www.nature.com/scientificreports OPEN Prior activity of olfactory receptor neurons is required for proper sensory processing and behavior in Received: 4 January 2018 Drosophila larvae Accepted: 14 May 2018 Published: xx xx xxxx 1 2,3 2,3 1,4 Nao Utashiro , Claire R. Williams , Jay Z. Parrish & Kazuo Emoto Animal responses to their environment rely on activation of sensory neurons by external stimuli. In many sensory systems, however, neurons display basal activity prior to the external stimuli. This prior activity is thought to modulate neural functions, yet its impact on animal behavior remains elusive. Here, we reveal a potential role for prior activity in olfactory receptor neurons (ORNs) in shaping larval olfactory behavior. We show that prior activity in larval ORNs is mediated by the olfactory receptor complex (OR complex). Mutations of Orco, an odorant co-receptor required for OR complex function, cause reduced attractive behavior in response to optogenetic activation of ORNs. Calcium imaging reveals that Orco mutant ORNs fully respond to optogenetic stimulation but exhibit altered temporal patterns of neural responses. These findings together suggest a critical role for prior activity in information processing upon ORN activation in Drosophila larvae, which in turn contributes to olfactory behavior control. Animals rely on their sensory neurons to detect external stimuli and change their behavior in response to the external world. However, sensory neurons are often activated prior to experiencing external stimuli. In many sensory systems, such neural activity prior to the stimulus, or prior activity, ae ff cts neural response to subsequent stimuli. For example, in the olfactory system of locusts, prior activity modulates response to odorants . In addi- tion, even in the absence of such background stimuli, many types of neurons exhibit spontaneous activity. For example, mitral cells in the mammalian olfactory bulb show patterned spontaneous activity in the absence of 2,3 odor stimuli . This spontaneous activity could also be regarded as a type of prior activity. These neural activities 4–7 prior to stimuli are observed in many sensory systems and cortical regions , yet their impacts on animal behav- ior remain unclear. Olfactory receptor neurons (ORNs) of Drosophila melanogaster larvae provide an attractive model for stud- ying functional links between neural activity and behavioral output. Drosophila larvae have only 21 ORNs that innervate the dorsal organs on each side of the head and project to individual glomeruli in the antennal lobe. Each ORN expresses its own olfactory receptor complex (OR complex) that consists of a cell-specific olfactory recep- 8 9–11 tor (OR) and the co-receptor Orco , with the cell-specific OR determining the odor specificity . Activation of single ORNs induces either attractive or aversive behavior, indicating that the neural activity of each ORN tightly relates to stereotyped behavior. For example, larvae that have only a single pair of functional ORNs express- ing Or42a exhibit robust attractive behavior to many odors . By contrast, optogenetic stimulation of individual ORNs expressing Or33b, or Or45a, which detect aversive odors, induced aversive behavior toward the stimulating light . Within ORNs, Orco is a key regulator of both evoked and spontaneous activity. In ORNs, Orco regulates 8 14,15 dendritic localization of ORs and forms heteromeric ligand-gated ion channels together with ORs . Orco is therefore necessary for odor-evoked activity. In addition, Orco promotes spontaneous activity in ORNs. Orco 8,16,17 mutation or pharmacological inhibition severely diminishes ORN spontaneous activity in Drosophila as well Department of Biological Sciences, School of Science, The University of Tokyo, 7-3-1 Hongo, Bunkyo-ku, Tokyo, 113- 0033, Japan. Department of Biology, University of Washington, 24 Kincaid Hall, Box 351800, Seattle, WA, 98195, USA. 3 4 Molecular and Cellular Biology Program, University of Washington, Seattle, WA, 98195, USA. International Research Center for Neurointelligence (WPI-IRCN), The University of Tokyo, 7-3-1 Hongo, Bunkyo-ku, Tokyo, 113-0033, Japan. Correspondence and requests for materials should be addressed to K.E. (email: email@example.com) ScIentIfIc REPO R Ts | (2018) 8:8580 | DOI:10.1038/s41598-018-26825-3 1 www.nature.com/scientificreports/ Figure 1. Calcium imaging of larval olfactory receptor neurons. (a) Schematic of the ex vivo calcium imaging preparation and the larval olfactory circuit. ORN, olfactory receptor neuron; LN, local neuron; PN, projection neuron. (b) Representative fluorescence changes from baseline (∆F/F ) of Or42a ORN in three different −3 −3 1118 animals. 