Synaptotagmin I is the Ca2+ sensor for fast, synchronous release of neurotransmitter; however, the molecular interactions that couple Ca2+ binding to membrane fusion remain unclear. The structure of synaptotagmin is dominated by two C2 domains that interact with negatively charged membranes after binding Ca2+. In vitro work has implicated a conserved basic residue at the tip of loop 3 of the Ca2+-binding pocket in both C2 domains in coordinating this electrostatic interaction with anionic membranes. Although results from cultured cells suggest that the basic residue of the C2A domain is functionally significant, such studies provide contradictory results regarding the importance of the C2B basic residue during vesicle fusion. To directly test the functional significance of each of these residues at an intact synapse in vivo, we neutralized either the C2A or the C2B basic residue and assessed synaptic transmission at the Drosophila neuromuscular junction. The conserved basic residues at the tip of the Ca2+-binding pocket of both the C2A and C2B domains mediate Ca2+-dependent interactions with anionic membranes and are required for efficient evoked transmitter release. Our results directly support the hypothesis that the interactions between synaptotagmin and the presynaptic membrane, which are mediated by the basic residues at the tip of both the C2A and C2B Ca2+-binding pockets, are critical for coupling Ca2+ influx with vesicle fusion during synaptic transmission in vivo. Our model for synaptotagmin's direct role in coupling Ca2+ binding to vesicle fusion incorporates this finding with results from multiple in vitro and in vivo studies.
- synaptic vesicle fusion
- anionic phospholipid interactions
- site-directed mutagenesis
- calcium dependence
- Western analysis
The synaptic vesicle protein, synaptotagmin, functions as the Ca2+ sensor for synchronous neurotransmitter release. Synaptotagmin contains two C2 domains, C2A and C2B, that coordinate Ca2+ ions. Whereas Ca2+ binding by the C2B domain is essential for synchronous transmitter release, Ca2+ binding by C2A plays only a modest role (Fernández-Chacón et al., 2002; Mackler et al., 2002; Robinson et al., 2002). Synaptotagmin's C2 domains interact with anionic phospholipids in a Ca2+-dependent manner in vitro (Perin et al., 1990; Earles et al., 2001; Fernández-Chacón et al., 2001; Bai et al., 2002), and deficits in Ca2+-triggered fusion in several synaptotagmin mutants parallel the decrease in Ca2+-dependent phospholipid binding (Fernández-Chacón et al., 2001; Mackler et al., 2002; Sørensen et al., 2003; Wang et al., 2003; Nishiki and Augustine, 2004; Li et al., 2006). Thus, a Ca2+-dependent interaction between synaptotagmin and phospholipids is postulated to be critical in mediating Ca2+-triggered vesicle fusion.
Specific residues within synaptotagmin are required for Ca2+-dependent phospholipid binding in vitro. At the tip of the Ca2+-binding loops of each C2 domain, there is a conserved basic residue (Fig. 1, ⊕) that is thought to mediate an electrostatic interaction between synaptotagmin and the anionic presynaptic membrane (Chae et al., 1998; Fernández-Chacón et al., 2001; Wang et al., 2003). This interaction may contribute to the electrostatic switch that drives vesicle fusion after Ca2+ influx (Davletov et al., 1998; Ubach et al., 1998). In C2A, this basic residue is likely functionally significant, because it is necessary for efficient Ca2+-triggered vesicle fusion in a variety of cultured cell types (Fernández-Chacón et al., 2001; Sørensen et al., 2003; Wang et al., 2003). The functional significance of this basic residue in C2B, however, is controversial, because studies from cultured cells provide contradictory results (Wang et al., 2003; Li et al., 2006). In addition, cultured cells do not necessarily reproduce the exact behavior of intact synapses (Banker and Goslin, 1998), so it is critical to test each of these residues for function in vivo.
Because (1) multiple residues located at the tip of the Ca2+-binding pockets, including these basic residues, in both the C2A and C2B domains are critical for Ca2+-dependent phospholipid interactions (Chae et al., 1998; Chapman and Davis, 1998; Davis et al., 1999; Fernández-Chacón et al., 2001; Bai et al., 2002; Frazier et al., 2003; Wang et al., 2003; Araç et al., 2006) (but see Li et al., 2006) and (2) multiple fusion assays implicate these tip residues in Ca2+-triggered fusion (Fernández-Chacón et al., 2001; Sørensen et al., 2003; Wang et al., 2003; Rhee et al., 2005; Martens et al., 2007), we directly tested the functional significance of each of these basic residues at an intact synapse by individually neutralizing them and measuring evoked release at the Drosophila neuromuscular junction. Here, we demonstrate that the conserved basic residues at the tip of the C2A and C2B Ca2+-binding pockets each mediate interactions with anionic phospholipids in vitro and are each critical for synaptotagmin function in vivo.
