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We recently established a novel method for generating functional human retinal ganglion cells (RGCs) from human induced pluripotent cells (hiPSCs). Here, we confirmed that RGCs can also be generated from human embryonic stem cells (hESCs). We investigated the usefulness of human RGCs with long axons for assessing the effects of chemical agents, such as the neurotrophic factor, nerve growth factor (NGF), and the chemorepellent factors, semaphorin 3A (SEMA3A) and SLIT1. The effects of direct and local administration of each agent on axonal projection were evaluated by immunohistochemistry, real-time polymerase chain reaction (PCR), and real-time imaging, in which the filopodia of the growth cone served as an excellent marker. A locally sustained agent system showed that the axons elongate towards NGF, but were repelled by SEMA3A and SLIT1. Focally transplanted beads that released SLIT1 bent the pathfinding of axons, imitating normal retinal development. Our innovative system for assessing the effects of chemical compounds using human RGCs may facilitate development of novel drugs for the examination, prophylaxis, and treatment of diseases. It may also be useful for observing the physiology of the optic nerve in vitro, which might lead to significant progress in the science of human RGCs.
Optic nerve diseases, including congenital anomalies1,2, neuritis3, and glaucoma4, are the principal causes of severe visual impairment in humans. Despite the varied pathogenesis of optic nerve diseases, including genetic abnormalities5,6, inflammation, trauma7, demyelination3, and glaucoma, retinal ganglion cell (RGC) injury, resultant cell death occurs in all these diseases8. At the early stage of most of these diseases, the axon of the RGC, rather than the cell body, is the first part of the cell to be injured, and this induces cell body apoptosis9,10. Therefore, a better understanding of RGC axons is the key to elucidating the pathogenesis and the pathological conditions underlying these optic nerve diseases. In addition, the main physiological role of RGCs is to transmit retinal information to the brain, and to this end, RGCs have developed unusually long axons11. Therefore, in order to elucidate the pathogenesis of optic nerve diseases and the physiological functions of RGCs, as well as to treat optic nerve diseases, it is important that research extends beyond the current studies of animal models that employ axonal crush12,13 to also focus on in vitro generation of RGCs with characteristically long axons.
Numerous animal models of optic nerve diseases have been established for in vivo studies, including high ocular pressure models of mice, rats, sheep, and pigs14–16, optic nerve crush models, and glutamate/aspartate transporter-deficient mice for the assessment of normal-tension glaucoma17. These animal models provide useful tools for investigating pathogenesis and the resulting pathological condition of human diseases. However, possible differences between animal and human cells pose serious obstacles to the interpretation of the results in a clinical context, particularly in term of the evaluation of pharmacokinetics and drug effects. Moreover, in those in vivo models, the pathological status and drug effects are assessed mainly by evaluating the structure of the inner retina or the optic nerve by histopathology and optical coherence tomography18, as real-time observation of RGCs and their axons has been difficult. Thus, an in vitro system has a clear advantage in terms of allowing a more detailed, precise, direct, and real-time observation of RGCs.
Several in vitro models have been suggested as the in vitro glaucoma model, in which the effect of hydrostatic pressure on RGCs isolated from the retina of mice and other rodents were analysed19. However, these isolated cells were only sustainable on culture dishes for a few weeks, and did not exhibit the characteristic axons20. Therefore, these cells are considered unsuitable for use as in vitro glaucoma models, because they may not have sufficient resilience to tolerate stress, including hydrostatic pressure19,21 and N-methyl-D-aspartate (NMDA) supplementation22. Sustainable human RGCs with their characteristically long axons would be the most suitable models for discovering candidate drugs, but the cells are available exclusively from the retina of human cadavers using immunopanning23 and the number of available human cells is limited. Moreover, the characteristics and functions of the axons of RGCs, which play a crucial role in mechanisms involving optic neuropathies, have not been demonstrated in RGCs isolated from human cadavers. Consequently, establishment of sustainable RGCs with axons from human stem cells is highly desired.
