SNAP-25 is a core component of the trimeric SNARE complex mediating vesicle exocytosis during membrane addition for neuronal growth, neuropeptide/growth factor secretion, and neurotransmitter release during synaptic transmission. Here, we report a novel microRNA mechanism of SNAP-25 regulation controlling motor neuron development, neurosecretion, synaptic activity, and movement in zebrafish. Loss of miR-153 causes overexpression of SNAP-25 and consequent hyperactive movement in early zebrafish embryos. Conversely, overexpression of miR-153 causes SNAP-25 down regulation resulting in near complete paralysis, mimicking the effects of treatment with Botulinum neurotoxin. miR-153-dependent changes in synaptic activity at the neuromuscular junction are consistent with the observed movement defects. Underlying the movement defects, perturbation of miR-153 function causes dramatic developmental changes in motor neuron patterning and branching. Together, our results indicate that precise control of SNAP-25 expression by miR-153 is critically important for proper neuronal patterning as well as neurotransmission.
Citation: Wei C, Thatcher EJ, Olena AF, Cha DJ, Perdigoto AL, Marshall AF, et al. (2013) miR-153 Regulates SNAP-25, Synaptic Transmission, and Neuronal Development. PLoS ONE 8(2): e57080. doi:10.1371/journal.pone.0057080
Editor: Erik C. Johnson, Wake Forest University, United States of America
Received: December 1, 2012; Accepted: January 16, 2013; Published: February 25, 2013
Copyright: © 2013 Wei et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was supported by grants from the National Institutes of Health (NIH) to JGP (GM 075790 and EY019759), KB (GM 54544), and BDC (NS038220) and by training fellowships to EJT (T32 GM08556) and ALP (F30 NS061403 and T32 GM07347). Antibodies were obtained from the Zebrafish International Resource Center NIH-NCRR, grant RR12546. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Trimeric soluble N-ethylmaleimide-sensitive factor attachment protein receptor (SNARE) complexes form the core machinery mediating vesicular exocytosis –. In the nervous system, SNARE complexes are involved in membrane addition during neuronal growth as well as both dense core vesicle (DCV) release of proteins and synaptic vesicle (SV) release of fast neurotransmitters. At synapses, the core SNARE protein SNAP-25 interacts with accessory proteins that together regulate SV exocytosis by linking Ca2+ sensing to membrane fusion and neurotransmitter release –. SNAP-25 is a specific target of Botulinum neurotoxin proteases that block vesicle release, resulting in rapid paralysis and death , . Misregulation of SNAP-25 is associated with several human diseases and neurodegenerative disorders including Huntington’s Disease , Alzheimer’s Disease , and diabetes .
SNAP-25 is required for action potential-evoked glutamatergic, cholinergic, and glycinergic transmission in neurons , . Mouse knockouts of SNAP-25 are therefore lethal although neuronal cultures from SNAP-25 null mutants maintain the ability to exhibit stimulus-independent transmitter release , . GABAergic inhibitory synapses express lower levels of SNAP-25 and may be more sensitive to calcium regulation, whereas glutamatergic excitatory synapses express higher amounts of SNAP-25 that alters calcium sensitivity . Part of this differential regulation could be due to accessory proteins that control SNAP-25 distribution and levels to modulate synaptic activity –. Transcriptional mechanisms regulating SNAP-25 levels have also been suggested to play key roles in the dynamic control of synaptic function –.
Several miRNAs have been shown to regulate synapse formation or homeostasis, mostly within the post-synaptic dendrite , , . On the presynaptic side, most forms of regulation center on modulation of calcium channels and calcium-dependent vesicle release , . In this study, we show that miR-153 inhibits SNAP-25 expression in the developing nervous system. Precise control of SNAP-25 by miR-153 is necessary not only for presynaptic vesicle release, but also for protein secretion, motor neuron patterning, and outgrowth.
miR-153 Regulates Embryonic Movement
miR-153 has been proposed to be one of a limited number of ancient miRNAs that evolved with the establishment of tissue identity . It is conserved among bilaterians displaying distinct expression patterns in neurosecretory brain cells of the deuterostome marine worm Platynereis dumerilii and the protostome annelid Capitella . In zebrafish, miR-153 is expressed in distinct regions of the developing nervous system and brain, including neurosecretory cells of the hypothalamus , . Using deep sequencing and in situ localization, we detected robust miR-153 expression in the developing zebrafish brain and reduced, but detectable levels in the spinal cord as early as the 18 somite stage, with progressively increasing expression thereafter ,  .
To determine the function of miR-153, we injected either synthetic miR-153 or antisense morpholinos against miR-153 into single cell embryos and allowed development to proceed for 1–2 days. Two different morpholinos were used to ensure specificity and we verified overexpression and knockdown of miR-153 using northern blots (Fig. S1). No gross morphological changes were observed in injected embryos and normal localization of neuronal markers was detected at the midbrain-hindbrain boundary, inner ear, and retina at 1–2 dpf (data not shown). Despite the lack of morphological changes, we observed striking behavioral movement defects in injected embryos. To quantify movement, embryos were recorded over time (Movie S1) with analyses restricted to embryos within the chorion at 24 hpf. Normal zebrafish embryos move within the chorion with a characteristic frequency of ~1 twitch/minute at 24 hpf (Fig. 1). Strikingly, embryos injected with miR-153 were almost completely motionless, with little or no spontaneous movement, although their hearts were beating normally and minimal movement could be elicited by touch stimulation (Fig. 1). In contrast, knockdown of miR-153 caused a dramatic and significant 7-fold increase in the frequency of spontaneous movement (Fig. 1). Interestingly, upon touch stimulation, miR-153 morphants would initially respond with unusually robust, hyperactive movements after which all motion would cease altogether for a period of time (whether touched or not), followed by a resumption of hyperactive movement upon stimulation. At 52 hpf, miR-153 overexpression fish embryos were still mostly motionless, while miR-153 knockdown embryos were still hyperactive (data not shown).
Embryonic movement was recorded at 1 dpf for each of the singly and multiple injected conditions shown (see Movies). The number of twitches per minute was counted and significance determined by comparing the noninjected control (NIC) embryos to all other conditions using ANOVA with Dunnett’s post-test. *, p<0.05; **, p<0.01. Movements were counted for approximately 60 embryos over 2–5 minutes for each condition.
miR-153 Targets snap-25
To identify mRNAs regulated by miR-153, we used target prediction algorithms, compared the expression patterns of both potential mRNA targets and miR-153, and assayed phenotypes from gain and loss of function experiments. Based on these criteria, snap-25 proved to be a bona fide target for miR-153 based on the results of reporter silencing experiments (Fig. 2) and consistent with conservation of miRNA recognition elements (MREs) from fish to humans (Fig. S2).
(A) GFP reporter constructs were created by fusing the reading frame of GFP to the snap-25a 3′UTR. Two predicted miRNA recognition elements (MREs) were identified in the snap-25a 3′ UTR. The miR-153 sequence is indicated in red and the corresponding snap-25a UTR sequence is shown in green. (B) Single cell zebrafish embryos were injected with mRNAs derived from GFP reporters lacking a UTR (GFP), fused to the full length snap-25a UTR (+snap-25), or mutant versions of the snap-25a UTR lacking individual MREs (snap-25aΔMRE1 and snap-25aΔMRE2) or both MREs (snap-25aΔMRE1&2). Embryos were injected in the presence or absence of exogenous miR-153 or morpholinos against miR-153 (miR-153MO). Fluorescence levels were examined at 1 dpf. Clusters of embryos (~60) are shown as well as a high magnification image of a single representative embryo. (C) Lysates from ~100 embryos were prepared from embryos treated as in B and GFP protein levels were determined by western blotting using antibodies against GFP or control antibodies against α-tubulin. (D) Quantitation of westerns was performed with a paired Student’s t-test (n = 5).