Materials and Methods
To neutralize the positive charge without disrupting the structure of the C2 domain (Fernández-Chacón et al., 2001), arginine residues 285 and 419 (Fig. 1, ⊕) of Drosophila synaptotagmin I (syt) were mutated to glutamines using PCR. To mutate arginine 285, a specifically mutated oligonucleotide (CGAGAACTGATCGAAGTCGAAAATGGC) was paired with a wild-type (WT) oligonucleotide that flanked a unique StyI site. The PCR product was gel purified and used as a macroprimer in a second round of PCR with a wild-type oligonucleotide that flanked a unique EcoRV site. This second-round, mutant PCR product was then subcloned into an otherwise wild-type Drosophila syt cDNA construct in pBluescript II (Mackler and Reist, 2001). To mutate arginine 419, a specifically mutated oligonucleotide (TGCAGCGGCCGATGGGTTCGGAGGTGCCAATCTGATCGTAGTCCACGACGGTCACAACG) containing a unique EagI site was paired with a wild-type oligonucleotide that flanked a unique EcoRV site. That mutant PCR product was then gel purified and subcloned into the Drosophila syt cDNA construct in pBluescript mentioned above. DNA sequencing confirmed that either R285Q or R419Q was the only mutation harbored in the entire region generated by PCR. Each mutant syt cDNA was subcloned into a pUAST vector to place the mutant syt gene under the control of the UAS promoter (Brand and Perrimon, 1993).
Generation of mutant transgenic lines.
Drosophila embryos were transfected with the mutant pUAST plasmids as described previously (Mackler and Reist, 2001). At least two lines carrying separate insertions of the mutant syt transgenes were isolated for each genotype. Expression of each transgene was localized to the nervous system using the elav promoter to drive Gal4, and the Gal4/UAS system was used to amplify expression levels (Brand and Perrimon, 1993; Yao and White, 1994). Standard genetic techniques were used to cross the transgenes into the sytnull background to express the transgene in the absence of endogenous synaptotagmin I for all experiments. The genotypes of the mutant lines were yw; sytAD4 elav GAL4/sytAD4; P[UAS sytA-R285Q]/+, and yw; sytAD4 elav GAL4/sytAD4; P[UAS sytB-R419Q]/+, which are written as P[sytA-RQ] and P[sytB-RQ], respectively, in the text. The genotype of the control was yw; sytAD4 elav GAL4/sytAD4; P[UAS sytwild-type]/+, which is written as P[sytWT] in the text.
Evoked and spontaneous excitatory junction potentials (EJPs) were recorded from muscle 6 of segments 3 and 4 of third instars in HL3 saline [5 mm KCl, 1.5 mm CaCl2, 70 mm NaCl, 20 mm MgCl2, 10 mm NaCHO3, 5 mm HEPES, 115 mm sucrose, and 5 mm trehalose (Stewart et al., 1994)] as described previously (Loewen et al., 2001). Briefly, third-instar larvae were dissected in Ca2+-free HL3 to expose the body wall musculature. After changing to HL3 saline containing 1.5 mm Ca2+, muscle 6 was impaled with a recording electrode having a resistance between 10 and 40 MΩ. Evoked EJPs were generated by stimulating segmental nerves with a suction electrode filled with HL3. The Ca2+ dependence curve was generated by evoking EJPs in external Ca2+ concentrations ranging from 0.6 to 5.0 mm. Muscles were impaled in 1.5 mm Ca2+ HL3, and recordings in several different Ca2+ concentrations were obtained from each muscle fiber. The trehalose was varied between 0.5 and 5.0 mm, although this had no effect on evoked release (data not shown). The predicted maximal response was calculated by fitting the Hill equation to the mean response at each extracellular Ca2+ concentration (Kalediagraph). The Ca2+ cooperativity coefficient was estimated from the slope of a double-log plot of EJP amplitude versus Ca2+ concentration (Kalediagraph). All events were collected using an AxoClamp 2B (Molecular Devices) and digitized using a MacLab4s analog-to-digital converter (ADInstruments). Spontaneous events were recorded in Chart Software, and evoked events were recorded in Scope software (ADInstruments). Spontaneous fusion events were identified manually, blind to genotype.
For immunolabeling of the neuromuscular junction, third instars of the indicated genotypes were dissected in Ca2+-free HL3 saline to expose their body wall muscles and fixed in 4% paraformaldehyde in PBS. This whole-mount preparation was incubated overnight in anti-synaptotagmin antibody [Dsyt-CL1 (Mackler et al., 2002)], diluted 1:1000 in PBST-NGS [PBS with 0.1% Triton, 1% BSA, and 1% normal goat serum (NGS from Jackson ImmunoResearch)], washed in PBST for 30–60 min, incubated in Alexa Fluor 488 goat-anti-rabbit antibody (Invitrogen) diluted 1:5000 in PBST-NGS for 1 h, washed in PBST for 1–2 h, mounted in Citifluor (Ted Pella), and then visualized on a Zeiss LSM 510Meta confocal microscope equipped with an argon laser (Zeiss Microimaging). Emissions were collected using a bandpass 505–530 emission filter at 40× with a pinhole set for 1 Airy unit.