We have recently established a novel method for generating RGCs with functioning and stable long axons from human induced pluripotent cells (hiPSCs). Our RGCs survive for approximately 50 days and are generated with an efficiency of 90%24. In this experiment, we employed 3-dimensional (3D) and 2-dimensional (2D) culture methods to culture floating aggregates of hiPSCs as embryoid bodies (EBs). EBs were induced into a retinal cell lineage and subsequently into 3D cultures of optic vesicles (OVs). OVs are the primordia of the retina and extrude from the EBs. EBs were then transferred to culture dishes as 2D cultures, which resulted in both the generation of RGCs at the marginal portion of the attached OVs and in the extension of long radial axons with physiological functioning.
Upon injury to the optic nerve, RGCs experience cell death, which is a physiologically irreversible phenomenon. Therefore, treatment of optic nerve diseases relies upon novel drug development for neuroprotection and nerve regeneration, and possibly upon the transplantation of human RGCs. In the current study, we show that RGCs can also be generated from human embryonic stem cells (hESCs) using the protocol we previously established for generating RGCs from hiPSCs24. We also investigated the utility of our RGCs, which contained numerous firm, long axons elongating in the same direction, for assessing the effects of administered neurotrophic and chemorepellent agents. We evaluated nerve growth factor (NGF) as a neurotrophic factor, and semaphorin 3A (SEMA3A) and SLIT1 as chemorepellent factors, in which various in vitro analyses of the nerve elongation pattern, nerve pathfinding, including real-time nerve pathfinding, and the growth cone, were carried out.
Human embryonic stem cells (hESCs) (HES0001_KhES-1) and induced pluripotent stem cells (iPSCs) (HPS0007_409B2, cell passage 29) were obtained from RIKEN BRC (Japan) and cultured as described previously24. Briefly, cells were maintained on mouse embryonic fibroblasts (MEFs) in primate ES medium (ReproCELL) supplemented with recombinant human basic fibroblast growth factor (Invitrogen). For passaging, cell colonies were detached using dissociation solution (ReproCELL) and detached clumps of hESCs and hiPSCs were broken into smaller portions. Cells were passaged at split ratios of 1:3 to 1:4.
The use of hESCs and hiPSCs in this study was approved by the Ethics Committee of the National Institute for Child and Health Development (NCCHD), Tokyo (approved #ES-Rin 261).
RGCs were induced from hESCs and hiPSCs based on methods that involve a serum-free floating culture of EB aggregates25 and our previously established approach24. For a short period, hESCs and hiPSCs were dissociated into single cells and were resuspended in retinal differentiation medium (RDM; G-MEM supplemented with 20% KSR, 0.1 mM nonessential amino acids, 1 mM pyruvate, 0.1 mM 2-mercaptoethanol, 100U/mL penicillin, and 100 mg/mL streptomycin). After separation from the feeder cells, floating hESCs and hiPSCs were collected and seeded into V-bottomed plates (Sumitomo Bakelite, Tokyo, Japan) at 9,000 cells per well. On the second day (D2) after initiating suspension (D0), Matrigel (BD Bioscience) was added, and on D12, the aggregates were transferred to 24-well plates (BD Bioscience) and the medium was replaced with RDM containing 1.0% Matrigel and 1.0% fetal bovine serum (FBS). On D15, CHIR99021 (3µM; Wako Pure Chemicals) and SAG (100 nM; Enzo Life Science) were added to the medium and the suspension culture was continued for another 3 days. EBs were transferred to retinal maturation medium (RMM; DMEM/F12-Glutamax medium containing the N2 supplement, 100U/mL penicillin, and 100mg/mL streptomycin) on D18 and cultured in the absence of FBS for 6 days. On D24, OVs started to extrude, and 1.0% FBS and retinoic acid (0.5µM; Sigma−Aldrich) was added to the RMM. On D27, adhesion culture was initiated when EBs were transferred to poly-d-lysine/laminin-coated 24-well plates with the supplementation of brain-derived neurotrophic factor (100ng/mL BDNF, R&D Systems) instead of retinoic acid.
Real-time polymerase chain reaction (PCR) was performed as previously described24 using an RNeasy Mini Kit and analysed using a One Step SYBR PrimeScript PLUS real-time PCR Kit (Takara Bio Inc.) and StepONE Sequence Detection System (Applied Biosystems). The primers used in this study are listed in Supplementary Table S1.
