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Current methods to examine and regulate the functional integration and plasticity of human embryonic stem cell (hESC)-derived neurons are cumbersome and technically challenging. Here we engineered hESCs and their derivatives to express the light-gated Channelrhodopsin-2 (ChR2) protein to overcome these deficiencies. Optogenetic targeting of hESC-derived neurons with ChR2 linked to the mCherry fluorophore allowed reliable cell tracking as well as light-induced spiking at physiological frequencies. Optically-induced excitatory and inhibitory post-synaptic currents could be elicited in either ChR2+ or ChR2- neurons in vitro and in acute brain slices taken from transplanted SCID mice. Furthermore, we created a clonal hESC line that expresses ChR2-mCherry under the control of the synapsin-1 promoter. Upon neuronal differentiation, ChR2-mCherry expression was restricted to neurons and was stably expressed for at least six months, providing more predictable light-induced currents than transient infections. This pluripotent cell line will allow both in vitro and in vivo analysis of functional development as well as the integration capacity of neuronal populations for cell-replacement strategies.
Human stem cell derived-neurons present both a model system for the study of functional neural development and plasticity [1, 2] as well as a viable source of therapeutically relevant cells for replacement following neurodegeneration . Toward these ends, traditional stimulation and recording techniques have demonstrated many basic physiological capabilities of these neurons including voltage-gated currents, action potential (AP) generation, and synaptic activity [1, 4]. Furthermore, multiple reports have provided evidence that stem cell-derived neurons can receive information from host cells. For example, Brustle and colleagues used co-cultures of either mouse (mESC) or human (hESC)-derived neurons with organotypic hippocampal slices. Stimulation of the intact perforant path fibers could elicit post-synaptic responses in the mESC or hESC-derived neurons deposited on the dentate gyrus [2, 5]. Responses in mESC-derived neurons could also be potentiated by paired-pulse facilitation . These findings are further supported by the fact that, in acute slice preparations from transplanted animals, hESC- and iPSC-derived neurons demonstrated spontaneous excitatory post-synaptic currents [6, 7], which were thought to derive from the host neurons. Thus, current methods have sufficed to establish a post-synaptic role for ESC- and iPSC-derived neurons in neural networks.
However, the inability to specifically stimulate stem cell-derived neurons has proven insufficient to demonstrate graft-to-host connectivity and slowed our understanding of the synaptic plasticity capabilities of these neurons. Attempts to do so have used extracellular stimulation of grafted cells [8, 9, 10] or technically challenging dual patch clamp recordings . While results from these early studies are suggestive of graft-to-host connectivity, the generalized nature of extracellular stimulation and lack of cell identity inevitably leads to questions of specificity . Dual patch clamp methods have failed to show point-to-point synaptic connections, likely due to low probability of connectivity between two randomly selected neurons . Further, no studies have reported pre- or post-synaptic plasticity due to enduring changes in stem cell-derived neurons themselves. Thus, new techniques are needed to accelerate the study of synaptic development, plasticity, and integration of human stem-cell derived neurons.
Channelrhodopsin-2 (ChR2), a light-gated cation channel [14, 15], presents an optical stimulation method that can be genetically-targeted (termed “optogenetics”) to specific neuronal populations to resolve these issues. Brief (5-15ms) light pulses applied to ChR2-expressing rodent neurons can reliably induce AP firing at physiological frequencies (up to 50Hz in some cases ) while preserving cell viability . Transgenic animals expressing ChR2 in specific neuronal subpopulations have been used to map local and distant neuronal circuits [17, 18], dissect the underlying rhythms of Parkinson's Disease , and restore function of damaged tissues . Furthermore, while standard physiological techniques have been integral to the characterization of functional adult neurogenesis in rodents , the advent of ChR2 technology was necessary to demonstrate that adult stem cell-derived neurons could form functional synaptic connections with adult neurons . Thus, ChR2 presents a unique tool for controlling the physiological output of specific groups of neurons that may now be readily generated from human stem cells.
