- Research article
- Open Access
Nonmuscle Myosin II helps regulate synaptic vesicle mobility at the Drosophilaneuromuscular junction
© Seabrooke et al; licensee BioMed Central Ltd. 2010
- Received: 24 September 2009
- Accepted: 16 March 2010
- Published: 16 March 2010
Although the mechanistic details of the vesicle transport process from the cell body to the nerve terminal are well described, the mechanisms underlying vesicle traffic within nerve terminal boutons is relatively unknown. The actin cytoskeleton has been implicated but exactly how actin or actin-binding proteins participate in vesicle movement is not clear.
In the present study we have identified Nonmuscle Myosin II as a candidate molecule important for synaptic vesicle traffic within Drosophila larval neuromuscular boutons. Nonmuscle Myosin II was found to be localized at the Drosophila larval neuromuscular junction; genetics and pharmacology combined with the time-lapse imaging technique FRAP were used to reveal a contribution of Nonmuscle Myosin II to synaptic vesicle movement. FRAP analysis showed that vesicle dynamics were highly dependent on the expression level of Nonmuscle Myosin II.
Our results provide evidence that Nonmuscle Myosin II is present presynaptically, is important for synaptic vesicle mobility and suggests a role for Nonmuscle Myosin II in shuttling vesicles at the Drosophila neuromuscular junction. This work begins to reveal the process by which synaptic vesicles traverse within the bouton.
- Synaptic Vesicle
- Myosin Light Chain Kinase
- Myosin Motor
- Recovery Index
- Vesicle Movement
Transport and assembly of synaptic vesicles has been the subject of several studies. Vesicles and their components are transported along axon microtubules to the nerve terminal, (for review see [1, 2]) where they participate in synaptic physiology, undergoing a cycle of exo- and endocytosis. However, vesicle traffic within terminal boutons is not well understood although recent advances in this area have been made [3, 4].
Classically, vesicles were believed to be relatively stationary until released [5–7]. However, more recent studies provided evidence for a mobile vesicle pool [8, 9] best described by a caged-diffusion model  and differential vesicle mobility in the reserve and recycling pool has been suggested within the frog motor nerve terminals . Additionally, Nunes et al.  observed dynamic vesicles in the Drosophila melanogaster bouton, and dynamic vesicles have been reported at ribbon synapses in lizards .
Vesicle movement may result from diffusion or directed transport. Actin polymerization in the nerve terminal may promote vesicle movement through a Listeria comet mechanism  or it may act as a substrate for myosin motors to shuttle vesicles. In light of a previous screen from our lab identifying Nonmuscle Myosin II (NMMII) as a candidate molecule important in neuromuscular junction (NMJ) development [15, 16], we have focused on determining a neuromuscular function for this actin-based myosin motor. NMMII is present in the nervous system of Xenopus, mouse, rat and chicken [17–19], and in the CNS of Drosophila . NMMII can both crosslink F-actin and has been shown to transport vesicles on F-actin [21–23].
This study was undertaken to determine whether NMMII contributes to synaptic vesicle mobility. We used the genetic model system Drosophila melanogaster to manipulate NMMII expression, pharmacology to inhibit NMMII activity, and the optically accessible neuromuscular synapse of third instar larvae to investigate vesicle dynamics. We show that NMMII is concentrated pre- and postsynaptically and importantly, we report that unstimulated synaptic vesicle mobility exhibited a dependence on NMMII expression. These results report the first evidence for NMMII having a function in synaptic vesicle dynamics at the Drosophila NMJ.
