28 days 32% (C-peptide+) Insulin release
C-peptide release
mESC Insulin-producing cell PDX1 Genetic recombination 16–24 days ND Insulin release
C-peptide expression		 No effect Miyazaki et al., 2004
mESC Insulin-producing cell PDX1-AcGFP fusion protein Stable transfection ~23 days 25~30% (Insulin+) Insulin release
Transplantation to diabetic mice		 Reduce blood glucose levels in diabetic mice Raikwar and Zavazava, 2012
hiPSC Insulin-producing cell PDX1-VP16a, NKX6.1 Lentiviral vector ~17 days ND Insulin release
C-peptide expression		 ND Walczak et al., 2016
hESC Pancreatic endocrine cell PDX1, NKX6.1, siPOU5F1 Synthetic mRNA ~13 days 5.6% (Insulin+) Insulin, glucagon, and somatostatin expression ND Ida et al., 2018
mESC Insulin-producing cell PDX1, NEUROG3 Genetic recombination ~18 days 43% (Insulin+) Insulin expression
C-peptide, glucagon, and somatostatin release		 ND Kubo et al., 2011
mESC Insulin-producing cell NKX2.2 Stable transfection ~14 days 1% (Dithizone+) Dithizoneb staining
Insulin release		 ND Shiroi et al., 2005
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a

PDX1 fused to the transactivator domain of the VP16 proteins from herpes simplex

b

A zinc-chelating agent known to stain β-cell

ND: Not Determined

SKELETAL AND CARDIAC MUSCLES

Muscular dystrophies including Duchenne muscular dystrophy and limb girdle muscular dystrophy are inherited disorders with skeletal muscle degeneration (Mercuri et al., 2013). PSC-derived skeletal muscles could be a promising source for transplantation therapy and disease modeling. Based on previous findings that MYOD1, a master transcription factor of myogenesis, can convert non-muscle cells into skeletal myocytes (Davis et al., 1987; Weintraub et al., 1989), whether MYOD1 induction could direct PSCs into skeletal muscles has been tested. MYOD1 overexpression facilitated myogenesis in mESC-derived embryoid bodies and generated skeletal muscle fibers (Dekel et al., 1992). However, only a subset of differentiating cells could be differentiated into skeletal muscles. Other studies have also confirmed that MYOD1 overexpression can induce myogenesis in mESCs (Ozasa et al., 2007; Yamamizu et al., 2013). Interestingly, MYOD1 is unable to induce the myogenic program in hESCs, although extensive myogenic conversion has been observed in human fibroblasts (Albini et al., 2013). However, co-expression of SWI/SNF component BAF60C (encoded by SMARCD3) and MYOD1 is capable of driving hESCs into muscle cells, suggesting that the presence of epigenetic barriers can block MYOD1 functions in hESCs (Albini et al., 2013). BAF60C2/MYOD1-directed myospheres showed spontaneous contraction as well as typical skeletal muscle markers (myogenin, MyH3, and MyH8) at 20 days after differentiation. Ectopic expression of the catalytic domain of histone demethylase JMJD3 also enabled MYOD1 to activate the myogenic program in hPSCs (Akiyama et al., 2016). However, another study has been reported that MYOD1 alone is sufficient to drive hiPSCs into skeletal muscles (Tanaka et al., 2013). Such difference could be attributed to different media conditions used for muscle differentiation or variability related to hESC and hiPSC lines. More studies are warranted in order to make a clear answer to this issue.

PAX3 is a key transcription factor that initiates myogenesis in early paraxial mesoderm. Consistently, forced expression of PAX3 in mESC-derived embryoid bodies can greatly promote myogenic differentiation (Darabi et al., 2008). Myo-genic progenitor cells can be further enriched from PAX3-directed cells by sorting out a PDGFαR+Flk1− population. Transplantation of PAX3-directed PDGFαR+Flk1− cells has shown potential for therapeutic engraftment in dystrophic mice (Darabi et al., 2008). Like PAX3, overexpression of PAX7 can also efficiently drive both human and mouse ESCs into muscle progenitor cells with muscle regeneration potential (Darabi et al., 2011, 2012).

