the drosophila epsin 1 is required for ubiquitin-dependent synaptic growth and function but not for...
TRANSCRIPT
# 2008 The Authors
Journal compilation # 2008 Blackwell Munksgaard
doi: 10.1111/j.1600-0854.2008.00832.xTraffic 2008; 9: 2190–2205Blackwell Munksgaard
The Drosophila Epsin 1 is Required forUbiquitin-Dependent Synaptic Growth andFunction but Not for Synaptic Vesicle Recycling
Hong Bao1, Noreen E. Reist2 and
Bing Zhang1,3,*
1Department of Zoology, University of Oklahoma,Norman, OK 73019, USA2Department of Biomedical Sciences, Colorado StateUniversity, Fort Collins, CO 80523, USA3Section of Neurobiology, University of Texas, Austin,TX 78712, USA*Corresponding author: Bing Zhang, [email protected]
The ubiquitin-proteasome systemplays an important role
in synaptic development and function. However, many
components of this system, and how they act to affect
synapses, are still not well understood. In this study, we
use the Drosophila neuromuscular junction to study the
in vivo function of Liquid facets (Lqf), a homolog of
mammalian epsin 1. Our data show that Lqf plays a novel
role in synapse development and function. Contrary to
prior models, Lqf is not required for clathrin-mediated
endocytosis of synaptic vesicles. Lqf is required to main-
tain bouton size and shape and to sustain synapse
growth by acting as a specific substrate of the deubiqui-
tinating enzyme Fat facets. However, Lqf is not a sub-
strate of the Highwire (Hiw) E3 ubiquitin ligase; neither is
it required for synapse overgrowth in hiw mutants.
Interestingly, Lqf converges on the Hiw pathway by
negatively regulating transmitter release in the hiw
mutant. These observations demonstrate that Lqf plays
distinct roles in two ubiquitin pathways to regulate
structural and functional plasticity of the synapse.
Key words: neuromuscular junction, synapse develop-
ment, synaptic plasticity, synaptic transmission, ubiquitin
Received 9 October 2007, revised and accepted for publica-
tion 11 September 2008, uncorrected manuscript published
online 15September 2008, publishedonline 15October 2008
The ubiquitin-proteasome system (UPS) serves to not only
degrade misfolded proteins but also dynamically regulate
protein levels and biological processes (1). In neurons, the
UPS has recently emerged as an important cellular mecha-
nism that regulates the structural and functional plasticity
and health of the nervous system in a variety of animals,
including mammals, Drosophila, Caenorhabditis elegans and
Aplysia (reviewed in 2,3). The UPS plays an active role in
synaptic plasticity through modification of synaptic trans-
mission (4,5) and regulation of protein levels in both pre- and
post-synaptic membranes (5–9). During neuronal develop-
ment, the UPS affects axonal outgrowth (10), dendritic
remodeling (11,12) and synapse formation and growth
(13–21). Finally, the UPS is implicated in a number of neu-
rological disorders (4,22–25) andWallerian degeneration (26).
At present, most UPS substrates associated with either
neuronal development or diseases remain unidentified.
Liquid facets (Lqf) possesses ubiquitin interaction motifs
and is a substrate of the deubiquitinating enzyme Fat
facets (Faf) (27,28). Lqf might regulate synaptic develop-
ment as overexpression of Faf in neurons stimulates
synaptic overgrowth at the Drosophila larval neuromuscu-
lar junction (NMJ) (16). Lqf is also a homolog of mammalian
epsin 1(27,29), which has multiple binding sites for
clathrin, adaptor protein (AP)2 and eps15 (reviewed in
30). Lqf appears to be the only homolog of epsin 1 in flies.
Furthermore, epsin 1 shares a highly conserved N-terminal
structure with the clathrin-assembly protein AP180 (30–33).
Importantly, epsin 1 binds to lipid membranes in vitro (34)
where it causes membrane curvature necessary for clathrin-
coated vesicle assembly (32). Both AP180 and epsin 1
promote clathrin cage assembly in vitro (35,36). These
observations highly suggest that epsin 1 plays a key role in
clathrin-mediated endocytosis (CME). Subsequent studies
of mammalian cultured cells, yeasts and fruit flies show that
epsin 1 and its homologs (including Lqf) are involved in the
endocytosis of select ligands (27,29,37–44). Hence, we
expect that deletion of Lqf would significantly block CME
of synaptic vesicles (SVs), homologous to the phenotypes of
the AP180 mutant like-ap180 (lap) (45–47).
Despite these implications from previous studies, it re-
mains untested whether Lqf also acts as a substrate during
Faf-induced synaptic growth and whether Lqf plays a role
in endocytosis of SVs. In this report, we investigated the
in vivo function of Lqf at theDrosophila larval NMJ, amodel
for studying synapse development and function (48,49).
Our results show that Lqf does not play a role in SV
recycling; rather, it regulates synapse development and
function through specific UPS pathways.
Results
Lqf is ubiquitously detected at a low level in both
pre- and post-synaptic membranes
Endocytotic proteins involved in CME of SVs are typically
enriched at presynaptic terminals at these NMJs in third
instar larvae [e.g. Dynamin, (50); LAP, (45); Dap160, (51)].
To reveal the cellular distribution of Lqf at Drosophila
2190 www.traffic.dk
larval NMJs, we used an Lqf polyclonal antibody for
immunocytochemistry (28). Lqf was uniformly present
at low levels at presynaptic membranes and nerves
marked by the neuronal membrane marker horseradish
peroxidase (HRP) (Figure 1A). While present at presyn-
aptic boutons, Lqf did not show the enrichment typically
seen for the endocytotic protein Dynamin (Figure 1B).
Additionally, Lqf was found at low levels in muscles,
along tracheal tubules and at postsynaptic densities
identified by the postsynaptic marker Discs large (Dlg;
Figure 1C). This pattern of Lqf subcellular localization
suggests that its functions may not be restricted to
endocytosis at nerve terminals.
To ascertain the specificity of the Lqf antibody, we
immunostained lqf mutant NMJs and measured Lqf
protein levels in lqf mutant alleles on western blots.
Several mutations in the lqf locus were generated and
described previously (27,40). Among these alleles, lqfARI
and lqfAG are severe loss-of-function mutations. When
placed over a deficiency in the region uncovering the lqf
locus, flies carrying these alleles grew slowly and died
during late larval stages. A few larvae lived to the third
instar stage with reduced body size and muscle size, but
all died before pupation. For example, the size of muscle
6/7 in abdominal segment 3 was reduced on average by
�32% (Figure S1). Immunoreactivity to the Lqf antibody
at the NMJ (identified by HRP staining) of the lqfARI/Df
mutant larva was nearly undetectable (Figure 1D). Con-
sistent with this immunocytochemistry, western blots
showed a significant reduction of Lqf proteins in third
instar larval brains and ventral nerve cords of lqfARI and
lqfAG alleles (Figure 1E). Hence, the antibody is specific
for Lqf at both larval synapses (this study) and developing
eyes (28,39).
lqf mutations slightly reduce transmitter release
at the larval NMJ
To test the hypothesis that Lqf is involved in CME of SVs,
we first characterized the lqf mutant NMJ using electro-
physiology. We examined spontaneous miniature excit-
atory junction potentials (mEJPs or minis) in the wild-type
control and lqfARI/Df larvae by recording from muscles
bathed in HL-3 saline containing 0.1 mM Ca2þ and 1 mm
tetrodotoxin (TTX) (45,47,52,53). The resting potential was
similar between the two genotypes (�65.6� 0.80 mV, n¼12, in the control and �64.3 � 0.97 mV, n ¼ 14, in the lqf
mutant). Minis in lqfARI/Df larvae were reduced in fre-
quency but larger in amplitude (Figure 2A,B). Although
rare, both the mutant and the control larvae displayed
minis with unusually large amplitudes (Figure 2A). Mini
frequency in the lqfARI/Dfmutant was significantly reduced
Figure 1: Lqf is present in both pre-
and post-synaptic membranes at the
larval NMJ. A) Immunoreacivity to Lqf
and the neuronal membrane marker
HRP at the wild-type larval NMJ on
muscle 4 (M4). Lqf (green) is present
in muscles, synaptic boutons and ner-
ves, whereas HRP (red) staining is re-
stricted to neuronalmembranes (nerves
and synaptic boutons). Motor nerves
and tracheal tubules are marked by ‘n’
and ‘t’, respectively. The inset on the
overlay panels shows close-up images
of localization signals (same for panels B
and C). B) Immunoreacivity to Lqf and
the endocytotic protein Dynamin at
the wild-type larval NMJ. Note that
Dynamin (red) is highly enriched at pre-
synaptic boutons. C) Lqf (green) is colo-
calized with Dlg (red) at the postsynaptic
density and at low levels in muscles. D)
Lqf immunoreactivity in the lqfARI/Df mu-
tant larval NMJ is significantly reduced
compared with HRP. The scale is 20 mm
for images in panels (A–C), 5 mm for
insets and 10mm for images in panel (D).
E) Lqf protein levels are nearly absent in
the brain and ventral nerve cords of two
lqf mutants (lqfARI/Df and lqfAG/Df ). The
western blot was reprobed for a-tubulin
to ensure that sample loading was simi-
lar among different genotypes.
Traffic 2008; 9: 2190–2205 2191
Novel Synaptic Roles for Drosophila Epsin 1
from 5.1 � 0.5 Hz (n ¼ 12) in the wild type to 3.4 � 0.4 Hz
(n ¼ 14) (p < 0.05). In contrast, mini amplitude was
increased from 1.4 � 0.1 mV (n ¼ 12) in the wild type to
2.1 � 0.3 mV (n ¼ 14) in lqfARI/Df larvae (p < 0.05).