10 EA, 10 concentration of ethyl acetate. Genotype: w ;Or42a-Gal4,UAS-GCaMP6f/+. 18,19 as a broad range of other insects, including Anopholes gambiae, and Manduca sexta . While Orco expression 20,21 may extend to tissues involved in other sensory modalities in some insects , Drosophila Orco expression is apparently restricted to OR-expressing ORNs, thus Orco mutation provides a tool to potently and specifically block evoked and spontaneous activity in ORNs. In this study, we aim to investigate potential roles for prior activity in the olfactory system by using Drosophila larval ORNs as the model system. We show that each larval ORN has different patterns of prior activity and that the OR complexes are the key components required for prior activity in larval ORNs. Optogenetic behavioral analysis indicates that Orco mutant larvae show reduced responses to ORN stimulation. Using a combination of optogenetic stimulation and ex-vivo calcium imaging, we show that Orco mutant ORNs exhibit altered temporal patterns of ORN activity in response to ORN stimulation. Our findings thus suggest a role for prior neural activity of ORNs in sensory processing and olfactory behavior control. Results Calcium imaging of larval olfactory receptor neurons. To examine neural activity in larval ORNs, we 2+ 2+ 22 performed calcium (Ca ) imaging of ORNs. To that end, we expressed the Ca indicator GCaMP6f in ORNs 23 2+ using the Gal4-UAS system and monitored Ca response in ORN axonal terminals in the larval brain (Fig. 1a). 24 2+ Consistent with a previous report , we detected robust Ca responses when the larval head was exposed to ethyl 9 2+ acetate, a strong attractant to larvae (Fig. 1b). In addition to the odor-evoked Ca responses, we also observed 2+ continuous Ca responses prior to the odor stimulation in ORNs (Fig. 1b). These responses may reflect sponta- neous activity or responses to other background odorants; we subsequently refer to these responses as prior activ- ity to reflect their presence prior to application of a defined odor. The prior activity in ORNs exhibited smaller amplitudes compared to the odor-evoked activity (Fig. 1b: Or42a, 61.1% of evoked activity on average, n = 11). In 2+ addition, video recordings of Ca responses in ORNs demonstrated that the frequency of prior activity in each ORN is different from one another (Supplementary Movie S1). These data suggest that larval ORNs likely have different profiles of prior activity with unique frequency. Orco is essential for prior activity in larval ORNs. Given that firing patterns of prior activity seem to be different in each ORN, we reasoned that ORN-specific molecules might contribute to generating the prior activity. One potential candidate is the OR complexes as each of 21 ORNs in the larval olfactory organ (dorsal organ) expresses a unique set of OR complexes . OR complexes are heteromeric ion channels that consist of the ORN-specific OR that determines the response spectrum of the ORN and the co-receptor Orco that is shared by 14,15,26 most ORNs . ScIentIfIc REPO R Ts | (2018) 8:8580 | DOI:10.1038/s41598-018-26825-3 2 www.nature.com/scientificreports/ 2+ To examine potential roles for OR complexes in generation of ORN prior activity, we performed Ca imaging in Orco mutant ORNs. Orco null mutations prevent OR complexes from localizing to ORN dendrites and Orco is required for formation of heteromeric channels with ORs. Hence, Orco mutation blocks odor-evoked responses 16,17 of ORNs. Orco mutation additionally blocks spontaneous activity in embryonic and adult ORNs . We likewise found that in Orco mutant ORNs prior activity was rarely detectable (Fig. 2a,b). Quantitative analysis indicated that the frequency of the prior activity in Orco mutant ORNs was significantly reduced compared to wild-type controls (Fig. 2c: WT, median 0.90, 1st quartile 0.48, 3rd 1.47; Orco mutants, median 0.060, 1st quartile 0.017, 3rd 0.083). We next performed power spectrum analysis of the prior activity and found that the characteristic peak observed in wild-type ORNs was