To facilitate myocardial differentiation, transient overexpression of ISL1, a cardiac progenitor marker, has been tested in mESCs. Transfection of mESC-derived embryoid bodies with a ISL1-expressing construct increased the expression of cardiomyocyte markers (ACTC1, MLC2V, MYH7, SMA), suggesting an instructive role of ISL1 in myocardial differentiation (Kwon et al., 2009). The effect of ISL1 on myocardial differentiation has also been confirmed in hESCs by ISL1 protein transduction (Fonoudi et al., 2013). A combined delivery of three transcription factors, GATA4, MEF2C, and TBX5, to mESC-derived embryoid bodies activated the cardiac program and increased the efficiency of cardiomyocyte derivation up to 60% (Bai et al., 2015). Another combination of five transcription factors, GATA4, MEF2C, TBX5, ESRRG and MESP1, has been tested in hPSCs. Delivery of these transcription factors to hPSC-derived mesoderm strongly promoted cardiomyocyte differentiation (Jin et al., 2018). Furthermore, a single transcription factor, SHOX2, greatly facilitated the derivation of cardiac pacemaker cells when it was delivered into mESC-derived embryoid bodies (Ionta et al., 2015). Most SHOX2-directed embryoid bodies exhibited spontaneous beating. When they were transplanted to the left ventricular apex of rat heart, SHOX2-directed embryoid bodies functioned as biopacemakers. Thus, many attempts with single or a combination of transcription factors have been made to produce functional muscle cells from PSCs. However, it seems that transcription factor-directed differentiation methods are not yet mature enough to produce highly pure muscle cells with functional maturity in a short culture period. New combinations of transcription factors together with small-molecule epigenetic inhibitors should be tested to further improve PSC-derived muscle derivation in the future. Transcription factor-directed methods for muscle cell differentiation are summarized in Table 3.

Table 3.

Transcription factor-directed PSC differentiation toward skeletal and cardiac muscle cells

Cell Line Final Cell Type Transcription Factor Delivery Method Time to Functional Cell Differentiation Efficiency Functional Test Therapeutic Effect Reference
mESC Skeletal muscle MYOD1 Plasmid transfection >13 days 20–50% Skeletal muscle marker expression ND Dekel et al., 1992
mESC Myocyte MYOD1 Genetic recombination ~5 days ~60% (MHC+Myogenin+) Skeletal muscle marker expression
Cell fusion assay with C2C12 mouse myoblast cells		 ND Yamamizu et al., 2013
hiPSC Skeletal myocyte MYOD1 PiggyBac vector ~9 days 70–90% (MHC+) Skeletal muscle marker expression
Cell fusion assay with C2C12 mouse myoblast cells
Transplantation to mice		 ND Tanaka et al., 2013
mESC Skeletal muscle MyoD Genetic recombination ~6 days 66% (MHC+)
23% (dystrophin+)		 Skeletal muscle marker expression
Transplantation to mice		 ND Ozasa et al., 2007
hESC Skeletal muscle BAF60C2, MYOD1 Lentiviral vector ~20 days 60.1%(MHC+) Skeletal muscle marker expression
Intracellular calcium recording
Contractile properties		 ND Albini et al., 2013
hESC Skeletal muscle JMJD3, MYOD1 JMJD3: PiggyBac vector
MYOD1: Synthetic mRNA		 ~5 days 57% (MHC+) Skeletal muscle marker expression
Contractile properties		 ND Akiyama et al., 2016
hESC, hiPSC Synthetic mRNA 34~64% (MHC+) Skeletal muscle marker expression
Cell fusion assay with C2C12 mouse myoblast cells
mESC Skeletal myogenic progenitor PAX3 Genetic recombination ~12 days 72.2% (Myogenin+)
78.4%(MHC+)		 Myogenic progenitor marker expression
Transplantation to mice
Contractile properties		 Improved isometric tetanic force and rotarod performance in mdx micea Darabi et al., 2008
mESC Skeletal myogenic progenitor PAX7 Genetic recombination ~5 days 84.4%(MHC+) Myogenic progenitor marker expression
Transplantation to mice
Contractile properties		 Improved isometric tetanic force in cardiotoxin-injured mdx mice Darabi et al., 2011
hESC, hiPSC Skeletal myogenic progenitor PAX7 Lentiviral vector ~14 days 87~91% (Myogenin+)
93~96% (MHC+)		 Myogenic progenitor marker expression
Transplantation to mice
Contractile properties		 Improved isometric tetanic force in immunodeficient mdx mice Darabi et al., 2012
mESC Cardiomyocyte ISL1 Plasmid transfection ~8 days 4.01%(Myh7+) Cardiomyocyte marker expression ND Kwon et al., 2009
hESC Cardiomyocyte ISL1 Protein transduction ~8 days 75% (beating area) Cardiomyocyte marker expression
Spontaneous contractile properties		 ND Fonoudi et al., 2013
mESC Cardiomyocyte GATA4, MEF2C, TBX5 Bacterial injection ~12 days 61% (MHC+) Cardiomyocyte marker expression
Spontaneous contractile properties		 ND Bai et al., 2015
hESC, hiPSC Cardiomyocyte GATA4, MEF2C, TBX5, ESRRG, MESP1 Bacterial injection ~14 days 55~62%(cTnT+) Cardiomyocyte marker expression
Spontaneous contractile properties		 ND Jin et al., 2018
mESC Cardiac pacemaker cell SHOX2 Adenoviral vector ~10 days 83% (beating embryoid body) Electrophysiological properties
Transplantation to the rat heart		 Induced biological pacing in rat hearts Ionta et al., 2015
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a