Nonmuscle Myosin II is localized pre- and postsynaptically at the NMJ
Expression level of Nonmuscle Myosin II in zipper alleles
Inhibition of Myosin with ML-9 results in a dose-dependent decrease in vesicle mobility
Rate parameters from FRAP curves fit with the double exponential curves
0 μM ML-9
0.38 ± 0.031
0.0040 ± 0.0010
0.72 ± 0.031
0.11 ± 0.40
10 μM ML-9
0.37 ± 0.0035
0.0035 ± 0.0010
0.40 ± 0.083
0.080 ± 0.023
50 μM ML-9
0.39 ± 0.030
0.0025 ± 0.0010
0.42 ± 0.087
0.080 ± 0.022
100 μM ML-9
0.51 ± 0.020
0.0025 ± 0.0005
0.29 ± 0.16
0.11 ± 0.050
0.40 ± 0.033
0.0047 ± 0.0012
0.58 ± 0.22
0.10 ± 0.039
Heterozygous Loss-of-Function (Het)
0.37 ± 0.043
0.0069 ± 0.0015
0.66 ± 0.33
0.12 ± 0.049
RNAi Knockdown (K/D)
0.46 ± 0.035
0.0031 ± 0.0008
0.28 ± 0.12
0.082 ± 0.045
0.49 ± 0.040
0.0023 ± 0.0010
0.35 ± 0.093
0.071 ± 0.030
Nonmuscle Myosin II contributes to synaptic vesicle dynamics
Although the bleach depth was not significantly different between the heterozygous loss-of-function allele, the RNAi knockdown sample and control samples, the O/E samples did show significantly lower bleach depth (See Additional file 6, Figure S1A showing the average bleach depth from FRAP experiments). We therefore further analysed the FRAP recoveries to ensure differences in bleach depth did not account for our results. To refine our analysis, we calculated the recovery index of the FRAP curve  which accounts for differences in bleach depth between genotypes. These calculations led to the same conclusions: the heterozygous loss-of-function allele of NMMII increased the recovery index, while both the RNAi knockdown and overexpression of NMMII reduced the recovery index (See Additional file 6, Figure S1B showing the recovery index from the FRAP curves).
Summary of results from manipulating NMMII expression
Expression of NMMII
This report has identified the presence of NMMII in the presynaptic terminal and indicates a function for NMMII in synaptic vesicle mobility at the NMJ of Drosophila melanogaster. NMMII has been implicated in synaptic transmission in rats , but has not previously been shown at the NMJ of Drosophila and this is the first evidence of NMMII having a function in synaptic vesicle mobility. Using Drosophila, as a genetically malleable tool, and the confocal imaging technique, FRAP, we were able to quantify the effect of NMMII on vesicle mobility. FRAP revealed that NMMII plays a complex role in vesicle dynamics and begins to clarify our knowledge of how synaptic vesicles may be available for release upon stimulation.
Vesicle mobility is affected by a complex interaction with Nonmuscle Myosin II
Immunocytological staining first identified that NMMII is found both pre- and postsynaptically in the Drosophila NMJ. Abolishment of postsynaptic NMMII expression through RNAi confirmed expression of NMMII presynaptically. With NMMII present in the presynaptic terminal, this suggests a possible function for NMMII in trafficking vesicles within the bouton. To determine whether NMMII impacts vesicle dynamics, we carried out in vivo imaging techniques to visualize synaptic vesicle mobility. We found an intriguing complex interaction between the expression level of NMMII and the dynamics of vesicle mobility. Inhibiting MLCK reduced vesicle mobility, consistent with Jordan et al. . More specifically, increasing either NMMII expression by 95% or reducing NMMII expression to 28% reduced vesicle mobility, while moderately reducing NMMII to 57% enhanced vesicle mobility. A limitation of the present study is an estimate of NMMII activity or levels specifically at nerve terminal boutons in the various mutant strains used. The postsynaptic presence of NMMII makes immunohistochemical techniques for measuring presynaptic NMMII difficult. We estimated neuronal NMMII levels using western blots of larval brains. This demonstrated that NMMII levels were up- and down-regulated significantly by the genotypes used. The 50% reduction in protein level from the heterozygous loss-of-function to the RNAi knockdown strains did not exhibit a statistical difference. However, we did find substantially different effects on vesicle mobility suggesting that the apparent difference in expression levels is functionally significant. Thus it appears that tight regulation of NMMII expression is essential in maintaining appropriate vesicle dynamics: a small reduction in NMMII levels enhances mobility whereas too much or too little impairs mobility. Together this supports a role for NMMII in normal synaptic vesicle mobility at the Drosophila NMJ.