To assess the presence of characteristic markers of RGCs (Fig. 1), the amount of mRNA, relative to D0, specific to each of the target genes, was calculated using the 2−ΔΔCT method. The expression of mRNA was assessed by evaluating threshold cycle (CT) values. The CT values were firstly normalised to the expression level of hypoxanthine phosphoribosyl transferase 1 (HPRT1), and the relative amount of mRNA specific to each of the target genes was calculated using the 2−ΔΔCT method. For evaluating the effects of chemical agents, the amount of mRNA relative to the amount of control mRNA was calculated. The sample size for all mRNA data was five (n=5).
Immunostaining was performed as described previously24 using frozen sections or entire cells fixed in 24-well plates and 3.5-cm film-bottom dishes (Matsunami Glass). The stained cells were viewed with an IX71 inverted research microscope (Olympus) and a DeltaVision ELITE fluorescence microscope (CORNES Technologies). Frozen sections were prepared as previously described24. Hematoxylin and eosin staining of 3-μm-thick specimens was performed as previously described24. Growth cone immunostaining was performed by attaching OVs to 3.5-cm film-bottom dishes on D28, 1 day after administration of chemical agents, and conducting double-staining with phalloidin and GAP43 antibody. The primary antibodies and their respective dilutions used in this study are listed in Table 1, and negative controls for these antibodies are indicated in Fig. S1.
Recombinant human NGF (R&D Systems), SEMA3A (R&D Systems), and human SLIT1 (R&D Systems), diluted in Dulbecco’s phosphate-buffered saline (DPBS, Life Technologies) were used as candidate agents with a potential to affect the axonal growth of hESC- and hiPSC-derived RGCs. DPBS was used as the control. These were added to RMM at final concentrations of 50, 100, or 200ng/ml for NGF and SEMA3A, and 0.2, 1, 2, or 5μg/ml for SLIT1. Further, SEMA3A and SLIT1 were supplemented on D27, at the time of attachment. For the supplementation assay of NGF, the induction protocol of RGCs was slightly modified, because the previously established protocol induced maximal growth of RGC axons. In particular, the supplementation of NGF was initiated on D24 without FBS or retinoic acid. On D27, attachment of floating EBs was achieved in the absence of FBS or BDNF26. Supplementation of these agents was continued until D30, 3 days after attachment, and the colonies were collected on D30.
A quarter piece of hydrogel (Hydrogel #SP PI5, MedGel) was used as a carrier. Recombinant human NGF, diluted in reduced Matrigel (BD Bioscience), was used at 10ng/ml, and SEMA3A, diluted in reduced Matrigel (BD Bioscience), was used at a concentration of 200ng/ml, while recombinant human SLIT1 (R&D Systems), diluted in Matrigel, was used at concentrations of 5µg/ml at a temperature of approximately 4°C. Matrigel without the agents was used as the control. Each EB was adhered to the centre of a well in 24-well plates. Matrigel was absorbed by the piece of hydrogel, which was placed at the edge of each well of the 24-well plates, in front of the attached OVs on D29 (Fig. S2). On D31, 2 days after the administration of the respective agents, colonies were fixed and immunostained using neurofilament protein L (NFL) antibodies. Each experiment was repeated at least five times.
Affi-gel Blue beads (Bio-Rad) were used as carriers for the sustained release of chemical agents. Beads were washed in DPBS and then incubated for 1 h at room temperature (20°C) in solutions containing chemical agents at different concentrations. Recombinant human NGF (R&D Systems) and SEMA3A (R&D Systems) diluted in DPBS were used at a concentration of 200ng/ml, and recombinant human SLIT1 (R&D Systems) diluted in DPBS was used at a concentration of 5μg/ml. Beads without the agents were used as the controls. Beads were transplanted on D28, one by one, at the site near the base of attached OVs using forceps (Inami) and fine needles (TERUMO) under a microscope (Olympus). Because the filopodia of axons are away from the attached OV on D29, i.e., the day of starting administration of the agents by means of hydrogel, we transplanted the beads on D28 when the filopodia are located close to the OVs. Each experiment was repeated at least five times.