mdx mice: mouse model for Duchenne muscular dystrophy (DMD)

ND: Not Determined

HEPATOCYTES

Liver transplantation is a promising treatment for end-stage liver diseases. PSC-derived hepatocytes could not only be unlimited sources for cell therapy, but also serve as an experimental model for metabolic diseases. Several key transcription factors for liver development have been tested to develop directed PSC differentiation methods. HEX (also known as HHEX) is an essential transcription factor that functions at the early stage of hepatic development. Forced expression of HEX in mESC-derived endoderm can dramatically increase the expression of genes related to hepatocyte maturation and function (Kubo et al., 2010). These findings have also been confirmed in hPSCs (Inamura et al., 2011). hPSCs were differentiated into definitive endoderm by Activin A followed by adenoviral delivery of HEX. Transient overexpression of HEX was sufficient to promote hepatocyte derivation. HEX-directed cells expressed both α-fetoprotein (AFP) and albumin (ALB) on day 12. Furthermore, P450 cytochrome enzymes known to play a critical role in liver metabolism were also expressed in HEX-directed hepatoblasts (Inamura et al., 2011). Further maturation of hepatoblasts into functional hepatocytes was achieved by overexpression of HNF4α, a key regulator of liver-specific genes (Takayama et al., 2012a). Interestingly, forced induction of HNF4α in mESCs was able to bypass the natural order of hepatic differentiation and activate the hepatic program directly from mESCs (Yamamizu et al., 2013). ALB secretion and the uptake of low-density lipoproteins were observed in HNF4α-directed cells as early as 7 days after differentiation. In their study, other transcription factors, such as FOXA1, GATA2, and GATA3, could also directly drive mESCs into hepatocytes (Yamamizu et al., 2013).

Sequential delivery of transcription factors has also been tested for efficient PSC differentiation toward hepatocytes (Takayama et al., 2011; 2012b). Forced induction of either SOX17 or FOXA2 was used to differentiate hPSCs into definitive endoderm. SOX17-directed endoderm cells were driven to hepatocytes by HEX overexpression (Takayama et al., 2011). In FOXA2-directed endoderm cells, HNF1α transduction efficiently generated hepatocytes (Takayama et al., 2012b). Furthermore, a single-step protocol with a combination of transcription factors for hepatocyte derivation has been reported (Tomizawa et al., 2016). Forced induction of four transcription factors, CEBPA, CEBPB, FOXA1, and FOXA3, directly differentiated hiPSCs into hepatocytes when they were cultured in a medium that could promote hepatic differentiation. Transcription factor-directed methods for hepatocyte differentiation are summarized in Table 4.

Table 4.