Although the mini amplitude was slightly increased, we
failed to detect a change in glutamate receptor levels in
muscle cells (Figure S2).
We next investigated action potential-evoked synaptic
transmission in lqf mutants. Evoked transmitter release
was measured as excitatory junction currents (EJCs)
from muscles voltage clamped at �80 mV in saline
containing 1 mM Ca2þ (Figure 2C). The amplitude of EJCs
was slightly reduced from 54.5 � 2.6 nA (n ¼ 9) in the
control larvae to 38.6 � 3.5 nA (n ¼ 9; p < 0.05) in lqfARI/
Df larvae and to 45.1 � 4.2 nA (n ¼ 21; p > 0.05) in lqfAG/
Df larvae (Figure 2D). Heterozygous lqf mutant alleles or
its deficiency (Df) were essentially similar to wild-type
control larvae and did not have a dominant effect on
evoked EJC amplitudes (Figure S3). It appears that lqfARI
is a more severe allele than lqfAG, consistent with
the conclusion reached by others studying heart de-
velopment in Drosophila (41). For this reason, we con-
ducted most of the remaining experiments with the
lqfARI allele.
Electrophysiological evidence that lqf mutations do
not block SV recycling at the larval NMJ
Given the previously suggested role for Lqf in CME, the
defects we have observed in synaptic transmission could
be caused by an impairment of SV recycling. We ad-
dressed this possibility by measuring the vesicle depletion
rate electrophysiologically. Upon repetitive and prolonged
nerve stimulation, the NMJ depletes SVs first in the readily
releasable pool, then the releasable pool and finally relies
on both translocation of SVs from the reserve pool and
recycling of SVs to sustain transmitter release. Mutations
reducing vesicle recycling have been shown to rapidly and
dramatically reduce transmitter release when challenged
with maintained nerve stimulation (54–58).
We recorded EJCs in HL-3 saline containing high Ca2þ so
that we could maximize the release probability and achieve
a rapid depletion of the vesicle pool. We initially stimulated
the motor nerve at 0.2 Hz to obtain a basal level and then at
10 Hz for 5 min to measure the depletion rate. This was
followed by a short period of nerve stimulation at 0.2 Hz to
measure the EJC recovery rate (Figure 3A,B). The ampli-
tude of EJCs for basal release was 125.2 � 5.72 nA (n ¼ 7
at 1.8 mM Ca2þ) and 124.2 � 4.9 nA (n ¼ 8 at 2 mM Ca2þ)
for the control and lqfARI/Df larvae, respectively. Three
Figure 2: lqf mutations alter synap-
tic transmission. A) A cumulative plot
of spontaneous minis and a histogram
of the average mini amplitude in the
wild-type (wt) and lqfARI/Df larvae. The
average amplitude of minis is signifi-
cantly increased in the lqfmutant (*p <
0.05). B) A histogram of mini frequen-
cies in the wild-type control and mutant
larvae. Mini frequency is significantly
reduced in the mutant compared with
the control larvae (*p < 0.05). C) Rep-
resentative traces of EJCs in the wild-
type control larvae and two lqf mutant
genotypes. D) A histogram of the aver-
age amplitude of EJCs. The lqfARI/Df
mutant significantly reduces the am-
plitude of EJCs compared with the
control larvae (*p < 0.05).
2192 Traffic 2008; 9: 2190–2205
Bao et al.
consecutive EJCs at the onset of the high frequency
stimulation (marked time 0), at 30 seconds and every
minute thereafter were averaged and then normalized to
the basal amplitude. Our results showed that transmitter
release in the control larvae dropped by�19% at the onset
of 10 Hz stimulation (indicated by time 0 in Figure 3B) and
soon reached �45% of the normal release within 30
seconds. Following this initial and rapid decline, trans-
mitter release was gradually reduced but maintained at
�38% of the normal release near the end of 5 min
stimulation. This steady state of release is thought to
reflect the balance of exocytosis and endocytosis of SVs
(54). EJC amplitude was rapidly recovered to nearly pre-
vious levels within 10–15 seconds.
In lqfAR1/Df mutant larvae, the initial drop of transmitter
release at the onset of stimulation (i.e. time 0) was similar
to that observed in the control larvae. However, trans-
mitter release dropped only to �55% of the basal level at
30 seconds and remained at a higher steady-state level
(�50%) compared with the control larvae. In other words,
the depletion rate in the lqf mutant is significantly slower
than that in the control larva (p < 0.05). Such a lack of
effects on vesicle depletion has also been shown in the
Drosophila amphiphysin mutant (59).
Delayed rebound of the EJC amplitude, which presumably
reflects impaired SV recycling, is expected for endocytotic
mutants (58). However, this did not occur in the lqf mutant
(Figure 3A,B). The kinetics of EJC amplitude recovery
following the 5-min prolonged depletion period was similar
to that in the wild type or slightly faster in the lqf mutant.
Consistent with these electrophysiological results, our re-
sults demonstrated that lqfmutants readily took up FM 1-43
dyes at the NMJ, similar to the control larvae (Figure S4).
Taken together, these results argue against the possibility
that deletion of lqf blocks SV recycling at the larval NMJ.
Ultrastructural evidence that lqf mutations do not
block SV recycling
To ascertain that indeed SV recycling is not blocked by lqf
mutations, we examined the SV pool at the ultrastructural
level. Previous studies have shown that nerve terminals in
endocytotic mutants typically contain significantly reduced
number of vesicle (45,55–58, 60–62). Although the shape
of boutons was altered (see Discussion below), the SV
pool in type Ib boutons was not reduced in the lqf mutant
compared with the control larvae (Figure 4A,B). Quantifi-
cation of over 10 random transmission electron micro-
scope (TEM) micrographs showed that the average
density of SVs (number of SVs per mm2) inside type Ib
boutons was significantly increased in the lqf mutant
(379.7 � 19.8, n ¼ 12) compared with that in control larvae
(306.4 � 23.8, n ¼ 14) (p < 0.05; Figure 4C). Judging from
the average diameter of SVs, we found no apparent
differences in SV size between these two genotypes
(Figure 4D). Hence, collective evidence from electrophys-
iology, ultrastructure and optical imaging strongly indicates
that contrary to its expected function, Lqf does not play
a detectable role in CME of SVs at Drosophila NMJs.
Synaptic bouton size is increased and bouton
shape is altered in the lqf mutant
To determine whether Lqf plays a role in synapse devel-
opment, we examined synaptic bouton number and mor-
phology using antibodies to the SV protein synaptotagmin I
as well as to HRP. Using antibodies to other SV proteins
[such as cysteine string protein (CSP) and synaptobrevin],
we failed to reveal obvious defects in mislocalization of
Figure 3: lqfmutants do not display a detectable defect in SV
endocytosis. A) The motor nerve is first stimulated at 0.2 Hz
(control), followed by 10 Hz stimulation for 5 min and then by 0.2
Hz until the EJC amplitude is recovered. Examples of EJC traces
from these three stimulation periods are shown here. [Ca2þ] is
1.8 mM for the wild type and 2 mM for the lqf mutant so that
their initial EJC amplitude is similar. B) The depletion rate of the SV
pool by repetitive stimulation of the motor nerve (10 Hz, 5 min)
is shown by normalizing the EJC amplitude to the control EJC
amplitude evoked at 0.2 Hz. The recovery kinetics is revealed by
low rate stimulation (0.2 Hz) following the SV pool depletion. n¼ 7
and 6 for the wild-type and the lqf mutant larvae, respectively.
These results are inconsistent with a role for Lqf in either
endocytosis or recycling of SVs at the NMJ.
Traffic 2008; 9: 2190–2205 2193
Novel Synaptic Roles for Drosophila Epsin 1
SV proteins to extrasynaptic axons, as previously shown to
the lap mutant [data not shown, (47)]. Our results showed
that synaptic bouton number was reduced in the lqf mutant
(Figure 5A–E). The average number of type Ib and Is
boutons found on muscle 4 was 54.0 � 2.8 (n ¼ 14) and
23.2� 1.7 (n¼ 22) for the control larvae and the lqfmutant
larvae, respectively (p < 0.001) (Figure 5B,E). On muscles
6/7, the total bouton number was also reduced from 104.3
� 11.1 (n ¼ 10) in the control larvae to 65.7 � 6.4 (n ¼ 13)
in the lqfARI/Df mutant (p < 0.001) (Figure 5D,E). This
represents a 57 and 37% reduction from the control larvae
for muscle 4 and muscles 6/7, respectively. Once calibrated
to the surface area of the muscle fiber (63), the difference in
bouton numbers became statistically insignificant except for
muscle 4 on segment 3 (Figure 5F). The results from
muscles 6/7 and 4 on segment 4 showed that the average
bouton number per muscle surface area was similar
between the lqf mutant and the control animal (Figure S5).
Similar findings on bouton numbers were also detected in
the lqfAG/Df allele (data not shown). Hence, lqf mutations
reduce larval body size and muscle growth but do not
significantly alter synaptic bouton numbers on all muscles.
One noticeable defect was that the size and shape of
synaptic boutons were altered. The average size of type Ib
and Is boutons was doubled from 5.68 � 0.27 mm2 (n ¼ 9)
in control to 13.25 � 1.26 mm2 (n ¼ 9) in the lqf mutant on
muscle 4 (p < 0.001) (Figure 5G). Bouton size on muscles
6/7 was also increased from 6.41 � 0.22 mm2 (n ¼ 10) in
control larvae to 9.21 � 0.35 mm2 (n ¼ 13) in the mutant
(p< 0.001) (Figure 5G). It appears that the most significant
change is the enlargement of those small boutons seen
normally between large boutons (compare lower panels in
Figure 5A,B and Figure 5C,D). This increase in bouton size
remained even when type Ib and Is boutons were consid-
ered separately.