There are two SNAP-25 paralogs in zebrafish (a and b isoforms) with similar, but not identical, 3′ UTRs , . For reporter assays, we fused the 3′ UTR from both snap-25 isoforms to the GFP reading frame (snap-25a data shown in Fig. 2A; snap-25b shown in Fig. S3). Synthetic mRNAs prepared from these reporters were injected into single cell embryos in the presence or absence of exogenous miR-153 or miR-153 morpholinos (MOs). Based on fluorescence levels in live embryos at 1 dpf, co-injection of miR-153 resulted in obvious down-regulation of GFP for both isoforms (Fig. 2B). To confirm that the loss of GFP was due to pairing with the predicted MREs, we created deletions of individual and combinations of MREs in snap-25a and snap-25b. Deletion of both MREs from snap-25a and all three MREs from snap-25b abolished the ability of miR-153 to silence expression (Fig. 2B; Fig. S3B). For snap-25a, we tested each of the individual MREs and found that deletion of a single MRE resulted in only modest silencing whereas deletion of both MREs caused a loss of silencing. We conclude that miR-153 targets both isoforms of snap-25 in an MRE-dependent manner.
If miR-153 targets snap-25, knockdown of endogenous miR-153 should lead to increased reporter fluorescence. To test this prediction, antisense morpholinos were co-injected with reporter mRNAs (Fig. 2). We found that knockdown of miR-153 caused a significant increase in GFP expression compared to embryos with wild type levels of endogenous miR-153. Lastly, we performed western blots using antibodies against GFP and analyzed protein levels in lysates prepared from pools of embryos treated as above (Fig. 2C,D). The levels of GFP mirrored the effects observed using fluorescence imaging in live embryos–reduced reporter expression in the presence of miR-153 and increased reporter expression upon knockdown of miR-153 (Fig. 2C,D). In all cases, the effects were dependent on intact MREs. Taken together, the in vivo reporter assays and western blots support the conclusion that snap-25 is a target of miR-153.
We next tested whether miR-153 targets endogenous snap-25. Single cell embryos were injected with either miR-153 or antisense morpholinos followed by western blots on pooled 1 dpf embryo lysates using antibodies against SNAP-25. Titration experiments were performed to optimize the levels of injected reagents (Figs. S4,S5). After optimization, protein levels were analyzed and fold changes in expression were determined compared to the amounts detected in noninjected controls (NIC) (Fig. 3). Under these conditions, excess miR-153 led to a ~50% decrease in SNAP-25 levels whereas knockdown of endogenous miR-153 increased SNAP-25 levels ~2-fold. To test for specificity we co-injected embryos with combinations of miR-153, snap-25a,b mRNAs, or morpholinos against both (Fig. 3). Injection of mRNAs encoding snap-25a,b resulted in a 2-fold elevation in SNAP-25 levels whereas injection of morpholinos that block the translation start site of snap-25 led to a ~50% decrease in SNAP-25 levels. Importantly, co-injection of combinations of RNAs and morpholinos could suppress these effects and rescue SNAP-25 levels (Fig. 3). For both suppression experiments, the effects were dose dependent. Even though snap-25a was more effective than snap-25b at rescuing endogenous SNAP-25 levels, combinations both were the most effective (Fig. 3). These results indicate specific targeting of snap-25 by miR-153. Although miR-153 is likely to have additional targets, the ability to specifically rescue the effects of overexpression and knockdown of both miR-153 and snap-25 indicates that the effects we observe are specific to targeting of snap-25 by miR-153.
(A) Embryo lysates were prepared from either NIC embryos or embryos injected with miR-153, miR-153MO, mRNAs encoding snap-25a and snap-25b, morpholinos against snap-25, or combinations thereof, as indicated. Western blots were performed using antibodies against SNAP-25 and α–tubulin. (B) Quantification of SNAP-25 levels from the western blots (n = 3) shown in A. Significance was determined by a two-tailed Student’s t-test. Error bars show s.e.m.
miR-153 Regulates snap-25 to Control Movement
Because we could specifically suppress the effects of overexpression or knockdown of miR-153 by co-injection of either snap-25a,b mRNA or morpholinos against snap-25a,b, we next sought to test whether the movement defects are caused by altered miR-153 levels could likewise be rescued in a snap-25 dependent manner. Embryonic movements were quantitated at 24 hpf after injection of antisense morpholinos against snap-25 (snap25MO) or with snap-25a,b mRNAs (Fig. 1; Movie S1). Knockdown of snap-25 resulted in dramatically decreased embryonic movements, similar to overexpression of miR-153 (Fig. 1). In contrast, overexpression of snap-25a,b increased movement approximately 5-fold over control NIC embryos (Fig. 1). For rescue experiments, co-injection of snap-25a,b mRNA with miR-153 restored near normal movement (Fig. 1; Movie S1). Similarly, co-injection of morpholinos against both snap-25 and miR-153 also restored normal movement (Fig. 1; Movie S1). Thus, not only were SNAP-25 protein levels restored to normal, but also movement defects were rescued, demonstrating specific targeting of snap-25 by miR-153.
SNAP-25 is a known target of Botulinum neurotoxin (BoNT) proteases A and E , . If miR-153 is targeting snap-25, the effects of increased miR-153 should mimic the effects of BoNT A. To test this prediction, injected zebrafish were exposed to BoNT A for 30 minutes at 27 hpf. One hour later, western blots were performed on pooled protein samples to determine whether it was possible to rescue SNAP-25 over-expression phenotypes associated with miR-153 knockdown or injection of snap25a,b mRNAs. Exposure to BoNT A dramatically reduced SNAP-25 levels, recapitulating the effects of miR-153 knockdown and over-expression (Fig. 4A,B). For movement, exposure to BoNT A rescued the hyperactive phenotypes observed after injection with MOs against miR-153 or overexpression of snap-25a&b mRNAs (Fig. 4C; Movie S1). Together, these experiments strongly support the conclusion that miR-153 specifically targets snap-25 to regulate embryonic movement.
(A) Single cell embryos were injected as indicated and then at 27 hpf, exposed to Botulinum neurotoxin A (BoNT) for 30 minutes. After recovery for 1 hour, western blots were performed on embryo lysates using antibodies against SNAP-25 or α–tubulin. (B) Quantitation of SNAP-25 levels from A, n = 3. **, p<0.01 (C) Embryonic movement in the presence or absence of BoNT A. The number of twitches per minute was counted as in Fig. 1 for embryos treated as indicated. Significance was determined by comparing mock embryos to all other conditions using ANOVA with Dunnett’s post-test, n = 15. *, p<0.05.
miR-153 Regulation of Motor Neuron Development
SNAP-25 is a well-characterized t-SNARE protein, with an established function in vesicular exocytosis –. In the developing nervous system, the SNARE complex mediates vesicular membrane addition driving neurite outgrowth and morphological patterning –, . Moreover, DCV-mediated release of signaling proteins and growth factors is important for axon guidance, path finding, and morphological development –. We therefore sought to determine whether snap-25 regulation by miR-153 would alter neuronal morphogenesis. Because zebrafish motor neuron development is well characterized –, we decided to focus on the effects of miR-153 on motor neurons during early zebrafish development.
We first injected miR-153 or morpholinos against miR-153 to observe the effects on the development and morphology of motor neurons in a transgenic zebrafish line in which motor neurons are specifically labeled with RFP (Tg(mnx1:TagRFP-T) . Perturbation of miR-153 levels caused striking changes in motor neuron structure and branching (Fig. 5A,B). Compared with NICs, overexpression of miR-153 dramatically changed the axonal architecture with significant decreases in branch numbers and length (Fig. 5C, D). Knockdown of miR-153 resulted in completely opposite effects with increased motor projection architectural complexity, increased axonal length, and increased branch numbers (Fig. 5B–D). To test whether the effects were specific, we conducted rescue experiments, as above. Injection of snap-25a,b mRNA or morpholinos against snap-25a/b produced virtually the same phenotypes observed in embryos subjected to miR-153 knockdown or overexpression, respectively. In contrast, co-injection of miR-153 and snap-25a,b mRNAs or morpholinos against miR-153 and snap-25a,b almost completely restored the normal patterning and branching of motor neurons (Fig. 5B–D). These results indicate that miR-153 regulates motor neuron development via control of snap-25a,b.