Similar levels of transgene expression were verified by Western blot analysis. The nervous system of a single third instar of the indicated genotype was homogenized in protein loading buffer (Bio-Rad). Proteins were separated via SDS-PAGE and transferred to a polyvinylidene difluoride membrane as described previously (Mackler and Reist, 2001). All antibodies were diluted in PBS containing 0.05% Tween and 10% NGS. Blots were probed with Dsyt-CL1 diluted between 1:1250 and 1:5000, and an anti-actin antibody (MAB 1501; Millipore Bioscience Research Reagents), diluted between 1:20,000 and 1:80,000. Actin levels were used to normalize for equal protein loading. These antibodies were visualized with HRP-tagged donkey anti-rabbit IgG, diluted 1:10,000 to 1:20,000, and HRP-tagged donkey anti-mouse IgG, diluted 1:2500 to 1:40,000 (Jackson ImmunoResearch). The HRP-tagged antibodies were detected using a Supersignal West Dura Extended Duration Substrate kit (Pierce) in an Epichemi3 Darkroom (UVP). The synaptotagmin:actin signal ratio was determined for each CNS, then normalized to the mean synaptotagmin:actin ratio of the P[sytWT] lanes on each blot to allow comparison of signal between multiple blots.
cDNA encoding the cytoplasmic domain of Drosophila synaptotagmin (C2AB, residues 191–474) was generated by PCR using primers AGCAGAGAATTCAGAAGCTGGGGCGCC and CCGCCGAAGCTTTTACTTCATGTTCTT. WT, C2A mutant (A-R285Q), and C2B mutant (B-R419Q) C2AB constructs were subcloned into the expression vector, pGEX-KG (kindly provided by Dr. Sandra Bajjalieh, University of Washington, Seattle, WA). Mammalian cDNA encoding WT, C2A mutant (A-R233Q), and C2B mutant (B-K366Q) C2AB in pGEX-KG (Li et al., 2006) was kindly provided by Dr. Thomas C. Südhof (UT Southwestern Medical Center, Dallas, TX). The C2AB domains were expressed as GST fusion proteins and purified using glutathione-Sepharose beads [GE Healthcare (Chapman et al., 1995)]. Recombinant synaptotagmin harbors tightly bound nucleic acid contaminants that may affect its properties (Ubach et al., 2001). These contaminants were removed by DNase/RNase and high-salt washes as described previously (Bai et al., 2004). Synthetic 1,2-dioleoyl-sn-glycero-3-phospho-l-serine [phosphatidylserine (PS)], 1,2-dioleoyl-sn-glycero-3-phosphocholine [phosphatidylcholine (PC)], and N-(lissamine rhodamine B sulfonyl)-1,2-dipalmitoyl-sn-glycero-3-phosphoethanolamine were purchased from Avanti Polar Lipids. A phospholipid mixture containing 15% negatively charged phospholipid was chosen to approximate the amount of negatively charged phospholipids found in neuronal membranes (Takamori et al., 2006). This mixture [15% PS + 84% PC + 1% N-(lissamine rhodamine B sulfonyl)-1,2-dipalmitoyl-sn-glycero-3-phosphoethanolamine] was dried under a stream of nitrogen and suspended in HEPES-buffered saline (50 mm HEPES/150 mm NaCl, pH 7.4). Large (100 nm) unilamellar liposomes were prepared using an extruder from Avanti Polar Lipids, as described previously (Davis et al., 1999). Rhodamine-labeled liposome-binding assays were performed as described previously (Hui et al., 2005) in 150 μl of HEPES-buffered saline (50 mm HEPES/150 mm NaCl, pH 7.4) using 6 μg of immobilized protein and 22 nm liposomes per data point. Bound liposomes were eluted with HEPES-buffered saline containing 1% Triton X-100. The solubilized lipids were collected, and binding was quantified by measuring the emission fluorescence intensity of rhodamine at 580 nm. To determine the apparent Ca2+ affinity for WT and mutant C2AB, we assayed for PS/PC binding as a function of the indicated Ca2+ concentrations. Free Ca2+ concentration was calculated by using WEBMAXC STANDARD software developed by Stanford University (http://www.stanford.edu/∼cpatton/webmaxc/webmaxcS.htm). Data were plotted and fitted with sigmoidal dose–response curves (variable slope) using PRISM 5.0 software (GraphPad). In all experiments, error bars represent the SD from at least three independent determinations.