Figure 4: Ultrastructural analysis reveals no evidence for a defect in SV pool in the lqfmutant. A and B) Electronmicrographs of the
longitudinal section of type Ib synaptic boutons in the control (wt) and lqfARI/Df larvae. Both synaptic boutons are occupied by a large
number of SVs with apparently similar sizes (see insets). C) The average SV density (number of SVs/mm2) is slightly increased in the lqf
mutant (*p< 0.05). D) The average diameter of SVs does not differ between the wild type and the lqfmutant. These ultrastructural results
are consistent with the electrophysiological observation, indicating that neither SV endocytosis nor recycling is blocked by the lqfmutation.
MTs, microtubules; SVs, synaptic vesicles.
2194 Traffic 2008; 9: 2190–2205
Bao et al.
We next examined the active zone number in the mutant
synapse and found that each bouton contained a slightly
higher number of active zones in the mutant (Figure S2).
As expected for reduced muscle size and bouton number,
the total number of active zones per muscle was signifi-
cantly reduced compared with that in the wild type. These
changes may account for the reduced transmitter release
in the mutant.
Figure 5: lqf mutations increase the size
and alter the shape of synaptic boutons.
A–D) Immunocytochemistry of synaptic mor-
phology shows that the total number of type
Ib and Is synaptic boutons on muscle 4 (M4)
and muscles 6/7 (M6/7) is reduced in the
lqfARI/Df mutant larvae (panels B and D)
compared with that in the control larvae
(wt, panels A and C). Additionally, the size
of synaptic boutons is enlarged on average in
the lqf mutant (see close-up panels). Finally,
some boutons have irregular rather than the
normal oval or round shapes. E) Histograms
of the average number of type Ib and Is
synaptic boutons on muscles 4 (M4) and
muscles 6/7 (M6/7) in segment 3. On aver-
age, the number of synaptic boutons is
significantly reduced in the lqf mutant com-
pared with that in the control larvae (***p <
0.001). F) Histograms of the average number
of synaptic boutons (type Ib and Is) normal-
ized to the surface area of muscles in seg-
ment 3. The difference remains significant in
muscle 4 but not in muscles 6/7 (**p< 0.01).
G) Histograms of the average size of type Ib
and Is synaptic boutons on muscles 4 (M4)
and muscles 6/7 (M6/7) in segment 3. On
average, the size of synaptic boutons is
significantly larger in the lqf mutant than that
in the control larvae (***p < 0.001).
Traffic 2008; 9: 2190–2205 2195
Novel Synaptic Roles for Drosophila Epsin 1
Finally, we found that some boutons changed from the
normal round shape to an irregular and elongated ‘potato-
like’ shape (Figure 5B). This change in bouton shape is
similar to those observed in the electron microscope
(Figure 4B). These alterations in bouton size and shape
suggest a novel role for Lqf in synaptic development.
Neuronal expression of the wild-type lqf gene
rescues the developmental and functional defects
in lqf mutants
To ensure that the defects found in the lqf mutant
specifically result from a disruption of the lqf gene, we
used either a complementary DNA rescue construct
[upstream activation sequence (UAS)-Lqf] or a genomic
rescue line carrying the wild-type lqf gene to rescue the
lqfARI/Df mutant phenotype (27). One copy of the geno-
mic lqf gene (Glqfþ) readily rescued the lqfARI/Df mutant
to viable adults. Using the Gal4-UAS-system (64), we
next conducted tissue-specific rescue. Muscle-
specific expression of Lqf driven by the myosin heavy
chain (MHC) Gal4 driver did not rescue the lqf mutant.
Occasionally, a few larvae (estimated to be <1%) lived
to become early pupae. However, all of them died soon
after pupation. In contrast, neuronal expression of Lqf
driven by the pan-neuronal ElavC155 Gal4 driver rescued
the mutant to viable adults when the flies were kept at
18–198C, suggesting a primary role for Lqf in neurons.
At room temperature (�228C), this rescue was not
successful, likely because of gain-of-function effects of
Lqf (Figure 8).
We then further examined the genomically rescued lqf
animals morphologically and physiologically. First, synaptic
boutons in the rescued larvae resumed the oval or round
shape typically seen in the wild-type larvae (Figure 6A,B).
Second, the body size of the rescued larvae was similar to
Figure 6: The wild-type lqf gene rescues
both the morphological and the functional
defects in the lqf mutant. A and B) Repre-
sentative images of NMJs on muscle 4 (M4,
panel A) and muscles 6/7 (M6/7, panel B) in
the lqfARI/Df mutant in which a copy of the
wild-type lqfþ gene has been introduced. The
rescued mutant is viable as adult and does not
display any gross anatomical and behavioral
abnormalities. Note the restoration of well-
spaced round- or oval-shaped boutons in a typ-
ical ‘beads-on-a-string’ arrangement at the
larval NMJ (compare with mutant boutons in
Figure 5). C and D). The amplitude of evoked
EJCs is restored to a level slightly but not
significantly higher than that in the control
larvae. E and F) Representative mini traces
and histograms of mini amplitude and fre-
quency. Recordings were conducted under
the same conditions as those shown in Figure 2.
*p < 0.05. n.s., not significantly different.
2196 Traffic 2008; 9: 2190–2205
Bao et al.
that of the control larvae. Consequently, the average muscle
size was also restored to near wild-type levels (data not
shown). The number of synaptic boutons was 45.9 � 3.4
(n ¼ 14) in muscle 4. This value is not statistically different
from that in the control larvae (p > 0.05). Third, evoked
synaptic currents were reversed to 64.5 � 7.5 nA (n ¼ 12),
which was slightly above but not statistically significant from
the average amplitude of EJCs in the control larvae (54.5 �2.6 nA, n ¼ 9; p > 0.05) (Figure 6C,D). Fourth, mini ampli-
tude was reversed to near wild-type levels (Figure 6E,F).
The mini frequency, however, was not rescued. Finally, the
rescued mutant flies were fully viable as adults, with no
apparently behavioral or morphological abnormalities. These
results indicate that the morphological and electrophysio-
logical defects detected in the lqf mutant are specifically
caused by the loss of function of Lqf.
Lqf is required for Faf-induced synaptic overgrowth
Neuronal overexpression of Faf promotes overgrowth
of synapses at Drosophila NMJs (16). This overgrowth
seems to depend on Faf’s deubiquitinating activity
because the yeast UBP2 has similar stimulating effects
on synaptic growth (21). The mitogen-activated protein
(MAP) kinase kinase kinase (MAPKKK) Wallenda (Wnd)
is also required downstream of Hiw (21). Lqf has
been demonstrated to be a specific substrate of the
deubiquitinating enzyme Faf (28). Could the overgrowth
induced by Faf overexpression also depend on a Faf–Lqf
interaction?
We tested this hypothesis by overexpressing Faf in the lqf
mutant background (ElavC155 Gal4/þ; lqfARI, EP(3)381/lqf
Df). Consistent with previous observations (16), neuronal
overexpression of Faf induced NMJ overgrowth in a wild-
type background (compare Figure 7A,B). In the absence of
Lqf, overexpression of Faf failed to stimulate synaptic
growth (Figure 7C). The number of synaptic boutons on
muscle 4 was significantly reduced by �78% to a level
similar to that found in the lqf mutant. Bouton numbers
were 99.1 � 10.4 (n ¼ 16) in Faf-overexpressing larvae
and 21.6 � 2.4 (n ¼ 15) when Faf was overexpressed in
the lqf mutant background (p < 0.001) (Figure 7D). After
normalizing to the surface area of respective muscle
fibers, the number of boutons per muscle surface area
remained significantly lower than that in the Faf-over-
expressing larvae (p < 0.01; Figure 7E). These results
suggest that Lqf acts downstream of Faf to promote
synaptic growth.
Figure 7: Lqf is required for Faf-
induced synaptic overgrowth. A)
A representative image of synaptic
morphology onmuscle 4 (M4) in the
wild-type (wt) larva revealed by the
neuronal membrane marker HRP
and the SV protein Syt I. B) Neuronal
overexpression of the deubiquitinat-
ing enzyme Faf induces overgrowth
of synaptic boutons (muscle 4 is
shown here). The arrow indicates
neuronal overexpression of Faf in
ElavC155 Gal4/þ; EP(3)381/þ flies
(same for panels C–E). C) The Faf-
induced synaptic overgrowth is fully
suppressed in the lqfARI/Df mutant
background. D) Histograms of the
average number of synaptic bou-
tons on muscle 4 (segment 3). E)
Histograms of the average number
of synaptic boutons normalized to
the surface area of muscle 4 (seg-
ment 3). ***p < 0.001. n.s., not
significantly different.
Traffic 2008; 9: 2190–2205 2197
Novel Synaptic Roles for Drosophila Epsin 1
To test whether this suppression of Faf-induced synaptic
overgrowth is mediated by a defect in CME, we overex-
pressed Faf in the lapmutant background in which CME is
severely impaired by deletion of the clathrin assembly
protein LAP (45). In the lap mutant background, over-
expression of Faf consistently induced overgrowth of
synapses (data not shown). Together with our electro-
physiological and ultrastructural data, these results sug-
gest that Lqf mediates Faf-induced synaptic overgrowth
by a mechanism that appears to be independent of CME.
Neuronal overexpression of Lqf promotes bouton
budding but does not mimic Faf-induced synapse
overgrowth
If Lqf acts as a substrate of Faf in synaptic overgrowth,
could overexpression of Lqf itself mimic the Faf effect?