(A) A transgenic zebrafish line, Tg(mnx1:TagRFP-T), that expresses RFP in motor neurons was used to monitor the effects of altered levels of miR-153 and snap-25 at 55 hpf. For all confocal images, developing motor neurons were examined from the same somites, as indicated. (B) Morphology of developing motor neurons under each of the indicated conditions. Arrows indicate increased branching after knockdown miR-153 (miR-153MO) or overexpression snap-25a,b mRNA. Arrowheads indicate the structural defects after miR-153 overexpression or knockdown of snap-25a,b (snap-25a,bMO). Scale bar: 20 µm. (C) Quantification of motor neuron axonal branch number under the different conditions shown in (B). Error bars show s.e.m. Significance was determined using ANOVA with Dunnett’s post-test, n = 5. *, p<0.01; **, p<0.005. (D) Quantification of motor neuron axon length relative to uninjected control under the different conditions shown in (B). Error bars show s.e.m. ANOVA with Dunnett’s post-test, n = 5. *, p<0.05; **, p<0.01.
To further dissect the function of miR-153 on motor neuron development, immunofluorescence was performed on whole-mount zebrafish embryos (55 hpf) with antibodies that label primary (Znp-1 or anti-synaptotagmin 2) or secondary (Zn-8 or Alcama) motor neurons . Compared to NIC embryos, a striking difference in primary motor neuron axon architecture was observed with both miR-153 overexpression (miR-153) and knockdown (miR-153MO)(Fig. 6). A significant decrease in branching was observed in miR-153 injected embryos whereas knockdown of miR-153 caused a dramatic increase in branching. Likewise, injection of snap-25a,b mRNA led to increased axonal growth and branching in primary motor neurons whereas knockdown of snap-25a,b caused decreased outgrowth and branching (Fig. 6). Co-injection experiments showed that snap-25a,b mRNA and morpholinos against snap-25 could partially counteract the effects of the corresponding gain and loss of miR-153.
(A) Immunofluorescence performed on whole mount zebrafish embryos at 55 hpf using Znp-1 antibodies to label primary motor neurons. Confocal images were acquired from the same somites for all embryos, as indicated. (B) Effects on primary motor neuron structure and branching under the indicated conditions. Scale bar: 40 µm.
For secondary motor neurons, rostral axon outgrowth was similarly stunted and/or irregularly spaced by miR-153 overexpression and slightly elongated by miR-153 knockdown (Fig. S6). Differences in the caudal region were minimal compared to earlier developing rostral neurons, possibly reflecting temporal limitations to injection experiments or perhaps increased vulnerability of rostral motor neurons to altered SNAP-25 levels. Focusing on rostral effects, injection of snap-25a,b mRNA phenocopied miR-153 knockdown and injection of morpholinos against snap-25 resulted in patterns that closely resembled miR-153 overexpression. Co-injection of morpholinos against both miR-153 and SNAP-25 largely restored normal secondary motor neuron patterning, although the injection of snap-25a,b mRNAs was not as effective at rescuing the defects that resulted from miR-153 overexpression (Fig. S6). This may indicate a possible additional function for miR-153 in regulating axonal growth and patterning during secondary motor neuron development.
Expression of miR-153 in Motor Neurons
To ensure that the effects of miR-153 on motor neuron patterning were due to expression of miR-153 in these cells, we FACS sorted cells from the trunks of 52 hpf (Tg(mnx1:TagRFP-T) embryos and conducted RT/qPCR. As shown in Fig. 7, there was a greater than 10-fold enrichment for miR-153 in RFP+ cells compared to RFP- cells. Prior work had shown that miR-153 is expressed in the brain and spinal cord but these results show that miR-153 is expressed in developing motor neurons.
To enrich for motor neurons, heads were removed from 52 hpf embryos just posterior to the otic vesicle and trunks were dissociated to facilitate sorting of RFP+ and RFP- cells. RNA was isolated from these cell fractions and RT/PCR was performed to determine miR-153 levels relative to U6 snRNA. Significance was determined by a two-tailed Student’s t-test with the error bars representing s.e.m.; p<0.02.
miR-153 Regulates Vesicular Exocytosis to Control Signaling
Since SNAP-25 has a well-established function in the fusion and release of numerous vesicle types, we next examined the role that miR-153 plays in modulating exocytosis. Owing to the core role of miR-153 in movement control, we first focused on synaptic activity at the neuromuscular junction (NMJ) in zebrafish embryos. For this analysis, we measured synaptic vesicle (SV) cycling using the styryl dye, FM1-43 , . At 55 hpf, embryonic NMJs were imaged with Alexa 594-conjugated α-bungarotoxin (α-Btx) to label postsynaptic acetylcholine receptor (AChR) clusters, while monitoring FM1-43 uptake into NMJ presynaptic boutons (Fig. 8). The terminals were acutely depolarized for 5 minutes with high [K+] saline (45 mM) to drive the SV cycle and load FM1-43, whereas only weak loading was evident in low [K+] conditions. In non-injected controls, fluorescence was observed along terminal axon branches with intense staining at individual synaptic varicosity boutons (Fig. 8A). Compared to NIC labeling, miR-153 overexpression resulted in a significant decrease in FM1-43 loading in presynaptic terminals, indicating slowing of the SV cycle (Fig. 8B). In sharp contrast, knockdown of miR-153 showed a significant increase in FM1-43 loading, indicating an elevated SV cycling rate (Fig. 8C). The significant difference between miR-153 knockdown and overexpression conditions indicates that miR-153 plays an important role in controlling the rate of vesicle cycling (Fig. 8D). Together, these results reveal a key function for miR-153 in the control of presynaptic vesicle release at the embryonic NMJ, consistent with a role for miR-153 in the regulation of embryonic movement. The overall effects on movement are therefore a combination of effects on motor neuron development and patterning as well as overall exocytic activity.
(A) FM1-43 loading of neuromuscular junction (NMJ) boutons in 55 hpf fish embryos. (B) Postsynaptic clusters of AChRs were labeled with Alexa 594-conjugated α-bungarotoxin. Overexpression of miR-153 caused decreased FM1-43 loading, indicating down-regulation of the synaptic vesicle cycle within NMJ boutons (arrowheads). (C) Knockdown of miR-153 (miR-153MO) promoted greater uptake of FM1-43 dye, indicating increased synaptic vesicle cycling. Scale bar: 10 µm. (D) Quantification of FM1-43 fluorescent intensity with a paired Student’s t-test. Error bars show s.e.m. *p<0.01; **p<0.02.
SNAP-25 has a highly conserved role mediating vesicular fusion in both neurons and other neurosecretory cells where it is critical for DCV release . To test whether miR-153 plays a role in this secretory context, we examined exocytosis in a rat neuroendocrine pituitary cell line (GH4C1) expressing human growth hormone (hGH) . Release of hGH in these cells provided a functional readout of exocytic activity (Fig. 9). GH4C1 cells were therefore transfected with miR-153, morpholinos against miR-153/snap-25, or vectors expressing snap-25a,b, followed by determination of hGH levels in the media by ELISA. Overexpression of miR-153 and knockdown of snap-25a,b (snap-25a,bMO) reduced the levels of hGH to below the amount detected in culture media from mock transfected cells (Fig. 9). In sharp contrast, knockdown of miR-153 and overexpression of snap-25 both significantly increased the amount of secreted hGH 8–10 fold over the mock transfected control (Fig. 9). The differences observed due to perturbation of miR-153 levels in the GH4C1 cell line compared to embryonic NMJs are most likely due to differences in the efficiency of miR-153/miR-153MO delivery between the two experiments, as well as developmental differences. Nevertheless, the effects in this case were fully suppressed by co-expression of either miR-153/snap-25a,b mRNA or MOs against miR-153/snap-25a,b, demonstrating specific regulation of snap-25 by miR-153. These data strongly support the conclusion that miR-153 functions to precisely control SNAP-25 levels to regulate vesicle exocytosis.
GH4C1 cells stably expressing human growth hormone (hGH) were transfected, as indicated. The effects of exogenous expression on hGH levels secreted into the culture media were determined by ELISA using hGH antibodies. Significance was determined by comparing mock transfected to all other treatments using ANOVA with Dunnett’s post-test. Error bars show s.e.m. *, p<0.01.
