- Open Access
Efficient derivation of dopaminergic neurons from SOX1− floor plate cells under defined culture conditions
© Li et al. 2016
- Received: 28 October 2015
- Accepted: 25 February 2016
- Published: 8 March 2016
Parkinson’s disease (PD) is a severe neurodegenerative disease associated with loss of dopaminergic neurons. Derivation of dopaminergic neurons from human embryonic stem cells (hESCs) could provide new therapeutic options for PD therapy. Dopaminergic neurons are derived from SOX− floor plate (FP) cells during embryonic development in many species and in human cell culture in vitro. Early treatment with sonic hedgehog (Shh) has been reported to efficiently convert hESCs into FP lineages.
In this study, we attempted to utilize a Shh-free approach in deriving SOX1− FP cells from hESCs in vitro. Neuroectoderm conversion from hESCs was achieved with dual inhibition of the BMP4 (LDN193189) and TGF-β signaling pathways (SB431542) for 24 h under defined culture conditions.
Following a further 5 days of treatment with LDN193189 or LDN193189 + SB431542, SOX1− FP cells constituted 70–80 % of the entire cell population. Upon treatment with Shh and FGF8, the SOX1− FP cells were efficiently converted to functional Nurr1+ and TH+ dopaminergic cells (patterning), which constituted more than 98 % of the entire cell population. However, when the same growth factors were applied to SOX1+ cells, only less than 4 % of the cells became Nurr1+, indicating that patterning was effective only if SOX1 expression was down-regulated. After transplanting the Nurr1+ and TH+ cells into a hemiparkinsonian rat model, significant improvements were observed in amphetamine induced ipslateral rotations, apomorphine induced contra-lateral rotations and Rota rod motor tests over a duration of 8 weeks.
Our findings thus provide a convenient approach to FP development and functional dopaminergic neuron derivation.
- Human embryonic stem cells
- Neural conversion
- Floor plate
- Dopaminergic neurons
Parkinson’s disease (PD) is the second most common central nervous system neurodegenerative disease and the most common sub-cortical neurodegenerative disease . The prevalence of PD is generally estimated at 0.3 % of the entire population, 1 % of the population over 60, and 4 % of those over 80 . PD is caused by loss of dopaminergic neurons from the substantia nigra and disease severity is correlated to the percentage of dopaminergic neuronal loss . PD in most people is idiopathic but environmental or genetic factors may contribute to the onset of dopaminergic neuron loss in certain cases. Currently, there is no proven preventative therapy or cure for this disease.
PD is typically managed pharmacologically with dopaminergic agonist replacement or by increasing production of dopamine in surviving dopaminergic neurons through administration of the dopamine precursor, L-3,4-dihydroxyphenylalanine (L-DOPA). In certain cases, deep brain stimulation and fetal tissue transplantation have been utilized in the clinical management of PD . The transplantation of donor fetal tissue is however associated with concerns regarding supply of sufficient quantities of tissue, inter-batch variability, safety and ethics. Human embryonic stem cells (hESCs) hold great promise in regenerative medicine. There is potential for application in PD therapy as hESCs have been differentiated into functional dopaminergic neurons with various protocols [5–7]. Of particular interest is the study by Kriks et al. that reported a floor plate (FP)-based strategy for the derivation of human DA neurons within 25 days , based on the earlier FP induction protocol developed by Fasano et al. that involved early sonic hedgehog (Shh) exposure .
As an alternative to Shh-induced FP induction, Teillet et al. showed that the FP develops in a cell-autonomous manner in the absence of a notochord, providing evidence that the lineage fate of some FP cells derived from the chordoneural hinge is predetermined . In this study, we employed a Shh-free approach in deriving FP cells with BMP and TGF-β dual inhibition. To determine the optimal timing of FP induction for our in vitro system, we utilized the dynamics of SOX1 expression as an indicator. Studies have shown that SOX1 is restricted to neural folds at the 2nd somite stage and restricted to the neural tube at the 10th-12th somite stages. At the 20th somite stage, SOX1 is down-regulated in the FP of the neural tube. Specifically, cells occupying the lateral regions of the FP express SOX1, whereas cells occupying the medial region do not [10, 11]. However, little is known about how SOX1 is associated with FP cells derived in situ within the developing human embryo or equivalent in vitro model systems.