To test this idea, we overexpressed Lqf in neurons using
UAS-Lqf and ElavC155 Gal4 and found that this did not
achieve the exuberant overgrowth of NMJs seen in Faf
overexpression larvae. However, we noted a large number
of satellite or miniature boutons, which resemble those
found in larvae overexpressing b-amyloid precursor-like
protein (65) and in a number of endocytotic mutants (66)
(Figure 8B,C). In some NMJs, synaptic boutons were
dramatically enlarged and shaped like ‘growth cones’, with
visible filopodia-like protrusions or tiny budding vesicles
(Figure 8B–D). In rare cases, we also detected giant
synaptic boutons, which had reduced levels of SV markers
(e.g. Syt I, Figure 8E). As with the neuronal rescue
experiment described above, the gain-of-function pheno-
type observed in this study was more pronounced at room
temperature or higher, suggesting that synapse develop-
ment depended on Lqf protein levels. The mechanisms
Figure 8: Neuronal overexpression of Lqf promotes budding of miniature synaptic boutons and the formation of ‘growth cone’-
like boutons. A) A representative image of NMJs onmuscle 4 in the control larvae (ElavC155 Gal4/þ) co-stained for the neuronal membrane
marker HRP and the SV protein synaptotagmin I (Syt I). One area of the NMJ (arrowhead) is enlarged and shown in the far right panel. B–E)
Examples of NMJs from larvae overexpressing Lqf in neurons using the pan-neuronal driver ElavC155 Gal4 (indicated by the arrow). Note the
dramatic changes in synaptic bouton morphology. Panel (B) shows a ‘lobster’-shaped NMJ with one enlarged bouton and numerous small
budding boutons. Particularly, the SV marker is found in these miniature boutons. Panel (C) shows an example where the motor axon
becomes ‘spine’ shaped because of the addition of small boutons along the entire length of the axon. Panel (D) shows that although the
NMJ on muscle 12 appears normal, muscle 13 has a large ‘leaf’-shaped giant synaptic bouton. Note the presence of small ‘filopodia’-like
protrusions. Panel (E) shows a ‘crab’-shaped giant synaptic bouton associated with short and thin protrusions. Note the spatial restriction of
the SV marker within the giant bouton.
2198 Traffic 2008; 9: 2190–2205
Bao et al.
involved in such dramatic changes in bouton shapes
and sizes are not clear. Nonetheless, the appearance of
mini boutons and filopodia-like protrusions suggests that
overexpression of Lqf stimulates bouton budding but fails
to induce full expansion and maturation of synaptic bou-
tons. These findings imply that Faf has at least one other
substrate that acts synergistically with Lqf in promoting
synaptic growth.
lqf does not suppress synaptic overgrowth
in the hiw mutant
To further explore the role of Lqf in the UPS-mediated
synaptic growth, we next studied the genetic interaction
between lqf and highwire (hiw) mutations. Hiw is a puta-
tive E3 ubiquitin ligase that inhibits synaptic growth in
Drosophila (13,16), C. elegans (14,15) and mammals
(15,18). In Drosophila, hiw and faf mutations interact
genetically (16). Overexpression of Faf mimics the synap-
tic overgrowth seen in the hiw mutant. faf null mutants,
which do not have an apparent phenotype in both synaptic
morphology and function, partially rescue the defect in
transmitter release in hiw mutants. However, faf does not
suppress NMJ overgrowth caused by the loss of hiw (16).
These results suggest that the Hiw-based ubiquitin path-
way may be parallel with the Faf-dependent ubiquitin
pathway in conditioning synaptic growth (67).
To further test this idea, we conducted genetic interactions
between hiw and lqf mutants. hiwND9, a partial loss-
of function allele (68), is adult viable as homozygotes with
minor locomotion defects (13). Our results showed that
the hiwND9; lqfARI/Df double mutant died before reaching
second instar larval stage. In hiwND9; lqfARI/lqfAG double
mutants, we observed mid second instars. lqfFDD9 is
a hypomorphic allele of lqf, which is fully viable as
homozygotes at room temperature, has weakly rough
eyes (27) and retains less than 10% of the Lqf protein
(28) (Figure 9A). hiwND9; lqfFDD9 double mutants showed
partial lethality as some of them died in the pupal case,
whereas others escaped to the adult stage. Even though
hiw and lqf mutations showed lethal genetic interactions,
the hiwND9 mutation did not suppress the rough eye
phenotype in lqfFDD9 homozygotes (data not shown) or
alter the Lqf protein levels measured in adult hiw mutant
head extracts (Figure 9A).
To examine the effect of lqf mutations on synaptic over-
growth in hiw mutants, we generated three double mu-
tants: hiwND9; lqfARI/lqfAG, hiwND9; lqfARI/lqfFDD9 and
hiwND9; lqfAG/lqfFDD9. None of these allelic combinations
significantly inhibited synaptic overgrowth in the hiwND9
mutant background (Figure 9B–G). In second instar larvae,
muscle 4 had 39.5 � 2.4 (n ¼ 11) and 36.8 � 4.1 (n ¼ 12)
boutons in the hiwND9 mutant and hiwND9; lqfARI/lqfAG
double mutants, respectively (Figure 9B,C,H). The synap-
tic bouton number increased to 102 � 4.8 (n ¼ 13) in the
third instar hiwND9 mutant (Figure 9D,E,I). In third instar
Figure 9: lqf mutations do not reduce the synaptic over-
growth in hiw mutants. A) Western blot analyses show that
Lqf levels are significantly reduced in adult head extracts of the
lqfFDD9 homozygote but remain unaltered in the hiwND9 homozy-
gote. The western blot was reprobed for a-tubulin to ensure that
sample loading was similar between the wild-type control flies and
the mutant flies. B, C and H) Synaptic growth in second instar
larval NMJs in the hiwND9 mutant (panel B) is not significantly
affected by lqfARI/lqfAGmutations (panel C). The NMJ is stained for
HRP in these and the following images. A histogram of synaptic
bouton numbers on muscle 4 in these mutants is shown in panel
(H). D, E and I) Synaptic growth in third instar larval NMJs in the
hiwND9 mutant (panel D) is not significantly affected by lqfARI/
lqfFDD9 mutations (panel E). A histogram of synaptic bouton
numbers on muscle 4 is shown in panel I. F and G) Representative
images of exuberant synaptic growth on muscles 12 and 13 (M12
and M13) in third instar larvae of hiwND9 mutants and hiwND9;
lqfAG/lqfFDD9 double mutants.
Traffic 2008; 9: 2190–2205 2199
Novel Synaptic Roles for Drosophila Epsin 1
larvae of hiwND9; lqfARI/lqfFDD9 double mutants, muscle 4
had 110.4 � 5.7 (n ¼ 12) synaptic boutons. None of these
differences was statistically significant (p > 0.05). Simi-
larly, synaptic overgrowth persisted on muscles 12 and 13
in the hiwND9; lqfAG/lqfFDD9 double mutant (Figure 9F,G).
These observations suggest that there are at least two
distinct pathways for ubiquitin-dependent synaptic growth
and that Lqf is unlikely to be a substrate for ubiquitination
by Hiw.
lqf partially rescues the synaptic transmission
defect in hiw mutants
Synaptic transmission is severely reduced in hiw mu-
tants (13). Because lqf and hiw mutations are synthetically
lethal, one might predict that lqf mutations could further
reduce transmitter release in the hiw mutant and thus
account for their lethal genetic interactions. However, faf
null alleles partially suppress the synaptic transmission
defect in hiw mutants (16). Lqf levels are reduced in faf
mutants (28), suggesting that lqf mutations may also
partially rescue the hiw physiological defect.
To distinguish these possibilities, we recorded minis and
EJPs in hiw; lqfARI/lqfFDD9 double mutants using lqfARI/
lqfFDD9 and hiw single mutants as controls. With the
exception of increased mini amplitude, other parameters
of synaptic transmission were not significantly altered in
the lqf hypomorphic mutant (Figure 10A–C). Consistent
with earlier observations (16), mini frequency and the
amplitude of evoked EJPs were both reduced in hiw
mutants (Figure 10A–C). This reduction in evoked EJP
amplitude in the hiw mutant was partially suppressed
by the lqf mutation. This suppression was significant as
the EJP amplitude in the hiw mutant was nearly doubled
(p < 0.05). However, lqfmutations had little effect on both
the mini frequency and the amplitude in hiw mutants,
suggesting that this suppression is rather specific to
calcium-evoked exocytosis.
Discussion
Lqf does not play a significant role in SV recycling
One important finding from this study is that Lqf does not
play a detectable role in SV endocytosis. Multiple lines of
evidence obtained from electrophysiological, ultrastruc-
tural and optical imaging studies support this conclusion.
To our knowledge, this is the first in vivo study of Lqf or
epsin 1 on SV recycling. Our finding is also clearly
surprising given that epsin 1 has been highly implicated
to play a key role in the initiation of clathrin-coated vesicle
formation and endocytosis (32,34). Does our observation
reflect the special property of the fly NMJ? Lqf lacking
either the ENTH domain or the clathrin-interacting
C-terminus has been shown to rescue the mutant pheno-
type in the developing eye (39). These rescue results are
intriguing, but they do not readily support a specific role for
Lqf in CME. In particular, there are no clear mechanisms on
how these truncated fragments could fulfill Lqf’s clathrin-
dependent functions. Interestingly, RNA interference and
small interfering RNA-induced knockdown of epsin 1 fails
to block the internalization of EGF receptors in HeLa cells
(69,70). There is also evidence that epsin 1 functions only
in clathrin-independent endocytosis (70,71). Furthermore,
Lqf has been shown to be required for endocytosis of
select receptors but not of all receptors (41–43). More
importantly, Lqf itself is not required for receptor-mediated
endocytosis. Rather, Lqf appears to signal select ligands
(such as Delta/Serrate/Lag2) for internalization or recycling
(42). Hence, these studies lend strong support to our
observations that Lqf does not play a significant role in
CME of SVs.