Here we have combined optogenetic targeting with directed neural differentiation of hESCs to provide a method to regulate their functional output for basic and translational studies. We used the pan-neuronal synapsin-1 (Syn) promoter  to drive ChR2 expression in cells with a variety of neurotransmitter phenotypes. Light stimulation of hESC-derived neurons expressing ChR2 could reliably drive AP frequencies from 5-30Hz, depending on cell maturity. ChR2 stimulation elicited both glutamatergic and GABAergic post-synaptic currents (PSCs) both in vitro and within transplanted tissue for at least six months. In addition, we created a pluripotent Syn-ChR2-mCherry cell line to circumvent the variable nature of lentiviral transduction and provide a resource for broader investigation into basic and translational studies of hESC-derived neurons.
The Syn-ChR2-mCherry transfer vector with humanized codons was created using methods described , whereby the CamKII promoter in the CaMKII hChR2-mCherry was excised (PacI, AgeI) and replaced by the Synapsin-1 promoter (−422 to +53; kindly donated by Dr. S. Kugler, University of Goettingen, Germany). Lentiviral production and transduction was performed essentially as described . Briefly, 10μg of Syn-ChR2-mCherry, 7.5 μg lentiviral vector pCMVΔ8.7, and 5μg vesicular stamtitis virus G protein (VSVg) were cotransfected into HEK293FT cells using calcium phosphate. Forty-eight to seventy-two hours after transfection, culture media containing viral particles was collected and filtered through a 0.45um filter (Millipore, Billerica, MA). Viral particles were concentrated by ultracentrifugation (SW28 rotor, Beckman) at 20,000g for 3 hours. Viral pellets were resuspended in the appropriate culture medium and titrated using the Lenti-X qRT-PCR kit (Clontech).
For transduction of hESCs, cells were incubated for 1 hr. with ROCK inhibitor , followed by treatment with 0.5% Trypsin-EDTA (Invitrogen) for five minutes and dissociated to single cells in hESC-media . The cell suspension was centrifuged (1000rpm for 5min.) and resuspended with 100μl of concentrated virus (106 transducing units/ml) and then incubated at 37°C for 30 min. Cells were then plated onto irradiated MEF feeder layers and allowed to grow for 10-14 days for colony formation. Individual colonies were expanded and differentiated to determine if lentiviral incorporation of ChR2 construct had occurred. hESCs (WA09 line, P16-40; Syn-ChR2-mCherry, P25-30) were maintained and differentiated as described [1, 27] with the addition of penicillin-streptomycin (100U-100ug/ml, Invitrogen) after viral transduction, and B27 supplement (Invitrogen) to differentiated neurons after day 21. Images of neurons derived from the Syn-ChR2-mCherry line were acquired on live cells using an inverted Nikon TE2000S (Nikon Instruments Inc., Melville, NY) Microscope with a Photometrics Coolsnap ES CCD camera (Photometrics, Tucson, Az). Comparisons of light-induced ChR2 currents were made between Syn-ChR2 neurons (passage 27-29) and wild type WA09 hESC-derived neurons (passage 31-33) and consisted of pooled means of 7-9 cell recordings per passage.
Immunolabeling of hESC-derived neural progenitor cultures was performed according to previously established methods [27, 28] using polyclonal synapsin-1 primary antibody (1:1000; Calbiochem, La Jolla, CA), an Alexa-Fluor donkey anti-rabbit 488 secondary antibody (1:1000; Invitrogen) and visualized using a Nikon confocal workstation (D-Eclipse C1, Nikon Instruments Inc.) running EZ-C1 software (v3.5).
Cell transplantation was performed similar to previously published methods . Briefly, 21-35 day-old neuroepithelial aggregates were dissociated with accutase (0.05%; Invitrogen) and resuspended in differentiation media [1, 27] at a concentration of 50,000/μl. 2μl of cell suspension was injected through microinjection needles with tip diameters of 50-100μm into the ventricles of 1-2 day old SCID mouse pups that were anesthetized on ice for 3-4 minutes prior to injections.