In this study, we report efficient induction of SOX1− FP cells for the derivation of dopaminergic neurons from hESCs. Dissociation of hESC into a single-cell suspension was carried out, followed by treatment (for 24 h) with a BMP4 inhibitor, LDN193189, and a TGF-β inhibitor, SB431542, (dual restriction) for neuroectoderm conversion under defined culture conditions. The cells were then subsequently cultured in the presence of LDN193189 and SB431542 (dual inhibition) for 5 days to achieve a SOX1− medial FP cell population. In addition, 5 days of treatment with FGF2 or transient treatment with its inhibitor PD173074 was investigated in our platform (patterning). We found that when the cells are SOX1+, treatment with Shh and FGF8 only yielded less than 4 % of Nurr1+ cells. It was only after SOX1 expression was down-regulated, that Shh and FGF8 treatment yielded more than 90 % Nurr1+ cells.
Cell lines, culture media and supplements, labware consumables and reagents
Undifferentiated hESC of the H1 and H9 line were purchased from Wicell Inc. (Madison, WI, USA). Unless otherwise stated, all culture media and supplements including serum and trypsin were purchased from Gibco BRL Inc. (Grand Island, NY, USA); all cell culture plastic labware consumables were purchased from BD Bioscience Inc. (Franklin Lakes, NJ, USA); and all reagents including growth factors were purchased from Sigma-Aldrich Inc. (St Louis, MO, USA). Cell cultures were carried out at 37 °C within a humidified 5 % CO2 incubator (Heraeus GmbH, Hanau, Germany).
Cell culture and GFP labeling
H1 and H9 hESCs were continuously co-cultured under Mytomycin-C inactivated Mouse Embryonic Fibroblast (MEF) feeders, as previously described . The hESCs culture medium is composed of Dulbecco’s modified Eagle’s medium (DMEM) F-12 supplemented with 20 % (v/v) knock-out serum replacement (KSR), 1 mM L-glutamine, 0.1 mM β-mercaptoethanol, 1 % (v/v) non-essential amino acid and 4 ng/ml recombinant basic fibroblast growth factor (rFGF2). Culture media were changed every day and cells were sub-cultured at 5–6 days intervals. For labeling, hESCs colonies were treated with 2 mg/ml collagenase IV for 20 min to allow the colonies to detach from the MEF feeders. The floating colonies were then collected and dissociated with trypsin/enzyme free cell dissociation buffer mixture (3:7) in the presence of Y-27632. A plasmid vector carrying the GFP gene was incubated with the hESCs for 24 h in Ultra-low Attachment plates. Transfected cells were then seeded again on MEF feeder layers for expansion from single cells to colonies. Green-fluorescent colonies were manually selected under fluorescent microscopy for expansion and differentiation.
Induction of FP neurons and patterning
hESCs were detached with 2 mg/ml collagenase type IV for 20mins and floating colonies were collected. The pellets were then dissociated with trypsin/enzyme free cell dissociation buffer mixture (3:7) in the presence of Y-27632. Dissociated cells were then re-suspended into DMEM/F-12 medium supplemented with 20 % (v/v) KSR containing 2nM LDN193189 for single restriction or 2nM LDN193189 and 10 μM SB431542 for dual restriction for 24 h on fibronectin-coated plates. For FP induction, cells were cultured in neural basal medium (NB, Life technologies Inc. Grand Island, NY, USA) supplemented with 1 mM L-glutamine, 1 % (v/v) non-essential amino acid, 1 % (v/v) N2 supplement with or without 0.5nM LDN193189 or 10 μM SB431542 for another 5 days. The FGF2 inhibitor, PD173074 (1 nM), was added immediately after dual restriction for 24 h only for lateral FP cell induction. For patterning, cells were subsequently cultured in NB supplemented with 1 % (v/v) NEAA, 1 mM L-glutamine, 1 % (v/v) B27 supplement, 200 ng/ml Shh, and 100 ng/ml FGF8. Shh and FGF8 were then withdrawn and replaced with 20 ng/ml brain derived neurotrophic factor (BDNF) and 20 ng/ml glial cell derived neurotrophic factor (GDNF), 1 μM Transforming growth factor beta-3, 200 μM ascorbic acid and 1 mM Dibutyryl cyclic adenosine monophosphate (dcAMP), to maintain the differentiated cells .