While these findings suggest a role for NMMII in synaptic vesicle mobility, it does not exclude the possibility that other myosin motors are also involved. In support of this, the general myosin inhibitor, ML-9, reduced synaptic vesicle mobility in a dose dependent manner with no stimulation of vesicle mobility at low concentrations. In addition, other myosin motors have been shown to associate with synaptic vesicles and be involved in synaptic transmission. For example, Myosin V can bind to a myosin receptor found on a subpopulation of high density vesicles  and is found to be associated with vesicles isolated from chick brain , but was not found to alter hippocampal synaptic transmission in mice . However, Myosin II has been associated with normal synaptic transmission. In cultured rat superior cervical ganglion neurones, myosin IIb was found to inhibit synaptic transmission . A reduction in synaptic transmission upon inhibition of Myosin II was also observed in rat cholinergic synapses , while MLCK was found to be involved in maintaining repetitive synaptic transmission . Myosin II has also been shown to be involved in vesicle mobility in other systems. Nonmuscle Myosin II has been shown to transport vesicles on actin filaments in clam oocytes  and Nonmuscle Myosin II has been shown to contribute to vesicle transport from the Golgi to the Endoplasmic Reticulum . Thus, while the present work identifies a function for NMMII in synaptic vesicle mobility, the precise mechanisms of myosin motors in synaptic transmission and the precise role of NMMII as a vesicle motor remains to be clarified. Since NMMII interacts with actin, it will also be important to investigate the affects of NMMII on actin stability and dynamics in the NMJ and to determine whether the affects of NMMII on vesicle mobility translate into affects on synaptic transmission.
Our results show that NMMII is found presynaptically at the Drosophila NMJ and plays a functional role at the NMJ. We report, for the first time, a function for NMMII in normal synaptic vesicle mobility in the unstimulated neuron, which is dependent on the expression level of NMMII. Further experimentation to address the function of NMMII at the NMJ, through electrophysiological assays, manipulating NMMII activity by its' kinases and phosphatases and measuring actin activity, is required to more clearly define the precise role of NMMII at the Drosophila NMJ.
Drosophila melanogaster were maintained at 22°C on Bloomington fly media. The heterozygous loss-of-function NMMII allele, zipper1/CyO (zip1/CyO) (FBal0018862) was acquired from the Bloomington stock center and rebalanced over Cyo-GFP. UASzipperRNAi (UASzipRNAi) was obtained from the Vienna Drosophila RNAi center (FBst0470845) and is a NMMII RNAi construct. The gain-of-function NMMII construct, zipper GS50077 (zip GS50077 ), was obtained from the Drosophila gene search project  and is a unidirectional UAS construct inserted upstream of NMMII. elav C155 Gal4; UASsynaptotagminGFP (elav C155 Gal4;UAS-sytGFP) was obtained from the Bloomington stock center (FBst0006923) and UASactinGFP (UAS-actGFP) was obtained from the Kyoto stock center for FRAP imaging of vesicle and actin dynamics respectively. A stock of UAS-actGFP/UAS-actGFP; elav 3A Gal4/TM3, Sb, Tb was generated to express actinGFP in the nervous system. The Gal4 drivers, elav 3A Gal4 (FBti0072910, Bloomington stock center) and elav C155 Gal4 drive expression of UAS constructs in the nervous system . 24BGal4 (FBti0002090, Bloomington stock center) was used to drive expression of NMMII alleles in muscle. Flies were crossed at 25°C and kept at identical growing conditions.
Third instar larva were dissected in HL3 buffer with no Ca2+ added , and fixed in 4% paraformaldehyde in phosphate-buffered saline (PBS). After fixation, the samples were transferred to 1% BSA diluted in PBT (PBS plus 0.1% Triton X-100). The following primary antibodies were used: rabbit anti-NMMII (1:1000, Roger Karess, Centre de National de Récherche Scientifique, Centre de Génétique Moléculaire), and mouse anti-Dlg (1:200, Developmental Studies Hybridoma Bank). Anti-HRP FITC (1:1000, MP Biomedical; Solon, OH) was used as a neural marker. The secondary antibodies used were; goat anti-mouse Alexa488 and goat anti-rabbit Alexa633 (1:1000, Invitrogen). Following antibody labelling, the preparations were washed in PBT and mounted in Vectashield (Vector Laboratories; Burlington, ON).