In this study, we show that miR-153 regulates the critical core SNARE component, SNAP-25, to modulate exocytosis and neuronal development. Increased miR-153 levels cause decreased SNAP-25 expression resulting in decreased embryonic movement, decreased neuronal secretion, and decreased neuronal growth/branching. Conversely, miR-153 knockdown causes elevated SNAP-25 expression resulting in hyperactive movement, increased neuronal secretion, and increased neuronal growth/branching. Accumulating evidence suggests that SNAP-25 misregulation plays a role in numerous human disease states including ADHD, schizophrenia, bipolar I disorder, Huntington’s disease, Alzheimer’s disease, and diabetes . Regulated expression of miR-153 provides an attractive model to mechanistically explain tight control of SNAP-25 levels.
SNAP-25 Functions during Development
It is well established that axon outgrowth during neuronal development occurs via SNARE-dependent addition of membrane for growth cone extension , . Axonal growth, pathfinding, and target recognition are secondarily modulated by SNARE-dependent release of developmental signals via dense core vesicle (DCV) exocytosis –. The outgrowth of both axons and dendrites is blocked by Botulinum neurotoxins A and C1, proteases specific for SNAP-25, demonstrating a direct role of SNAP-25 in neuronal morphogenesis , , . Likewise, inhibition of SNAP-25 by antisense oligonucleotides blocks axonal outgrowth . In stark contrast, neuronal outgrowth was surprisingly not inhibited in SNAP-25 null mice . The explanation for this inconsistency is not clear. Our results show a clear requirement for SNAP-25 in motor neuron outgrowth and branching in zebrafish. It is possible that the requirement for SNAP-25 may be species specific but we found that altered levels of miR-153 caused similar branching defects in rat PC12 cells as observed in zebrafish motor neurons, strongly arguing against this (data not shown). Perhaps the differences are due to cell-specific requirements for SNAP-25. In the retina, for example, SNAP-25 is expressed in a dynamic spatiotemporal pattern and such differential expression may underlie specific development of cholinergic amacrine cells and photoreceptors . An intriguing possibility based on the results presented here is that developmental, stage-specific and/or cell-specific expression of miR-153 may similarly regulate SNAP-25 levels, which then drives developmental and cell-specific effects.
SNAP-25 in Synaptic Vesicle Exocytosis
SNAP-25 is one of three SNARE proteins that contribute α-helices that mediate fusion between synaptic vesicles and presynaptic membranes , . Blockage of synaptic transmission by Clostridium and Botulinum neurotoxins first established that SNARE proteins are critical for neurotransmitter release . Cleavage of SNAP-25 by Botulinum neurotoxin A causes a paralytic phenotype that resembles the loss of movement we observe in zebrafish embryos expressing excess miR-153. SNAP-25 haploinsufficient mice show no observable phenotypic defects but complete loss of SNAP-25 blocks evoked synaptic transmission . Moreover, overexpression of SNAP-25 inhibits normal calcium responsiveness and can impair memory-associated synaptic plasticity . These findings suggest that modulation of SNAP-25 levels are important for overall SNARE function, especially in generating differences in calcium dependence between neuronal and non-neuronal secretory vesicular fusion events. Matteoli and colleagues (2009) have shown that SNAP-25 is differentially expressed between excitatory glutamatergic and inhibitory GABAergic neurons in a developmental-specific manner . These results remain controversial, as earlier studies did not observe this difference, but the data are consistent with an important role for SNAP-25 as a required component for both glutamatergic and GABAergic transmission , . Mechanisms for how SNAP-25 levels might be regulated in a development- and/or cell-specific manner are uncertain, but our data strongly support miRNA regulation as a likely candidate and a critical mechanism controlling SNAP-25 levels. A recent report describing the effects of chronic overexpression of SNAP-25 in the rat dorsal hippocampus demonstrated the critical importance of controlling SNAP-25 levels . Elevated expression of SNAP-25 produced increased levels of secreted glutamate with cognitive deficits similar to those observed in ADHD and schizophrenia. We propose that miR-153 control of SNAP-25 levels allows for precise regulation of SNAP-25 during development and exocytosis.
miRNAs Regulation of Neuronal Morphogenesis and Synaptic Activity
Localized translation control in synaptic dendrites is common, requiring repression of mRNA translation during transport. miRNA mediated inhibition of translation is an attractive mechanism that can precisely control gene expression in neurons. Consistent with this hypothesis, many miRNAs are neuron or brain specific . Moreover, the effector complexes that carry out repression of translation (RNA Induced Silencing Complexes; RISCs) are composed of several subunits that have been implicated in both neuronal function and disease , , . For example, nervous system specific miRNAs have been shown to regulate the maturation of dopamine neurons in the midbrain as well as control serotonin transport by regulating the serotonin transporter , . Likewise, miR-1, miR-124, miR-125b, miR-132, bantam, miR-34 and the miR-310 cluster have all been implicated in the modulation of synaptic homeostasis –. Similarly, synaptic plasticity is reportedly regulated by miR-134 through targeting of SIRT1 or Limk1, which control dendritic spine morphogenesis , . In addition, miR-124 in retinal ganglion cell growth cone was shown to act through CoREST to regulate the intrinsic temporal sensitivity to Sema3A, a guide cue during axonal pathfinding and morphogenesis . Our work demonstrates that miR-153 is a member of this subset of miRNAs implicated in neuronal function but by a distinctly different mechanism through targeting of snap-25. miR-153 also likely targets other mRNAs , but SNAP-25 regulation alone is required and sufficient to explain the role of miR-153 regulation of movement, motor neuron morphogenesis, and SNARE-mediated secretion.
Materials and Methods
The Animal Care and Use Committee monitors all animal care and research at Vanderbilt. Vanderbilt University has on file with the Office for Protection from Research Risks of the NIH an Assurance of Compliance with Public Health Service regulations and requirements and provisions of the Animal Welfare Act. All zebrafish experiments in this paper were approved by the Vanderbilt University Institutional Animal Care and Use Committee (IACUC) under protocol M-09-398. In accordance with that protocol, all necessary means were taken to avoid pain. For any manipulations that might induce pain, animals were anesthetized with a 0.15% solution of Tricaine (3-amino-benzoic acidethylester). The approved method for euthanizing zebrafish is incubation in ice water.
Single cell zebrafish male and female embryos were injected with 200 pg of miR-153, 5 ng each of miR-153MO and miR-153loopMO and/or 100 pg of in vitro-transcribed, capped GFP reporter mRNA with or without the snap-25a or b 3′UTR. Zebrafish snap-25a,b 3′ UTR sequences were amplified by PCR and subcloned downstream of the GFP ORF in pCS2+ . Rescue experiments used injections of 3 ng of snap-25StartMO and snap-255’UTRMO, 150 pg of snap-25a,b mRNA, 250 pg of snap-25a mRNA, or 300 pg of snap-25b mRNA without 3′UTRs.
Two different morpholinos against miR-153 were utilized. One was perfectly complementary to the mature sequence; the second was complementary to a portion of the mature sequence and then extending into the precursor loop. Targeting of snap-25a,b mRNAs was performed using morpholinos against the region including the start codon.
Botulinum Toxin Analysis
Embryos injected at the 1-cell stage were treated with purified Botulinum neurotoxin A (Metabiologics, Inc., Madison, WI). Initial titration experiments were performed testing a range of BoNT A concentrations with final selection of 1 ng per 10 ml of water for 30 minutes at either 24-hpf or 48-hpf. Embryos were washed 10 times in fresh water and then allowed to recover for 1 hour prior to protein extraction or video capture to monitor movement.
qRT-PCR and Northern Blots
Total RNA extracted from both RFP+ and RFP- cells was reverse transcribed and qPCR reactions were carried out using Taqman miRNA assays (Life Technologies, NY) using the CFX96 Real-time PCR system (Bio-Rad), as previously described . Northern blots were also performed as described , .
Embryos were dechorionated, deyolked, and sonicated in lysis buffer as described . Approximately 100 embryos were pooled and one-tenth of the resulting samples were loaded into each lane. Membranes were probed with antibodies against α-tubulin (Abcam, ab15246), GFP (Torrey Pines, TP401) or SNAP-25 (Alomone Labs). For detection, anti-rabbit or anti-mouse HRP-conjugated secondary antibodies were used, followed by visualization with ECL.