Gene expression analysis by polymerase chain reaction
mRNA was extracted from samples using Qiagen RNeasy® Mini Kits (Qiagen Inc., Hilden, Germany). Following the manufacture’s instructions, total mRNA was immediately quantified by nanodrop and 2 μl of each mRNA sample was loaded to a 1.5 % agarose gel for integrity checking. 500 ng of mRNA was reverse transcribed to cDNA using the Biorad iScript™ cDNA synthesis kits (Biorad Inc., Hercules, CA, USA). Briefly, 40 μl of cDNA was synthesized with programmed temperature changes of 5 min at 25 °C, then 30 min at 42 °C and followed by 85 °C for 5 min to heat-inactivate the reverse transcriptase. For qRT-PCR, 20 μl volume of reaction mix was utilized (including 10 μl Fast SYBR® Green Master Mix (2X) (Life technologies Inc. Grand Island, NY, USA), 5nM forward and reverse primers 0.4 μl each, and RNAase free water). cDNA was denatured at 95 °C for 10mins, followed by 40 cycles of denaturation at 95 °C for 10 s and 60 °C for 1 min. All runs were performed on a StepOnePlus™ Real-Time PCR System (Life technologies Inc. Grand Island, NY, USA) with GAPDH utilized as the loading control. Fold differences were calculated relative to control samples. All primers utilized are listed in Additional file 1: Table S1. For conventional PCR, a volume of 20 μl was utilized (including 10 μl Fermentas Master Mix (2X) (Thermo-Scientific Inc., Waltham, MA, USA), 25nM forward and reverse primers 0.4 μl each, and RNAase free water). The PCR product was loaded on a 1.5 % agarose gel and imaged with a Bio-rad Gel-Doc system (Biorad Inc., Hercules, CA, USA).
Cells were detached by trypsinization for 5 min at 37 °C. After fixation in 4 % (w/v) PFA for 10 min at room temperature, the cells were immediately chilled on ice for 1 min, followed by 10mins permeabilization in 0.2 % Triton X-100 in 1X PBS. The cells were then incubated with the appropriate primary antibodies for 4 h at room temperature followed by incubation with corresponding secondary antibodies for 1 h, prior to analysis with a CyAn™ Flow Cytometer (Beckman-Coulter Inc., Indianapolis, IN, USA). All secondary antibodies used were tested for cross reactivity and non-specific immunoreactivity. Approximately, 10,000 cells were gated for analyzing each marker.
Cells/brain slices were washed with 1X phosphate buffered saline (PBS) three times and fixed with 4 % (w/v) Paraformaldehyde (PFA) for 10mins at room temperature. Following 10mins permeabilization with 0.2 % Triton X-100 in PBS, the cells were blocked for 1 h with 5 % (v/v) goat serum and 2 % (w/v) bovine serum albumin (BSA). Diluted primary antibodies were then added to the culture and incubated at 4 °C overnight. After 4 washes with 1X PBS, diluted secondary antibodies against the specific primary antibodies were added and incubated in the dark at room temperature for 1 h. All secondary antibodies used were tested for cross reactivity and nonspecific immunoreactivity. The nuclear stain DAPI was added 10mins prior to the final wash. Images were captured under fluorescence microscopy. The antibodies used are listed in Additional file 2: Table S2.
Live imaging analysis for neurite outgrowth
Differentiating dopaminergic cells from monolayer culture of FP origin were analyzed for neurite outgrowth. Cells generated by a neurosphere protocol were imaged together for comparison . Differentiating dopaminergic neurons in 24-well plates were continuously cultured in a Cell IQ Imagen system (Chip-Man Technologies INC., Tampere, Finland) for 5 days in a Cell IQ incubator with 5 % CO2 mixed with air at 37 °C. 2 × 2 grid images were sampled continuously every 15 min on selected colonies collected over a period of 5 days with 10X magnification using the Cell IQ Imagen system. Superimposed images were then analyzed using the Neurite Finder™ module of the Cell IQ Analyser.
In vitro patch clamp
Differentiated dopaminergic cells were immersed in an external solution of 125 mM NaCl, 3 mM KCl, 1.25 mM NaH2PO4, 1.5 mM MgCl2, 2 mM CaCl2, 24 mM NaHCO3, and 10 mM D-Glucose, with pH adjusted to 7.4. Whole-cell voltage clamping was conducted with the membrane potential clamped at -60 mV as the resting potential of the differentiated neurons. The currents were recorded with borosilicate pipettes with resistances of 2–6MΩ, which were pulled from borosilicate glass capillaries with a Flaming Brown micropipette puller. The pipettes were filled with an internal solution with the same composition as the external solution. Transplanted neurons were clamped using a MultiClamp 700A amplifier in conjunction with a Digidata 1322A interface (Molecular Devices Inc., Sunnyvale, CA, USA). Currents were recorded and analyzed using the pCLAMP software (Molecular Devices Inc., Sunnyvale, CA, USA).