Images were acquired on a Carl Zeiss LSM510 confocal. Z-sections were obtained on a F-Fluar 40×/1.3 Oil for NMMII localization. The pinhole aperture acquired images of 1 μm thickness and image sections were projected onto a single plane. 1-3 images were collected per larva.
For each treatment, five brains from third instar larvae were lysed in protein lysis buffer (50 mM Tris-Cl, 1% NP-40, 150 mM NaCl) with complete protease inhibitor. Samples were separated on a 10% SDS-polyacrylamide gel, and transferred to PVDF membrane. NMMII was detected with rabbit anti-NMMII antibody (1:10000, Roger Karess, Centre de National de Récherche Scientifique, Centre de Génétique Moléculaire), and a goat anti-rabbit HRP-coupled secondary (1:1500 BioRad). α-β-Tubulin was used as a loading control (1:100, Developmental Studies Hybridoma Bank). Antibodies were visualized using chemiluminescent detection (ECL Plus, Amersham). Control and experimental bands were imaged either simultaneous or individually on the same blot. Blots were scanned and digitized with a Molecular Dynamics Phosphoimager. Band intensities were quantified using ImageJ.
Fluorescence Recovery After Photobleaching
FRAP was conducted on a Carl Zeiss LSM 510 confocal microscope equipped with an Argon2 laser and a LP505 filter. To immobilize the preparation, wandering third instar larvae were dissected in HL3 with no Ca2+ added  and glued to slygard-coated slides using Nexabrand tissue glue (WPI, Sarasota, FL). The glued preparations were placed under an Achroplan 100×/1.0 W Ph objective with an 8× digital zoom. FRAP recordings were made, from segments 3 or 4, of type I boutons at muscle 7/6 for vesicle dynamics. Images were collected at 1.12 μs/pixel with a pinhole of 1 airy unit and a resolution of 512 × 512. Sixty images were collected over two minutes with a 1 sec delay between image acquisitions. To select the area for bleaching, a region of interest (ROI) 24 × 30 pixels was selected on the digital image. Four baseline scans were acquired using 5% or 10% of full laser power. Before the fifth scan, the laser increased to 97% of maximal and rapidly iterated the ROI 9 times, after which, returning to 5% or 10% of maximal power to complete the remaining 56 scans. A maximum of three type I boutons were recorded per hemi-segment and a maximum of 6 boutons per larvae. All FRAP experiments were completed within 2 hours of the larval dissection.
Where T = total fluorescence in the bouton, I = fluorescence in the bleached fraction and BG = background fluorescence outside the bouton. This accounts for photobleaching throughout the FRAP experiment and for movement of bleached molecules out of the FRAP ROI.
Where A, B = constants that represent the apparent bleached fraction, K1, K2 = rates, t = time.
To access vesicle dynamics under myosin inhibition, the myosin light chain kinase inhibitor, ML-9, was applied to the preparation before beginning FRAP experiments. A stock concentration of 50 mM ML-9 in DMSO was diluted into HL3  with no Ca2+ added, to make 100 μM, 50 μM and 10 μM ML-9 solutions. The preparations were incubated in the dark with ML-9 for 30 minutes prior to FRAP.
All statistical analyses were performed in GraphPad Prism 4.0. For non-linear regression, FRAP was double normalized  and compiled for curve fitting . In all cases, the double exponential curve outlined in McNally (2008)  was accepted over the single exponential curve. Error is represented as the 95% confidence interval for the curve. Rates are expressed as inverse seconds. In double exponential curves, the initial phase has been indicated here with A and K1 and the second phase of the curve have been indicated by B and K2. For analysis of variance, one-way ANOVA was completed. P < 0.05 was accepted as statistically significant.
We acknowledge Owen Randlett for his preliminary work with ML-9, Nicola Haines, Ronald Gonzalez, Colin DeMill and Marta Kisiel for feedback on the manuscript and Nicole Novroski for making fly food. We would like to thank Roger Karess for providing the Nonmuscle Myosin II antibody, the Developmental Studies Hybridoma Bank for antibodies, and the Bloomington, Kyoto, Vienna and Gene Search Stock Centers for fly stocks. This work was supported by funds from the Canadian Institutes of Health Research program to BAS.
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