GFP Reporter Analyses
Reporter analyses and western blots were as described . To generate the snap-25a,b GFP reporters, the GFP ORF was fused to the 3′ UTR sequence of zebrafish snap-25a or b. snap-25a,b UTRs were cloned from zebrafish whole embryo RNA preparations using oligo d(T) primed reverse transcription followed by PCR amplification with gene specific primers. Images were acquired with a Leica MZFIII dissecting scope equipped with a fluorescent laser using a Qimaging camera with Qimaging software and imported into Adobe Photoshop for orientation and cropping.
Embryos were fixed in 4% PFA overnight at 4°C and then permeabilized in 0.5% TritonX-100 for 60 minutes followed by treatment with protease K (20 µg/ul) for 10 minutes at room temperature. Samples were washed in PBT-DMSO before blocking overnight at 4°C (PBT-DMSO, 2% BSA, 5% goat serum). Primary antibodies (SNAP-25, 1:1000; SV-2, 1:300; ZNP-1, 1:2000; ZN-8, 1:25) were incubated overnight at 4°C, washed with PBT-DMSO, and then embryos were incubated with Cy5 or Cy3-conjugated donkey anti-mouse or rabbit antibodies (Jackson Immuno) for 4 hrs at room temperature. Before mounting and visualization, embryos were washed with PBT-DMSO. PC12 cells were fixed in 4% PFA for 15 mins, washed in PBS before incubating with primary antibodies for 1 hr, washed, incubated with secondary antibodies for 1 hr, Hoechst dye for 5 mins, washed, and visualized.
Tissue Dissociation and Motor Neuron Isolation
Tg(mnx1:TagRFP-T) zebrafish embryos of 52 hpf were dechorionated, deyolked, and then dissected just posterior to the otic vesicle to collect trunks (excluding the hearts). Tissues were kept in buffer (1×PBS, pH 6.4, 1%BSA) and then dissociated using 16 U/ml papain and 0.2 U/ml Dispase (Worthington, NJ) for 30 mins at 28°C on a rotator. After complete dissociation of the tissue by careful pipetting up and down, cells were pelleted at 8000×g for 2 mins. Resuspended cells were then treated with 1 mg/ml leupeptin (Worthington, NJ) and 100 U/ml DNaseI (Sigma-Aldrich) in PBS at pH 7.4 containing 2 mg/ml MgCl2 for 10 mins at room temperature and then kept on ice for RFP+ and RFP- cell isolation. Gating was based on cell size and fluorescence intensity, determined by the control sample of dissociated cells from WT fish at the same developmental stage.
FM1-43 Dye Labeling
Embryos at 55 dpf were incubated in HBSS (137 mM NaCl, 5.4 mM KCl, 1 mM MgSO4, 0.44 mM KH2PO4, 0.25 mM Na2HPO4, 4.2 mM NaHCO3, 1.3 mMCaCl2, 5 mM Na-HEPES) containing 0.2% Tricaine and glued onto sylgard coated glass chambers before removing the skin using a glass needle. FM1-43 and α-bungarotoxin (α-Btx) labeling procedures were as previously published , except the preloading incubation of FM1-43 dye was omitted and the Advasep incubation period was elongated to 15 mins. For data analysis, axons with puncta labeled with α-Btx were considered as synaptic boutons. FM1-43 puncta with sizes of 0.5–2 µm were collected for analysis using Image J.
Cell Culture and ELISA
PC12 cells (ATCC CRL-1721) were maintained using Ham’s F12K media with 15% horse serum and 5% FBS, and transfected individually or in combination with miRNAs, mRNAs, and morpholinos. Transfections were performed with 300 nM miR-153, biotinylated snap-25 MOs and miR-153 MOs and 1.5 µg of snap-25a,b using Lipofectamine 2000 . Co-transfection of a GFP plasmid was used to determine transfection efficiencies. Efficiencies less than 50% were discarded. One day after transfection, 50 ng/ml nerve growth factor was added to media to induce differentiation. Neurite outgrowth was assayed at day 5 by immunostaining with antibodies against acetylated α-tubulin. Stably transfected GH4C1 cells were a gift from Dr. K. Kannenberg . ELISAs were performed after 5 days of transfection and human growth hormone was assayed following the Diagnostic Systems ELISA kit.
Northern blot of miR-153 overexpression and knockdown. Perturbation of miR-153 expression levels by injection of miR-153 or MOs against different regions of pre-miR-153 was verified by northern blot. U6 served as a loading control.
Conservation of snap-25 3′ UTR sequences. The 3′ UTRs from mouse, human and zebrafish snap-25a (A) and snap-25b (B) are shown with the MREs that pair with miR-153 boxed in green. Conserved nucleotides are marked by an asterisk. The exact pairings between the MREs and miR-153 are shown in Figure 2 and Figure S3. Despite different levels of conservation, both MREs in snap-25a pair extensively with miR-153 in the seed region.
miR-153 targets snap-25b. (A) GFP reporter constructs were created by fusing the reading frame of GFP to the snap-25b 3′UTR. Three predicted miRNA recognition elements (MREs) were identified in the snap-25b 3′ UTR. The miR-153 sequence is indicated in red and the corresponding snap-25a UTR sequence is shown in green. (B) Single cell zebrafish embryos were injected with mRNAs derived from GFP reporters lacking a UTR (GFP), fused to the full length snap-25b UTR (GFP+snap-25b), or mutant version of the snap-25b UTR lacking all MREs (GFP+snap-25bΔMRE1, 2&3). Embryos were injected in the presence or absence of exogenous miR-153 or morpholinos against miR-153 (miR-153MO). Fluorescence levels were examined at 1 dpf. Clusters of embryos (~30) are shown. (C)Lysates from ~100 embryos were prepared from embryos treated as in B and GFP protein levels were determined by western blotting using antibodies against GFP or control antibodies against α-tubulin.
Dose-dependent rescue of miR-153 knockdown. (A) Single cell embryos were injected with a constant level of miR-153MO and increasing amounts (increments of 2 ng) of snap-25MOs. Embryo lysates from ~60 embryos in each group were prepared and SNAP-25 protein levels determined by western blotting. (B) Quantitation of westerns (n = 3) from A. The grey circle represents the amount of snap- 25MO (10 ng) used in co-injection rescue experiments.
Dose-dependent rescue of miR-153 over-expression. (A) Single cell embryos were injected with a constant level of miR-153 and increasing amounts (increments of 50 pg) of snap-25a, snap-25b, or snap-25a&b mRNA. Embryo lysates from ~60 embryos were prepared from embryos in each treatment group and SNAP-25 protein levels were determined by western blotting. (B) Quantitation of westerns (n = 3) from A. The grey circles represent the amounts used in co-injection rescue experiments (75 pg each of snap-25a and b, 250 pg of snap-25a, and 300 pg of snap-25b).
miR-153 regulates secondary motor neuron development. (A) Immunofluorescence was performed on whole mount zebrafish embryos at 55 hpf using Zn-8 antibodies to label secondary motor neurons. Confocal images were acquired from the same somites for all embryos, as indicated. (B) miR-153 knockdown (miR-153MO) and snap-25a,b overexpression significantly increased the growth of secondary motor neuron axons (arrows). Overexpression of miR-153 or knockdown of snap-25a,b (snap-25a,bMO) caused severe defects in axon development and architecture (asterisks). Scale bar: 40 µm.