Dopamine secretion assay
Dopamine secretion into the culture media was analyzed using a Dopamine ELISA Kit (GenWay Biotech Inc., San Diego, CA, USA) following the manufacture’s instructions with slight modifications. For amantadine treated samples, 5 or 10 μM of amantadine was added to the culture media. Culture media were collected every 3 days after induction for quantification of dopamine secretion. Briefly, dopamine from culture media was first extracted with 12 well pre-coated extraction plates. Following a few washes, bound dopamine was extracted by 200 μl of release buffer. Enzyme solution, 100 μl of the extracted samples and dopamine anti-serum were added to pre-coated 96 well plates and incubated for 2 h at room temperature. Enzyme conjugate and PNPP substrate solution were added sequentially with washes in-between. The reaction was stopped by addition of PNPP stop solution and absorbance of samples were read at 405 nm using Infinite™ 200 plate readers (Tecan Inc., Männedorf, Switzerland). The amounts of secreted dopamine were calculated based on a standard curve plotted with a series of known dopamine dilutions supplied by the manufacturer.
Transplantation into Hemi-Parkinsonian rats, behavioral analysis, patch clamp and histological staining
Sprague Dawley rats were purchased from the animal holding unit (AHU) of the National University of Singapore, and were housed in biological safety level 2 pathogen-free facilities with free access to food and water under a 12 h light/dark cycle, and with standard room temperature of 23 ± 1 °C. Ethical approval for all animal experiments were obtained from the Institutional Animal Care and Use Committee (IACUC) of the National University of Singapore. All animal studies were in compliance with the “Animal Research: Reporting In Vivo Experiments” (ARRIVE) guidelines. Animals (250 g) were anaesthetized and immobilized with a stereotactic instrument. 20 μg of 6-OHDA was stereotaxically injected at the bregma (AP +1.00 mm, ML +3.00 mm, DV +4.5 mm), at a concentration of 5 μg/μl with the aid of the Angle Two Software for unilateral lesion. Only animals with a mean contralateral rotation score of 7 or more body turns per minute at 3 weeks post-lesion were included in the study. Initially, lesions were created on 25 rats. However by 3 weeks post-lesion, only 12 rats that met the criteria of >7 rounds of contra-literal rotation induced by 0.5 mg/lg apomorphine were utilized for cell transplantation. At 12 days post-lesion, dopaminergic cells (250,000 cells/4 μl) were grafted into the same lesion site. 0.5 mg/kg of apomorphine or 0.25 mg/kg of amphetamine were injected subcutaneously or intraperitoneally and their contralateral and ipslateral rotation behavior was monitored over a 45 min period using an EthoVsion XT system (Noldus Inc., Wageningen, Netherlands). Rotation scores were expressed as full body turns per minute. To measure balance and coordination, animals were placed on a horizontally rotating rod that accelerated from 2rmp to 40 rpm within 2 min. The latency of fall off from the rod was recorded for 6 trials with 10 min rest between each trial.
Eight weeks after transplantation of GFP-labeled cells, brain samples were sectioned at 200 μm with a vibratome in 10 % (v/v) glycerol in PBS. Whole-cell voltage clamping was conducted with the membrane potential clamped at -60 mV as the resting potential of the differentiated neurons. The currents were recorded with borosilicate pipettes with resistances of 2–6MΩ, filled with an internal solution containing (in): 140 mM K Gluconate, 20 mM HEPES, 2 mM MgCl2, 4 mM K2ATP, 2 mM NaCl, 1 mM EGTA, and 2 mM NaCl, with pH and osmolarity of the solutions being adjusted to 7.2 and 290 mOsm respectively. The external solution was composed of 150 mM NaCl, 5 mM KCl, 2 mM CaCl2, 10 mM HEPES, 1 mM MgCl2, 10 mM glucose with the pH and osmolarity of the solution being adjusted to 7.2 and 310 mOsm respectively. Transplanted neurons were clamped using a MultiClamp 700A amplifier in conjunction with a Digidata 1322A interface (Molecular Devices Inc., Sunnyvale, CA, USA). Currents were recorded and analyzed using the pCLAMP software (Molecular Devices Inc., Sunnyvale, CA, USA).