The conserved basic residues at the tips of synaptotagmin's C2A and C2B Ca2+-binding pockets are both required for efficient synaptic transmission
A highly conserved basic residue is present in loop 3 of the Ca2+-binding pocket in both the C2A and C2B domains of synaptotagmin I (Fig. 1, ⊕). To examine the role of these residues during synaptic transmission at an intact synapse, we separately mutated the conserved basic residue in each C2 domain to a glutamine and assessed evoked release at the Drosophila neuromuscular junction. We will denote the mutation of these residues as sytA-RQ and sytB-RQ. All experiments were performed on third instars expressing the indicated form of synaptotagmin from a transgene in the absence of endogenous synaptotagmin I. To indicate their transgenic origin, we will refer to the C2A mutants as P[sytA-RQ], the C2B mutants as P[sytB-RQ], and the transgenic controls as P[sytWT]. Finally, because the random insertion of a transgene could potentially disrupt another functionally important gene, two independent insertions of each mutant transgene were examined to ensure that any deficits found resulted from the mutation rather than the insertion site.
Evoked EJPs and spontaneous miniature excitatory junction potentials (mEJPs) were recorded from larval neuromuscular junctions in HL3 saline containing 1.5 mm Ca2+. Mutation of either of the conserved basic residues that mediate synaptotagmin's electrostatic interaction with anionic phospholipids decreased the evoked response (Fig. 2). The mutation within the C2A domain reduced evoked release by ∼50% compared with the transgenic wild-type control. Evoked release in P[sytA-RQ] was 13.6 ± 2.1 mV (line 7) or 11.5 ± 0.6 mV (line 8) compared with 27.4 ± 1.5 mV in P[sytWT] (Fig. 2B, asterisks) (p < 0.0001). This decrease is similar to the result observed in cultured cells from mice and rats harboring a homologous mutation (Fernández-Chacón et al., 2001; Sørensen et al., 2003; Wang et al., 2003; Han et al., 2004). The mutation within the C2B domain reduced evoked release by ∼80% compared with the transgenic control. Evoked release in the P[sytB-RQ] mutants was 5.4 ± 0.7 mV (line 3) or 4.4 ± 0.7 mV (line 4), compared with 27.4 ± 1.5 mV in P[sytWT] (Fig. 2B, double asterisks) (p < 0.0001). This decrease is consistent with results from cultured rat neuroendocrine cells, PC12 cells (Wang et al., 2003), but in direct contrast to the results from cultured mouse neurons, hippocampal autapses (Li et al., 2006). The level of evoked release remaining in the P[sytB-RQ] mutants is significantly less than that in the P[sytA-RQ] mutants (Fig. 2B, asterisks vs double asterisks) (p < 0.01). No difference in mean EJP amplitude was found between the insertions of a given genotype for either P[sytA-RQ] or P[sytB-RQ] (p > 0.2). Thus, the reduction in evoked release results from the specific synaptotagmin mutations and not from insertion of the transgene disrupting an unspecified gene.
Mutation of either of the conserved basic residues increases the rate of spontaneous release at third-instar neuromuscular junctions (Fig. 3A). The mutation within the C2A domain at least doubled the rate of mEJPs, with a frequency of 3.5 ± 0.4 Hz (line 7) or 2.8 ± 0.3 Hz (line 8) in P[sytA-RQ] compared with 1.4 ± 0.1 Hz in P[sytWT] (Fig. 3A, asterisks) (p < 0.0001). The mutation within the C2B domain increased the rate of mEJPs by ∼40%, to 1.9 ± 0.2 Hz (line 3) or 2.0 ± 0.3 Hz (line 4) compared with 1.4 ± 0.1 Hz for P[sytWT] (Fig. 3A, double asterisks) (p < 0.05). Although the trend toward a less severe increase in mEJP frequency in the C2B mutants suggests that these mutants may maintain more of a vesicle-clamping function, the frequency of mEJPs in the P[sytA-RQ] and P[sytB-RQ] mutants was not significantly different (p > 0.05, single asterisks vs double asterisks, one-way ANOVA). No difference in mEJP frequency was found between independent insertions of the synaptotagmin gene for P[sytA-RQ] or P[sytB-RQ] (Fig. 3A) (p > 0.2). The amplitude of mEJPs was unchanged in the mutants (P[sytWT], 1.10 ± 0.03 mV; P[sytA-RQ] line 7, 1.00 ± 0.08 mV; P[sytA-RQ] line 8, 1.24 ± 0.06 mV; P[sytB-RQ] line 3, 1.09 ± 0.06 mV; P[sytB-RQ] line 4, 1.10 ± 0.07 mV; p > 0.1, one-way ANOVA). In addition, we compared the frequency of quantal amplitudes for each mutant line (Fig. 3B) (P[sytWT], P[sytA-RQ] line 8, and P[sytB-RQ] line 3 shown). The constant mEJP amplitude indicates that neither the C2A nor the C2B mutation perturbs synaptic vesicle filling or the postsynaptic machinery and is consistent with previous studies of spontaneous release characteristics in sytA-RQ mutants (Sørensen et al., 2003).