Embryo Movements in different conditions. 0:00–0:11. NIC Embryo Movements at 24 hpf Noninjected control (NIC) zebrafish embryos at 24 hpf were filmed for one minute. Twitching was counted from individual embryos over multiple movies, as quantitated in Figure 1. 0:11–0:21. Effects of miR-153 Overexpression on Movement at 24 hpf Single cell zebrafish embryos were injected with miR-153 and filmed for one minute at 24 hpf. Twitching was counted from individual embryos over multiple movies, as quantitated in Figure 1. 0:22–0:32. Effects of Knockdown of miR-153 on Movement at 24 hpf Single cell zebrafish embryos were injected with miR-153MOs and filmed for one minute at 24 hpf. Twitching was counted from individual embryos over multiple movies, as quantitated in Figure 1. 0:33–0:42. Effects of Decreased SNAP-25 Expression on Movement at 24 hpf Single cell zebrafish embryos were injected with snap-25a,bMO and filmed for one minute at 24 hpf. Twitching was counted from individual embryos over multiple movies, as quantitated in Figure 1. 0:42–0:52. Effects of Increased SNAP-25 Expression on Movement at 24 hpf Single cell zebrafish embryos were injected with snap-25a,b mRNA and filmed for one minute at 24 hpf. Twitching was counted from individual embryos over multiple movies, as quantitated in Figure 1. 0:52–1:02. Effects of co-Injection of miR-153 and snap-25a,b on Movement at 24 hpf Single cell zebrafish embryos were co-injected with miR-153 and snap-25a,b mRNA and filmed for one minute at 24 hpf. Twitching was counted from individual embryos over multiple movies, as quantitated in Figure 1. 1:02–1:12. Effects of co-Injection of miR-153MO and snap-25a,bMO on Movement at 24 hpf Single cell zebrafish embryos were co-injected with miR-153MO and snap-25a,bMO and filmed for one minute at 24 hpf. Twitching was counted from individual embryos over multiple movies, as quantitated in Figure 1. 1:12–1:22. NIC Embryo Movements at 28 hpf Noninjected control (NIC) zebrafish embryos at 28 hpf were filmed for one minute at the same time that the following Movies were created. Twitching was counted from individual embryos, as quantitated in Figure 4C. 1:22–1:32. Effects of Botulinum Toxin Treatment on Movement at 28 hpf Single cell zebrafish embryos were injected with injection dye and treated with Botulinum toxin A at 27 hpf. After a 30 min treatment, embryos were washed and allowed to recuperate for 1 hour before being filmed. Twitching was counted from individual embryos, as quantitated in Figure 4C. 1:33–1:42. Effects of Botulinum Exposure and co-Injection of miR-153MO on Movement at 28 hpf Single cell zebrafish embryos were injected with miR-153MOs and treated with Botulinum toxin A at 27 hpf. After a 30 min treatment, embryos were washed and allowed to recuperate for 1 hour before being filmed. Twitching was counted from individual embryos, as quantitated in Figure 4C. 1:42–1:52. Effects of Botulinum Exposure and co-Injection of snap-25a,b mRNA on Movement at 28 hpf Single cell zebrafish embryos were injected with snap-25a,b mRNA and treated with Botulinum toxin A at 27 hpf. After a 30 min treatment, embryos were washed and allowed to recuperate for 1 hour before being filmed. Twitching was counted from individual embryos, as quantitated in Figure 4C.
We thank Drs. Sarah Kucenas, Bruce Appel, and Victor Ambros for critical comments and suggestions and Dr. Jeff Rohrbough and Dr. Ricardo Pineda for help with the FM1-43 experiments. We also thank Drs. Li-En Jao and Susan Wente for providing the mnx1:TagRFP-T fish.
Conceived and designed the experiments: CW EJT JGP. Performed the experiments: CW EJT AFO DJC ALP AFM. Analyzed the data: CW EJT AFO BDC KB JGP. Contributed reagents/materials/analysis tools: CW EJT ALP. Wrote the paper: CW KB JGP.
- 1. Sudhof TC, Rothman JE (2009) Membrane fusion: grappling with SNARE and SM proteins. Science 323: 474–477. doi: 10.1126/science.1161748
- 2. Wickner W, Schekman R (2008) Membrane fusion. Nat Struct Mol Biol 15: 658–664. doi: 10.1038/nsmb.1451
- 3. Jahn R, Scheller RH (2006) SNAREs–engines for membrane fusion. Nat Rev Mol Cell Biol 7: 631–643. doi: 10.1038/nrm2002
- 4. Matteoli M, Pozzi D, Grumelli C, Condliffe SB, Frassoni C, et al. (2009) The synaptic split of SNAP-25: different roles in glutamatergic and GABAergic neurons? Neuroscience 158: 223–230. doi: 10.1016/j.neuroscience.2008.03.014
- 5. Choi UB, Strop P, Vrljic M, Chu S, Brunger AT, et al. (2010) Single-molecule FRET-derived model of the synaptotagmin 1-SNARE fusion complex. Nat Struct Mol Biol 17: 318–324. doi: 10.1038/nsmb.1763
- 6. Vrljic M, Strop P, Ernst JA, Sutton RB, Chu S, et al. (2010) Molecular mechanism of the synaptotagmin-SNARE interaction in Ca2+-triggered vesicle fusion. Nat Struct Mol Biol 17: 325–331. doi: 10.1038/nsmb.1764
- 7. Schiavo G, Stenbeck G, Rothman JE, Sollner TH (1997) Binding of the synaptic vesicle v-SNARE, synaptotagmin, to the plasma membrane t-SNARE, SNAP-25, can explain docked vesicles at neurotoxin-treated synapses. Proc Natl Acad Sci U S A 94: 997–1001. doi: 10.1073/pnas.94.3.997
- 8. Blasi J, Chapman ER, Link E, Binz T, Yamasaki S, et al. (1993) Botulinum neurotoxin A selectively cleaves the synaptic protein SNAP-25. Nature 365: 160–163. doi: 10.1038/365160a0
- 9. Schiavo G, Santucci A, Dasgupta BR, Mehta PP, Jontes J, et al. (1993) Botulinum neurotoxins serotypes A and E cleave SNAP-25 at distinct COOH-terminal peptide bonds. FEBS Lett 335: 99–103. doi: 10.1016/0014-5793(93)80448-4
- 10. Smith R, Klein P, Koc-Schmitz Y, Waldvogel HJ, Faull RL, et al. (2007) Loss of SNAP-25 and rabphilin 3a in sensory-motor cortex in Huntington's disease. J Neurochem 103: 115–123. doi: 10.1111/j.1471-4159.2007.04703.x
- 11. Dessi F, Colle MA, Hauw JJ, Duyckaerts C (1997) Accumulation of SNAP-25 immunoreactive material in axons of Alzheimer's disease. Neuroreport 8: 3685–3689. doi: 10.1097/00001756-199712010-00006
- 12. Ostenson CG, Gaisano H, Sheu L, Tibell A, Bartfai T (2006) Impaired gene and protein expression of exocytotic soluble N-ethylmaleimide attachment protein receptor complex proteins in pancreatic islets of type 2 diabetic patients. Diabetes 55: 435–440. doi: 10.2337/diabetes.55.02.06.db04-1575
- 13. Washbourne P, Thompson PM, Carta M, Costa ET, Mathews JR, et al. (2002) Genetic ablation of the t-SNARE SNAP-25 distinguishes mechanisms of neuroexocytosis. Nature Neuroscience 5: 19–26.
- 14. Keller JE, Cai F, Neale EA (2004) Uptake of botulinum neurotoxin into cultured neurons. Biochemistry 43: 526–532. doi: 10.1021/bi0356698
- 15. Sørensen JB, Nagy G, Varoqueaux F, Nehring R, Brose N, et al. (2003) Differential Control of the Releasable Vesicle Pools by SNAP-25 Splice Variants and SNAP-23. Cell 114: 75–86. doi: 10.1016/s0092-8674(03)00477-x
- 16. Augustin I, Rosenmund C, Sudhof TC, Brose N (1999) Munc13–1 is essential for fusion competence of glutamatergic synaptic vesicles. Nature 400: 457–461. doi: 10.1038/22768
- 17. Gitler D, Takagishi Y, Feng J, Ren Y, Rodriguiz RM, et al. (2004) Different presynaptic roles of synapsins at excitatory and inhibitory synapses. Journal of Neuroscience 24: 11368–11380. doi: 10.1523/jneurosci.3795-04.2004
- 18. Schoch S, Castillo PE, Jo T, Mukherjee K, Geppert M, et al. (2002) RIM1alpha forms a protein scaffold for regulating neurotransmitter release at the active zone. Nature 415: 321–326. doi: 10.1038/415321a
- 19. Atouf F, Czernichow P, Scharfmann R (1997) Expression of neuronal traits in pancreatic beta cells. Implication of neuron-restrictive silencing factor/repressor element silencing transcription factor, a neuron-restrictive silencer. J Biol Chem 272: 1929–1934. doi: 10.1074/jbc.272.3.1929
- 20. Chong JA, Tapia-Ramirez J, Kim S, Toledo-Aral JJ, Zheng Y, et al. (1995) REST: a mammalian silencer protein that restricts sodium channel gene expression to neurons. Cell 80: 949–957. doi: 10.1016/0092-8674(95)90298-8
- 21. Wu J, Xie X (2006) Comparative sequence analysis reveals an intricate network among REST, CREB and miRNA in mediating neuronal gene expression. Genome Biol 7: R85.