10 μm brain slices sectioned with a vibrotome were also stained with haematoxylin and eosin to determine whether there is any teratoma formation by the transplanted cells. Briefly, sections were fixed in 4 % (w/v) paraformaldehyde and washed in PBS for 4 times followed by 1 min staining with haematoxylin. Samples were then rinsed in distilled deionised water until no dye can be extracted from the samples, followed with eosin staining for 2mins. Samples were then washed, dehydrated and mounted on glass slides.
Numerical data of experimental and control groups were analyzed with one-way Anova Bonferroni post-hoc multi-group comparison, utilizing the SPSS software. A value of P < 0.05 was considered statistically significant.
LDN193189 treatment restricts hESC lineage fate to neuroectoderm
Dual inhibition produces medial FP cells
FGF2 inhibits neural induction and inhibiting FGF2 signaling sustains NP state
Characterization of FP cell derived dopaminergic neurons in vitro
FP derived dopaminergic neurons are functional in vitro, survive after transplantation and ameliorate behavioral deficits in PD rats
After transplantation of cells into the stratum of the host, tissue samples were collected from animals at week 4, 6, and 8 to assess cell survival and integration with β-III tubulin immunostaining. At 4 weeks, a large number of cells were found to have survived within the host with positive staining for β-III tubulin (Fig. 5c). After 6 weeks, integration was clearly observable with transplanted cell interspersed with host cells (Fig. 5d). Some cells were found to have migrated from the injection site to the surrounding host tissue by week 8. Confocal microscopy revealed that some cells have migrated across the host nucleus (Fig. 5e). After H&E staining of the host tissue, no obvious teratoma formation was found at both low and high magnifications (Fig. 5f). Over 8 weeks, clear action potentials were recorded from grafted cells within the host. When tissues were extracted for electrophysiological studies of the grafted cells, action potentials were induced when the cells were exposed to a current of 150 pA for 400 ms (Fig. 5g). The appearance of the action potentials indicates that the cells already had the key functional property of neurons.
Within the FP, there are two distinct populations of cells located in the lateral and medial regions of the FP. It is generally agreed that all FP cells express netrin1, FOXA2 and Shh. However, there is controversy over the origin of FP cells during early embryonic development, particularly the role of notochord in FP induction . Inhibition studies revealed that FP differentiation is impeded along the entire AP axis in mice and chick upon pharmacological blockade of Shh (which is mainly expressed in the notochord) [24, 25]. Gain of function studies demonstrated that high concentrations of Shh induced formation of FP tissue/cells from neural explants and in vitro hESCs culture [8, 26]. Contrarily, loss of function studies in zebra fish revealed unaffected ventral midline differentiation with certain effects on lateral FP induction . Additionally, the finding that surgical ablation of notochord resulted in lack of FP formation was challenged by Nicole and colleagues, who postulated that the absence of FP in notochord ablation experiments was due to removal of FP precursors of nodal origin rather than termination of Shh secretion .
It has been shown that Shh is required for lateral FP cell induction, but not for medial FP cells . Medial FP cells are still formed in the absence of a differentiated notochord, thus indicating that Shh signaling originating from the neural tube is not a prerequisite for MFP induction [30, 31]. Additionally, medial FP cells failed to develop in the case of mutations affecting the nodal-related molecule of the TGF-β family despite high levels of Shh expression . It was also reported that signaling from the notochord or medial FP cells can induce lateral FP cells . These data suggest that with differentiating FP cells within in vitro culture, the induction of medial FP cells will also increase the population of lateral FP cells. In this study, it was observed that FP cells, both medial and lateral, can be induced without extrinsic Shh treatment, thus supporting the hypothesis that the developmental fate of FP cells are pre-determined before being exposed to patterning signals from the notochord. It is well established that dorsalization is mediated by BMP and TGF-β signaling, which originate from the epidermis and roof plate [34, 35]. Contrarily, antagonists of the BMP and TGF-β family are known to be secreted from the organizer to protect surrounding cells from dorsalization . BMP4 inhibition from the organizer is required to induce neural differentiation of epiblast cells. However, synchronized TGF-β inhibition stabilizes and accelerates neural induction towards FP lineage fates.