A protocol similar to the one described for the local and sustained agent release assay was used to observe time-lapse analysis of axonal growth. A piece of hydrogel containing SLIT1 (5μg/ml) diluted in Matrigel was placed in front of attached OVs on D29. Time-lapse observation was performed for 18 h in a STX Stage Top Incubator (TOKAI HIT) and imaged using an IX71 inverted research microscope (Olympus).
All statistical analyses were performed using PASW statistics 18 (IBM) software with values expressed as mean±standard deviation (SD). Groups of measurements were compared using one-way analysis of variance (ANOVA) followed by Tukey’s honestly signify difference (Tukey-HSD) test for normally distributed variables, and Dunnett’s T3 test for variables of non-normal distribution. Probability values equal to or smaller than 5% were considered significant. In the current experiment, there was no non-parametric data.
We attempted to generate RGCs from hESCs using the same protocol as used for the generation of RGCs from hiPSCs24. Real-time PCR revealed that characteristic RGC markers, such as ATOH7 27, BRN3B 28, TUJ1, γ-synuclein (SNCG)29, and ISLET1 30, were expressed more on D30 as compared with their expression on D0. In particular, the expression level of BRN3B—a highly specific marker for RGCs28—was increased more than 1000-fold (Fig. 1a). These results correspond to results reported for markers of hiPSC-derived RGCs24. Immunohistochemistry on D30 revealed that BRN3B-positive RGCs tended to be located on the peripheral margin of attached OVs. Similar findings were noted in SNCG, and ATOH7 and ISLET1-positive cells that were also detected at the margin and the centre of attached OVs. Staining of TUJ1 was evident at the radiating axons that developed from the attached OVs. Double-staining with ATOH7 and TUJ1 indicated that TUJ1-positive axons originated from ATOH7-positive RGCs. (Fig. 1b). These results demonstrated that RGCs can be generated from hESCs using the same protocol that is used to generate RGCs from hiPSCs. Furthermore, we confirmed that hESC-derived RGCs possess the same physiological functions, including axonal transport and action potentials, as those reported for hiPSC-derived RGCs24 (Fig. S3, and Supplementary Movie 1). Using puff application of 1 mM glutamate, we also observed an inward current and repetitive action potentials (Fig. S4).
Combining the results of our current and previous studies confirms that hESC- and hiPSC-derived RGCs expressed characteristic molecular and electrophysiological markers of RGCs. Therefore, hESC-derived RGCs were ready for use in the in vitro evaluation of the effects of neurotrophic and chemorepellent agents.
We first investigated the availability of hESC- and hiPSC-derived RGCs in order to evaluate the effects of totally and locally administrated growth factor. NGF (a growth factor regulating the growth and survival of nerve cells31) was added to floating aggregates in the culture media on D24, at concentrations of 0, 50, 100, and 200ng/ml. After attachment to the well on D27, supplementation was continued for another 3 days. Immunohistochemistry by NFL-staining revealed a starkly increased number and length of axons following the supplementation of NGF to each well (Fig. 2a). Growth of axons of hESC- and hiPSC-derived RGCs was significantly promoted by 200ng/ml NGF supplementation, and there was no difference between hESC- and hiPSC-derived RGCs (Fig. S5f).
These results were supported by real-time PCR data of the axonal markers NFL 32 and TAU 33. In RGCs generated from hESCs and from hiPSCs, the NFL expression levels were upregulated with NGF supplementation at concentrations of 50, 100, and 200ng/ml, as compared with samples from control conditions (ANOVA, Dunnett’s T3 test, P≤0.05). The expression pattern did not change in a dose-dependent manner. The expression of TUJ1 tended to be upregulated by NGF supplementation; however, the increase was not statistically significant (Fig. 2b). The upregulation of NFL by NGF supplementation was clearly inhibited by K252, which is an established NGF receptor antagonist (Fig. S6).
We investigated the usefulness of our hESC- and hiPSC-derived RGCs for evaluation of the effects of totally and locally administrated suppression factors. SEMA3A, which guides axonal growth by chemorepulsion via growth cone collapse34, was added to each well of hESC- and hiPSC-derived RGCs on D27, and supplementation was continued for 3 days at concentrations of 0, 50, 100, or 200ng/ml. Immunohistochemistry using NFL staining revealed that the number and length of axons markedly decreased after SEMA3A supplementation (Fig. 3a). Growth of axons of hESC- and hiPSC-derived RGCs are significantly decreased by 200ng/ml SEMA3A supplementation, and there was no difference between hESC- and hiPSC-derived RGCs (Fig. S5d).
