Skip to main content
Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

A Homolog of FHM2 Is Involved in Modulation of Excitatory Neurotransmission by Serotonin in C. elegans

  • Elena G. Govorunova,

    Affiliation Department of Molecular Pharmacology, Albert Einstein College of Medicine, Bronx, New York, United States of America

  • Mustapha Moussaif,

    Affiliation Department of Molecular Pharmacology, Albert Einstein College of Medicine, Bronx, New York, United States of America

  • Andrey Kullyev,

    Affiliation Department of Molecular Pharmacology, Albert Einstein College of Medicine, Bronx, New York, United States of America

  • Ken C. Q. Nguyen,

    Affiliation Department of Neuroscience, Albert Einstein College of Medicine, Bronx, New York, United States of America

  • Thomas V. McDonald,

    Affiliations Department of Molecular Pharmacology, Albert Einstein College of Medicine, Bronx, New York, United States of America, Department of Medicine, Albert Einstein College of Medicine, Bronx, New York, United States of America

  • David H. Hall,

    Affiliation Department of Neuroscience, Albert Einstein College of Medicine, Bronx, New York, United States of America

  • Ji Y. Sze

    Affiliation Department of Molecular Pharmacology, Albert Einstein College of Medicine, Bronx, New York, United States of America


The C. elegans eat-6 gene encodes a Na+, K+-ATPase α subunit and is a homolog of the familial hemiplegic migraine candidate gene FHM2. Migraine is the most common neurological disorder linked to serotonergic dysfunction. We sought to study the pathophysiological mechanisms of migraine and their relation to serotonin (5-HT) signaling using C. elegans as a genetic model. In C. elegans, exogenous 5-HT inhibits paralysis induced by the acetylcholinesterase inhibitor aldicarb. We found that the eat-6(ad467) mutation or RNAi of eat-6 increases aldicarb sensitivity and causes complete resistance to 5-HT treatment, indicating that EAT-6 is a component of the pathway that couples 5-HT signaling and ACh neurotransmission. While a postsynaptic role of EAT-6 at the bodywall NMJs has been well established, we found that EAT-6 may in addition regulate presynaptic ACh neurotransmission. We show that eat-6 is expressed in ventral cord ACh motor neurons, and that cell-specific RNAi of eat-6 in the ACh neurons leads to hypersensitivity to aldicarb. Electron microscopy showed an increased number of synaptic vesicles in the ACh neurons in the eat-6(ad467) mutant. Genetic analyses suggest that EAT-6 interacts with EGL-30 Gαq, EGL-8 phospholipase C and SLO-1 BK channel signaling to modulate ACh neurotransmission and that either reduced or excessive EAT-6 function may lead to increased ACh neurotransmission. Study of the interaction between eat-6 and 5-HT receptors revealed both stimulatory and inhibitory 5-HT inputs to the NMJs. We show that the inhibitory and stimulatory 5-HT signals arise from distinct 5-HT neurons. The role of eat-6 in modulation of excitatory neurotransmission by 5-HT may provide a genetic explanation for the therapeutic effects of the drugs targeting 5-HT receptors in the treatment of migraine patients.


Serotonin (5-hydroxytryptamine, 5-HT) functions as a neuromodulator by inhibiting and enhancing synaptic transmission of other neurotransmitters. Dysregulation of 5-HT signaling has been implicated in pathophysiology of many disorders, including migraine [1]. Migraine is a polygenic trait. Familial hemiplegic migraine (FHM) is a rare autosomal dominant subtype of migraine associated with genetic lesions in three genes, FHM1 encoding the α1 subunit of the voltage-gated Ca2+ channel CACNA1A, FHM2 encoding the α2 subunit of the Na+,K+-ATPase ATP1A2, and FHM3 encoding the α1 subunit of the voltage-gated Na+ channel SCN1A [2]. According to the current view, mutations in these genes result in excessive excitatory neurotransmission in the brain leading to migraine pain [3]. However, verification of this hypothesis, as well as analysis of the relationship between migraine and 5-HT signaling is difficult due to the complexity of mammalian nervous systems. The nematode C. elegans is an attractive genetic model to study neuronal functions in vivo. The first two FHM genes are conserved in this organism and are designated as unc-2 and eat-6, respectively. Analysis of unc-2 mutants has been undertaken for modeling of FHM1 migraine channelopathy [4]. In this study, we focused on the FHM2 homolog eat-6 to gain new insights into biochemical and physiological mechanisms of migraine pathology.

The Na+,K+-ATPase is a sodium pump that uses energy derived from ATP hydrolysis to extrude cytoplasmic Na+ in exchange for extracellular K+ across the plasma membrane [5]. In human there are four genes encoding Na+,K+-ATPase α subunits [6]. The α1 isoform is the ubiquitous housekeeping enzyme. FHM2 is the α2 isoform, which together with the α3 isoform is enriched in neuronal and muscular systems, and the α4 isoform is confined to testis. In the adult brain α2 is mostly expressed in glia; besides, it is present in skeletal muscle, heart and other tissues. The C. elegans genome harbors four other Na+,K+-ATPase α subunit genes besides eat-6 [7]. EAT-6 appears to be the closest functional homolog of FHM2, as no other α subunit genes are expressed in excitable cells [8]. EAT-6 and FHM2 share 72% identity, 84% homology at the protein level. A homozygous eat-6 deletion mutant is reported to be embryonic lethal/early larval arrest ( Four other eat-6 mutations were initially isolated for feeble contractions and delayed relaxations of the pharyngeal muscles [9], and subsequently shown to affect the membrane potential of these cells [10]. A recent study demonstrated that eat-6 is localized at the NMJs in the bodywall muscles and regulates synaptic efficacy [8]. Taken together, these studies convinced us that further research into eat-6 function in C. elegans might provide a deeper insight into the mechanisms of migraine in humans.

Here we provide evidence that eat-6 may also act in locomotory cholinergic neurons, and that mutations in eat-6 disrupt inhibitory 5-HT input to the control of excitatory synaptic transmission at C. elegans bodywall NMJs.


Molecular lesions of eat-6 alleles

Sequencing of mutant genomic DNA confirmed that ad467, ad601 and ad997 alleles are missense mutations leading to the following amino acid substitutions in the EAT-6 protein: L359F, G522E and S761F, respectively [11]. In addition, we identified that the ad792 allele carries a missense mutation that results in the R569H substitution. All four eat-6 mutations substitute amino acid residues that are conserved in human FHM2. Three out of four mutated residues are in the intracellular 4–5 loop (Figure 1), which contains the nucleotide-binding domain and the phosphorylation site essential for the enzymatic activity [5], [12]. The majority of mutations found in human migraine patients are also located in this region [13]. The sites of the ad467 and ad601 mutations are very close to the sites of pathological human mutations, and the ad792 mutation substitutes the same residue as the FHM2(R593W) mutation [14].

Figure 1. Predicted topology of EAT-6/FHM2 and location of mutations.

A schematic depiction of the human FHM2 protein generated by the TOPO2 program ( The sites of mutations found in migraine patients [13] are shown by black circles. Corresponding residues of eat-6 mutations are shown by black triangles.

eat-6(ad467) mutant is hypersensitive to aldicarb and does not respond to 5-HT

Aldicarb, an inhibitor of acetylcholinesterase, causes paralysis in C. elegans due to accumulation of acetylcholine (ACh) at the locomotory NMJs, and is therefore frequently used to measure the steady state ACh release in living C. elegans animals [15], [16]. In WT animals exogenous 5-HT slowed down the paralytic effect of aldicarb (Figure 2a). By contrast, 5-HT treatments did not reduce the sensitivity to paralysis induced by levamisole, a specific agonist of the nicotinic ACh receptor UNC-29 in the bodywall muscles (data not shown) [17]. These results suggest that 5-HT signaling inhibits ACh release by the motor neurons [17]. Out of four tested eat-6 alleles, the ad467 mutant showed the strongest defects in the function of the pharyngeal muscles [10]; we found that ad467 animals were hypersensitive to aldicarb and completely resistant to 5-HT treatment (Figure 2b,c). The ad997 and ad792 mutations that modestly disrupted the function of the pharyngeal muscles [10] did not cause significant hypersensitivity to aldicarb, although the ad997 mutation reduced the response to 5-HT treatment (Figure 2c). Interestingly, the ad601 mutation that least affected the function of the pharyngeal muscles [10] caused the strongest hypersensitivity to aldicarb (Figure 2c) [8].

Figure 2. eat-6(ad467) is hypersensitive to aldicarb and resistant to 5-HT.