Cultured neurons were recorded in a modified Hanks Balanced Salt Solution (HBSS) that contained (in mM): 140 NaCl, 3 KCl, 2 CaCl2, 1 MgCl2, 15 HEPES, and 23 glucose, pH 7.4, 300 mOsm. Application of pharmacological antagonists diluted in extracellular solution was achieved using a gravity-fed drug barrel system. Tetrodotoxin (1 μM), bicuculine (20 μM), and 6-cyano-7-nitroquinoxaline-2,3-dione (CNQX, 50 μM) were obtained from Sigma. Acute slice preparations were prepared in cutting solution (CS) and artificial cerebrospinal fluid (aCSF) described previously . Coronal slices were prepared from isoflurane-anesthetized mice whereby the frontal cortex was removed and brains were mounted rostral side down on the slicing stage in ice-cold CS. Slices were cut with a sapphire knife (Leica Microsystems, Deerfield, IL) mounted in a vibrating microtome (VT1000S; Leica Microsystems) also in ice-cold CS. Slices were transferred the to a 35°C chamber containing CS for 30 min., after which time the chamber was allowed to cool to room temperature. Slices were secured in a custom perfusion chamber with a fine polyethylene mesh (Siskiyou Design) and perfused with aCSF (315 mosm) continuously bubbled with 95% O2/5% CO2.
All recordings were performed at 21–23°C using pipettes with resistances of 3–5 MΩ that were filled with an intracellular recording solution containing the following (in mM): 121 K-gluconate, 22 KCl, 10 Na+-HEPES, 10 EGTA, pH 7.2, 290 mOsm. Recordings were obtained using a MultiClamp 700B amplifier (Molecular Devices) and output to a PC running pClamp 9 (Molecular devices); signals were filtered at 4 kHz, sampled at 100 kHz using a Digidata 1322A analog-to-digital converter (Molecular Devices). Access resistance was monitored prior to and following recordings and cells with resistances greater than 25MΩ at either point were discarded from analyses. Series resistance was compensated >60% except during post-synaptic current (PSC) recordings where it was not compensated. All data were stored on a computer hard disk and analyzed with clampfit 9.0 (Molecular Devices) or MiniAnalysis (Synaptosoft, Fort Lee, NJ) software. The liquid junction potential was post-hoc adjusted according to previously published methods (; JPCalc in Clampex; Molecular Devices). For light-induced AP quantitation, current injections were used to maintain RMP at approximately −60mV. PSC analysis was performed using minianalysis software (Synaptosoft). Statistical analysis was performed using one-way ANOVAs and Fisher's LSD post-hoc tests. Data from the Syn-ChR2-mCherry cell line (Figure 5C) represents three replicates of at least eight cells per trial.
Light stimulation was achieved by a custom LED device using a 1 Watt blue fiber optic LED (470 nm; Cree Lighting Inc., Morrisville, NC) coupled to a fiber optic cable. The end of the fiber optic cable was placed 2-5mm from ChR2-expressing neurons in the recording chamber. Power to the LED was provided by a TIP110 transistor (National Semiconductor, Santa Clara, CA). Light intensity was modulated by a potentiometer, and ranged from 0.1 to 1 mW/mm2, with the most stimulations using 0.4 mW/mm2. A National Instruments USB-6501 DAQ provided the trigger pulses, with timing controlled by custom LabView software (LabView, National Instruments, Austin, TX).
To examine the utility of ChR2 across multiple neuronal populations we created a lentiviral vector with the ChR2 gene tethered to the mCherry fluorophore controlled by the pan-neuronal synapsin-1 promoter (Figure 1A). To verify the specificity of this construct, hESCs were differentiated to neural progenitors, infected with lentiviruses carrying the Syn-ChR2-mCherry cassette at day 21, and allowed to mature for 1 week. At day 28, cells displayed robust mCherry expression that was only observed in post-mitotic neurons (PMNs) that also expressed synapsin-1, but not in proliferating neuroepithelial cells (Figure 1B; [1, 32]).