These results were supported by RT-RCR data of the axonal markers NFL, TAU, and TUJ1. In RGCs generated from hESCs and from hiPSCs, the expression level of NFL was significantly downregulated at a concentration of 200ng/ml SEMA3A, compared with the control (ANOVA, Tukey-HSD test, P≤0.05). The downregulation tended to be dose-dependent. Expression of TAU and TUJ1 was significantly downregulated at a concentration of 200ng/ml SEMA3A (ANOVA, Tukey-HSD test, P≤0.05). Expression levels tended to be lower relative to control levels for all three concentrations tested; however, this trend was not statistically significant for concentrations of 50 and 100ng/ml (Fig. 3b).
We investigated the usefulness of our hESC- and hiPSC-derived RGCs for evaluation of the effects of a totally and locally administered nerve bending factor during pathfinding. SLIT1, which plays an important role in axonal guidance by sending repulsive signals to the axon35, was added to each well of hESC- and hiPSC-derived RGCs on D27 at concentrations of 0.0, 0.2, 1.0, and 5.0μg/ml. Immunohistochemistry using NFL staining revealed no inhibition of axonal growth, as compared with the control. However, we observed a change in axon morphology; rather than growing straight, several axons grew windingly, indicating axon misguidance (Fig. 4a). The grown axonal length of hESC- and hiPSC-derived RGCs was not decreased by supplementation with 5μg/ml SLIT1 (Fig. S5e). These results were supported by RT-RCR data of the axonal markers NFL, TAU and TUJ1; expression levels tended to be similar to those of the control at all concentrations (Fig. 4b).
We next investigated the effects of local and sustained delivery of NGF from hydrogel or focally transplanted beads. A piece of hydrogel containing NGF (10ng/ml) was placed inside the well in front of the OV 2 days after attachment, on D29, and culture was continued for 2 more days. NGF hydrogel promoted axonal growth of hESC- and hiPSC-derived RGCs (Fig. 5b,f, respectively), as compared with controls (Fig. 5a,e, respectively). Phalloidin and GAP43 staining confirmed that filopodia of hESC- and hiPSC-derived RGCs (Fig. 5c,g, respectively) were normally organised and their growth was slightly promoted after NGF treatment (Fig. 5d,h, respectively). Beads containing NGF (200ng/ml) were transplanted beside the OV 1 day after attachment, but no obvious effect was observed (Fig. S7).
We next investigated the effects of local and sustained delivery of SEMA3A from hydrogel or focally transplanted beads. A piece of hydrogel containing SEMA3A (200ng/ml) was placed inside the well in front of the OV 2 days after attachment on D27, and culture was continued for 2 more days. SEMA3A-hydrogel locally inhibited elongation of axons, as revealed by immunohistochemistry, indicating the chemorepellent effects of SEMA3A on axonal growth (Fig. 6a,b,d,e). The morphology of the filopodia was not maintained and collapsed after SEMA3A supplementation (Fig. 6c,f). Effects were similar for hESC- and hiPSC-derived RGCs. Beads containing SEMA3A (200ng/ml) were transplanted beside the OV 1 day after attachment, but no obvious effect was observed (Fig. S8).
We next investigated the effects of local and sustained delivery of SLIT1 from hydrogel or focally transplanted beads. A piece of hydrogel containing SLIT1 (5μg/ml) was placed inside the well in front of the OV 2 days after attachment on D27; the culture was then continued for 2 more days. SLIT1-hydrogel did not inhibit axonal growth. However, a subset of axons progressed as if avoiding the hydrogel (Fig. 7a,b,d,e), in both hESC- and hiPSC-derived RGCs, which was calculated using hESC-derived RGSs (Fig. S9). The morphology of the lamellipodia, rather than filopodia, was not maintained, and collapsed following SLIT1 supplementation (Fig. 7c,f). Similar effects were noted for hESC- and hiPSC-derived RGCs. Beads containing SLIT1 (5μg/ml) were transplanted beside the OVs (Fig. 8) 1 day after attachment. In RGCs derived from both hESCs and hiPSCs, axons located close to the beads formed a bend, avoiding the area close to SLIT1-beads (Fig. 8b,d, respectively), compared with the control (Fig. 8a,c, respectively).