The decreased evoked release observed in P[sytA-RQ] and P[sytB-RQ] mutants is not the result of protein misexpression
It is conceivable that the decreased evoked release demonstrated in both the P[sytA-RQ] and P[sytB-RQ] mutants results from protein misexpression. To assess the expression level of each transgenic line, we probed Western blots of larval CNSs with an anti-synaptotagmin antibody (Fig. 4A) (P[sytWT], P[sytA-RQ] line 8, and P[sytB-RQ] line 3 shown). The two independent lines of both P[sytA-RQ] and P[sytB-RQ] used for the electrophysiological experiments expressed approximately the same amount of transgenic synaptotagmin as the transgenic control line (Fig. 4B). Thus, the deficits in evoked release seen in both the P[sytA-RQ] and P[sytB-RQ] mutants are not the result of insufficient expression of the transgene. To determine whether the mutant proteins were appropriately localized to synaptic sites, the neuromuscular junctions of mutant and control transgenic larvae were immunolabeled with an anti-synaptotagmin antibody. In all lines, transgenic synaptotagmin was properly localized to the neuromuscular junction (Fig. 4C) (P[sytWT], P[sytA-RQ] line 8, and P[sytB-RQ] line 4 shown). Thus, the decrease in evoked release did not result from either a deficiency in gene dosage or improper localization.
The sytA-RQ and sytB-RQ mutations decrease the Ca2+ affinity of neurotransmitter release
Release of neurotransmitter has long been known to be a Ca2+-dependent, cooperative process (Dodge and Rahamimoff, 1967). The Ca2+ cooperativity (“n”) of release may represent the mean number of Ca2+ ions used to trigger a vesicle fusion event (Dodge and Rahamimoff, 1967; Stevens and Sullivan, 2003; Tamura et al., 2007). To assess the Ca2+ dependence of the release properties in the sytA-RQ and sytB-RQ mutants, evoked release was measured at a variety of extracellular Ca2+ concentrations, ranging from 0.6 to 5.0 mm. At all Ca2+ concentrations, these mutants exhibit a decrease in evoked transmitter release compared with control (Fig. 5A). To determine whether mutation of either of these basic residues changes the Ca2+ cooperativity of release, we plotted the mean EJP amplitude versus extracellular Ca2+ concentration on a double-log plot in nonsaturating Ca2+ ranges (Fig. 5B). As estimated from the slope of these double-log plots, n = 3.2 for P[sytWT], n = 3.0 for P[sytA-RQ], and n = 2.9 for P[sytB-RQ], similar to previously recorded values (n = 3.0–3.6) at wild-type neuromuscular junctions in Drosophila (Littleton et al., 1994; Stewart et al., 2000; Yoshihara and Littleton, 2002; Okamoto et al., 2005). Thus, neither of the mutations changes the Ca2+ cooperativity of release. This finding is consistent with the hypothesis that synaptotagmin's interaction with phospholipids functions downstream of Ca2+ binding and does not affect the number of Ca2+ ions needed to trigger vesicle fusion.
To assess the apparent Ca2+ affinity of release, we fit the Hill equation to the data and normalized to the predicted maximal response within each line. Figure 5C shows that the apparent Ca2+ affinity of release in vivo was decreased in both the P[sytA-RQ] (EC50 = 2.0 ± 0.1 mm) and P[sytB-RQ] (EC50 = 2.3 ± 0.2 mm) mutants compared with the transgenic wild-type control (EC50 = 1.4 ± 0.1 mm). A rightward shift of the EC50 for Ca2+-evoked transmitter release was previously seen for sytA-RQ mutants in several cell culture systems, including hippocampal autapses, chromaffin cells, and PC12 cells (Fernández-Chacón et al., 2001; Sørensen et al., 2003; Wang et al., 2003), and our studies now show that the sytA-RQ mutation decreases the Ca2+ affinity of release at an intact synapse. In addition, our experiments demonstrate that the sytB-RQ mutation also results in a severe disruption of Ca2+-evoked transmitter release at an intact synapse, indicating that the function of the basic residue at the tip of loop 3 is conserved.