(a) and (b) The time course of aldicarb-induced paralysis of animals pretreated with 5 mg/ml 5-HT (black circles) and without 5-HT treatment (open squares) in wild type (a) and eat-6(ad467) animals (b). The error bars indicate SEM (n>3 replicates). T50 is the time course when 50% of the worms were paralyzed. We use reciprocal T50 values as a measurement for the rate of paralysis. (c) Relative reciprocal T50 values of aldicarb-induced paralysis of worms pretreated with 5-HT (hatched bars) and those without 5-HT treatment (black bars). The values of 5-HT-treated WT worms and mutants are normalized to that of WT worms without 5-HT treatment. The error bars indicate SEM (n>3 replicates). ad467 and ad601 were hypersensitive to aldicarb compared to WT (* p<0.05, ** p<0.001). 5-HT treatment significantly reduced the rate of aldicarb-induced paralysis in WT and ad792 animals, compared to their untreated siblings (p<0.0005), whereas no significant reduction by 5-HT treatment was found in the ad467, ad601 and ad997 alleles. Student's t-test. (d) Influence of 5-HT on egg laying in eat-6 mutant alleles. The bars show the number of eggs in the uterus (black bars), and the number of eggs laid per h per animal incubated in M9 buffer (open bars) and in M9 buffer supplemented with 5 mg/ml 5-HT (hatched bars). C. elegans generally does not lay eggs in M9 [18]. The error bars indicate SEM (n>3 replicates, 8 animals of each genotype for each condition per trial).

To further characterize the effect of eat-6 mutations on sensitivity to 5-HT, we tested the egg-laying response of the mutants to 5-HT treatment. In WT animals, exogenous 5-HT stimulated egg laying (Figure 2d) [18]. The ad467 mutant laid practically no eggs in response to 5-HT, whereas all the other three eat-6 alleles laid some (Figure 2d, hatched bars). To exclude the possibility that the failure of ad467 animals to lay eggs in response to 5-HT was simply due to a reduced number of fertilized eggs, we counted the number of eggs in the uterus of one-day old adult hermaphrodite worms. Although all four eat-6 alleles had reduced number of eggs in the uterus, ad467 worms carried at least as many fertilized eggs as ad792 and ad997 mutants (Figure 2d, black bars). Therefore, we concluded that the eat-6(ad467) mutation disrupts 5-HT regulation in the egg-laying circuit as well as 5-HT-induced modulation of ACh neurotransmission at the bodywall NMJs. The differential effects of the eat-6 mutations on the function of the pharyngeal muscles [10], the sensitivity to aldicarb and the responses to 5-HT suggest allele-specific modification of EAT-6 function in particular cellular mechanisms, rather than a simple reduction of its activity.

Both reduction and excess of EAT-6 protein cause hypersensitivity to aldicarb and resistance to 5-HT

To further investigate the relationship between EAT-6 function and phenotypes seen in eat-6 mutants, we used RNA interference (RNAi) to knock down eat-6 gene activity. The strain rrf-3(pk1426) has enhanced neuronal sensitivity to RNAi [19]. The rrf-3 worms fed with E. coli expressing dsRNA targeted to eat-6, but not the empty vector (mock RNAi), showed abnormalities similar to, but stronger than those seen in the eat-6 mutants. They had a smaller body size, a reduced number of eggs in the uterus, hypersensitivity to aldicarb and resistance to 5-HT (data not shown; Figure 3a), indicating that a reduction of EAT-6 function brings about all these phenotypes.

Figure 3. Phenotypic analysis of eat-6 RNAi and overexpression.

(a) Relative reciprocal T50 values of aldicarb-induced paralysis of animals untreated (black bars) or pretreated with 5-HT (hatched bars). The error bars indicate SEM (n>3 replicates). Both RNAi and overexpression of eat-6 conferred hypersensitivity to aldicarb compared to WT (* p<0.05, ** p<0.01). Pretreatment of 5-HT reduced aldicarb sensitivity in WT animals (p<0.005), but not in eat-6 RNAi animals. Student's t-test. (b) The ratio of the amplitude of the excitation and recovery peaks (black bars, left axis), and the fraction of EPSPs that failed to trigger APs (hatched bars, right axis). The error bars indicate SEM (n = 15). (c–h) Representative EPG recordings. EPSP designates an excitatory postsynaptic potential, E designates the peak corresponding to the muscle excitation (depolarization), R designates the peak corresponding to muscle recovery.

We next sought to rescue eat-6 mutant phenotypes by a WT eat-6 transgene, Ex[eat-6(+)]. As it has been shown previously [10], this transgene rescued the pharyngeal defects of the ad467 mutant (Figure 3b,e). However, we found that the same transgenic animals remained hypersensitive to aldicarb and resistant to 5-HT (Figure 3a). One possible reason for this could be less efficient expression of the eat-6 transgene in the locomotory system. But, when we crossed this transgene into WT background, we observed an increased sensitivity to aldicarb in the transgenic animals compared to WT animals (Figure 3a). This result suggests that overexpression of eat-6 may also perturb ACh synaptic transmission at the locomotory NMJs.

Extrachromosomal arrays usually carry multiple copies of the transgene, so to test whether the aldicarb hypersensitivity of the eat-6 mutant can be corrected by a single copy of the WT gene, we took advantage of the nT1 genetic balancer, in which part of the chromosome V carrying the eat-6 locus is translocated to the chromosome IV [20]. The homozygous eat(ad467) mutant carrying a single copy of the nT1 balancer contains two copies of the eat-6(ad467) mutant gene and one copy of the WT eat-6 gene from the balancer; these animals showed significantly reduced aldicarb hypersensitivity, compared to the eat(ad467) mutant without the balancer (Figure S1). This result is consistent with the idea that eat-6(ad467) is a reduction-of-function mutation [10] and suggests that a low dosage of the WT gene, in contrast to a high dosage introduced by an extrachromosomal array, can correct aldicarb sensitivity of the ad467 mutant.

We also characterized pharyngeal electrical activity in animals with excess or reduced EAT-6. In contrast to the effect on aldicarb sensitivity, expression of Ex[eat-6(+)] in WT background did not change EPG (Figure 3b,f), which again points to distinctive functions of EAT-6 in the pharyngeal and locomotory circuits. Furthermore, eat-6 RNAi altered EPG differently from that seen in eat-6 mutants. In WT and mock-treated rrf-3 control animals almost every excitatory postsynaptic potential (EPSP) triggered an action potential (AP) in the pharyngeal muscles (Figure 3b,c,h) [21]. Even the strong eat-6(ad467) mutation did not change the probability of AP generation, but reduced the rate of AP decay, which corresponds to a reduced amplitude of the recovery (R) peak in EPG (Figure 3b,d) [10]. In contrast, in eat-6 RNAi worms about 50% of EPSPs failed to elicit APs in the pharyngeal muscles (Figure 3b,g). When APs were generated in eat-6 RNAi worms, their R peaks were not reduced (Figure 3b,g). In fact, the mean relative amplitude of the R peak in the eat-6 RNAi animals was even larger than that in WT and mock-treated control (Figure 3b). Outside of the pharynx, some effects of eat-6 mutations and eat-6 RNAi also differ. For example, the mutant worms showed no apparent motility defects [10], whereas RNAi animals were severely uncoordinated. These observations suggest that the phenotypes caused by the ad467 mutation reflect allelic-specific defects. It is possible that the mutation alters specific enzyme properties, such as affinities for K+ and Na+ or voltage dependence, as shown for several mutations in mammalian homologs of eat-6 [22], [23]. However, it remains possible that some differences between the phenotypes of ad467 worms and that of RNAi-treated animals are due to resistance of some neurons to RNAi even in the rrf-3 background.

Cell-specific RNAi of eat-6 in ACh neurons causes hypersensitivity to aldicarb

As the first step to determine cellular sites of EAT-6 function in ACh signaling, we constructed a GFP reporter under the control of the eat-6 promoter (peat-6::gfp) and generated multiple transgenic lines from independent injections of this construct. Like that of many other GFP reporters, the expression of peat-6::gfp was mosaic, but was consistent in terms of cell types in at least three lines that were carefully examined in several generations. In agreement with a previous study [8], we observed GFP fluorescence in the pharyngeal, bodywall and vulval muscles. In addition, we found eat-6 expression in many neurons, including the ventral cord ACh neurons, as well as in several head and tail neurons (Figure 4). This expression pattern raised the possibility that eat-6 may regulate neurotransmission both pre- and postsynaptically.