It should be noted that recent studies reveal that the
epsin 1-interacting protein Eps15 is required for SV
recycling in both C. elegans (72) and Drosophila (73,74).
However, Eps15 is required to maintain the level of
endocytotic proteins in nerve terminals (74). Strikingly,
key endocytotic proteins such as Dynamin and Dap160
are reduced in synaptic boutons by �90 and �80%,
respectively, in eps15mutants. These observations make
it difficult, if not impossible, to assign a direct role for
Eps15 in CME.
Lqf plays a novel role in a specific UPS pathway to
regulate NMJ growth
Synapse development is a highly regulated process
involving a large number of molecules (48,63,75–77).
The first suggestion that Lqf could have a potential role
in synapse development came from studies of its deubi-
quitinating enzyme Faf (16). This notion was further
supported by a direct biochemical demonstration that
Lqf is a specific substrate of Faf (28). Our studies provide
the first experimental test of this hypothesis by showing
that Lqf acts downstream of Faf in promoting synaptic
overgrowth. This effect on NMJ growth appears to be Faf
dependent as lqf mutations alone do not dramatically
affect bouton numbers. It is interesting to note that
neuronal overexpression of Lqf promotes bouton budding
but does not mimic the exuberant synaptic overgrowth
induced by overexpression of Faf. Hence, we suggest
that Lqf is necessary but insufficient for synaptic over-
growth, raising the possibility that Lqf is not the only
substrate of Faf in motoneurons (hence the hypothetical
molecule X in Figure 10D).
Another important finding emerging from this study is that
two distinct UPS pathways may be employed at the
Drosophila larval NMJ to regulate synapse growth. The
Hiw/RPM-1/Phr1 proteins have a conserved role in inhibit-
ing presynaptic development in Drosophila, C. elegans and
mammals (13–15,18,68). In C. elegans (19) and Drosophila
(21), the substrates of RPM-1/Hiw have been shown to be
2200 Traffic 2008; 9: 2190–2205
Bao et al.
MAP kinases and MAPKKK. Our study indicates that Lqf is
unlikely a substrate of Hiw in conditioning synaptic growth.
In contrast, the Faf pathway is a positive regulator of
synaptic growth at the NMJ (16) in which Lqf is an
essential substrate (this study). Hence, we suggest that
Hiw and Faf/Lqf are two distinct UPS pathways that
regulate synapse development in Drosophila.
However, the relationship between the Faf and Hiw path-
ways in synapse development is rather complex. Intriguingly,
the MAPKKK Wnd is required for synaptic overgrowth
mediated by both Hiw and Faf pathways (21). One possibility
is that Wnd acts downstream of Lqf to fulfill the function of
both the Hiw and the Faf pathways. However, this idea is
inconsistent with the observation that unlike lqfmutants, the
wnd null mutant itself has no morphological or electrophys-
iological defect. More importantly, wnd mutations do not
suppress the transmitter release defect seen in the hiw
mutant (21), whereas the lqf mutant does. Alternatively, we
suggest that Hiw and Faf act through two parallel pathways
and that the suppression of Faf-induced overgrowth by the
wnd mutation may be mediated by Fos/Jun kinase signaling
(Figure 10D). Based on the observation that overexpression
of Ubp2A increases neuronal Wnd levels (21), it is possible
that Faf may also use Wnd as a substrate for synaptic
overgrowth (78). However, this has yet to be tested
experimentally.
Dissociation of synaptic growth from function
Recent genetic studies have revealed an interesting feature
of synapse growth and function that closely depends on
protein turnover by specific UPS pathways. InDrosophila, faf
or lqf mutations are capable of partially suppressing the
defect in transmitter release in hiw mutants. This partial
suppression is specific and should not be viewed simply as
a reduction of transmitter release in faf or lqf mutant back-
grounds by hiw mutations. If there were no partial suppres-
sion by faf or lqfmutations, the amplitude of EJPs would be
similar to that in hiw single mutants. Because faf null
mutations reduce Lqf levels (28), it is reasonable to suggest
that Lqf acts downstream of Faf to inhibit synaptic trans-
mission in hiw mutants. Unlike the functional interactions
with hiw, however, faf or lqfmutations do not affect synaptic
overgrowth in hiw mutants [(16); this study]. Differing from
lqf and fafmutations,wndmutations fully suppress synaptic
overgrowth but do not affect synaptic physiology in the hiw
mutant (21). Hence, different ubiquitin pathways can specif-
ically dissociate synapse growth from function.
The physiological stimuli involved in such selective modu-
lation of synapse growth and function remain to be
Figure 10: lqf mutations partially suppress the synaptic
release defect in hiwmutants. A) lqfmutations partially rescues
the EJP amplitude in hiw mutants. The top panel shows the
representative traces of EJPs from control larvae (wt), a lqf
hypomorph (lqfARI/lqfFDD9), hiwND9; lqfARI/lqfFDD9 double mutants
and hiwND9. The bottom panel shows the average amplitude of
EJPs in these genotypes. Note that the EJP amplitude in the hiw
mutant is nearly double by the lqf mutation. The [Ca] was 0.8 mM.
B) Histograms of the average mini amplitude in the above four
genotypes. C) Histograms of the average mini frequency in the
above four genotypes. D) A proposed model of the regulation of
synaptic growth and function by Faf/Lqf- and Hiw-dependent
ubiquitin-proteasome pathways, based on our results and those
of DiAntonio et al. (16, 21, 68). 1). We propose that Lqf acts
downstream of Faf to stimulate synaptic growth and maintain
synaptic transmission. However, there appears to be least one
other substrate (marked X) of Faf that acts synergistically with Lqf.
2). Hiw downregulates the MAPKKK Wnd, which in turn activates
the Jun kinase (JNK) and fos to stimulate synaptic growth by
transcriptional regulation (21). Because wnd neither alters synap-
tic transmission by itself nor suppresses synaptic release defects
in hiwmutants (21), the Hiw pathway appears to regulate synaptic
function and growth by two different mechanisms. 3). Faf, but not
Lqf, converges on the Hiw pathway to regulate Wnd-dependent
synaptic growth. 4). Lqf converges on the Hiw pathway to
negatively regulate transmitter release in the hiw mutant. See
Discussion. Filled arrows represent stimulatory or enhancing
effects. ‘T-stops’ represent inhibitory effects. *p < 0.05; ***p <
0.01. n.s., not significantly different.
Traffic 2008; 9: 2190–2205 2201
Novel Synaptic Roles for Drosophila Epsin 1
identified. Given the conserved role of the UPS in synaptic
plasticity across animal species (4,22,79–83), the findings
reported in this study may have general neurobiological
implications. In particular, we note that the Faf homolog in
mouse, Usp9x or Fam is differentially expressed in differ-
ent regions of the brain (20). Such spatial distribution
patterns may provide a means for Usp9x to locally regulate
synaptic function. Importantly, Usp9x is localized at syn-
apses, where calcium influx rapidly regulates its enzymatic
activity and deubiquitination of epsin 1 (84). Hence, Faf and
Lqf/epsin 1 are good candidate mediators of activity-
dependent synaptic plasticity.
Materials and Methods
Fly strains and geneticsThree alleles of the lqfmutant, lqfARI, lqfAG and lqfFDD9, a Df uncovering the
lqf locus, Df(3L) pbl-X1 (85), and a genomic rescue line (P{wþ, genomic
lqfþ}) were described previously (27). In this study, we generated lqfmutant
larvae in w and w/þ background. To minimize possible effects of genetic
background, we also used w or w/þ as our ‘wild-type’ control animals. The
lqfmutant alleles and the Df were balanced with TM6B, Hu, Tb. lqf alleles in
trans to the Df chromosome were selected as non-Tubby larvae. Post-
synaptic rescue was conducted by crossing w; UAS-lqf; lqfARI/TM6B, Hu,
Tb flies with þ; lqf Df, MHC-Gal4/TM6B, Hu, Tb. Neuronal rescue was
achieved by driving UAS-lqf expression with the pan neuronal driver
ElavC155 Gal4 in the lqfARI/Df background. Genomic rescue was conducted
by introducing one copy of P{wþ, genomic lqfþ} in lqfARI/Df mutants.
EP(3)381 was used for Faf overexpression (16). Other strains used in this
study include hiwND9 (a hypomorphic allele of hiw) (13,68) andMHC-Gal4 (63).
BiochemistryTo determine Lqf protein levels in wild-type control and lqfmutants, at least
five larval brains and ventral nerve cords were dissected in ice-cold PBS
solution and transferred directly to 20–30 mL sample buffers in an
Eppendorf tube. Larval brains and ventral nerve cords were ‘ground’
carefully using a straightened paper clip, spun down and the supernatant
equivalent to one larval brain and ventral nerve cord was loaded on a
SDS–PAGE gel (10–12%), followed by standard western blotting. Blots
were probed with antibodies to Lqf (guinea pig, 1:4000) (28) and a-tubulin
(mouse, 1:4000; Sigma). To determine Lqf levels in hiw flies, adult fly heads
were used instead of larval brains and ventral nerve cords.