The sytA-RQ and sytB-RQ mutations decrease the Ca2+ affinity of phospholipid binding
To determine whether the conserved basic residue at the tip of each C2 domain participates in the electrostatic interaction between synaptotagmin and anionic phospholipids, we measured the Ca2+ affinity of C2AB domain binding to PS/PC liposomes in vitro. Similar to previous reports from mammalian systems (Chae et al., 1998; Davletov et al., 1998; Fernandez et al., 2001; Fernández-Chacón et al., 2001; Wang et al., 2003), the Drosophila sytA-RQ mutation decreased the Ca2+ affinity of C2AB binding to negatively charged phospholipids (Fig. 6A) (WT EC50 = 238 ± 20 μm Ca2+; sytA-RQ EC50 = 368 ± 35 μm Ca2+). Using Drosophila C2AB domains, the sytB-RQ mutation decreased the Ca2+ affinity of binding to negatively charged phospholipids to a similar extent as the sytA-RQ mutation (Fig. 6A) (WT EC50 = 238 ± 20 μm Ca2+; sytB-RQ EC50 = 344 ± 32 μm Ca2+). Compared with mammalian systems, this result is consistent with the findings of Wang et al. (2003) but in conflict with the findings of Li et al. (2006). To directly examine whether or not the Drosophila and mammalian systems differ, we also measured the Ca2+ affinity of mammalian C2AB domain binding to PS/PC liposomes. As shown in Figure 6B, both the sytA-RQ and the sytB-KQ mutations decreased the Ca2+ affinity of C2AB binding to negatively charged phospholipids to a similar extent (WT EC50 = 98 ± 6 μm Ca2+; sytA-RQ EC50 = 154 ± 10 μm Ca2+; sytB-KQ EC50 = 147 ± 7 μm Ca2+). The EC50 values measured in this study are higher than those previously reported (Fernández-Chacón et al., 2001; Wang et al., 2003) because of a lower, and more physiological (Takamori et al., 2006), percentage of negatively charged phospholipids in our liposomes. Thus, in Drosophila and mammals, mutation of either the C2A or the C2B conserved basic residue decreases the Ca2+ affinity of interactions with anionic phospholipids.
Several reports indicate that residues at the tip of the Ca2+-binding pockets, including the conserved basic residues, in both C2 domains of synaptotagmin are critical for Ca2+-dependent phospholipid interactions in vitro and Ca2+-triggered fusion in cultured cells (Chapman and Davis, 1998; Fernández-Chacón et al., 2001; Bai et al., 2002; Frazier et al., 2003; Sørensen et al., 2003; Wang et al., 2003; Rhee et al., 2005; Araç et al., 2006). Studying cultured cells provides valuable insight into possible protein functions, yet some of the properties of vesicle fusion in PC12 cells and chromaffin cells are quite different from those mediating fast transmitter release at a synapse. Even cultured neurons do not necessarily faithfully reproduce all aspects of synaptic behavior at an intact synapse. For example, at cultured hippocampal autapses, the amplitude of mEJPs is larger (Bekkers et al., 1990), the paired-pulse ratio is decreased (Sippy et al., 2003), and long-term potentiation cannot be reliably elicited (Bekkers and Stevens, 1990) compared with recordings from hippocampal slices. Additionally, synaptotagmin mutant autapses exhibit no change in mEJP frequency (Geppert et al., 1994), whereas synaptotagmin mutations increased the mEJP frequency at several other synapses, including excitatory and inhibitory synapses between cultured cortical neurons, the calyx of Held, and mature neuromuscular junctions in Drosophila and mice (DiAntonio and Schwarz, 1994; Pang et al., 2006a,c) (but see Marek and Davis, 2002). Therefore, it is critical to test the function of the basic residues at the tips of the C2 domains at an intact synapse to determine their role in synaptic transmission in vivo.
The C2A and C2B domains are structurally highly homologous and exhibit many similar biochemical interactions in vitro (Geppert et al., 1991; Sutton et al., 1995; Chae et al., 1998; Shao et al., 1998; Ubach et al., 1998; Fernandez et al., 2001; Cheng et al., 2004). Analyses of these interactions have provided critical insights into the molecular mechanisms mediating synaptic vesicle fusion. Conditions in vitro, however, can affect biochemical interactions. Interactions between the C2A basic residue and negatively charged phospholipids can differ when isolated C2A domains are used: Fernández-Chacón et al. (2001) found that the Ca2+ affinity of the interaction was decreased in sytA-RQ mutants, whereas Zhang et al. (1998) found no change. But studies using tandem C2AB domains all show a decrease in Ca2+-dependent phospholipid binding (Fernández-Chacón et al., 2001; Wang et al., 2003; Li et al., 2006). The homologous C2B residue shows variable results using tandem C2AB domains: similar to our results in Drosophila (Fig. 6A), Wang et al. (2003) found that this mutation decreased Ca2+-dependent interactions with negatively charged phospholipids, whereas Li et al. (2006) found no change. We therefore repeated these experiments using the C2AB constructs from Li et al. (2006) and found that the Ca2+ affinity of this interaction decreased (Fig. 6B). Thus, Ca2+-dependent interactions between these positively charged residues and negatively charged phospholipids appear to be quite sensitive to experimental conditions. Still, most studies find a decrease in Ca2+-dependent phospholipid interactions when either the C2A or C2B basic residue is neutralized.