Figure 4. eat-6 is expressed in muscles and neurons.

(a) Photomicrographs of animals expressing GFP driven by the eat-6 promoter. (b) Top, a photomicrograph of GFP driven by the eat-6 promoter; middle, a photomicrograph of mCherry driven by the unc-17 promoter; and bottom, merge of the top and middle images.

EAT-6 function at the postsynaptic site of ACh neurotransmission at the bodywall NMJs has been reported by others [8]. In agreement with the report [8], we observed that eat-6(ad467) mutant animals were hypersensitive to paralysis induced by levamisole, a specific agonist of the nicotinic ACh receptor UNC-29 (Figure 5a). Furthermore, like the Ex[eat-6(+)] transgene, a transgene expressing the WT eat-6 cDNA under the bodywall muscle-specific myo-3 promoter (Muscle::eat-6) also caused strong hypersensitivity to levamisole in the WT background (Figure 5). This result was unexpected, as Doi and Iwasaki reported successful rescue of the levamisole hypersensitivity of the eat-6(ad467) and eat-6(ad601) mutants by expressing eat-6 in the muscles [8]. While the reason for the difference is not clear, one possible explanation could be dosage differences of eat-6 in the transgenic arrays.

Figure 5. eat-6 in both muscles and neurons regulates synaptic transmission.

Synaptic transmission was assayed by scoring paralysis induced by levamisole (a) or aldicarb (b) at concentrations indicated in each panel. The relative reciprocal T50 values were calculated as described in Figure 2a. The error bars indicate SEM (n>3 replicates). * p<0.05, ** p<0.001, compared to WT. Student's t-test.

We went on to test whether eat-6 also functions in the ACh neurons to regulate neurotransmission. We knocked down eat-6 expression in the ACh neurons using cell-specific RNAi [24]. Both transgenic lines in which eat-6 was silenced in the ACh neurons were hypersensitive to aldicarb, but not to levamisole (Figure 5a,b). These results suggest that, in addition to its role in the bodywall muscles, EAT-6 in the ACh neurons may also influence ACh neurotransmission.

Next, we expressed the eat-6 cDNA under the control of the promoter of the vesicular ACh transporter gene unc-17 (ACh::eat-6). Like Ex[eat-6(+)] and Muscle::eat-6, ACh::eat-6 did not correct aldicarb hypersensitivity or 5-HT resistance in eat-6 mutant animals (Figure S2). However, four transgenic lines expressing ACh::eat-6 in the WT background all showed strong hypersensitivity to aldicarb, but not to levamisole (Figure 5a,b). The unc-17(e245) mutant significantly reduces ACh release, and therefore is resistant to aldicarb-induced paralysis [25], [26]. When the ACh::eat-6 transgene was crossed into the unc-17(e245) background, the transgenic animals became completely resistant to aldicarb (Figure S3). These results are consistent with the model that EAT-6 functions in both the bodywall muscles and the ACh neurons, and that either increased or decreased EAT-6 function may perturb ACh neurotransmission. However, since we were unable to rescue the aldicarb hypersensitivity of the eat-6 mutants by expressing EAT-6 in the ACh neurons, other experiments are necessary to determine the mechanisms by which EAT-6 regulates presynaptic neurotransmission.

The synaptic architecture of the eat-6(ad467) mutant

To probe for a possible role of eat-6 in synaptic architecture we examined the expression and localization of GFP-tagged post- and presynaptic markers in eat-6(ad467) animals. We found that UNC-29::GFP fluorescence at the bodywall NMJs was slightly increased in the ad467 animals relative to WT (Figure S4), although this difference was not statistically significant. This result is in agreement with a published study [8].

We also examined fluorescence of the GFP-tagged synaptic vesicle marker synaptobrevin snb-1 expressed in a subset of the cholinergic motor neurons under the unc-4 promoter [27]. No significant difference in SNB-1::GFP fluorescence was found between ad467 and WT worms (data not shown), which is again consistent with the previous report [8]. These results indicate that the eat-6(ad467) mutation does not cause any gross defect in morphology of the NMJs.

To test whether hypersensitivity to aldicarb in the eat-6(ad467) mutant is resulted from alterations in synaptic vesicle formation or distribution, we carried out ultrastructural analysis of the ACh synapses by transmission electron microscopy (TEM). We found that the mean number of vesicles per synaptic profile was greater in the mutant relative to WT (Figure 6c). In C. elegans, the nerve processes in the nerve ring and along the ventral cord show large variations in axon diameter in correlation with vesicle content at synapses. The axon plasma membrane at a synaptic site is molded tightly around vesicle clusters, so the more vesicles, the larger the axon caliber [28], [29] (Hall, unpublished). Indeed, the mean area of the axon profile at ACh synapses in eat-6 mutant animals is significantly larger than that in WT (Figure 6d). This result suggests that EAT-6 might play a role in regulation of the abundance of synaptic vesicles at the NMJs. The reason for the discrepancy between an increased number of synaptic vesicles revealed by EM analyses and the insignificant change in GFP-tagged synaptobrevin by fluorescence microscopy is not clear at present. One possibility could be that subtle changes in intensity of the GFP reporters may not be discernible with our experimental setting. Another attractive hypothesis would be less synaptobrevin per synaptic vesicle in eat-6 mutants.

Figure 6. The eat-6(ad467) mutant accumulates more synaptic vesicles at ACh NMJs.

(a) and (b) Representative synaptic profiles of WT and ad467 mutant worms obtained by high-pressure freezing EM. Arrows point to the active zone. (c) The average number of synaptic vesicles per profile and SEM, * p<0.005. (d) The average area of the synaptic profile and SEM. ** p<0.001. The data were collected from 24 and 23 synaptic profiles, respectively, in WT and ad467 worms. Four animals per each genotype were analyzed. Student's t-test.

EAT-6 acts upstream of EGL-30 Gαq in a genetic pathway

To gain more insights into molecular mechanisms by which EAT-6 regulates synaptic transmission, we have sought for mutations in other genes that might block aldicarb hypersensitivity in the eat-6(ad467) mutant. Gαq EGL-30 promotes production of diacylglycerol (DAG), which facilitates ACh release from the ventral cord motor neurons [30], [31]. The egl-30(ad806) loss-of-function mutant animals are resistant to aldicarb [32]. We found that egl-30(ad806) eliminated aldicarb hypersensitivity of ad467 (Figure 7a). The egl-8 phospholipase Cβ is a downstream target of egl-30 in the presynaptic pathway, and egl-8 loss-of-function mutants show phenotypes similar, albeit weaker, to those of egl-30 mutants [32], [33]. The egl-8(n488)lf mutation also suppressed hypersensitivity of the eat-6 mutant to aldicarb (Figure 7a). These results suggest that eat-6 acts upstream of egl-30 in the genetic pathway. egl-30 expression has been shown in neurons, pharyngeal and vulval muscles, but not in the bodywall muscles [34]. Interestingly, the egl-30;eat-6 and egl-8;eat-6 double mutants remained hypersensitive to levamisole (Figure S5).

Figure 7. Genetic interaction between eat-6 and egl-30, egl-8 and slo-1.

Relative reciprocal T50 values of paralysis induced by aldicarb. The error bars indicate SEM (n>3 replicates). * p<0.05, ** p<0.005, compared to WT. The p value between two tested groups is indicated on the top of the bars. In (a) the difference between egl-30(ad806) and ad467;ad806 is significant (p<0.5). Student's t test.

There are no predicted voltage-gated Na+ channels in the C. elegans genome [35], and no Na+ APs are generated in C. elegans neurons [36]. Nevertheless, EAT-6 Na+,K+-ATPase may influence neurotransmitter release from the motor neurons by changing the resting membrane potential, and/or by influencing the activity of other ion channels or transporters. To explore a possible role of EAT-6 in this process, we analyzed the interaction between EAT-6 and SLO-1. SLO-1 is a large-conductance, Ca2+-activated K+ channel that acts presynaptically to repolarize active neurons, leading to closure of the voltage-gated Ca2+ channels and thus terminating neurotransmitter release [37]. Loss of slo-1 function causes prolonged ACh release and hypersensitivity to aldicarb [37]. Conversely, worms carrying the slo-1(ky399) gain-of-function mutation are resistant to aldicarb [38], presumably because of a shortened duration of ACh synaptic release. When we crossed the ad467 mutation into the slo-1(ky399) background, the double mutant remained as hypersensitive to aldicarb as the single eat-6(ad467) mutant (Figure 7b), in contrast to the eat-6(ad467);egl-30(ad806) double mutant that became resistant (Fig. 7a). This result suggests that EAT-6 activity is required for the gain-of-function effect of slo-1(ky399).