largely absent in Orco mutant ORNs (Fig. 2d), indicating that not only the amplitude but also the rhythmicity of the prior activity was extinguished in Orco mutant ORNs. Recording the prior activity from single ORNs, Or42a and Or42b ORN, further revealed that the reduced prior activity in Orco mutant ORNs was detectable at the single neuron level (Fig. 2e,f ). The reduced prior activity in Orco mutant ORNs was restored to the wild-type level by expressing UAS-Orco in ORNs (Fig. 2c,e and f ). These data suggest that OR-complex expression in each ORN is essential for producing their unique prior activity as well as evoked activity in ORNs. While it is possible that Orco could directly influence membrane potential on its own, given that 14,15,19 Orco family proteins can form functional cation channels in the absence of OR expression , whether such channels are actually formed in ORNs remains to be determined. Orco mutant larvae exhibit reduced response to ORN activation. In order to investigate potential roles for the prior activity in larval behavior, we next examined whether Orco mutant larvae might have defects in olfactory behavior evoked by ORN activation. To activate wild-type and Orco mutant ORNs, we expressed the red light-gated cation channel CsChrimson in ORNs under the control of the Orco-Gal4 driver and illuminated larvae with red light (617 nm) (Fig. 3a). We placed these transgenic larvae in the center of a Petri dish divided into quadrants receiving either red light illumination or no illumination (Fig. 3a). In this choice assay system, quad- rants receiving red light illumination are bounded by dark quadrants, therefore ORNs expressing CsChrimson are optogenetically activated as long as larvae stay in the illuminated areas. We first checked CsChrimson expression and found no significant difference in CsChrimson expression levels in wild-type and Orco mutant ORNs (Supplementary Fig. S1). We then performed the choice assay with wild-type lar- vae harboring CsChrimson in ORNs. Consistent with the previous reports , wild-type larvae carrying CsChrimson in ORNs showed a strong preference to the illuminated areas compared to control larvae that tended to stay in the dark areas (Fig. 3b,c), suggesting that optogenetic activation of ORNs causes an attractive bias in larvae. We next examined Orco mutant larvae carrying CsChrimson in ORNs and found that, unlike wild-type larvae, Orco mutant larvae exhibited no significant preference between illuminated and dark areas (Fig. 3b,c). Similar data were obtained with wild-type and Orco mutant larvae expressing CsChrimson in single ORNs such as Or42a and Or42b, both of 9,25 which are dominant ORNs activated by attractive odorants such as ethyl acetate (Fig. 3d,e). The reduced attrac- tion to the illuminated areas in Orco mutant larvae was fully rescued to wild-type levels by expressing UAS-Orco in ORNs (Fig. 3c–e), suggesting the cell-autonomous role of OR complexes in ORNs. Together with our finding that OR complexes are essential components to generate the prior activity in ORNs, these observations suggest potential roles for the prior activity of ORNs in control of olfactory behavior evoked by ORN activation. Orco mutant larvae are defective in turning behavior at the light/dark boundary. What behavioral changes might cause Orco mutant larvae to spend less time in illuminated areas compared to wild-type? To address this, we analyzed larval behavior at the boundary of illuminated and dark quadrants. First, we examined behavior of larvae moving from the dark to the illuminated areas. Video recording of individual traces indicated that ~75% of larvae harboring CsChrimson passed into the illuminated areas in both wild-type and Orco mutant larvae, while ~50% of wild-type and Orco mutant larvae lacking CsChrimson crossed the boundaries (Fig. 4a). These data indicate that loss of OR-complex functions has no significant effect on larval moving from the dark to the illuminated areas. We next focused on the larvae moving from the illuminated quadrants toward the dark quadrants. Almost 100% of wild-type larvae harboring CsChrimson in ORNs made an obvious turn when they approached from the illuminated to the dark areas (Fig. 4b; 95.5%, n = 49). In contrast, only ~50% Orco mutant larvae harboring CsChrimson passed into the dark areas (Fig. 4b; 51.0%, n = 69). These observations suggest