Additional studies indicate that Ca2+-dependent interactions between each C2 domain and anionic membranes are conserved and mediated by residues at the tip of the Ca2+-binding pockets. Immediately adjacent to the conserved basic residues (Fig. 1, ⊕), there are hydrophobic residues (Fig. 1A, □). In both C2 domains, these hydrophobic residues interact with phospholipids in a Ca2+-dependent manner by inserting into the hydrophobic core of the membrane (Bai et al., 2002). Increasing the hydrophobicity of three residues located around the rim of each Ca2+-binding pocket substantially increased the Ca2+ affinity of these interactions (Rhee et al., 2005). Together, these results provide strong support for the hypothesis that Ca2+-dependent interactions between phospholipids and both the C2A and C2B domains are mediated by residues located at the tip of the Ca2+-binding pockets.
But are these interactions between synaptotagmin and anionic membranes relevant for synaptic transmission? Results from cultured cells suggest that residues at the tip of the C2A Ca2+-binding pocket maybe functionally significant; the sytA-RQ mutation decreased evoked transmitter release by decreasing the apparent Ca2+ affinity of release (Fernández-Chacón et al., 2001; Sørensen et al., 2003; Wang et al., 2003). The homologous mutation in C2B has been examined twice in culture with directly contradictory results. At cultured hippocampal autapses, this mutation showed no decrease in Ca2+-evoked release (Li et al., 2006). However, in cultured PC12 cells, the C2B mutation decreased Ca2+-evoked release (Wang et al., 2003). Thus, the functional relevance of the C2B interaction remained inconclusive.
To determine whether the results from cultured cells are relevant for synaptic transmission in vivo, we tested the function of the basic residue at the tip of each Ca2+-binding pocket at intact neuromuscular junctions. We found that the sytA-RQ mutation decreases the Ca2+ affinity of release at the neuromuscular junction. Importantly, we found that the sytB-RQ mutation also decreases Ca2+-evoked transmitter release by decreasing Ca2+ affinity. Western analysis and immunohistochemical localization studies demonstrate approximately equal levels of transgene expression and appropriate synaptic localization in multiple, independent mutant and control lines. Therefore the decrease in evoked release is a direct result of the mutation. Thus, both the C2A and C2B positively charged residues mediate Ca2+-dependent interactions with anionic phospholipids and are required for efficient evoked transmitter release at intact synapses.
Our results are consistent with those from PC12 cells expressing the mutant C2B protein (Wang et al., 2003). When using high K+ to trigger release, these authors found that the rate of evoked release was decreased by ∼50% in both the C2A and C2B basic residue mutations. Interestingly, the cumulative amount of release was lower in C2B mutants than in C2A mutants, although this effect was not quantified. Yet our results at intact synapses, like the results from PC12 cells, are in direct contrast with the lack of effect seen at hippocampal autapses (Li et al., 2006).
Importantly, the replacement of three hydrophobic residues around the rim of either the C2A or the C2B Ca2+-binding pocket with residues of increased hydrophobicity increased both the Ca2+ affinity of phospholipid binding in vitro and the Ca2+ affinity of evoked release at autapses (Rhee et al., 2005). Thus, even at hippocampal autapses, the tip of the C2B Ca2+-binding pocket can interact with phospholipid membranes during synaptic transmission.
Our results indicate that the function of this basic residue is conserved in each C2 domain. Yet other studies have discovered dramatic functional differences between the C2 domains during synaptic transmission. The most striking difference is the relative importance of Ca2+ binding in triggering vesicle fusion. Mutations within the C2A Ca2+-binding motif resulted in either subtle or no disruptions in evoked release (Fernández-Chacón et al., 2002; Robinson et al., 2002; Stevens and Sullivan, 2003; Pang et al., 2006b). Yet mutations within the C2B Ca2+-binding motif inhibited evoked release by up to 99% (Mackler and Reist, 2001; Nishiki and Augustine, 2004; Tamura et al., 2007). Thus, Ca2+ binding by the C2B domain plays the crucial role in triggering fast, synchronous vesicle fusion.