Although overexpression of eat-6 in the WT background caused hypersensitivity to aldicarb as did the ad467 mutation (Figure 3a), the slo-1(ky399);Ex[eat-6(+)] transgenic animals exhibited aldicarb sensitivity similar to that of WT animals (Figure 7b), suggesting that an excess of EAT-6 can compensate for or offset the effect of the ky399 mutation. Similarly, the ky399 mutation also suppressed aldicarb hypersensitivity induced by ACh::eat-6 (Figure 7b). Therefore, although both reduction and excess of EAT-6 function cause hypersensitivity to aldicarb, their mechanisms differ.

Exogenous 5-HT acts via egl-30, tom-1 and slo-1

Exogenous 5-HT inhibits the paralytic effects of aldicarb but does not affect the sensitivity to levamisole (data not shown) [17], suggesting that 5-HT regulates presynaptic ACh release. The resistance to 5-HT treatment observed in ad467 and eat-6 RNAi animals (Figures 2 and 3) could reflect a specific role of EAT-6 in 5-HT signaling or a general phenotype of aberrant synaptic transmission. To discriminate between these possibilities, we analyzed the effects of 5-HT on aldicarb-induced paralysis in mutants defective in different aspects of ACh neurotransmission. It has been reported that worms carrying egl-30 loss- or gain-of-function mutations showed opposite egg-laying phenotypes, but were both resistant to stimulation of egg laying by 5-HT treatment [30]. Similarly, we found that although loss- and gain-of-function egl-30 mutants were, respectively, resistant and hypersensitive to aldicarb [32], they were both insensitive to 5-HT treatment (Figure 8). Since aldicarb hypersensitivity of eat-6(ad467) worms was suppressed by egl-30(ad806), but not by slo-1(ky399), we tested whether 5-HT can modify aldicarb sensitivity in slo-1 mutants. We found that both loss- and gain- of-function slo-1 mutants were resistant to 5-HT treatment (Figure 8). Furthermore, mutants of the syntaxin-binding protein TOM-1, which regulates synaptic vesicle priming [39], were also resistant to 5-HT treatment (Figure 8). We conclude that mutations that disrupt regulated neurotransmitter release by either enhancing or attenuating it may compromise the effects of 5-HT treatment. Interestingly, WT animals expressing Ex[eat-6(+)] remained partially responsive to 5-HT treatment (Figure 3a), indicating that excessive amounts of normal EAT-6 protein does not disrupt 5-HT signaling. These results support the notion that 5-HT acts via presynaptic mechanisms to modulate synaptic transmission [17], and suggest that EAT-6 is a component in the pathway regulated by 5-HT.

Figure 8. Mutants of egl-30, tom-1 and slo-1 are insensitive to 5-HT treatment.

Relative reciprocal T50 values and SEM of aldicarb-induced paralysis of worms pretreated with 5-HT (hatched bars) and that without 5-HT treatment. The values of 5-HT-treated WT worms and mutants are normalized to that of WT worms without 5-HT treatment. n>3 replicates. None of the tested mutants showed significant difference between 5-HT-treated and untreated worms, Student's t test.

Deletion of the G protein-coupled 5-HT receptor SER-4 suppresses aldicarb hypersensitivity of eat-6 mutants

The C. elegans genome encodes one ionotropic 5-HT receptor and seven predicted G protein-coupled 5-HT receptors [40]. To identify receptors responsible for modulation of ACh neurotransmission by exogenous 5-HT, we analyzed available deletion mutants of these genes by the aldicarb assay. The sensitivity to aldicarb itself was not significantly changed in any of the tested 5-HT receptor mutants compared to that of WT (Figure 9a,c). However, the functional null allele ser-4(ok512) [41] was completely resistant to 5-HT treatment (Figure 9a). Transgenic expression of WT ser-4 gene rescued 5-HT sensitivity of the ser-4(ok512) mutant (Figure 9a), indicating that SER-4 function is required for exogenous 5-HT to downregulate ACh neurotransmission. To determine whether SER-4 acts in the ACh neurons, we generated transgenic animals expressing ser-4 cDNA specifically in these neurons (ACh::ser-4) in the ok512 background. The 5-HT response in such animals was fully restored (Figure 9a). Deletion mutants of ser-1, ser-5, ser-7 and mod-1 also showed reduced sensitivity to 5-HT treatment (Figure 9c), suggesting that multiple 5-HT receptors are at work at the NMJs.

Figure 9. Role of 5-HT receptors in response to exogenous 5-HT.

(a) The response to 5-HT treatment of ser-4 mutants and the mutants expressing a WT ser-4 transgene. Aldicarb-induced paralysis of worms pretreated with 5-HT (hatched bars) and those without 5-HT treatment (black bars) were scored by calculating the percentage of worms paralyzed after 60 min of exposure to aldicarb. The error bars indicate SEM (n>3 replicates). Noticeably, the aldicarb sensitivity of ok512;Ex[ser-4(+)] #1 worms without 5-HT treatment is significantly (p<0.05) higher than that of WT. (b) Mutations in ser-4 and tph-1 suppress aldicarb hypersensitivity of eat-6 mutant worms. Aldicarb-induced paralysis was scored after 100 min of exposure to the drug. The error bars indicate SEM (n>3 replicates). (c) The response to 5-HT treatment of mutants of other 5-HT receptors. Aldicarb-induced paralysis of worms pretreated with 5-HT (hatched bars) and that without 5-HT treatment was scored by calculating the percentage of worms paralyzed after 60 min of exposure to the drug. The error bars indicate SEM (n>3 replicates). The values of 5-HT-treated WT worms and mutants are normalized to that of WT worms without 5-HT treatment. Student's t-test.

To elucidate the relationship between 5-HT signaling and EAT-6, we generated an eat-6(ad467);ser-4(ok512) double mutant. Surprisingly, although the ser-4(ok512) mutant itself showed WT sensitivity to aldicarb, the ser-4 mutation significantly suppressed aldicarb hypersensitivity of the eat-6(ad467) mutant (Figure 9b; Figure S6). Likewise, null mutants of the tryptophan hydroxylase gene tph-1 that cannot biosynthesize serotonin [42] showed WT sensitivity to aldicarb, but the tph-1 mutation significantly attenuated aldicarb hypersensitivity of the eat-6(ad467) mutant (Figure 9b). These results indicate that there is indeed a genetic interaction between eat-6 and endogenous 5-HT signaling.

Specific serotonergic neurons are responsible for stimulatory and inhibitory 5-HT inputs

Suppression of aldicarb hypersensitivity of the eat-6(ad467) mutant by the ser-4 mutation raises a possibility for a stimulatory 5-HT input to ACh neurotransmission. Genetic analysis of C. elegans has demonstrated that distinct serotonergic neurons regulate specific aspects of behavior [43] and that multiple 5-HT receptors may exert opposite effects on the same behavior [44]. To understand how serotonergic neurons regulate ACh neurotransmission, we analyzed the role of 5-HT signal from specific neurons. In C. elegans hermaphrodites, 5-HT is primarily produced in the ADF chemosensory neurons, the NSM secretory neurons in the head region, and the HSN motor neurons responsible for egg laying [42], [45]. In addition, the single RIH neuron and a pair of the AIM interneurons can absorb extracellular 5-HT via the serotonin reuptake transporter (SERT) MOD-5, but cannot synthesize it (Kullyev et al., unpublished).

To test for contributions of specific serotonergic neurons in modulation of neurotransmission, we expressed tph-1 cDNA either in the ADF neurons or the NSM neurons in a tph-1 null background. To prevent neurons from absorbing extracellular 5-HT, we introduced individual neuron-specific tph-1 transgenes into the tph-1;mod-5 double mutant. We confirmed the presence of 5-HT in specific neurons by staining the transgenic animals with anti-5-HT antibodies (data not shown). When the tph-1 transgene was expressed in the ADF neurons in the tph-1;mod-5 background, the worms became strongly hypersensitive to aldicarb (Figure 10). Conversely, when 5-HT was excluded from the ADF neurons, but present in the other neuronal classes, the worms were slightly resistant to aldicarb, as compared to WT (Figure 10). A similar degree of resistance was also observed in the TRPV channel ocr-2 mutants, which has reduced 5-HT specifically in the ADF neurons [46]. These results indicate that endogenous 5-HT released from the ADF neurons stimulates ACh synaptic transmission at the NMJs, whereas 5-HT from the NSM/RIH/AIM neurons inhibits the stimulatory 5-HT inputs.