We found that dual restriction under defined culture conditions committed the lineage fate of hESCs to neuroectoderm in only 24 h. Further culture under dual inhibition sustained neural differentiation in favor of the FP lineage fate. Additionally, upon addition of FGF2, the majority of the anterior neural lineage markers were down-regulated, suggesting that after neural induction of hESCs, in the early phase of neurogenesis, high levels of FGF2 inhibits the anterior neural fate by up-regulating pluripotency markers OCT4 and NANOG expression. It has been shown that FGF2 acts as a morphogen for the anteroposterior axis of the CNS and that FGF2 induces gastrula ectoderm cells to express posterior neural markers in Xenopus . Other studies have shown that FGF2 caudalizes intermediate neural tissue, inducing spinal cord formation from anterior tissue . In our in vitro culture system, endogenous FGF2 could act in two ways simultaneously, ensuring cell survival and inducing differentiation into caudal neural tissues. In this study, when FGF2 inhibitor is added to the culture for only 24 h, significant FP induction was observed and maintained. Our data thus indicates that neural conversion occurs in the presence of weak FGF signaling combined with BMP inhibition, and that pre-gastrulation FGF signaling is required in the ectoderm for the emergence of neural lineage fates . Hence, inhibition of FGF signaling should be in a temporal manner to ensure cell survival during neural induction. In combination with ventralization factors that block BMP and TGF-β signaling, SOX1− FP cells were induced after 5 days and these cells can be further induced into dopaminergic neurons efficiently. In contrast, despite the expression of other FP genes, dopaminergic cells cannot be efficiently induced in culture when cells are still expressing SOX1 and Nurr1.
Following the pioneering study of Kriks et al. , a number of other studies have also attempted to utilize a similar floor plate-based strategy for the derivation dopaminergic neurons from human pluripotent stem cells [40–43]. Nevertheless, all of these studies [40–43] including that of Kriks et al. , carried out floor plate induction through stimulation of the Shh signaling pathway, either through the direct use of recombinant Shh protein itself, or it’s agonist purmorphamine. Our study differs from these previous studies by utilizing a Shh-free approach to floor plate induction, through dual inhibition of the BMP4 (LDN193189) and TGF-β signaling pathways (SB431542).
The results of this study demonstrated that the hESC-derived dopaminergic neurons are functional in vitro, can survive after transplantation and integrate within the host brain. This is thus consistent with a previous study which showed that grafted dopaminergic neurons possess an intrinsic capacity for innervation of the adult striatum . Significant functional improvements were observed in amphetamine induced ipslateral rotations, apomorphine induced contra-lateral rotations and Rota rod motor tests over a duration of 8 weeks post-transplantation, and it is anticipated that the grafted cells would continue to provide functional improvement at later time points, because the long-term survival and health of dopaminergic neuron transplants in Parkinson’s disease patients over several years have been conclusively demonstrated . Nevertheless, it is unclear whether the observed amelioration of behavioral deficits in the rat PD model arise directly from new synaptic connectivity conferred by the transplanted cells, or is instead due to other pro-survival, neuroprotective or trophic effects of paracrine secretions emanating from the transplanted cells. Although the results of this study appear promising, we still need to investigate what affects the survival of grafted cells in host, how the grafted cell integrate with host and how the dopamine release from grafted cells are controlled. By using an optogenetic tool, we could be able to shut down the biological function of the grafted neurons within the host brain and successfully created a temporal lapse of behavioral restoration in animal models. In a previous study , Wentz and colleagues developed a wirelessly powered control LED system for delivering light into specific areas of the brain. Perhaps, we could utilize similar instrumentation for future optogenetic studies to dissect the cellular and molecular function of grafted dopaminergic neurons within the rat brain.
We have demonstrated that when cells were predominantly SOX1− under dual inhibition with both LDN193189 and SB431542, FP cells can be generated efficiently. Following patterning with Shh and FGF8, midbrain dopaminergic neurons can be efficiently derived at a very high yield. Our findings thus provide a convenient approach to FP development and functional dopaminergic neuron derivation.
We thank Dr. Wang Shangshang for technical assistance in behavioral studies and helpful discussions. This work was supported by the National University Health System Research Fund R221000085733, the National University Research Fund R221000024133, R221000050133, and NUHS Neuroscience Phenotyping Core (NUHS Centre Grant NMRC/CG/013/2013)
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