The key difference between the C2 domains likely resides within their polylysine motifs. The C2B polylysine motif mediates a unique set of interactions that are not shared by the C2A domain, including Ca2+-independent interactions with phosphatidylinositol 4,5-bisphosphate (PIP2) and soluble N-ethylmaleimide-sensitive factor attachment receptor (SNARE) proteins (Zhang et al., 2002; Bai et al., 2004; Rickman et al., 2004). Because the polylysine motif is on the side of the C2B domain, interactions with the SNARE proteins could hold the C2B Ca2+-binding pocket in close proximity to the presynaptic membrane, priming vesicles for immediate fusion after Ca2+ influx (Fig. 7A) (Loewen et al., 2006). Then, after Ca2+ influx, the conserved basic residues of each C2 domain mediate similar Ca2+-dependent interactions with anionic phospholipids (Fig. 6) (Wang et al., 2003), which pulls the synaptic vesicle toward the membrane (Fig. 7B). The insertion of hydrophobic residues on the tips of the C2 domains may destabilize the presynaptic membrane, aiding the fusion reaction (Bai et al., 2002; Martens et al., 2007). The relative positioning of the C2A versus C2B domains with respect to the SNARE complex may determine the relative importance of the Ca2+-binding sites, and the basic residues reported in this study, for triggering vesicle fusion in vivo. This model is consistent with the data from multiple in vitro and in vivo systems, and a remarkably similar model, postulating a more distally positioned C2A domain, has recently been proposed (Dai et al., 2007).
In summary, synchronous vesicle fusion triggered by Ca2+ requires the coordinated interactions of many presynaptic molecules. Examination of isolated interactions in vitro provides insight into possible molecular mechanisms for fusion; however, only the analysis of synaptic transmission at intact synapses can determine which interactions are likely to function in vivo. Our findings demonstrate that the positively charged residue located at the tip of each Ca2+-binding pocket mediates Ca2+-dependent interactions with negatively charged membranes and is required for efficient synaptic transmission. These findings indicate that the function of this region of C2A and C2B is likely conserved and support the hypothesis that Ca2+-dependent interactions between the tips of each C2 domain with anionic phospholipids are requisite for efficient excitation–secretion coupling during synaptic transmission.
This work was supported by grants from American Heart Association (0440168N), March of Dimes, National Institutes of Health (NS-045865, GM 56827, and MH 61876), and National Science Foundation (9982862). E.R.C. is an Investigator of the Howard Hughes Medical Institute. We thank Laurie Biela for her technical assistance, Dr. Thomas Südhof for the mammalian synaptotagmin GST-C2AB constructs, and Dr. Sandra Bajjalieh for providing the GST-KG vector.
- Correspondence should be addressed to Dr. Noreen E. Reist, Molecular, Cellular, and Integrative Neuroscience Program, Department of Biomedical Sciences, Colorado State University, Fort Collins, CO 80523-1617.
- Araç et al., 2006.↵
- Bai et al., 2002.↵
- Bai et al., 2004.↵
- Banker and Goslin, 1998.↵
- Bekkers and Stevens, 1990.↵
- Bekkers et al., 1990.↵
- Bhalla et al., 2006.↵
- Brand and Perrimon, 1993.↵
- Chae et al., 1998.↵
- Chapman and Davis, 1998.↵
- Chapman et al., 1995.↵
- Cheng et al., 2004.↵
- Dai et al., 2007.↵
- Davis et al., 1999.↵
- Davletov et al., 1998.↵
- DiAntonio and Schwarz, 1994.↵
- Dodge and Rahamimoff, 1967.↵
- Earles et al., 2001.↵
- Fernandez et al., 2001.↵
- Fernández-Chacón et al., 2001.↵
- Fernández-Chacón et al., 2002.↵
- Frazier et al., 2003.↵
- Geppert et al., 1991.↵
- Geppert et al., 1994.↵
- Han et al., 2004.↵
- Hui et al., 2005.↵
- Li et al., 2006.↵
- Littleton et al., 1994.↵
- Loewen et al., 2001.↵
- Loewen et al., 2006.↵
- Mackler and Reist, 2001.↵
- Mackler et al., 2002.↵
- Marek and Davis, 2002.↵
- Martens et al., 2007.↵
- Micheva et al., 2001.
- Nishiki and Augustine, 2004.↵
- Okamoto et al., 2005.↵
- Pang et al., 2006a.↵
- Pang et al., 2006b.↵
- Pang et al., 2006c.↵
- Perin et al., 1990.↵
- Rhee et al., 2005.↵
- Rickman et al., 2004.↵
- Rickman et al., 2006.↵
- Robinson et al., 2002.↵
- Shao et al., 1998.↵
- Sippy et al., 2003.↵
- Sørensen et al., 2003.↵
- Stevens and Sullivan, 2003.↵
- Stewart et al., 1994.↵
- Stewart et al., 2000.↵
- Sutton et al., 1995.↵
- Takamori et al., 2006.↵
- Tamura et al., 2007.↵
- Ubach et al., 1998.↵
- Ubach et al., 2001.↵
- Wang et al., 2003.↵
- Yao and White, 1994.↵
- Yoshihara and Littleton, 2002.↵
- Zhang et al., 1998.↵
- Zhang et al., 2002.↵