Figure 10. 5-HT from the ADF and the NSM/RIH/AIM neurons antagonistically regulates ACh neurotransmission.

Relative reciprocal T50 values of aldicarb-induced paralysis of worms expressing the tph-1 gene in specific neurons. The error bars indicate SEM (n>3 replicates). * p<0.05, ** p<0.005, compared to WT by Student's t-test. The presence or absence of 5-HT in specific neurons is designated by “+” or “-”, respectively.


FHM was the first human disease linked to mutations in a specific subunit of Na+,K+-ATPase [47]. Later it became evident that the same α2 subunit is associated with a much broader spectrum of pathologies, including other forms of migraine, epilepsy and ataxia [48]. In addition, mutations in the α3 subunit have been found in patients suffering from rapid-onset dystonia Parkinsonism [49]. Finally, genetic variations in all three subunits of Na+,K+-ATPase expressed in brain have been linked to bipolar disorders [50]. Cellular and molecular mechanisms by which specific mutations cause disease phenotypes remain poorly understood. In this study, we showed that EAT-6, a C. elegans homolog of human FHM2, controls excitatory synaptic transmission and its modulation by 5-HT, both of which are altered in migraine patients.

Both reduction and excess of EAT-6 Na+,K+-ATPase alter synaptic transmission

There is an ongoing debate in the literature on whether FHM2 mutations cause pathology by a loss- or a gain-of function mechanism [51]. Several FHM2 alleles have been studied by expressing the mutant genes in oocytes or cell culture. Some of the FHM2 mutations clearly result in reduced function of the enzyme, ranging from a complete loss of pump current to subtle changes in the voltage gating, cation affinities or enzyme turnover [52]. On the other hand, certain effects of FHM2 mutations argue for gain-of-function activity [51]. In this study, we found that both silencing eat-6 by RNAi and eat-6 overexpression increased sensitivity to an ACh esterase inhibitor, suggesting enhanced ACh neurotransmission. These findings may provide a clue to reconcile some paradoxical observations of the pathogenic FHM2 alleles.

A primary cause of the migraine aura is “cortical spreading depression” (CSD), a wave of transient neuronal depolarization that spreads over the brain cortex and presumably activates the trigeminovascular system resulting in migraine headache. Mutations in all FHM genes have been predicted to cause increased levels of the neurotransmitter glutamate and K+ in the synaptic cleft leading to increased propensity for CSD [53]. In the case of FHM1 this hypothesis has been validated by analysis of knock-in mice [54]. However, for FHM2 such studies have not yet been reported. Our genetic analyses of EAT-6 supports a model that the FHM2 Na+,K+-ATPase may regulate synaptic transmission both pre- and postsynaptically.

What are the molecular mechanisms by which eat-6 mutations may enhance ACh neurotransmission at the NMJ? A postsynaptic role for eat-6 has been shown convincingly before by others [8]. Our ACh neuron-specific eat-6 RNAi results suggest that eat-6 may also function in the ACh neurons to regulate neurotransmission. We observed an increased number of synaptic vesicles in the eat-6(ad467) mutant. Although the mechanism by which Na+,K+-ATPase regulates the abundance of synaptic vesicles is unclear, our genetic analyses shed some light on a possible role of EAT-6 in regulation of ACh neurotransmission. The aldicarb hypersensitivity by reduced EAT-6 function could be, at least in part, ascribed to exaggeration of EGL-30 Gαq signaling to the EGL-8 phospholipase, because a reduction of egl-30 and egl-8 function suppressed aldicarb hypersensitivity of the eat-6(ad467) mutant. Moreover, we found that a slo-1(gf) mutant overexpressing EAT-6 exhibited WT aldicarb sensitivity, although slo-1(gf);eat-6 double mutant worms were as hypersensitive to aldicarb as the eat-6 single mutant. These results suggest that, while both reduced and excessive EAT-6 function may increase ACh neurotransmission, their mechanisms differ. One possibility would be that the hyperactivity of SLO-1 compensates for the effects caused by increased EAT-6 function, whereas a reduced transmembrane K+ gradient in eat-6 mutant animals renders this hyperactive SLO-1 channel inefficient. It has been reported that EAT-6 possesses a novel function that is unrelated to the pump function of this enzyme [8]. We speculate that overexpression and the mutation of EAT-6 differentially affect this yet undefined EAT-6 function, which in turn perturb particular aspects of cellular mechanisms in ACh neurotransmission. However, since we were unable to rescue the aldicarb hypersensitivity of the eat-6 mutants by expressing EAT-6 in the ACh neurons, other experiments are necessary to determine its role in regulation of presynaptic neurotransmission.

Opposing 5-HT inputs to ACh neurotransmission

We demonstrated that eat-6 not only regulates ACh neurotransmission, but it is also involved in modulation of this process by exogenous and endogenous 5-HT. Our observation of eat-6 mutants as well as mutants of many synaptic components being completely resistant to 5-HT treatment suggests that eat-6 is one component mediating the inhibitory input of 5-HT to ACh neurotransmission. This result could be relevant to the therapeutic effects of drugs targeting 5-HT receptor subtypes in the treatment of migraine [55].

Analysis of the G protein-coupled 5-HT receptor ser-4 revealed dual stimulatory and inhibitory 5-HT inputs to ACh neurotransmission. One the one hand, ser-4 appears to be the primary receptor that mediates inhibition of ACh neurotransmission by exogenous 5-HT. On the other hand, deletion of ser-4 significantly suppressed aldicarb hypersensitivity of the eat-6(ad467) mutant, suggesting that SER-4 activity is required for the increased aldicarb sensitivity of the eat-6 mutant. Such dual activities of 5-HT receptors have been observed in mammals. For example, the 5-HT1A receptor can both stimulate and inhibit adenylyl cyclase [56]. Further experiments are required to discern the precise mechanisms of SER-4 action in stimulatory and inhibitory 5-HT signaling. One thought is that ser-4 may function in different neurons to inhibit or stimulate ACh neurotransmission. In rodents, in vivo binding assays showed that the 5-HT1A receptor expressed in different neurons in the CNS has different affinities to 5-HT. It is plausible that different levels of 5-HT differentially activate SER-4 in different neurons to modulate ACh neurotransmission. Consequently, the ser-4 mutation would abolish both the inhibitory and stimulatory 5-HT inputs to ACh neurotransmission, while loss of EAT-6 may selectively block the inhibitory 5-HT input. Interestingly, we found that specific serotonergic neurons are responsible for stimulatory and inhibitory 5-HT inputs to ACh neurotransmission at the bodywall NMJs. Genetic analyses in C. elegans have demonstrated that 5-HT released from specific neurons regulates specific behavior [43], while many 5-HT receptors synergistically or antagonistically regulate the same behavior [41], [44]. It may be sensible that different serotonergic neurons regulate different receptor subtypes at different cellular targets coordinating synaptic activity according to dynamic changes in the environment.

Materials and Methods


C. elegans strains were maintained at 20°C as described [57]. Wild-type (WT) animals were the Bristol Strain N2. Mutants used were: AQ279 unc-29(x29);Ex[unc-29::gfp;rol-6(d)], CX6741 tph-1(mg280);Ex[ADF::tph-1], CX7749 tph-1(mg280);Ex[NSM::tph-1], DA1239 eat-6(ad467);adEx1239[eat-6(+); rol-6(d)], eat-6(ad467), eat-6(ad601), eat-6(ad792), eat-6(ad997), VC836 eat-6(ok1334)/nT1[qIs51], egl-8(n488), egl-30(ad806), egl-30(tg26), mod-1(ok103), mod-5(n3314), MT15434 tph-1(mg280), NM670 Ex[punc-4::snb-1::gfp;lin-15(+)], ocr-2(yz5), rrf-3(pk1426), ser-1(ok345), ser-3(ok1995), ser-3 (ok2007), ser-4(ok512), ser-5(tm2647), ser-5(tm2654), ser-7(tm1325), slo-1(js379), slo-1(ky399), tom-1(ok285), unc-17(e245).