We have previously demonstrated that hESC-derived neurons progressively mature over an extended time course compared to rodent neurons. This ability is correlated with relatively hyperpolarized resting membrane potentials (RMPs) and increased expression of sodium (Na+) and potassium (K+) currents compared to younger cells . Thus, to determine the functional characteristics of ChR2 in hESC-derived neurons we recorded 10-week old mCherry+ cells (Figure 1C) during exposure to 470nm light (0.4mW/mm2). At a holding potential of −70mV, a 500ms light stimulus elicited inward currents with two components: a larger current with fast decay kinetics, and a smaller-amplitude sustained current (Figure 1Di), consistent with previous findings in rodent neurons . In current-clamp, light stimuli elicited similar potentials (Figure 1Dii), and most cells (10/11) displayed a clear threshold deflection indicative of AP generation (Figure 1E, left trace, arrow). Treatment of cells with 1μM Tetrodotoxin (TTX) eliminated the majority of the fast component of the depolarization, suggesting a true ChR2-induced AP (Figure 1E, right trace). Recordings from mCherry− cells revealed no light-induced currents, and stimulation of mCherry+ cells with 650nm light also had no effect (not shown), indicating the specificity of ChR2-induced currents.
To test the ability of ChR2 to trigger trains of APs in hESC-derived neurons, cells were recorded in current-clamp mode at 10 weeks of differentiation but were now presented with brief (5-10ms) light pulses . At this time point, light stimuli triggered individual APs with high reliability up to 10Hz but the fidelity of light-induced APs dropped precipitously at frequencies greater than 10Hz (Figure 1F, H). However, after 25 weeks of differentiation, cells could routinely fire 20Hz trains of ChR2-induced APs (Figure 1G, H), with a subpopulation (2/11) that could fire reliably at 30Hz and nearly at 50Hz (Supplemental Figure 1). Thus, the probability of light-induced AP generation was significantly increased in older cultures at frequencies of 20Hz-40Hz (Figure 1H; 20Hz: p=0.03; 30Hz: p=0.006; 40Hz: p=0.04, n=7-14 cells per group). Lastly, the number of extraneous APs generated during light pulses was extremely small (Figure 1I), with cells averaging less than one extra AP during light pulse trains at all frequencies tested. Together, these data suggest that Syn-ChR2-mCherry is specifically expressed in human PMNs and can induce rapid physiological responses on millisecond timescales with high fidelity and low “noise”.
Using our differentiation protocol we have previously demonstrated that without the addition of exogenous morphogens hESCs preferentially adopt a uniformly forebrain fate . These cultures are comprised of both glutamatergic and GABAergic neurons, exhibited by the presence of spontaneous excitatory and inhibitory post-synaptic currents (ePSCs and iPSCs; ). In voltage-clamp mode, we observed that cells expressing ChR2 routinely displayed increases in PSC incidence during and following trains of light-induced escape action currents (Supplemental Figure 2, Figure 2Ai, arrows). PSCs could also be seen when light stimuli failed to initiate escape action currents, suggesting that other ChR2+ cells in close proximity to the recorded cell initiated synaptic currents (Figure 2Aii). Alternatively, these PSCs could have arisen from autaptic currents from the recorded cell, although this remains untested. All PSCs recorded could be blocked by a combination of the AMPA and GABA receptor antagonists CNQX (50μM) and bicuculine (20μM), regardless of the presence of an escape current (Figure 2Aiii-iv), which were verified by treatment with TTX (Figure 2Aiv). Furthermore, we were able to detect light-induced PSCs in subpopulations of ChR2− cells (Figure 2B). A small minority (n=2 of 36) reliably induced ePSCs that were specifically blocked by CNQX (Figure 2Ci), whereas a larger proportion (n=8 of 36) reliably induced iPSCs that could be blocked by bicuculine (Figure 2Cii). Thus, both glutamatergic and GABAergic populations of cells that expressed ChR2 and could be induced to release neurotransmitter in response to light stimulation.