- 22. Vo NK, Cambronne XA, Goodman RH (2010) MicroRNA pathways in neural development and plasticity. Curr Opin Neurobiol.
- 23. Qureshi IA, Mehler MF (2009) Regulation of non-coding RNA networks in the nervous system–what's the REST of the story? Neurosci Lett 466: 73–80. doi: 10.1016/j.neulet.2009.07.093
- 24. Schratt G (2009) microRNAs at the synapse. Nat Rev Neurosci 10: 842–849. doi: 10.1038/nrn2763
- 25. Cohen JE, Lee PR, Chen S, Li W, Fields RD (2011) MicroRNA regulation of homeostatic synaptic plasticity. Proc Natl Acad Sci U S A 108: 11650–11655. doi: 10.1073/pnas.1017576108
- 26. Catterall WA, Few AP (2008) Calcium channel regulation and presynaptic plasticity. Neuron 59: 882–901. doi: 10.1016/j.neuron.2008.09.005
- 27. Verhage M, Sorensen JB (2008) Vesicle docking in regulated exocytosis. Traffic 9: 1414–1424. doi: 10.1111/j.1600-0854.2008.00759.x
- 28. Christodoulou F, Raible F, Tomer R, Simakov O, Trachana K, et al. (2010) Ancient animal microRNAs and the evolution of tissue identity. Nature 463: 1084–1088. doi: 10.1038/nature08744
- 29. Kapsimali M, Kloosterman WP, de Bruijn E, Rosa F, Plasterk RH, et al. (2007) MicroRNAs show a wide diversity of expression profiles in the developing and mature central nervous system. Genome Biol 8: R173. doi: 10.1186/gb-2007-8-8-r173
- 30. Wienholds E, Kloosterman WP, Miska E, Alvarez-Saavedra E, Berezikov E, et al. (2005) MicroRNA Expression in Zebrafish Embryonic Development. Science 309: 310–311. doi: 10.1126/science.1114519
- 31. Thatcher E, Flynt A, Li N, Patton J, Patton J (2007) MiRNA expression analysis during normal zebrafish development and following inhibition of the Hedgehog and Notch signaling pathways. Dev Dyn 236: 2172–2180. doi: 10.1002/dvdy.21211
- 32. Wei C, Salichos L, Wittgrove CM, Rokas A, Patton JG (2012) Transcriptome-wide analysis of small RNA expression in early zebrafish development. RNA 18: 915–929. doi: 10.1261/rna.029090.111
- 33. Risinger C, Salaneck E, Soderberg C, Gates M, Postlethwait JH, et al. (1998) Cloning of two loci for synapse protein Snap25 in zebrafish: comparison of paralogous linkage groups suggests loss of one locus in the mammalian lineage. J Neurosci Res 54: 563–573. doi: 10.1002/(sici)1097-4547(19981201)54:5<563::aid-jnr1>3.3.co;2-z
- 34. Bark C, Bellinger FP, Kaushal A, Mathews JR, Partridge LD, et al. (2004) Developmentally regulated switch in alternatively spliced SNAP-25 isoforms alters facilitation of synaptic transmission. Journal of Neuroscience 24: 8796–8805. doi: 10.1523/jneurosci.1940-04.2004
- 35. Hepp R, Langley K (2001) SNAREs during development. Cell Tissue Res 305: 247–253. doi: 10.1007/s004410100359
- 36. Lu B (2003) BDNF and activity-dependent synaptic modulation. Learn Mem 10: 86–98. doi: 10.1101/lm.54603
- 37. Asakura T, Waga N, Ogura K, Goshima Y (2010) Genes required for cellular UNC-6/netrin localization in Caenorhabditis elegans. Genetics 185: 573–585. doi: 10.1534/genetics.110.116293
- 38. Mai J, Fok L, Gao H, Zhang X, Poo MM (2009) Axon initiation and growth cone turning on bound protein gradients. J Neurosci 29: 7450–7458. doi: 10.1523/jneurosci.1121-09.2009
- 39. Cohen-Cory S, Kidane AH, Shirkey NJ, Marshak S (2010) Brain-derived neurotrophic factor and the development of structural neuronal connectivity. Dev Neurobiol 70: 271–288. doi: 10.1002/dneu.20774
- 40. Lewis KE, Eisen JS (2003) From cells to circuits: development of the zebrafish spinal cord. Prog Neurobiol 69: 419–449. doi: 10.1016/s0301-0082(03)00052-2
- 41. Eisen JS (1991) Developmental neurobiology of the zebrafish. J Neurosci 11: 311–317.
- 42. Eisen JS, Myers PZ, Westerfield M (1986) Pathway selection by growth cones of identified motoneurones in live zebra fish embryos. Nature 320: 269–271. doi: 10.1038/320269a0
- 43. Appel B, Korzh V, Glasgow E, Thor S, Edlund T, et al. (1995) Motoneuron fate specification revealed by patterned LIM homeobox gene expression in embryonic zebrafish. Development 121: 4117–4125.
- 44. Westerfield M, McMurray JV, Eisen JS (1986) Identified motoneurons and their innervation of axial muscles in the zebrafish. J Neurosci 6: 2267–2277.
- 45. Myers PZ, Eisen JS, Westerfield M (1986) Development and axonal outgrowth of identified motoneurons in the zebrafish. J Neurosci 6: 2278–2289.
- 46. Jao LE, Appel B, Wente SR (2012) A zebrafish model of lethal congenital contracture syndrome 1 reveals Gle1 function in spinal neural precursor survival and motor axon arborization. Development 139: 1316–1326. doi: 10.1242/dev.074344
- 47. Trevarrow B, Marks DL, Kimmel CB (1990) Organization of hindbrain segments in the zebrafish embryo. Neuron 4: 669–679. doi: 10.1016/0896-6273(90)90194-k
- 48. Gaffield MA, Betz WJ (2006) Imaging synaptic vesicle exocytosis and endocytosis with FM dyes. Nat Protoc 1: 2916–2921. doi: 10.1038/nprot.2006.476
- 49. Li W, Ono F, Brehm P (2003) Optical measurements of presynaptic release in mutant zebrafish lacking postsynaptic receptors. J Neurosci 23: 10467–10474.
- 50. Burgoyne RD, Morgan A (2003) Secretory granule exocytosis. Physiol Rev 83: 581–632.
- 51. Kannenberg K, Wittekindt NE, Tippmann S, Wolburg H, Ranke MB, et al. (2007) Mutant and Misfolded Human Growth Hormone is Rapidly Degraded Through the Proteasomal Degradation Pathway in a Cellular Model for Isolated Growth Hormone Deficiency Type II. Journal of Neuroendocrinology 19: 882–890. doi: 10.1111/j.1365-2826.2007.01602.x
- 52. Gray LJ, Dean B, Kronsbein HC, Robinson PJ, Scarr E (2010) Region and diagnosis-specific changes in synaptic proteins in schizophrenia and bipolar I disorder. Psychiatry Res 178: 374–380. doi: 10.1016/j.psychres.2008.07.012
- 53. Kimura K, Mizoguchi A, Ide C (2003) Regulation of growth cone extension by SNARE proteins. J Histochem Cytochem 51: 429–433. doi: 10.1177/002215540305100404
- 54. Osen-Sand A, Catsicas M, Staple JK, Jones KA, Ayala G, et al. (1993) Inhibition of axonal growth by SNAP-25 antisense oligonucleotides in vitro and in vivo. Nature 364: 445–448. doi: 10.1038/364445a0
- 55. Osen-Sand A, Staple JK, Naldi E, Schiavo G, Rossetto O, et al. (1996) Common and distinct fusion proteins in axonal growth and transmitter release. J Comp Neurol 367: 222–234. doi: 10.1002/(sici)1096-9861(19960401)367:2<222::aid-cne5>3.0.co;2-7
- 56. Igarashi M, Kozaki S, Terakawa S, Kawano S, Ide C, et al. (1996) Growth cone collapse and inhibition of neurite growth by Botulinum neurotoxin C1: a t-SNARE is involved in axonal growth. J Cell Biol 134: 205–215. doi: 10.1083/jcb.134.1.205
- 57. Igarashi M, Tagaya M, Komiya Y (1997) The soluble N-ethylmaleimide-sensitive factor attached protein receptor complex in growth cones: molecular aspects of the axon terminal development. J Neurosci 17: 1460–1470.