The following eat-6(ad467) double mutants were generated in this study: eat-6(ad467);egl-30(ad806), eat-6(ad467);egl-8(n488), eat-6(ad467);slo-1(ky399), eat-6(ad467);tph-1(mg280), eat-6(ad467);ser-4(ok512), eat-6(ad467);nT1. In the case of the deletion alleles n488, mg280 and ok512 that can be identified by PCR, we first isolated homozygous ad467 based on its slow pharyngeal pumping, small body size and fewer eggs (all these phenotypes manifest in eat-6 RNAi worms), then isolated the homozygous deletion mutations. In the case of the missense alleles ky399 and ad806, we first isolated cross-progeny showing the phenotypes of the homozygous ky399 (uncoordinated locomotion [38]), and egl-30 (sluggish movement and an increased number of eggs in the uterus [30]), and then picked homozygous ad467 animals from their progeny. To construct the ad467;nT1 strain, we generated males in the ok1334;nT1 strain, which carries the homozygous ok1334 mutation maintained by a single copy of the nT1 translocation marked by GFP. These males were crossed with ad467 hermaphrodites. The isolation of the homozygous ad467 progeny carrying nT1 was based on two criteria: first, worms should not carry the ok1334 deletion as determined by PCR; second, as the strain carries a single copy of nT1, the progeny that do not carry nT1 should show the ad467 phenotypes. All the missense alleles were confirmed by sequencing.

RNAi experiments

The rrf-3 strain with enhanced neuronal sensitivity to RNA interference [58] was used to silence eat-6, as described [59]. Briefly, NGM plates containing 6 mM IPTG were seeded with bacterial cultures expressing the empty vector L4440 or eat-6 RNAi construct from the RNAi feeding library constructed by J. Ahringer's group at the University of Cambridge and incubated overnight. 5–7 gravid rrf-3 hermaphrodites were allowed to lay eggs on these plates for one day and removed afterwards. The progeny on the plates were analyzed when they became adults after three days.

Constructs and transgenes

All the constructs were generated by PCR, and purified PCR fragments were used to generate transgenic animals. Unless specified otherwise, pinx-16::gfp, which is expressed in the intestine [60], was used as a transformation marker. The transcriptional reporter peat-6::gfp was generated by fusion of 1548 bp upstream of the translation start of eat-6, the same promoter element contained in Ex[eat-6(+)] [10], with the sequence of GFP and UNC-54 3′-untranslated regulatory element (UTR) in the plasmid pPD95.75 (from A. Fire, Stanford University School of Medicine, Stanford, CA). For tissue-specific expression full-length eat-6 cDNA was amplified from RNA isolated from WT animals by RT-PCR (SuperScript III First-Strand Synthesis System, Invitrogen) and fused with unc-54 3′ UTR and either the unc-17 [25] or myo-3 [61] promoter. punc-17::mCherry was generated by fusion of the unc-17 promoter element with the sequence of mCherry and unc-54 3′-UTR. The Ex[ser-4(+)] transgene has been described previously [41]. For cell-specific expression in ACh neurons full-length ser-4 cDNA amplified from WT RNA was fused with the unc-17 promoter and unc-54 3′ UTR. The construction and characterization of the transgenes expressing tph-1 in the ADF (under the srh-142 promoter) or NSM (under the ceh-2 promoter) neurons have been described [43].

To knock down eat-6 expression specifically in ACh neurons, we used a cell-specific RNAi approach [24]. Briefly, an eat-6 exon-rich 1089 bp genomic fragment, which was used to generate the eat-6 RNAi clone in the RNAi feeding library [59], was fused in the forward and reverse orientations by two different PCR reactions with the unc-17 promoter and unc-54 3′ UTR, so that the eat-6 gene fragment can be transcribed by the unc-17 promoter in the sense and antisense orientations. The two constructs were coinjected into worms in equal concentrations (∼100 ng/µl).

Fluorescence microscopy

GFP fluorescence was monitored using a 63× objective lens with an AxioImager Z1 miscroscope (Zeiss). Images were captured at 2×2 binning with an AxioCam MR digital camera using the AxioVision software (Zeiss). The neutral density filter #5 of the microscope was used to reduce the intensity of fluorescence excitation light to mitigate bleaching. The same exposure time (500 ms) was used for all samples. The ImageJ software (NIH) was used for image analysis.

Drug-induced paralysis assays

Sensitivity to drugs was determined by scoring paralysis after placing the animals on plates containing aldicarb or levamisole (Sigma) at the concentrations indicated in the figures. L4 stage animals were transferred to plates seeded with food and incubated at 20°C overnight, and resultant young adults were analyzed. An animal was scored as being paralyzed if no movement was detected after prodding with a platinum wire. In all experiments except that in Figure 9a,c, the time course of paralysis was measured by scoring percentage of animals paralyzed on the plates every 20 minutes over a three-hour period. To assay the inhibition of aldicarb effects by serotonin, animals were first incubated for 2 h on plates containing 5 mg/ml of serotonin creatine sulfate (Sigma), and were then transferred to plates containing both aldicarb (1 mM) and serotonin (5 mg/ml), and the time course of paralysis was assayed. For each genotype at least 3 independent trials were carried out, each performed in duplicate with 10 animals per assay plate. The results of mutants were compared with that of WT animals assayed in parallel.

Egg laying assay

Egg-laying behavior was evaluated by two well-established methods (18, 41). In both cases L4 stage animals were picked onto fresh plates seeded with food and allowed to develop at 20°C, and one-day old adults were analyzed. To test the response to 5-HT, animals were placed individually into wells of a 96-well plate, with each well containing 100 µl of a solution (M9 buffer or M9 buffer containing 5 mg/ml of serotonin). The number of eggs laid was scored after 1 h. To score the number of eggs carried in the uterus, individual one-day old adults were placed into a drop of solution containing commercial bleach and 2N NaOH on a glass slide. The bleach solution dissolved the body of the adult animal, and eggs, which were protected by their eggshells, were scored immediately. Eight animals per genotype for each condition were assayed in each trial.

Extracellular EPG recording

Extracellular recording of the electrical activity of the pharynx was made from intact worms as previously described [62]. One-day old adult worms were incubated in M9 buffer containing 10 mM 5-HT to stimulate pharyngeal pumping. The signals were acquired with an Axopatch 200B amplifier (Molecular Devices, Sunnyvale, CA) in voltage-clamp mode at 10 kHz sampling rate and were digitized using a Digidata 1322A AD/DA acquisition system controlled by a PC running Clampex 10.0 software (Molecular Devices), and analyzed using pClamp 10.0 software. The EPG reflects the time derivative of the membrane potential of the pharyngeal muscles. The EPG of WT worms consists of a large positive E peak, corresponding to muscle excitation, a plateau phase, and a large negative R spike, corresponding to muscle repolarization. In addition, recording EPG allows us to monitor neuronal inputs to the muscles. In particular, a small positive peak preceding the E peak represents an excitatory post-synaptic potential (EPSP) [21]. It results from activation of nicotinic receptors in the muscle membrane by ACh released from the MC neuron [63]. The amplitudes of the E and R spikes were measured in each of the first 5 action potentials recorded from each of 15–20 worms per genotype. Data collected from each individual worm were pooled together, and the mean R/E ratio was calculated for each genotype. To determine the percentage of the failed EPSPs, recording has been done till at least 30 action potentials were generated. All but the last EPSP in the series were counted, and those that were not immediately followed by the E spike were considered failed.

EM analysis

For transmission EM one-day old adult animals were fixed by high-pressure freezing and freeze-substitution, using 2% osmium tetroxide in acetone as the primary fixative [64]. Serial sections (80 nm thickness) of fixed animals were collected on copper slot grids and stained with 4% uranyl acetate in 70% methanol, followed by washing and incubating with lead citrate. Images were captured using a Philips CM10 transmission electron microscope at 80 kV equipped with a Morada 11 MPixel TEM CCD camera driven by the iTEM software (Olympus Soft Imaging Solutions). A set of serial sections containing a presynaptic density was defined as a synapse, and the number of vesicles per synaptic profile was calculated in the middle section of each set using NIH ImageJ software. Neuronal classes (VA or VB, both cholinergic; or VD, GABAergic) were identified by tracing the processes along the anterior ventral cord in a series of about 500 serial sections per animal [65].

Statistical analyses

Statistical analyses were performed using Origin 7.0 software (OriginLab Corporation, Northampton, MA). Significance was tested using an unpaired two sample Student's t test. Throughout the article data are expressed as mean ± SEM.

Supporting Information

Figure S1.