Immunocytochemistry and analysisThird instar larvae at wandering stage were dissected as described (52),
fixed with Bouin’s fixative for 15–20 min at room temperature, rinsed with
phosphate buffer plus Tween (PBT), blocked with 2%BSA and stained with
primary antibodies overnight at 48C, washed and incubated with secondary
antibodies (45,47). The primary antibodies included guinea pig anti-Lqf
[1:150; (28)], rabbit anti-Shi [1:300; (50)], goat anti-HRP (1:200; Sigma), goat
anti-HRP conjugated with fluorescein isothiocyanate (FITC) (1:400; Jackson
ImmunoResearch Laboratories), rabbit anti-synaptotagmin I [1:500; (86)],
mouse monoclonal antibody (mAB) 22C10 [1:50; (87); the Developmental
Studies of Hybridoma Bank at the University of Iowa], mAb for Dlg [4F3,
1:50; (88)], mAb nc82 for Bruchpilot [Brp, 1:20; (89)] and rabbit against
glutamate receptor III [GluRIII, 1:500; (90)]. Secondary antibodies included
donkey anti-goat immunoglobulin G (IgG) conjugated with FITC (1:100),
donkey anti-guinea pig IgG conjugated with FITC (1:100) and donkey anti-
rabbit IgG conjugated with tetramethylrhodamine isothiocyanate (TRITC)
(1:100) (Jackson ImmunoResearch Laboratories). Stained preparations
were mounted on standard glass slides with Vectashield medium (Vector
Laboratories) and examined on a fluorescence microscope (Nikon or Zeiss).
The final images were taken on a confocal microscope (Leica 4D TCS).
Unless otherwise noted, all morphological analyses of the NMJ (i.e., bouton
size and number) were conducted on muscles 6/7 or muscle 4 in abdominal
segments 3 and 4. Data from the same segment were averaged and
compared to ensure minimal variations from segment to segment. At least
five different larvae were used for the control ‘wild-type’ group, and
typically, more larvae were used for the mutant groups.
ElectrophysiologyA standard third instar larval body wall preparation was used for electro-
physiological recordings and two-electrode voltage clamp recordings
(45,47,52). The preparation was bathed in HL-3 solution (53). The concen-
tration of calcium contained in the HL-3 solution is specified in the Text
describing the experiments for Figures 2, 3, 6 and 10. For mini recordings,
TTX (1 mm) was added to prevent unwanted evoked release (45). The input
resistance of each muscle was monitored and those with 5 MV or higher
were retained for final data analysis. The input resistance of the recording
microelectrode (backfilled with 3 M KCl) was 20–25 MV. The current
injection electrode (also filled with 3 M KCl) used in voltage clamp experi-
ments had an input resistance of 15–20 MV. Muscle synaptic potentials or
currents were recorded using an Axon Clamp 2B amplifier (Axon Instru-
ments) and acquired by a Dell PC computer equipped with pClamp
software. The MINI ANALYSIS program (Synaptosoft) was used to measure
the amplitude of individual mEJPs or minis. Minis with a slow rise time
arising from neighboring electrically coupled muscle cells were excluded
from analysis (45). The final figures were prepared using ORIGIN (OriginLab)
and PHOTOSHOP (Adobe).
Electron microscopy and analysisThird instar tissues were processed according to standard procedures
(91). Briefly, they were dissected in ice-cold, Ca2þ-free HL-3 saline, fixed
for 1 h in ice-cold 1% acrolein, 2.5% glutaraldehyde in 0.1 M cacodylate
(Cac) buffer, pH 7.2, post-fixed in 0.5% OsO4, 0.8% KFeCn in 0.1 M Cac
for 1 h, incubated in 5% uranyl acetate for 1 h to overnight, dehydrated
and embedded in EmBed 812 araldite. Seventy nanometer sections were
post-stained with uranyl acetate and Reynold’s lead citrate. Boutons
were imaged at 12 K magnification using a JEOL JEM 2000 EX-II TEM
operated at 100 kV. Negatives were scanned at 1500 dpi into a Macintosh
G4 computer using an AGFA Duoscan T2500. Images were adjusted for
brightness, contrast, sharpness and evenness of illumination using
PHOTOSHOP.
To evaluate SV density, a small square box (250 � 250 pixel) was placed
manually at four to five different locations on the electron micrograph of
synaptic boutons. The number of SVs was counted, averaged and
converted into an average number of SVs per square micrometer area
(which is the SV density presented in Figure 4D). The central ‘core’ regions
(Figure 4B,C) were avoided because they often do not have SVs. Vesicle
diameter reported here is the outer diameter.
FM 1-43 uptakeTo measure FM 1-43 dye uptake at the larval NMJ, we adapted the
methods described previously (45,58,92). Briefly, third instar larval prep
was dissected and pinned down on a Sylgard dish, incubated with 5 mmFM
1-43 dye (Invitrogen) for 5 min in Jan’s standard fly saline (52) containing
2 mM Ca2þ and 90 mM KCl. The NMJ preparation was then washed three to
five times with 0 Ca2þ saline and examined on a Zeiss AxioImager
microscope equipped with a �63 water immersion objective (Achroplan,
0.9 NA) and AXIOVISION software (Zeiss Inc.). Four different larvae from each
genotype (wild type and the lqf mutant) and at least three NMJs from each
larva were examined.
StatisticsUnless otherwise specified, data are presented as mean � SEM and
considered significantly different from each other when p value is smaller
than 0.05 in unpaired Student’s t-tests using the ORIGIN software. In
addition, the Kolmogorov–Smirnov test was administrated when comparing
mini sizes between preparations using MINI ANALYSIS program.
2202 Traffic 2008; 9: 2190–2205
Bao et al.
Acknowledgments
We thank Richard Daniels and Mingshan Xue for their initial contributions to
this project, Suzanne Royer for technical assistance with electron micros-
copy, and Erin Overstreet and Janis Fischer for providing the lqf mutant
alleles, UAS-lqf and the genomic rescue lines. We also wish to thank our
colleagues, Mani Ramaswami (University of Arizona) for the Shi antibody
and Brian McCabe (Columbia) and Corey Goodman (University of California
Berkeley/HHMI) for providing the mAb to Dlg and hiw alleles, Aaeron
DiAntonio (Washington University) for the GluRIII antibody, Erich Buchner
(Universitat Wurzburg) for the Bruchpilot nc82 mAb, Wes Thompson
(University of Texas), Randy Hewes (University of Oklahoma), Rudolf Bohm
(OU) and two anonymous reviewers for helpful comments on the manu-
script. This research was supported by a startup fund from OU, in part by
National Science Foundation (NSF) grants (CAREER Award IBN-0093170
and IOS-0822236) and National Institutes of Health (NIH) grant (ES014441)
to B. Z. and in part by NIH grant R01-NS045865 to N. E. R., and H. B. thanks
T. H. Lee Williams, Vice President for Research at OU, for her salary
support.
Supporting Information
Additional Supporting Information may be found in the online version of
this article:
Figure S1: Muscle size is significantly reduced in lqf mutant. Panel A
shows the average muscle size of muscles 6/7 in abdominal segments 3
whereas panel B shows the average muscle size of muscles 6/7 in
abdominal segments 4. In both segments, the lqf mutant muscle size is
significantly reduced compared to that in the wild type. ***p < 0.001.
Figure S2: Immunoreactivity to the active zone protein Bruchpilot
(Brp; panels A and C) and glutamate receptor III (GluRIII; panels B and
D) at the larval NMJ. There are no apparent differences in the level of
these two proteins between the wild type and lqf mutant. The total active
zone number (defined by Brp puncta) on muscle 4 (segment 3) is
significantly reduced in the lqf mutant (panel E). **p < 0.05. However,
the normalized active zone number per synaptic bouton in the lqf mutant is
similar to or slightly higher than that in the wild type (panel F).
Figure S3: Lqf mutations or its deficiency do not have a dominant
effect on evoked synaptic transmission. Top panels show the represen-
tative traces of EJCs, whereas the bottom panels show the average
amplitude of EJCs obtained from wt, lqfARI/þ, lqfARI/Df, Df/þ and lqfþ;
lqfARI/Df (lqf rescue) larvae.
Figure S4: FM 1-43 dye uptake is normal at the lqf mutant
NMJ. Examples of FM 1-43-stained NMJs from muscles 4 and 12 are
shown here for the wild type (panels A and C) and the lqf mutant (panels B
and D).
Figure S5: Synaptic bouton number is not significantly reduced in the
lqf mutant when normalized to the muscle surface area. The average
number of synaptic boutons is significantly reduced on muscles 6/7 in
segment 4 in the lqf mutant (panel A). **p < 0.05. However, the average
number of boutons normalized to the muscle surface area is unaffected by
the lqf mutation (panel B).
Please note: Wiley-Blackwell are not responsible for the content or
functionality of any supporting materials supplied by the authors. Any
queries (other than missing material) should be directed to the correspond-
ing author for the article.
References
1. Pickart CM. Back to the future with ubiquitin. Cell 2004;116:181–190.
2. Yi JJ, Ehlers MD. Emerging roles for ubiquitin and protein degradation
in neuronal function. Pharmacol Rev 2007;59:14–39.
3. DiAntonio A, Hicke L. Ubiquitin-dependent regulation of the synapse.
Annu Rev Neurosci 2004;27:223–246.
4. Wilson SM, Bhattacharyya B, Rachel RA, Coppola V, Tessarollo L,
Householder DB, Fletcher CF, Miller RJ, Copeland NG, Jenkins NA.
Synaptic defects in ataxia mice result from a mutation in Usp14,
encoding a ubiquitin-specific protease. Nat Genet 2002;32:420–425.
5. Speese SD, Trotta N, Rodesch CK, Aravamudan B, Broadie K. The
ubiquitin proteasome system acutely regulates presynaptic protein
turnover and synaptic efficacy. Curr Biol 2003;13:899–910.
6. Burbea M, Dreier L, Dittman JS, Grunwald ME, Kaplan JM. Ubiquitin
and AP180 regulate the abundance of GLR-1 glutamate receptors at
postsynaptic elements in C. elegans. Neuron 2002;35:107–120.
7. EhlersMD. Activity level controls postsynaptic composition and signaling
via the ubiquitin-proteasome system. Nat Neurosci 2003;6:231–242.