Transcription factor-directed PSC differentiation toward hepatocytes

Cell Line Final Cell Type Transcription Factor Delivery Method Time to Functional Cell Differentiation Efficiency Functional Test Therapeutic Effect Reference
mESC Hepatocyte HEX Genetic recombination ~14 days ND Hepatocyte marker expression
Liver metabolism-related gene expression		 ND Kubo et al., 2010
hESC, hiPSC Hepatocyte HEX Adenoviral vector ~18 days ~84% (ALB+)
~80% (CYP3A4+)
~88% (CYP7A1+)
~92% (Cytokeratin18+)		 Hepatocyte marker expression
Liver metabolism-related gene expression
Liver metabolite production		 ND Inamura et al., 2011
hESC, hiPSC Hepatocyte SOX17, HEX, HNF4A Adenoviral vector ~20 days ~80% (ALB+)
~80% (CYP3A4+)
~80% (CYP7A1+)
~80% (CYP2D6+)		 Hepatocyte marker expression
LDL uptake
Liver metabolism-related gene expression
Liver metabolite production
Glycogen storage
Indocyanine green (ICG) uptake		 ND Takayama et al., 2012a
hESC, hiPSC Hepatocyte SOX17, HEX Adenoviral vector ~18 days ND Hepatocyte marker expression
Liver metabolism-related gene expression		 ND Takayama et al, 2011
hESC, hiPSC Hepatocyte FOXA2, HNF1A Adenoviral vector ~20 days ~90% (ALB+) Hepatocyte marker expression
LDL uptake
Liver metabolism-related geneexpression
Liver metabolite production
Glycogen storage
Indocyanine green (ICG) uptake
Urea secretion
Drug metabolism capacity		 ND Takayama et al., 2012b
hiPSC Hepatocyte CEBPA, CEBPB, FOXA1, FOXA3 Plasmid transfection ~7 days ND Hepatocyte marker expression ND Tomizawa et al., 2016
mESC Hepatocyte Either HNF4A, FOXA1, GATA2, or GATA3 Genetic recombination 7–14 days ND Hepatocyte marker expression
Albumin secretion
LDL uptake
Glycogen storage		 ND Yamamizu et al., 2013
HNF4A Synthetic mRNA ~11 days Hepatocyte marker expression
Glycogen storage
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ND: Not Determined

CONCLUSIONS

During development, fully differentiated cells emerge through several intermediate stages. For example, ESCs first produce early neuroectoderm that gives rise to region-specific neural progenitor cells. Neural progenitor cells further differentiate into post-mitotic neurons, a type of fully differentiated cells in the brain. Even in this simplified description, the end-stage cell fate is derived through three sequential cell fate transitions. An outstanding question in developmental biology is if multiple transitions are necessary for the acquisition of fully differentiated cell fates. A growing body of recent evidence shows that cell fate acquisition/conversion can occur directly by forced expression of transcription factors, suggesting that multiple developmental steps are unnecessary for generating fully differentiated cells. In this review, we also described examples of direct conversion of PSCs into mature cell types by transcription factors. Overexpression of transcription factors related to late developmental stages could bypass early developmental processes and rapidly produce functionally mature cells from PSCs. This is especially prominent in neuronal differentiation because many studies have shown that single proneural transcription factor is sufficient to convert PSCs into functional neurons with almost 100% efficiency. However, transcription factor-directed PSC differentiation seems to be less effective in other lineages. Although transcription factor induction can promote lineage differentiation, protocols are not yet mature in terms of efficiency or functional maturity. In some cases, transcription factors failed to initiate the differentiation program in PSCs likely due to epigenetic barriers. Small-molecule epigenetic inhibitors could be helpful to reset PSCs to be responsive to late-stage transcription factors.

Despite major advantages of transcription factor-directed differentiation over conventional methods, current methods are not ready for clinical applications yet. Besides a few tests for functionality, extensive systemic analyses including transcriptome and epigenome should be performed to validate if transcription factor-directed cells are safe and mature as their in vivo counterparts. Furthermore, virus-mediated transcription factor delivery might be inappropriate for clinical settings. Alternative delivery methods such as protein transduction and synthetic RNA transfection are under active investigation. Given that simple and scalable differentiation procedures with high purity are major bottlenecks for therapeutic applications of PSC-derived cells, transcription factor-directed PSC differentiation methods could be used as a promising strategy for future cell therapy.

ACKNOWLEDGMENTS

This work has been supported by the National Research Foundation of Korea (NRF) grant funded by the Korea government (MSIT) (NRF-2019R1C1C1002377), the POSCO Science Fellowship of POSCO TJ Park Foundation, and the POSTECH Basic Science Research Institute Grant.

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