A single copy of the genomic eat-6 gene rescues the aldicarb hypersensitivity of the eat-6(ad467) mutant. Relative reciprocal T50 values of aldicarb-induced paralysis of worms with different ratios of WT to mutant eat-6 gene. An extra copy of the eat-6(+) locus was introduced by the nT1 translocation into the eat-6 (ok1334) deletion background or into the eat-6(ad467) background. Heterozygous ad467 animals were included as a control. The genotypes of the tested strains are schematically represented at left. The chromosomes IV and V are shown as long black and white bars, respectively. A short black bar represents the WT eat-6 gene, the horizontally hatched short bar: the eat-6(ad467) allele, and the white short bar: the eat-6(ok1334) allele. The short obliquely hatched bar represents the gfp marker. The error bars indicate SEM (n>3 replicates).

(0.48 MB TIF)

Figure S2.

Expression of eat-6 cDNA in ACh neurons or body-wall muscles does not rescue the aldicarb hypersensitivity of eat-6 mutants. Relative reciprocal T50 values of aldicarb-induced paralysis of worms pretreated with 5-HT (hatched bars) and those without 5-HT treatment (black bars). The values of 5-HT-treated WT worms and mutants are normalized to that of WT worms without 5-HT treatment. The error bars indicate SEM (n>3 replicates).

(0.21 MB TIF)

Figure S3.

Time courses of aldicarb-induced paralysis of the unc-17(e245) and unc-17(e245);ACh::eat-6 transgenic animals. The error bars indicate SEM (n = 3 replicates).

(0.15 MB TIF)

Figure S4.

Intensity of UNC-29::GFP fluorescence in eat-6(ad467) background, as compared to WT. Measurements were performed in 18 ad467 and 47 WT worms. In each worm, an anterior section of the ventral cord (∼100 µm length) was photographed. The values of punctal fluorescence intensity were calculated from profiles drawn across the middle of the puncta along the ventral cord of individual worms. The error bars indicate SEM between worms.

(0.36 MB TIF)

Figure S5.

Mutations in egl-30 or egl-8 do not suppress hypersensitivity of the eat-6(ad467) worms to levamisole. Relative reciprocal T50 values of paralysis were calculated as shown in Fig. 2. The error bars indicate SEM (n>3 replicates). * p<0.05, ** p<0.005, compared to WT.

(0.41 MB TIF)

Figure S6.

Time courses of aldicarb-induced paralysis of eat-6 and eat-6;ser-4 mutants on1 mM (a) and 0.25 (b) mM aldicarb. The difference between the two hypersensitive strains, which is not significant on 1 mM of the drug, is clearly resolved on the lower concentration. The error bars indicate SEM (n>3 replicates).

(0.30 MB TIF)


We thank L. Avery, C. Bargmann, O. Hobert, R. Horvitz, M. Nonet, W. Schafer, and the Caenorhabditis Genetics Center for worm strains. Special thanks to S. Mitani and the Tokyo Women's Medical University for deletion alleles of 5-HT receptors, and to L. Gunther, who provided expert help in high pressure freezing for TEM. We thank J.J. Gargus for inspiring discussions during the early phase of this work and critical reading of the manuscript.

Author Contributions

Conceived and designed the experiments: EG MM AK JYS. Performed the experiments: EG MM AK KCQN. Analyzed the data: EG MM AK TM DH JYS. Contributed reagents/materials/analysis tools: TM DH JYS. Wrote the paper: EG MM TM DH JYS.