8. ColledgeM, Snyder EM, Crozier RA, Soderling JA, Jin Y, Langeberg LK,
Lu H, Bear MF, Scott JD. Ubiquitination regulates PSD-95 degra-
dation and AMPA receptor surface expression. Neuron 2003;40:
595–607.
9. Juo P, Kaplan JM. The anaphase-promoting complex regulates the
abundance of GLR-1 glutamate receptors in the ventral nerve cord of
C. elegans. Curr Biol 2004;14:2057–2062.
10. D‘Souza J, Hendricks M, Le Guyader S, Subburaju S, Grunewald B,
Scholich K, Jesuthasan S. Formation of the retinotectal projection
requires Esrom, an ortholog of PAM (protein associated with Myc).
Development 2005;132:247–256.
11. Watts RJ, Hoopfer ED, Luo L. Axon pruning during Drosophila meta-
morphosis: evidence for local degeneration and requirement of the
ubiquitin-proteasome system. Neuron 2003;38:871–885.
12. Kuo CT, Jan LY, Jan YN. Dendrite-specific remodeling of Drosophila
sensory neurons requiresmatrixmetalloproteases, ubiquitin-proteasome,
and ecdysone signaling. Proc Natl Acad Sci U S A 2005;102:15230–
15235.
13. Wan HI, DiAntonio A, Fetter RD, Bergstrom K, Strauss R, Goodman
CS. Highwire regulates synaptic growth in Drosophila. Neuron 2000;
26:313–329.
14. Schaefer AM, Hadwiger GD, Nonet ML. rpm-1, a conserved neuronal
gene that regulates targeting and synaptogenesis in C. elegans.
Neuron 2000;26:345–356.
15. Zhen M, Huang X, Bamber B, Jin Y. Regulation of presynaptic terminal
organization by C. elegans RPM-1, a putative guanine nucleotide
exchanger with a RING-H2 finger domain. Neuron 2000;26:331–343.
16. DiAntonio A, Haghighi AP, Portman SL, Lee JD, Amaranto AM,
Goodman CS. Ubiquitination-dependent mechanisms regulate synaptic
growth and function. Nature 2001;412:449–452.
17. van Roessel P, Elliott DA, Robinson IM, Prokop A, Brand AH.
Independent regulation of synaptic size and activity by the anaphase-
promoting complex. Cell 2004;119:707–718.
18. Burgess RW, Peterson KA, Johnson MJ, Roix JJ, Welsh IC, O’Brien TP.
Evidence for a conserved function in synapse formation reveals Phr1 as
a candidate gene for respiratory failure in newborn mice. Mol Cell Biol
2004;24:1096–1105.
19. Nakata K, Abrams B, Grill B, Goncharov A, Huang X, Chisholm AD,
Jin Y. Regulation of a DLK-1 and p38 MAP kinase pathway by the
ubiquitin ligase RPM-1 is required for presynaptic development. Cell
2005;120:407–420.
20. Xu J, Taya S, Kaibuchi K, Arnold AP. Spatially and temporally specific
expression in mouse hippocampus of Usp9x, a ubiquitin-specific pro-
tease involved in synaptic development. J Neurosci Res 2005;80:47–55.
Traffic 2008; 9: 2190–2205 2203
Novel Synaptic Roles for Drosophila Epsin 1
21. Collins CA, Wairkar YP, Johnson SL, DiAntonio A. Highwire restrains
synaptic growth by attenuating a MAP kinase signal. Neuron 2006;51:
57–69.
22. Jiang YH, Armstrong D, Albrecht U, Atkins CM, Noebels JL, Eichele G,
Sweatt JD, Beaudet AL. Mutation of the Angelman ubiquitin ligase in
mice causes increased cytoplasmic p53 and deficits of contextual
learning and long-term potentiation. Neuron 1998;21:799–811.
23. Dawson TM, Dawson VL. Molecular pathways of neurodegeneration in
Parkinson’s disease. Science 2003;302:819–822.
24. Bruijn LI, Miller TM, Cleveland DW. Unraveling the mechanisms
involved in motor neuron degeneration in ALS. Annu Rev Neurosci
2004;27:723–749.
25. Petrucelli L, Dawson TM. Mechanism of neurodegenerative disease:
role of the ubiquitin proteasome system. Ann Med 2004;36:315–320.
26. Zhai Q, Wang J, Kim A, Liu Q, Watts R, Hoopfer E, Mitchison T, Luo L,
He Z. Involvement of the ubiquitin-proteasome system in the early
stages of Wallerian degeneration. Neuron 2003;39:217–225.
27. Cadavid AL, Ginzel A, Fischer JA. The function of theDrosophila fat facets
deubiquitinatingenzyme in limitingphotoreceptorcell number is intimately
associated with endocytosis. Development 2000;127:1727–1736.
28. Chen X, Zhang B, Fischer JA. A specific protein substrate for
a deubiquitinating enzyme: Liquid facets is the substrate of Fat facets.
Genes Dev 2004;16:289–294.
29. Chen H, Fre S, Slepnev VI, Capua MR, Takei K, Butler MH, Di Fiore PP,
De Camilli P. Epsin is an EH-domain-binding protein implicated in
clathrin-mediated endocytosis. Nature 1998;394:793–797.
30. De Camilli P, Chen H, Hyman J, Panepucci E, Bateman A, Brunger AT.
The ENTH domain. FEBS Lett 2002;513:11–18.
31. HymanJ,ChenH,DiFiorePP,DeCamilliP,BrungerAT.Epsin1undergoes
nucleocytosolic shuttling and its eps15 interactor NH(2)-terminal homol-
ogy (ENTH) domain, structurally similar to Armadillo and HEAT repeats,
interacts with the transcription factor promyelocytic leukemia Zn(2)þfinger protein (PLZF). J Cell Biol 2000;149:537–546.
32. FordMG,Mills IG, Peter BJ, Vallis Y, PraefckeGJ, Evans PR,McMahonHT.
Curvature of clathrin-coated pits driven by epsin. Nature 2002;419:361–366.
33. Mao Y, Chen J, Maynard JA, Zhang B, Quiocho FA. A novel all helix
fold of the AP180 amino-terminal domain for phosphoinositide
binding and clathrin assembly in synaptic vesicle endocytosis. Cell
2001;104:433–440.
34. Itoh T, Koshiba S, Kigawa T, Kikuchi A, Yokoyama S, Takenawa T. Role
of the ENTH domain in phosphatidylinositol-4,5-bisphosphate binding
and endocytosis. Science 2001;291:1047–1051.
35. Ye W, Lafer EM. Bacterially expressed F1-20/AP-3 assembles clathrin
into cages with a narrow size distribution: implications for the regulation
of quantal size during neurotransmission. J Neurosci Res 1995;41:15–26.
36. Kalthoff C, Alves J, Urbanke C, Knorr R, Ungewickell EJ. Unusual
structural organization of the endocytic proteins AP180 and epsin 1.
J Biol Chem 2002;277:8209–8216.
37. Wendland B, Steece KE, Emr SD. Yeast epsins contain an essential
N-terminal ENTH domain, bind clathrin and are required for endocy-
tosis. EMBO J 1999;18:4383–4393.
38. Shih SC, Katzmann DJ, Schnell JD, SutantoM, Emr SD, Hicke L. Epsins
and Vps27p/Hrs contain ubiquitin-binding domains that function in
receptor endocytosis. Nat Cell Biol 2002;4:389–393.
39. Overstreet E, Chen X,Wendland B, Fischer JA. Either part of a Drosophila
epsin protein, divided after the ENTH domain, functions in endocytosis of
delta in the developing eye. Curr Biol 2003;13:854–860.
40. Overstreet E, Fitch E, Fischer JA. Fat facets and Liquid facets promote
Delta endocytosis and Delta signaling in the signaling cells. Develop-
ment 2004;131:5355–5366.
41. Tian X, Hansen D, Schedl T, Skeath JB. Epsin potentiates Notch
pathway activity in Drosophila and C. elegans. Development 2004;
131:5807–5815.
42. Wang W, Struhl G. Drosophila Epsin mediates a select endocytic
pathway that DSL ligands must enter to activate Notch. Development
2004;131:5367–5380.
43. Wang W, Struhl G. Distinct roles for Mind bomb, Neuralized and Epsin
in mediating DSL endocytosis and signaling in Drosophila. Develop-
ment 2005;132:2883–2894.
44. Wang H, Traub LM, Weixel KM, Hawryluk MJ, Shah N, Edinger RS,
Perry CJ, Kester L, ButterworthMB, Kleyman TR, Frizzell RA, Johnson JP.
Clathrin-mediated endocytosis of ENaC: role of epsin. J Biol Chem 2006;
281:14129–14135.
45. Zhang B, Koh YH, Beckstead RB, Budnik V, Ganetzky B, Bellen HJ.
Synaptic vesicle size and number are regulated by a clathrin adaptor
protein required for endocytosis. Neuron 1998;21:1465–1475.
46. Karunanithi S, Marin L, Wong K, Atwood HL. Quantal size and variation
determined by vesicle size in normal and mutant Drosophila glutama-
tergic synapses. J Neurosci 2002;22:10267–10276.
47. Bao H, Daniels RW, MacLeod GT, Charlton MP, Atwood HL, Zhang B.
AP180 maintains the distribution of synaptic and vesicle proteins in the
nerve terminal and indirectly regulates the efficacy of Ca2þ-triggered
exocytosis. J Neurophysiol 2005;94:1888–1903.
48. Keshishian H, Broadie K, Chiba A, Bate M. The drosophila neuromus-
cular junction: a model system for studying synaptic development and
function. Annu Rev Neurosci 1996;19:545–575.
49. Budnik V, Ruiz-Canada C. The Fly Neuromuscular Junction: Structure
and Function, 2nd edn. San Diego: Elsevier; 2006.