In the above experiments, SLIT1 acted as a chemorepellent for axonal growth in hESC- and hiPSC-derived RGCs. Therefore, real-time axonal pathfinding was imaged in vitro during local and sustained release of SLIT1 from hydrogels placed in front of attached OV for 18 h. We found that a subset of axons actively regressed while other axons actively changed their path to avoid the SLIT1-hydrogel both in hESC- and hiPSC-derived RGC cultures (Supplementary Movie 2).
In the current study, we first demonstrated that RGCs could also be generated from hESCs using the same protocol as for the generation of RGCs from hiPSCs. Minute differences between these two types of cells have been reported previously, such as variations in the expression patterns of non-coding RNAs36,37. However, organogenesis of the islets of the pancreas, nephrons, and, the pituitary gland has been reported from both hiPSCs, and hESCs. In accordance with these reports, most of the RGC markers tested, including by means of assays of genes expression, protein expression, axonal transport, and action potential firing, were similar for RGCs derived from hESCs and from hiPSCs24. Therefore, RGCs can be generated from both stem cell types, and the RGCs should be equally useful as a model of human RGCs.
The technique for the in vitro generation of RGCs from hiPSCs produced these cells with 90% efficacy and cells remained stable for around 50 days24; RGCs were similarly generated from hESCs (data not shown). We then evaluated the effects of neurotrophic and chemorepellent agents on the RGCs derived from hESCs and hiPSCs, generated in this study. To assess the general effect of each of these agents, we added them to each culture well, and to observe the local effects of the agents, we used hydrogel and focally transplanted beads as carriers for these agents. The hydrogel was placed in front of the attached OV, which enabled us to observe the nerve pathfinding in the context of the sustained release agents from the gel. On the other hand, focally transplanted beads enabled us to observe the effect of the agents on axonal pathfinding of the RGCs released from the inner portion of primordium of the retina, i.e., the attached OV.
We initially examined the possible application of the RGCs from hESCs and hiPSCs for the assessment of neurotrophic agents in vitro using NGF as a neurotrophic factor. NGF supplementation to the entire dish promoted axonal growth in RGCs, even at the lowest concentration tested (50ng/ml). The mRNA expression levels of axonal structure-related genes supported this result. When release of 10ng/ml NGF was locally sustained using hydrogel, RGC axon growth toward the hydrogel was also promoted. NGF is an important growth factor regulating growth and survival of nerve cells through tropomyosin receptor kinase A (TrkA)31 and p75NTR receptor binding. TrkA positively regulates cell survival38,39; in contrast, p75NTR induces nerve cell death by apoptosis40,41. Some researchers have demonstrated that NGF treats glaucoma effectively42,43, while others have published negative results44. This ambiguity can probably be explained by the bilateral effect of NGF45. Axons were successfully promoted by 200ng/ml NGF supplementation to the entire dish, but the promotion was observed at a lower dose (10ng/ml NGF) in locally placed hydrogel assay, which may be because of the positive and negative effects of NGF on RGC survival.
For the NGF assay, we first applied NGF to the dish from D27, the day of attachment, in line with our original induction method, but no significant axonal promotion was observed (data not shown). We considered that the effects of NGF may have been masked by the BDNF contained in the culture medium26,46 and by other neurotrophic factors that may have been present in FBS. We therefore excluded BDNF and FBS from the cultures from D24, and added NGF. This in vitro assessment system enabled us to analyse the effects of NGF on the promotion of axons of RGCs precisely in vitro.