  1. 1. Hamel E (2007) Serotonin and migraine: biology and clinical implications. Cephalalgia 27: 1293–1300.
  2. 2. Pietrobon D (2007) Familial hemiplegic migraine. Neurotherapeutics 274–284.
  3. 3. van de Ven R, Kaja S, Plomp J, Frants R, van den Maagdenberg A, et al. (2007) Genetic models of migraine. Arch Neurol 64: 643–646.
  4. 4. Estevez M (2006) Invertebrate modeling of a migraine channelopathy. Headache 46:: Suppl 1S25–31.
  5. 5. Kaplan J (2002) Biochemistry of Na,K-ATPase. Annu Rev Biochem 71: 511–535.
  6. 6. Blanco G (2005) Na,K-ATPase subunit heterogeneity as a mechanism for tissue-specific ion regulation. Semin Nephrol 25: 292–303.
  7. 7. Okamura H, Yasuhara J, Fambrough D, Takeyasu K (2003) P-type ATPases in Caenorhabditis and Drosophila: implications for evolution of the P-type ATPase subunit families with special reference to the Na,K-ATPase and H,K-ATPase subgroup. J Membr Biol 191: 13–24.
  8. 8. Doi M, Iwasaki K (2008) Na+/K+ ATPase regulates the expression and localization of acetylcholine receptors in a pump activity-independent manner. Mol Cell Neurosci 38: 548–558.
  9. 9. Avery L (1993) The genetics of feeding in Caenorhabditis elegans. Genetics 133: 897–917.
  10. 10. Davis M, Somerville D, Lee R, Lockery S, Avery L, et al. (1995) Mutations in the Caenorhabditis elegans Na,K-ATPase alpha-subunit gene, eat-6, disrupt excitable cell function. J Neurosci 15: 8408–8418.
  11. 11. Shima Y, Tada Y, Furuki M, Hara Y, Ohta H (1998) A missense mutation of the gene for Na+,K+-ATPase alpha-subunit causes abnormal feeding behavior in Caenorhabditis elegans. Biochem Biophys Res Commun 248: 778–782.
  12. 12. Morth J, Pedersen B, Toustrup-Jensen M, Sørensen T, Petersen J, et al. (2007) Crystal structure of the sodium-potassium pump. Nature 450: 1043–1049.
  13. 13. Morth J, Poulsen H, Toustrup-Jensen M, Schack V, Egebjerg J, et al. (2009) The structure of the Na+,K+-ATPase and mapping of isoform differences and disease-related mutations. Philos Trans R Soc Lond B Biol Sci 364: 217–227.
  14. 14. Vanmolkot K, Kors E, Turk U, Turkdogan D, Keyser A, et al. (2006) Two de novo mutations in the Na,K-ATPase gene ATP1A2 associated with pure familial hemiplegic migraine. Eur J Hum Genet 14: 555–560.
  15. 15. Miller K, Alfonso A, Nguyen M, Crowell J, Johnson C, et al. (1996) A genetic selection for Caenorhabditis elegans synaptic transmission mutants. Proc Natl Acad Sci USA 93: 12593–12598.
  16. 16. Sieburth D, Ch'ng Q, Dybbs M, Tavazoie M, Kennedy S, et al. (2005) Systematic analysis of genes required for synapse structure and function. Nature 436: 510–517.
  17. 17. Nurrish S, Segalat L, Kaplan J (1999) Serotonin inhibition of synaptic transmission: Galpha(0) decreases the abundance of UNC-13 at release sites. Neuron 24: 231–242.
  18. 18. Trent C, Tsuing N, Horvitz H (1983) Egg-laying defective mutants of the nematode Caenorhabditis elegans. Genetics 104: 619–647.
  19. 19. Sijen T, Fleenor J, Simmer F, Thijssen K, Parrish S, et al. (2001) On the role of RNA amplification in dsRNA-triggered gene silencing. Cell 107: 465–476.
  20. 20. Edgley M, Baillie D, Riddle D, Rose A (2006) Genetic balancers. In: Fay D, editor. WormBook: The C. elegans Research Community. pp.
  21. 21. Raizen D, Lee R, Avery L (1995) Interacting genes required for pharyngeal excitation by motor neuron MC in Caenorhabditis elegans. Genetics 141: 1365–1382.
  22. 22. Segall L, Mezzetti A, Scanzano R, Gargus J, Purisima E, et al. (2005) Alterations in the alpha2 isoform of Na,K-ATPase associated with familial hemiplegic migraine type 2. Proc Natl Acad Sci U S A 102: 11106–11111.
  23. 23. Tavraz N, Friedrich T, Dürr K, Koenderink J, Bamberg E, et al. (2008) Diverse functional consequences of mutations in the Na+/K+-ATPase alpha2-subunit causing familial hemiplegic migraine type 2. J Biol Chem 283: 31097–31106.
  24. 24. Esposito G, Di Schiavi E, Bergamasco C, Bazzicalupo P (2007) Efficient and cell specific knock-down of gene function in targeted C. elegans neurons. Gene 395: 170–176.
  25. 25. Alfonso A, Grundahl K, Duerr JS, Han HP, Rand JB (1993) The Caenorhabditis elegans unc-17 gene: a putative vesicular acetylcholine transporter. Science 261: 617–619.
  26. 26. Sandoval GM, Duerr JS, Hodgkin J, Rand JB, Ruvkun G (2006) A genetic interaction between the vesicular acetylcholine transporter VAChT/UNC-17 and synaptobrevin/SNB-1 in C. elegans. Nat Neurosci 9: 599–601.
  27. 27. Nonet M (1999) Visualization of synaptic specializations in live C. elegans with synaptic vesicle protein-GFP fusions. J Neurosci Methods 89: 33–40.
  28. 28. White J, Southgate E, Thompson J, Brenner S (1986) The structure of the nervous system of the nematode Caenorhabditis elegans. Phil Trans Roy Soc B 314: 1–340.
  29. 29. Hall D, Hedgecock E (1991) Kinesin-related gene unc-104 is required for axonal transport of synaptic vesicles in C. elegans. Cell 65: 837–847.
  30. 30. Brundage L, Avery L, Katz A, Kim U, Mendel J, et al. (1996) Mutations in a C. elegans Gqalpha gene disrupt movement, egg laying, and viability. Neuron 16: 999–1009.
  31. 31. Perez-Mansilla B, Nurrish S (2009) A network of G-protein signaling pathways control neuronal activity in C. elegans. Adv Genet 65: 145–192.
  32. 32. Lackner M, Nurrish S, Kaplan J (1999) Facilitation of synaptic transmission by EGL-30 Gqalpha and EGL-8 PLCbeta: DAG binding to UNC-13 is required to stimulate acetylcholine release. Neuron 24: 335–346.
  33. 33. Miller K, Emerson M, Rand J (1999) Goalpha and diacylglycerol kinase negatively regulate the Gqalpha pathway in C. elegans. Neuron 24: 323–233.
  34. 34. Bastiani C, Gharib S, Simon M, Sternberg P (2003) Caenorhabditis elegans Galphaq regulates egg-laying behavior via a PLCbeta-independent and serotonin-dependent signaling pathway and likely functions both in the nervous system and in muscle. Genetics 165: 1805–1822.
  35. 35. Bargmann C (1998) Neurobiology of the Caenorhabditis elegans genome. Science 282: 2028–2033.
  36. 36. Goodman M, Hall D, Avery L, Lockery S (1998) Active currents regulate sensitivity and dynamic range in C. elegans neurons. Neuron 20: 763–772.
  37. 37. Wang Z, Saifee O, Nonet M, Salkoff L (2001) SLO-1 potassium channels control quantal content of neurotransmitter release at the C. elegans neuromuscular junction. Neuron 32: 867–881.
  38. 38. Davies A, Pierce-Shimomura J, Kim H, VanHoven M, Thiele T, et al. (2003) A central role of the BK potassium channel in behavioral responses to ethanol in C. elegans. Cell 115: 655–666.
  39. 39. Gracheva E, Burdina A, Holgado A, Berthelot-Grosjean M, Ackley B, et al. (2006) Tomosyn inhibits synaptic vesicle priming in Caenorhabditis elegans. PLoS Biol 4: e261.
  40. 40. Carre-Pierrat M, Baillie D, Johnsen R, Hyde R, Hart A, et al. (2006) Characterization of the Caenorhabditis elegans G protein-coupled serotonin receptors. Invert Neurosci 6: 189–205.
  41. 41. Dempsey C, Mackenzie S, Gargus A, Blanco G, Sze J (2005) Serotonin (5-HT), fluoxetine, imipramine and dopamine target distinct 5-HT receptor signaling to modulate Caenorhabditis elegans egg-laying behavior. Genetics 169: 1425–1436.
  42. 42. Sze J, Victor M, Loer C, Shi Y, Ruvkun G (2000) Food and metabolic signalling defects in a Caenorhabditis elegans serotonin-synthesis mutant. Nature 403: 560–564.
  43. 43. Zhang Y, Lu H, Bargmann C (2005) Pathogenic bacteria induce aversive olfactory learning in Caenorhabditis elegans. Nature 438: 179–184.
  44. 44. Harris G, Hapiak V, Wragg R, Miller S, Hughes L, et al. (2009) Three distinct amine receptors operating at different levels within the locomotory circuit are each essential for the serotonergic modulation of chemosensation in Caenorhabditis elegans. J Neurosci 29: 1446–1456.
  45. 45. Albertson D, Thomson J (1976) The pharynx of Caenorhabditis elegans. Philos Trans R Soc Lond B Biol Sci 275: 299–325.
  46. 46. Zhang S, Sokolchik I, Blanco G, Sze J (2004) Caenorhabditis elegans TRPV ion channel regulates 5-HT biosynthesis in chemosensory neurons. Development 131: 1629–1638.
  47. 47. De Fusco M, Marconi R, Silvestri L, Atorino L, Rampoldi L, et al. (2003) Haploinsufficiency of ATP1A2 encoding the Na+/K+ pump alpha2 subunit associated with familial hemiplegic migraine type 2. Nat Genet 33: 192–196.
  48. 48. Montagna P (2004) The physiopathology of migraine: the contribution of genetics. Neurol Sci 25,S93-6: S93–96.
  49. 49. de Carvalho Aguiar P, Sweadner K, Penniston J, Zaremba J, Liu L, et al. (2004) Mutations in the Na+/K+ -ATPase alpha3 gene ATP1A3 are associated with rapid-onset dystonia parkinsonism. Neuron 43: 169–175.
  50. 50. Goldstein I, Lerer E, Laiba E, Mallet J, Mujaheed M, et al. (2009) Association between sodium- and potassium-activated adenosine triphosphatase alpha isoforms and bipolar disorders. Biol Psychiatry 65: 985–991.
  51. 51. Gargus J (2009) Genetic calcium signaling abnormalities in the central nervous system: seizures, migraine, and autism. Ann N Y Acad Sci 1151: 133–156.
  52. 52. Segall L, Scanzano R, Kaunisto M, Wessman M, Palotie A, et al. (2004) Kinetic alterations due to a missense mutation in the Na,K-ATPase alpha2 subunit cause familial hemiplegic migraine type 2. J Biol Chem Oct 15;(42): 279: 43692–43696.
  53. 53. van den Maagdenberg A, Haan J, Terwindt G, Ferrari M (2007) Migraine: gene mutations and functional consequences. Curr Opin Neurol 20: 299–305.
  54. 54. Tottene A, Conti R, Fabbro A, Vecchia D, Shapovalova M, et al. (2009) Enhanced excitatory transmission at cortical synapses as the basis for facilitated spreading depression in Ca(v)2.1 knockin migraine mice. Neuron 61: 762–773.
  55. 55. Goadsby P (2007) Recent advances in understanding migraine mechanisms, molecules and therapeutics. Trends Mol Med 13: 39–44.
  56. 56. Frazer A, Maayani S, Wolfe B (1990) Subtypes of receptors for serotonin. Annu Rev Pharmacol Toxicol 30: 307–348.
  57. 57. Brenner S (1974) The genetics of Caenorhabditis elegans. Genetics 77: 71–94.
  58. 58. Simmer F, Tijsterman M, Parrish S, Koushika S, Nonet M, et al. (2002) Loss of the putative RNA-directed RNA polymerase RRF-3 makes C. elegans hypersensitive to RNAi. Curr Biol 12: 1317–1319.
  59. 59. Kamath R, Ahringer J (2003) Genome-wide RNAi screening in Caenorhabditis elegans. Methods 30: 313–321.
  60. 60. Peters M, Teramoto T, White J, Iwasaki K, Jorgensen E (2007) A calcium wave mediated by gap junctions coordinates a rhythmic behavior in C. elegans. Curr Biol 17: 1601–1608.
  61. 61. Okkema P, Harrison S, Plunger V, Aryana A, Fire A (1993) Sequence requirements for myosin gene expression and regulation in Caenorhabditis elegans. Genetics 135: 385–404.
  62. 62. Raizen D, Avery L (1994) Electrical activity and behavior in the pharynx of Caenorhabditis elegans. Neuron 12: 483–495.
  63. 63. McKay J, Raizen D, Gottschalk A, Schafer W, Avery L (2004) eat-2 and eat-18 are required for nicotinic neurotransmission in the Caenorhabditis elegans pharynx. Genetics 166: 161–169.
  64. 64. Weimer R (2006) Preservation of C. elegans tissue via high-pressure freezing and freeze-substitution for ultrastructural analysis and immunocytochemistry. Methods Mol Biol 351: 203–221.
  65. 65. Hall D (1995) Electron Microscopy and 3D Image Reconstruction. C elegans: Modern Biological Analysis of an Organism Methods in Cell Biology. New York: Academic Press. pp. 395–436.