In addition to pharmacological blockade, we were able to verify that these were truly PSCs (and not ChR2 currents themselves) by their temporal kinetics as well as the delay between stimulus and current onset. In response to 10ms light stimulations PSCs had rapid rise times (Figure 2D, mean = 3.03±0.49ms, baseline to peak, n=8) as well as a significant delay between light onset and PSC onset (Figure 2D; mean delay=21.9±4.2ms; median delay=16.3ms, n=10). In contrast, onset delay for ChR2 currents were uniformly rapid, similar to previous findings (~50us; ) and ChR2 current rise times were significantly slower (mean=10.61±0.39ms, n=10), making them clearly distinguishable from light-induced PSCs (Supplemental Figure 2). Interestingly, PSC onset delay varied noticeably, ranging from 11.2ms to 46.8ms, likely resulting from a number of factors including across-neuron AP “jitter” (defined as the standard deviation of spike latency). Jitter between hESC-derived neurons (6.3±1.7ms, n=14) was noticeably greater than what was observed in hippocampal neurons (~3.4ms; ). However, mean spike latency (16.9±1.7ms, n=14) and within-cell jitter (2.8±0.5ms, n=14) did not appear to be different from previous reports. Thus, increased jitter between hESC-derived neurons likely results from the heterogeneity of the population (e.g. glutamatergic and gabaergic). Importantly, it should be noted that within individual cells, mean PSC onset delay was extremely uniform (0.94±0.18ms, n=10), suggesting that synaptic transmission at individual synapses was temporally consistent.
To demonstrate the utility of ChR2 expression in hESC-derived neurons within the context of host circuitry we recorded individual neurons in acute slice preparations 3-6 months after transplantation into perinatal SCID mice (Figure 3A). hESC-derived neurons at these time points displayed mature physiological phenotypes including low RMPs (mean=−60.7±2.9mV, n=19), robust Na+ (137.2±12.2pA/pF, n=20) and K+ currents (66.2±7.6pA/pF, n=20). Furthermore, hESC-derived neurons displayed spontaneous APs and PSCs, indicating the formation of functional neural networks within host brains (Figure 3B-C). Furthermore, similar to in vitro cultures, APs could be readily induced in mCherry+ neurons by 470nm light at physiological frequencies (Figure 3D). Light-induced APs could also be elicited in the on-cell configuration without manipulation of the RMP (Figure 3E), indicating that the endogenous RMP of these cells was sufficient to allow rapid repolarization following light stimulation. Furthermore, light-induced PSCs could be reliably induced in ChR2− cells adjacent to ChR2+ neurons (Figure 3F; light intensity: 1mW/mm2).
While ChR2− neurons were not verified as mouse or human, the data are proof of concept that this is a useful tool to examine the synaptic integration properties of transplanted hESC-derived neurons. Importantly, we can be confident that light-induced currents derived solely from human cells due to a lack of expression observed in anatomically identifiable mouse neurons (e.g. hippocampal formation) and the fact that previous reports found no transfer of heterologously expressed opsins between synaptically connected neuronal populations . It should be noted that for slice recordings, we observed greater failure rates at light intensities <1mW/mm2 (not shown) and larger variation in PSC amplitude was observed at light intensities of 1mW/mm2 (Figure 3F), which was likely due to diffraction of light within the slice . Lastly, no exogenous retinal was given to SCID mice following transplantation, indicating that endogenous levels were sufficient to reveal ChR2 currents in acute slice preparations.
While viral infection of hESC-derived neurons successfully demonstrated the utility of ChR2 in transplantable human neurons, there is inherent variability in transduction efficiency and expression using this method. Thus, we sought to create a clonal hESC line that would express ChR2 following differentiation to synapsin+ neurons. Infection of hESCs followed by trypsinization in the presence of the ROCK inhibitor  allowed us to select clones transduced with the Syn-ChR2-mCherry virus. Selection and subsequent differentiation of these cells revealed multiple clones that became mCherry+ during neuronal differentiation. A single clone was chosen based on mCherry fluorescence intensity as well as neuronal differentiation potential without contaminating cell populations. This clone did not display mCherry expression at the hESC stage nor during the early phases of neural induction (Figure 4, ES cells, EBs, NE). However, upon plating neuroepithelial aggregates after 3 weeks, mCherry expression was observed in the majority of cells with visible neurites (Figure 4, NE+PMNs, column 4). mCherry expression was maintained in cells for the duration of experiments (Figure 4, NE+PMNs, column 5), and increased in intensity with many cells becoming visible by eye after 2 months.