Secondly, we examined the effects of the chemorepellent agents SEMA3A and SLIT1 on RGCs. Supplementation of SEMA3A to the whole dish inhibited axonal growth of RGCs in a dose-dependent manner. Inhibition of axonal growth was confirmed both by immunohistochemical analysis and by analysis of the mRNA expression levels of axonal makers NFL, THJ1, and TAU. In contrast, SLIT1 affected neither axonal elongation nor expression levels of axonal markers. Judging from immunohistochemical analysis, SLIT1 only seemed to affect pathfinding of some axons, resulting in complex axonal elongation patterns. In further experiments on local sustained release of SEMA3A and SLIT1, most axons seemed to be repelled by SEMA3A release, in contrast to a subset of axons affected by SLIT1 release. Although growth cone collapse was directly observed by double-staining of phalloidin and GAP43, both under SEMA3A and SLIT1 supplementation, these results may indicate that SEMA3A indiscriminately induces collapse of axonal cones, while SLIT1 only induces the collapse of specific cones expressing the roundabout (Robo) receptor.
Semaphorins and SLITs are highly conserved proteins in both vertebrates and invertebrates47,48; members of both of these families achieved chemorepulsion via growth cone collapse, in concert with neuropilins 1/2 and A-plexins49 and Robo receptor35,47, respectively. In comparison with the semaphorins, which also play a crucial role in the development and morphogenesis of various organs34,50–52, SLITs are more locally expressed in the central nervous system, including in the eye53,54. Expression of SEMA3A has been detected in the RGCs of rat and zebra fish retina55,56, and RGC growth was repelled by SEMA3A in Xenopus RGCs57. Expression of SEMA3A has also been detected near the optic chiasm and in the optic tectum of zebra fish56. SLIT/Robo signalling also plays a crucial role in navigating RGC axons in the developing retina. SLIT1 and −2 are expressed in the RGC itself and in the inner nuclear layer, and they determine the polarity of axons in the nerve fibre layer58. SLITs are also expressed at the optic chiasm and the optic tract and act as chemorepellent factors. Although both SAMA3A and SLIT1 appear to influence RGC development in a similar fashion, SEMA3A seems to have more impact on RGC development than SLIT1, according to the results of the current in vitro experiment. Further experiments are needed to determine why different results were obtained for the two molecules. Nonetheless, this study demonstrates that the in vitro assessment system developed here significantly facilitates evaluation of the effects of these molecules on human RGCs.
In the assay for screening of chemical agents, the effect of each axon guidance factor on RGCs was clearly assessed, in which the length of axons and its molecular markers changed, depending on the respective dosages. Local administration of those axon guidance factors further confirmed the effect of each axon guidance facto on the axons; NGF promoted axonal elongation in the direction of the agent and SEMA3A and SLIT1 had a chemorepellent effect on axons. Direct observation of growth cones revealed that these phenomena were achieved through changes in the shape of the filopodia. These novel in vitro observations were possible only because the RGCs established in this study developed elongated axons with numerous growth cones; similar observations would have been impossible using RGCs isolated from animal and human retinas. It was possible to culture a large number of RGCs using our protocol, and it may be possible to enhance the method in future, for instance, through pharmaceutical analysis of RGCs supplemented with various candidate drugs, using molecular experiments, including microarrays.
In contrast to total and local axon guidance factor administration, focal transplantation of beads containing each axon guidance factor allows more precise observation of the effects on nerve pathfinding. To investigate focal effects of NGF, SEMA3A, and SLIT1 on axonal pathfinding of RGCs, we transplanted beads containing the respective molecules close to the attached OVs from which the RGCs developed. In our experiments, focal sustained release of NGF and SEMA3A had little impact on axonal pathfinding, while focal sustained release of SLIT1 resulted in the rerouting of RGC axons. As discussed above, SLIT1 is expressed at the inner nuclear layer of the developing retina, and plays a crucial role in determining the polarity of axons, by restricting axon progression into the nerve fibre layer59. In addition, SLITs are expressed in the optic chiasm, causing Robo-expressing growth cone collapse and resulting in commissural axons60. In the current study, SLIT1-containing beads were transplanted at the time of initial axonal development. Therefore, focal sustained SLIT1 possibly mimics the phenomenon in vitro.
Time-lapse observation for monitoring SLIT1-induced axon repulsion was performed with the use of a locally sustained axon guidance factor system. Our analysis revealed that different axons reacted differently to SLIT1-containing hydrogel, in which some growing axons changed path and avoided the SLIT1-containing hydrogel, while others regressed. In the developing retina, primitive RGCs develop into several types of RGCs and 90% of RGCs underwent apoptosis61. RGCs generated in vitro by our system could mimic the in vivo developing RGCs. Thus, real-time observation of such cultures might aid our understanding of unknown developmental events of RGCs in vitro.