- 58. Zhou Q, Xiao J, Liu Y (2000) Participation of syntaxin 1A in membrane trafficking involving neurite elongation and membrane expansion. J Neurosci Res 61: 321–328. doi: 10.1002/1097-4547(20000801)61:3<321::aid-jnr10>3.0.co;2-l
- 59. Martinez-Arca S, Coco S, Mainguy G, Schenk U, Alberts P, et al. (2001) A common exocytotic mechanism mediates axonal and dendritic outgrowth. J Neurosci 21: 3830–3838.
- 60. Grosse G, Grosse J, Tapp R, Kuchinke J, Gorsleben M, et al. (1999) SNAP-25 requirement for dendritic growth of hippocampal neurons. J Neurosci Res 56: 539–546. doi: 10.1002/(sici)1097-4547(19990601)56:5<539::aid-jnr9>3.0.co;2-y
- 61. Greenlee MH, Wilson MC, Sakaguchi DS (2002) Expression of SNAP-25 during mammalian retinal development: thinking outside the synapse. Semin Cell Dev Biol 13: 99–106. doi: 10.1016/s1084-9521(02)00015-0
- 62. Schiavo G, Matteoli M, Montecucco C (2000) Neurotoxins affecting neuroexocytosis. Physiol Rev 80: 717–766.
- 63. McKee AG, Loscher JS, O'Sullivan NC, Chadderton N, Palfi A, et al. (2010) AAV-mediated chronic over-expression of SNAP-25 in adult rat dorsal hippocampus impairs memory-associated synaptic plasticity. J Neurochem 112: 991–1004. doi: 10.1111/j.1471-4159.2009.06516.x
- 64. Tafoya LC, Shuttleworth CW, Yanagawa Y, Obata K, Wilson MC (2008) The role of the t-SNARE SNAP-25 in action potential-dependent calcium signaling and expression in GABAergic and glutamatergic neurons. BMC Neuroscience 9: 105. doi: 10.1186/1471-2202-9-105
- 65. Delgado-Martinez I, Nehring RB, Sorensen JB (2007) Differential abilities of SNAP-25 homologs to support neuronal function. J Neurosci 27: 9380–9391. doi: 10.1523/jneurosci.5092-06.2007
- 66. Bicker S, Schratt G (2008) microRNAs: tiny regulators of synapse function in development and disease. J Cell Mol Med 12: 1466–1476. doi: 10.1111/j.1582-4934.2008.00400.x
- 67. Ashraf SI, McLoon AL, Sclarsic SM, Kunes S (2006) Synaptic protein synthesis associated with memory is regulated by the RISC pathway in Drosophila. Cell 124: 191–205. doi: 10.1016/j.cell.2005.12.017
- 68. Baudry A, Mouillet-Richard S, Schneider B, Launay JM, Kellermann O (2010) miR-16 targets the serotonin transporter: a new facet for adaptive responses to antidepressants. Science 329: 1537–1541. doi: 10.1126/science.1193692
- 69. Kim J, Inoue K, Ishii J, Vanti WB, Voronov SV, et al. (2007) A MicroRNA feedback circuit in midbrain dopamine neurons. Science 317: 1220–1224. doi: 10.1126/science.1140481
- 70. Wayman GA, Davare M, Ando H, Fortin D, Varlamova O, et al. (2008) An activity-regulated microRNA controls dendritic plasticity by down-regulating p250GAP. Proc Natl Acad Sci U S A 105: 9093–9098. doi: 10.1073/pnas.0803072105
- 71. Rajasethupathy P, Fiumara F, Sheridan R, Betel D, Puthanveettil SV, et al. (2009) Characterization of small RNAs in Aplysia reveals a role for miR-124 in constraining synaptic plasticity through CREB. Neuron 63: 803–817. doi: 10.1016/j.neuron.2009.05.029
- 72. Simon DJ, Madison JM, Conery AL, Thompson-Peer KL, Soskis M, et al. (2008) The microRNA miR-1 regulates a MEF-2-dependent retrograde signal at neuromuscular junctions. Cell 133: 903–915. doi: 10.1016/j.cell.2008.04.035
- 73. Impey S, Davare M, Lasiek A, Fortin D, Ando H, et al. (2010) An activity-induced microRNA controls dendritic spine formation by regulating Rac1-PAK signaling. Mol Cell Neurosci 43: 146–156. doi: 10.1016/j.mcn.2009.10.005
- 74. Parrish JZ, Xu P, Kim CC, Jan LY, Jan YN (2009) The microRNA bantam functions in epithelial cells to regulate scaling growth of dendrite arbors in drosophila sensory neurons. Neuron 63: 788–802. doi: 10.1016/j.neuron.2009.08.006
- 75. Tsurudome K, Tsang K, Liao EH, Ball R, Penney J, et al. (2010) The Drosophila miR-310 cluster negatively regulates synaptic strength at the neuromuscular junction. Neuron 68: 879–893. doi: 10.1016/j.neuron.2010.11.016
- 76. Agostini M, Tucci P, Steinert JR, Shalom-Feuerstein R, Rouleau M, et al. (2011) microRNA-34a regulates neurite outgrowth, spinal morphology, and function. Proc Natl Acad Sci U S A 108: 21099–21104. doi: 10.1073/pnas.1112063108
- 77. Schratt GM, Tuebing F, Nigh EA, Kane CG, Sabatini ME, et al. (2006) A brain-specific microRNA regulates dendritic spine development. Nature 439: 283–289. doi: 10.1038/nature04367
- 78. Gao J, Wang WY, Mao YW, Graff J, Guan JS, et al. (2010) A novel pathway regulates memory and plasticity via SIRT1 and miR-134. Nature 466: 1105–1109. doi: 10.1038/nature09271
- 79. Baudet ML, Zivraj KH, Abreu-Goodger C, Muldal A, Armisen J, et al. (2012) miR-124 acts through CoREST to control onset of Sema3A sensitivity in navigating retinal growth cones. Nat Neurosci 15: 29–38. doi: 10.1038/nn.2979
- 80. Doxakis E (2010) Post-transcriptional regulation of alpha-synuclein expression by mir-7 and mir-153. J Biol Chem 285: 12726–12734. doi: 10.1074/jbc.m109.086827
- 81. Rupp RA, Snider L, Weintraub H (1994) Xenopus embryos regulate the nuclear localization of XMyoD. Genes and Development 8: 1311–1323. doi: 10.1101/gad.8.11.1311
- 82. Sempere LF, Sokol NS, Dubrovsky EB, Berger EM, Ambros V (2003) Temporal regulation of microRNA expression in Drosophila melanogaster mediated by hormonal signals and broad-Complex gene activity. Dev Biol 259: 9–18. doi: 10.1016/s0012-1606(03)00208-2
- 83. Flynt A, Li N, Thatcher E, Solnica-Krezel L, Patton J (2007) Zebrafish miR-214 modulates Hedgehog signaling to specify muscle cell fate. Nat Genet 39: 259–263. doi: 10.1038/ng1953
- 84. Tsuji M, Inanami O, Kuwabara M (2001) Induction of neurite outgrowth in PC12 cells by alpha -phenyl-N-tert-butylnitron through activation of protein kinase C and the Ras-extracellular signal-regulated kinase pathway. J Biol Chem 276: 32779–32785. doi: 10.1074/jbc.m101403200