that the reduced pref- erence to the illuminated areas in Orco mutant larvae is attributed at least in part to the reduced turning behavior at the boundary when they move from the illuminated quadrants to the dark quadrants. Temporal dynamics of ORN response to continuous stimulations are altered in Orco mutant larvae. To address how the prior activity in ORNs could affect the turning behavior, we examined neural responses of ORNs evoked by optogenetic stimulation in wild-type and Orco mutant larvae. We first tested whether Orco mutant ORNs could respond to single optogenetic stimulations. We simultaneously expressed 28 2+ channelrhodopsin-2 (ChR2) and GCaMP6f in ORNs and measured Ca responses induced by blue light stimu- lation of larvae (Fig. 5a). A previous report also showed that larvae expressing ChR2 in their ORNs were attracted to the blue-light stimulation . Thus, behavioral and neural responses to ChR2 likely mirror the responses to 2+ CsChrimson. Blue light application induced Ca responses in both wild-type and Orco mutant ORNs (Fig. 5a). 2+ Intriguingly, the average amplitude of Ca responses was higher in Orco mutant ORNs than in wild-type (Fig. 5b,c: wild-type, median 67.6%, 1st quartile 46.7%, 3rd quartile 67.6%, n = 64; Orco mutants, median 105.6%, 1st quartile 71.1%, 3rd quartile 138.0%, n = 34). Furthermore, Orco mutant ORNs consistently responded to repeated blue light applications, whereas wild-type ORNs exhibited large variability in the amplitude of their responses (Fig. 5d,e). These data indicate that Orco mutant ORNs respond to stimulation better than wild-type, and it is thus unlikely that reduced preference toward illuminated areas in Orco mutant larvae is simply due to reduced excitability in Orco mutant ORNs. ScIentIfIc REPO R Ts | (2018) 8:8580 | DOI:10.1038/s41598-018-26825-3 3 www.nature.com/scientificreports/ Figure 2. Orco is essential for prior activity in larval ORNs. (a) Schematic of Orco-OR channel of ORNs in wild-type (WT) and Orco mutant larvae. The channel contributes to the prior activity of ORNs. (b) Representative fluorescence changes from baseline (∆F/F ) of ORNs in wild-type (WT) and Orco mutant larvae. (c) Quantification of the frequency of the prior activity of ORNs in the wild-type (WT, blue; n = 57), Orco mutant (Orco, red; n = 57) and Orco expression-rescued strain (Rescue, black; n = 43). Box plots show the median (white line), 1st, and 3rd quartile (box), the data range (whiskers), and outliers (circles). Outliers are data points located outside the whisker range. (d) Average power spectra of the prior activity of ORNs in wild-type (WT, blue; n = 132) and Orco mutant (Orco, red; n = 118). Means ± SEM. Genotypes: WT, w ;Orco- 1118 1 1 1118 Gal4,UAS-GCaMP6f/+ Orco, w ;Orco-Gal4,UAS-GCaMP6f/+;orco /orco . Rescue, w ;Orco-Gal4,UAS- 1 1 GCaMP6f/UAS-Orco;orco /orco . (e and f) Quantification of frequency of the prior activity of a single ORN, 1118 1118 Or42a (e) and Or42b ORN (f). Genotypes: WT, w ;Or42a/b-Gal4/ UAS-GCaMP6f. Orco, w ;Or42a/b-Gal4/ 1 1 1118 1 1 *** UAS-GCaMP6f;orco /orco . Rescue, w ;Or42a/b-Gal4,UAS-Orco/UAS-GCaMP6f;orco /orco . P < 0.001, Wilcoxon rank-sum test with Bonferroni correction; n.s., not significant. ScIentIfIc REPO R Ts | (2018) 8:8580 | DOI:10.1038/s41598-018-26825-3 4 www.nature.com/scientificreports/ Figure 3. Orco mutant larvae exhibit reduced response to ORN activation. (a) Right, expression of CsChrimson in ORNs. Left, agarose gel arena for optogenetic choice assay. (b) Representative plots of WT (left) and Orco mutant (right) larval positions over a period of 5 min. (c) Performance index (PI) of larvae expressing 1118 1118 CsChrimson in their ORNs. Genotypes: WT, w ;Orco-Gal4/UAS-CsChrimson,Tsh-Gal80. Orco, w ;Orco- 1 1 1118 Gal4/UAS-CsChrimson,Tsh-Gal80;orco /orco . Rescue, w ;Orco-Gal4,UAS-Orco/UAS-CsChrimson,Tsh- 1 1 Gal80;orco /orco . (d and e) Performance index (PI) of larvae expressing CsChrimson in a single ORN, Or42a 1118 1118 (d) and Or42b (e). Genotypes: WT, w ;Or42a/b-Gal4/UAS-CsChrimson,Tsh-Gal80. Orco, w ;Or42a/b- 1 1 1118 Gal4/UAS-CsChrimson,Tsh-Gal80;orco /orco . Rescue, w ;Or42a/b-Gal4,UAS-Orco/UAS-CsChrimson,Tsh- 1 1 *** Gal80;orco /orco . P < 0.001, Wilcoxon’s rank-sum test with Bonferroni correction; n.s. not significant. Next, we examined how Orco mutant ORNs could respond to continuous stimulation. This stimulation par - adigm likely reflects our behavioral assay rather than the pulse stimulations, as Orco mutant larvae exhibited turning defects when they encountered the light-dark boundary ae ft r continuous ORN stimulations in the illu - minated areas (Fig. 4). Similar to the pulse stimulations (Fig. 5), Orco mutant ORNs responded to continuous stimulations more strongly than wild-type ORNs at the onset of the stimulations (Fig. 6a–d). However, during 2+ the course of the continuous stimulation, Ca responses in Orco mutant ORNs gradually decreased, whereas 2+ Ca responses in wild-type ORNs exhibited some fluctuation but were sustained at a certain level (Fig. 6b–d). Furthermore, wild-type and Orco mutant ORNs exhibited distinct responses to termination of prolonged stim- 2+ ulation. In wild-type ORNs, Ca responses were quickly diminished to levels below the pre-stimulus baseline, 2+ whereas Ca responses in Orco mutant ORNs were gradually reduced but did not return to the baseline for an extended period of time (Fig. 6b–d). Given that reduction of the turning behavior in Orco mutant larvae was specifically observed at the light-dark boundary where the larvae suddenly lost continuous ORN stimulation, the dier ff ent neural responses right after termination of the continuous stimulation in wild-type and Orco mutant ORNs might contribute to the changed turning behavior upon ORN activation. One might imagine that ion channel gene expression in Orco mutant ORNs could account for the die ff rent patterns of activation. To test this, we assayed for changes in ion channel gene expression between wild-type and Orco mutant dorsal organs using RNA-Seq analysis (Supplementary Fig. S2a), and found no significant changes in ion channel gene expression in Orco mutant dorsal organs; among 148 ion channel genes queried, only Orco and 4 OR genes exhibited significant differential expression between wild-type and Orco mutant samples (Supplementary Fig. S2b, Supplementary Table 1). These results suggest that the differences in neural responses in Orco mutant ORNs are unlikely to be caused by changes in ion channel expression. ScIentIfIc REPO R Ts | (2018) 8:8580 | DOI:10.1038/s41598-018-26825-3 5 www.nature.com/scientificreports/ Figure 4. Orco mutant larvae are defective in turning behavior at the light/dark boundary. (a) Probability of entering illuminated quadrants from dark quadrants. (b) Probability of turning back into illuminated 1118 1118 quadrants. Genotypes: WT, w ;Orco-Gal4/UAS-CsChrimson, Tsh-Gal80. Orco, w ;Orco-Gal4/UAS- 1 1 *** 46 CsChrimson,Tsh-Gal80;orco /orco . P < 0.001, Fisher’s exact test with Benjamini−Hochberg correction ; n.s. not significant. PNs respond to ORN stimulations in Orco mutant larvae. In the Drosophila olfactory system, projec- 30,31 tion neurons (PNs) relay olfactory information from ORNs to higher-order brain areas . To confirm that the neural responses of ORNs are transferred to PNs in Orco mutants, we explored whether functional synapses were formed between ORNs and PNs. To this end, we expressed the presynaptic marker, Bruchpilot::GFP (Brp::GFP) , in Or42a ORNs and observed the localization of the marker signals. We found that the Brp signals were local- ized at the axonal terminals in both wild-type and Orco mutant ORNs, though the signals in Orco mutant ORNs seemed to be more condensed compared to wild-type (Supplementary Fig. S3). This result suggests that the syn- apses between ORNs and PNs are formed in Orco mutants. Next, we examined whether PNs could respond to continuous stimulations of ORNs. We expressed ChR2 2+ 2+ in ORNs and the Ca -responsive red fluorescent protein RGECO1 in PNs, and measured PN Ca responses induced by blue light stimulation of ORNs (Fig. 7). The PN responses were similar to ORN responses in regard to temporal patterns during stimulation. At the onset of the ORN activation, the response of PNs was larger in Orco mutant compared to wild-type. However, PN responses in Orco mutants were gradually decreased and finally became weaker compared to wild-type. These results suggest that functional connectivity between ORNs and PNs is likely retained in Orco mutants. Discussion To realize proper sensory processing, neural circuits in the brain decode evoked responses based on the neural activity prior to the stimulation. Such prior activity is generally observed in olfactory, auditory, visual, and