In the current and in a previous study, we established a method for generating human RGCs derived from hESCs and hiPSCs. In this study, we have developed an in vitro evaluation system for human RGCs that allows analysis of the effects of biomolecules in vitro and that may be useful for potential drug discoveries. We confirmed that the general effects of the agents were analysable through supplementation of each well. The nerve pathfinding and the growth cone were observed by locally used hydrogel and Affi-Gel blue. Chemorepellent factors were easier to analyse than neurotrophic factors. In addition, we established a real-time observation system for the human RGCs in vitro, in which the physiological selection process of RGCs was observed.
It has been difficult to obtain live, human neuronal cells, particularly RGCs, to date. However, due to the differentiation method we established in this study and to the methods other groups have developed62–64, the availability of human RGCs may now be significantly improved. Gill et al. developed stepwise retinal differentiation of hESCs, from which RGCs are selected by the MACS isolation method, by labelling THY1.1. Although these RGCs have long axons and physiological function, as do ours, the axons seems to be heterogeneous64. Sluch et al. also attempted to obtain purified RGCs derived from CRISPR-engineered hESCs, in which axons of the RGCs elongated through nanofibre matrices, and concluded that forskolin may be a potent promoter of RGC differentiation63. Compared with the previous reports, our system has a limitation regarding purification or isolation of RGCs, because they are accompanied by several cells inside the attached OVs and EBs. On the other hand, a remarkable advantage of our method for generating RGCs, which is achieved only by co-culture of EBs and OVs, is that it obtains uniform, straight-radiating, abundant, and long axons in RGCs from the attached OVs. These enriched axons allowed us to observe the physiology of the axons of human RGCs in real-time and to analyse the effects of neuroactive agents on RGCs, including the promotion and inhibition of axons and their pathfinding, and the effects of neuroactive agents applied at different times, concentrations, and combinations. Until fairly recently, animal experiments and clinical trials have been necessary for the exploration of new drugs, including neuroprotective agents, because human cells were difficult to obtain, and thus the effect of the drugs on human cells could not be determined. The current approach for using RGCs derived from hESCs and hiPSCs for developing new drugs is costly and time-consuming, and has prevented the speedy exploration of new drugs. The potential drug screening system that we propose may shortcut the process.
The generation of iPSCs by reprogramming patient tissue is now a routine procedure65 and new drugs have been explored in vitro for the treatment of diseases, such as Parkinson’s and Alzheimer’s disease, which are resistant to medication; this is an obvious advantage of using iPSCs. For example, using cortical neurons derived from fibroblasts of patients with autosomal dominant or sporadic Alzheimer’s disease, docosahexaenoic acid has been demonstrated to be effective in a subset of patients66. Forebrain neurons derived from patients with Parkinson’s disease have been used to screen potential new drugs. In these screenings, Nedd4, and NAB2 were identified as candidate drug molecules67. Our method of generating human RGCs, with their characteristic axons, provides a potential system for the in vitro screening of drugs that may have neuroprotective and neuro-regenerative functions in the human RGC; such screening is already underway in our laboratory. The system presented in the current study may aid our understanding of the physiological development of RGC axons and enable us to develop new drugs that would significantly improve the quality of life of patients with treatment-resistant optic neuropathies.
This work was supported by JSPS KAKENHI (grant numbers 22390327 and 24659770), and a grant from the National Center for Child Health and Development (number 28-2).
T.Y. and T.T. performed experiments, analysed and interpreted data, and wrote the manuscript. E.M. performed experiments, and analysed and interpreted data. F.T. and S.W. designed and performed the electrophysiological recordings and contributed to the writing of the manuscript. S.N. interpreted data. N.A. designed experiments and supervised the project. All authors read and approved submission of the manuscript.
The authors declare that they have no competing interests.
Tadashi Yokoi and Taku Tanaka contributed equally to this work.
Electronic supplementary material
Supplementary information accompanies this paper at 10.1038/s41598-017-16727-1.
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