To test the functionality of this Syn-ChR2-mCherry cell line, we recorded from neurons between 5-6, 10-12 weeks, and 3-5 months of differentiation. While mCherry expression was detectable by 4 weeks (Figure 4), fluorescence intensity was relatively weak and required detection via CCD camera. Likewise, light stimulation of 5-6 week-old cells clamped at a holding potential of −70mV revealed relatively small ChR2-mediated currents (Figure 5A-B; mean amplitude=27.6±3.4pA). Furthermore, stimulation of these cells rarely (n=1/11) produced AP generation (Figure 5Ci), likely due to the diminutive nature of the ChR2 current as well as low levels of Na+ and K+ channel expression and RMPs at or above Na+ channel threshold in these immature neurons . However, mean ChR2-induced current amplitude was increased at later time points (10-12 weeks), and were not different from transiently infected cells of similar developmental age (Figure 5B; p>0.05, n=3, see methods). However, the variability of ChR2-induced currents compared to transient infections at the same time point was significantly decreased (5-6 weeks: p=0.003; 10-12 weeks: p=0.02; 3-5 months: p=0.005; n=3 at each timepoint) suggesting a greater uniformity of expression in the Syn-ChR2-mCherry cell line. Lastly, to establish that our Syn-ChR2 line was capable of generating neurons of multiple transmitter phenotypes that were also fully functional (pre- and post-synaptically), we recorded spontaneous PSCs in cultures of Syn-ChR2 cells alone or in co-culture with normal WA09 hESC-derived neurons. In Syn-ChR2 cultures we observed spontaneous PSCs with two distinct temporal profiles, indicative of glutamatergic and GABAergic synapses (Figure 5C, upper traces) similar to previous studies . Indeed, PSCs with relatively fast kinetics were specifically blocked by CNQX (Figure 5C, middle traces) while those with slower kinetics were blocked by bicuculine (Figure 5C, lower traces). While Syn-ChR2 neurons were unable to trigger light-induced APs at 6 weeks, the majority of cells (7/8) at 10-12 weeks could fire at least one AP in response to trains of light stimulation, and some (2/8) could maintain firing rates of up to 10 Hz, although the APs appeared immature in nature (e.g. lack of rapid repolarization, Figure 5Dii). At later timepoints (>3 months), some individual mCherry+ cells became visible to the naked eye, and most (7/10) could fire repetitive trains of APs in response to ChR2 stimulation (Figure 5Diii), wherein APs appeared more mature with faster kinetics and reduced refraction times. Lastly, in co-cultures with wild-type WA09-derived neurons (Figure 5E, upper panels), recordings from non-ChR2 neurons revealed the presence of repeatable light-induced PSCs that could be blocked with bicuculine (Figure 5E, traces), demonstrating their ability to form functional synapses with neurons from other sources.
The present study demonstrates the utility of optogenetic technology for controlling the functional output of transplantable stem cell-derived neurons. In addition to the creation of a pluripotent cell line whose excitability can be optically regulated when differentiated to neurons, our results represent the first demonstration that hESC-derived neurons are fully competent to form functional neural networks in vivo. Previous reports demonstrated that hESC-derived neurons could fire APs and could receive synaptic input from host neurons in acute slice preparations  or when deposited onto rat hippocampal slice cultures [2, 6]. We have extended these findings to show that hESC-derived neurons transplanted to neonatal SCID mice can act as a functional unit of output, capable of sending synaptic information to adjacent neurons. The fact that this activity can be regulated by ChR2 activation provides a tool for assessing the activity-dependent nature of synaptic integration and functional recovery following transplantation. This was possible in the absence of exogenous retinol which is required in some systems , indicating that endogenous retinol levels in SCID mouse brains are sufficient for ChR2 activation. Furthermore, survival of ChR2-expressing neurons was maintained for up to 6 months in vivo, raising hopes for longitudinal behavioral studies employing implantable LED or diode laser devices .