50. Estes PS, Roos J, van der Bliek A, Kelly RB, Krishnan KS, RamaswamiM.
Traffic of dynamin within individual Drosophila synaptic boutons
relative to compartment-specific markers. J Neurosci 1996;16:
5443–5456.
51. Roos J, Kelly RB. The endocytic machinery in nerve terminals
surrounds sites of exocytosis. Curr Biol 1999;9:1411–1414.
52. Jan LY, Jan YN. Properties of the larval neuromuscular junction in
Drosophila melanogaster. J Physiol 1976;262:189–214.
53. Stewart BA, Atwood HL, Renger JJ, Wang J,Wu CF. Improved stability
of Drosophila larval neuromuscular preparations in haemolymph-like
physiological solutions. J Comp Physiol [A] 1994;175:179–191.
54. Delgado R, Maureira C, Oliva C, Kidokoro Y, Labarca P. Size of vesicle
pools, rates of mobilization, and recycling at neuromuscular synapses
of a Drosophila mutant, shibire. Neuron 2000;28:941–953.
55. VerstrekenP, Kjaerulff O, Lloyd TE, Atkinson R, Zhou Y,Meinertzhagen IA,
Bellen HJ. Endophilin mutations block clathrin-mediated endocytosis
but not neurotransmitter release. Cell 2002;109:101–112.
56. Marie B, Sweeney ST, Poskanzer KE, Roos J, Kelly RB, Davis GW.
Dap160/intersectin scaffolds the periactive zone to achieve high-
fidelity endocytosis and normal synaptic growth. Neuron 2004;43:
207–219.
57. Koh TW, Verstreken P, Bellen HJ. Dap160/intersectin acts as a stabi-
lizing scaffold required for synaptic development and vesicle endocy-
tosis. Neuron 2004;43:193–205.
58. Dickman DK, Horne JA, Meinertzhagen IA, Schwarz TL. A slowed
classical pathway rather than kiss-and-run mediates endocytosis at
synapses lacking synaptojanin and endophilin. Cell 2006;123:
521–533.
59. Leventis PA, Chow BM, Stewart BA, Iyengar B, Campos AR, Boulianne
GL. Drosophila Amphiphysin is a post-synaptic protein required for
normal locomotion but not endocytosis. Traffic 2004;2:839–850.
60. Koenig JH, Ikeda K. Disappearance and reformation of synaptic
vesicle membrane upon transmitter release observed under rever-
sible blockage of membrane retrieval. J Neurosci 1989;9:3844–
3860.
61. Jorgensen EM, Hartwieg E, Schuske K, Nonet ML, Jin Y, Horvitz HR.
Defective recycling of synaptic vesicles in synaptotagmin mutants of
Caenorhabditis elegans. Nature 1995;378:196–199.
2204 Traffic 2008; 9: 2190–2205
Bao et al.
62. Rikhy R, Kumar V, Mittal R, Krishnan KS. Endophilin is critically required
for synapse formation and function in Drosophila melanogaster.
J Neurosci 2002;22:7478–7484.
63. Schuster CM, Davis GW, Fetter RD, Goodman CS. Genetic dissection
of structural and functional components of synaptic plasticity. I. Fasciclin
II controls synaptic stabilization and growth. Neuron 1996;17:641–654.
64. Brand AH, Perrimon N. Targeted gene expression as a means of
altering cell fates and generating dominant phenotypes. Development
1993;118:401–415.
65. Torroja L, Packard M, Gorczyca M, White K, Budnik V. The Drosophila
beta-amyloid precursor protein homolog promotes synapse differenti-
ation at the neuromuscular junction. J Neurosci 1999;19:7793–7803.
66. Dickman DK, Lu Z, Meinertzhagen IA, Schwarz TL. Altered synaptic
development and active zone spacing in endocytosis mutants. Curr Biol
2006;16:591–598.
67. Fischer JA, Overstreet E. Fat facets does a Highwire act at the
synapse. Bioessays 2002;24:13–16.
68. Wu C, Wairkar YP, Collins CA, DiAntonio A. Highwire function at the
Drosophila neuromuscular junction: spatial, structural, and temporal
requirements. J Neurosci 2005;25:9557–9566.
69. Huang F, Khvorova A, Marshall W, Sorkin A. Analysis of clathrin-
mediated endocytosis of epidermal growth factor receptor by RNA
interference. J Biol Chem 2004;279:16657–16661.
70. Sigismund S, Woelk T, Puri C, Maspero E, Tacchetti C, Transidico P,
Di Fiore PP, Polo S. Clathrin-independent endocytosis of ubiquitinated
cargos. Proc Natl Acad Sci U S A 2005;102:2760–2765.
71. Chen H, De Camilli P. The association of epsin with ubiquitinated cargo
along the endocytic pathway is negatively regulated by its interaction
with clathrin. Proc Natl Acad Sci U S A 2005;102:2766–2771.
72. Salcini AE, HilliardMA, Croce A, Arbucci S, Luzzi P, Tacchetti C, Daniell L,
De Camilli P, Pelicci PG, Di Fiore PP, Bazzicalupo P. The Eps15 C.
elegans homologue EHS-1 is implicated in synaptic vesicle recycling.
Nat Cell Biol 2001;3:755–760.
73. Majumdar A, Ramagiri S, Rikhy R. Drosophila homologue of Eps15 is es-
sential for synaptic vesicle recycling. Exp Cell Res 2006;312:2288–2298.
74. Koh TW, Korolchuk VI, Wairkar YP, Jiao W, Evergren E, Pan H, Zhou Y,
Venken KJ, Shupliakov O, Robinson IM, O’Kane CJ, Bellen HJ. Eps15
and Dap160 control synaptic vesicle membrane retrieval and synapse
development. J Cell Biol 2007;178:309–322.
75. Davis GW, Schuster CM, Goodman CS. Genetic dissection of structural
and functional components of synaptic plasticity. III. CREB is necessary
for presynaptic functional plasticity. Neuron 1996;17:669–679.
76. Goda Y, Davis GW. Mechanisms of synapse assembly and disassem-
bly. Neuron 2003;40:243–264.
77. Koh YH, Gramates LS, Budnik V. Drosophila larval neuromuscular
junction: molecular components and mechanisms underlying synaptic
plasticity. Microsc Res Tech 2000;49:14–25.
78. Collins CA, DiAntonio A. Synaptic development: insights from Dro-
sophila. Curr Opin Neurobiol 2007;17:35–42.
79. Zhao Y, Hegde AN, Martin KC. The ubiquitin proteasome system
functions as an inhibitory constraint on synaptic strengthening. Curr
Biol 2003;13:887–898.
80. Pak DT, Sheng M. Targeted protein degradation and synapse
remodeling by an inducible protein kinase. Science 2003;302:
1368–1373.
81. Fonseca R, Vabulas RM, Hartl FU, Bonhoeffer T, Nagerl UV. A balance of
protein synthesis and proteasome-dependent degradation determines
the maintenance of LTP. Neuron 2006;52:239–245.
82. Lu Z, Je HS, Young P, Gross J, Lu B, Feng G. Regulation of synaptic
growth and maturation by a synapse-associated E3 ubiquitin ligase at
the neuromuscular junction. J Cell Biol 2007;177:1077–1089.
83. Rezvani K, Teng Y, Shim D, De Biasi M. Nicotine regulates multiple
synaptic proteins by inhibiting proteasomal activity. J Neurosci 2007;
27:10508–10519.
84. Chen H, Polo S, Di Fiore PP, De Camilli PV. Rapid Ca2þ-dependent
decrease of protein ubiquitination at synapses. Proc Natl Acad Sci U S A
2003;100:14908–14913.
85. Hime G, Saint R. Zygotic expression of the pebble locus is required for
cytokinesis during the postblastoderm mitoses of Drosophila. Devel-
opment 1992;114:165–171.
86. Mackler JM, Drummond JA, Loewen CA, Robinson IM, Reist NE. The
C(2)B Ca(2þ)-binding motif of synaptotagmin is required for synaptic
transmission in vivo. Nature 2002;418:340–344.
87. Fujita SC, Zipursky SL, Benzer S, Ferrus A, Shotwell SL. Monoclonal
antibodies against the Drosophila nervous system. Proc Natl Acad Sci
U S A 1982;79:7929–7933.
88. Parnas D, Haghighi AP, Fetter RD, Kim SW, Goodman CS. Regulation of
postsynaptic structure and protein localization by the Rho-type guanine
nucleotide exchange factor dPix. Neuron 2001;32:415–424.
89. Wagh DA, Rasse TM, Asan E, Hofbauer A, Schwenkert I, Durrbeck H,
Buchner S, Dabauvalle MC, Schmidt M, Qin G, Wichmann C, Kittel R,
Sigrist SJ, Buchner E. Bruchpilot, a protein with homology to ELKS/
CAST, is required for structural integrity and function of synaptic active
zones in Drosophila. Neuron 2006;49:833–844. Erratum in: Neuron
2006;51:275.
90. Marrus SB, Portman SL, Allen MJ, Moffat KG, DiAntonio A. Differential
localization of glutamate receptor subunits at the Drosophila neuro-
muscular junction. J Neurosci 2004;24:1406–1415.
91. Reist NE, Buchanan J, Li J, DiAntonio A, Buxton EM, Schwarz TL.
Morphologically docked synaptic vesicles are reduced in synaptotag-
min mutants of Drosophila. J Neurosci 1998;18:7662–7673.
92. Ramaswami M, Krishnan KS, Kelly RB. Intermediates in synaptic
vesicle recycling revealed by optical imaging of Drosophila neuromus-
cular junctions. Neuron 1994;13:363–375.
Traffic 2008; 9: 2190–2205 2205
Novel Synaptic Roles for Drosophila Epsin 1