The combination of hESC and ChR2 technologies has broad potential for basic research as well as applied science. First, hESC/ChR2 technology will simplify the study of functional development and plasticity of human neurons both in vitro and in vivo. For instance, we delineated a temporal dependence of ChR2-mediated AP production in hESC-derived neurons. This technique could be extended to examine synaptic development , plasticity , or the crosstalk between cation influx (e.g. calcium) and the activation of other receptors such as metabotropic glutamate receptors . ChR2 activation may also facilitate the study of activity-dependent signal transduction and gene expression cascades such as those that occur during neuronal differentiation of stem cells . Lastly, it will allow researchers to definitively determine the integration capacity of hESC-derived neurons following transplantation, similar to studies conducted on newly born adult hippocampal neurons . Previous attempts to demonstrate graft-to-host connectivity relied upon technically challenging dual patch clamping methods or non-specific extracellular stimulations . Now, as we demonstrate in the present study, it is possible to genetically restrict stimulation to the stem cell-derived population while simultaneously amplifying output by activating many transplanted neurons simultaneously. This will increase the probability of demonstrating functional connectivity between various neuronal subclasses, as well as to examine local microcircuitry.
For translational studies, the Syn-ChR2-mCherry hESC line can be combined with directed differentiation of various neuronal subtypes (e.g. midbrain dopamine neurons) and implantable light stimulation devices . This will provide researchers with a minimally invasive tool to examine cell replacement strategies for neurodegenerative disorders in vivo. By modulating the amount of light excitation of ChR2+ neurons one might be able to regulate the therapeutic effects, and potentially minimize side effects, of transplanted cells. This may be further aided by subsequent genetic modifications that allow for cell-type specific cell sorting to enhance population purity . Furthermore, ChR2 technology may assist in dissecting the optimal patterns of neural activity (e.g. tonic vs. phasic spiking) necessary for functional recovery of disease models of neurodegeneration such as Huntington's disease (HD), Amyotrophic Lateral Sclerosis (ALS), as well as PD. Furthermore, newly-developed optrode technologies [43, 44] can be used to detect real time neural excitation during in vivo stimulation as a method to correlate behavioral responses with the degree of hESC-derived neuronal stimulation, similar to in vivo mapping of neural circuitry .
While stem cell-based optogenetic technology represents a significant advancement for regulating the physiological state of transplantable cells, significant challenges still exist for its application. For instance, ChR2 expression level, light intensity, and cellular RMP may all affect the fidelity of light-induced AP firing in individual cells [12, 18]. We have attempted to circumvent one of those issues by creating a cell line with relatively uniform ChR2 expression. While expression increased with developmental age, the variability of ChR2-induced currents was significantly decreased compared with transient infection at each time point tested and most could respond to light intensities consistent with previous reports in rodent neurons [16, 18]. Thus, a clonal stem cell line offers a source of human neurons with predictable functional responses to light stimulation.
We would like to thank Laura Stenton, Kyle Mangan, and Matthew Jones for technical assistance with acute slice recordings, Baoyang Hu for assistance with animal transplantation, and Thomas Richner for assistance with the LED stimulation device and light monitoring. The project was supported by NINDS, NS045926 and NS057778, and partly by a core grant to the Waisman Center from the National Institute of Child Health and Human Development (P30 HD03352). Austin Johnson was supported by Rath Distinguished Graduate Student Fellowship.
The project was supported by NINDS, NS045926 and NS057778, and partly by a core grant to the Waisman Center from the National Institute of Child Health and Human Development (P30 HD03352).
Jason P. Weick: Conception and design, collection and/or assembly of data, data analysis, manuscript writing, final approval of manuscript
M. Austin Johnson: Conception and design, collection and/or assembly of data, manuscript writing, final approval of manuscript
Steven P. Skroch: Provision of study material, data analysis and interpretation, final approval of manuscript
Justin C. Williams: Provision of study material, final approval of manuscript
Karl Deisseroth: Provision of study material, final approval of manuscript
Su-Chun Zhang: Conception and design, financial support, data analysis and interpretation, manuscript writing, final approval of manuscript
DISCLOSURE OF POTENTIAL CONFLICTS OF INTEREST
The authors indicate no potential conflicts of interest.