cor- 5,7,33–35 34–37 tical neurons . In certain cases, the prior activity is thought to modify the evoked response to stimuli . However, the contribution of prior activity to output behavior remains largely unknown because of difficulty in manipulating prior activity in vivo and lack of a simple model for assessing the effect of prior activity. In this study, we have provided the following evidence that support the potential role for prior activity in control of olfactory behavior. First, we showed that prior activity in ORNs is likely mediated at least in part by OR complexes, as prior activity was significantly reduced in Orco mutant ORNs (Fig. 2). Second, we found that Orco mutant larvae, which had reduced prior activity in ORNs, showed less attractive behavior to illuminated areas ScIentIfIc REPO R Ts | (2018) 8:8580 | DOI:10.1038/s41598-018-26825-3 6 www.nature.com/scientificreports/ Figure 5. Temporal dynamics of ORN response to pulse stimulations. (a) Expression of ChR2 and GCaMP6f in ORNs. (b) Average fluorescence changes (∆F/F ) to blue light stimulation in WT (blue; n = 64), Orco mutant (red; n = 40), and control larvae that did not carry UAS-ChR2 (black; n = 50). Means ± SEM. (c) Quantification of maximum ∆F/F (∆F/F ) of ORNs in the control, WT, and Orco mutant larvae. (d and e) Representative 0 0max traces of ∆F/F of a single ORN in WT (d) and Orco mutant (e). ORNs are stimulated with the blue light 1118 1118 pulses at four time points. Genotypes: Control, w ;Orco-Gal4,UAS-GCaMP6f/Orco-Gal4. WT, w ;Orco- Gal4,UAS-GCaMP6f/Orco-Gal4,UAS-hChR2[H134R]. Orco, w ;Orco-Gal4,UAS-GCaMP6f/Orco-Gal4,UAS- 1 1 hChR2[H134R];orco /orco . in a choice test arena in which illumination drives optogenetic activation of ORNs (Fig. 3). Third, we demon- strated that the behavioral changes in Orco mutant larvae were attributed to reduced turning behavior when larvae approached the boundary from the light area (Fig. 4). The behavioral defects in Orco mutant larvae were fully rescued by introducing one copy of Orco gene in ORNs, indicating the cell-autonomous function of Orco in ORNs (Fig. 3). How could the prior activity mediated by OR complexes ae ff ct the turning behavior? It seems unlikely that the prior activity ae ff cts ORN excitability as Orco mutant ORNs showed substantial activity in response to optoge- netic activation (Fig. 5). One possibility is that the prior activity could directly modify the firing patterns of ORNs upon activation. Indeed, temporal patterns of the optogenetically-evoked activity in wild-type larvae seemed to uc fl tuate probably due to the prior activity, whereas Orco mutant ORNs exhibited consistent firing patterns upon activation (Fig. 6). An alternative but not mutually exclusive scenario is that the prior activity might ae ff ct expression levels of functional proteins, such as ion channels. Temporal patterns of neuronal activity are basically determined by the combinatory activities of multiple ion channels . While our RNA-Seq analysis showed that the expression levels of ion channels were not significantly different between wild-type and Orco mutant ORNs, Orco mutant ORNs exhibited different temporal patterns of neural responses from wild-type ORNs (Fig. 6). Thus, one possibility is that prior activity might regulate post-transcriptional control of channel expression or modulate ion channel function by another mechanism, such as post-translational modification and/or trafficking, and hence change the temporal pattern of neural responses. Another possibility is that connectivity between ORNs and PNs might be influenced by the prior activity. Previous studies suggested that prior activities in neurons, including sponta- 39–41 neous activity, ae ff ct synaptic formation . Furthermore, blocking neural activity of ORNs led to alterations in the morphology of ORN axon terminals in Drosophila embryos . Consistent with these results, we observed alterations in the distribution of presynaptic marker signals in axonal terminals of Orco mutant ORNs compared to wild-type ORNs (Supplementary Fig. S3). We, therefore, cannot exclude the possibility that prior activity might modify the connectivity between ORNs and PNs. However, Orco mutant PNs responded to continuous ORN activation, suggesting that functional connectivity between ORNs and PNs in Orco mutants is intact. Thus, dep- rivation of prior activity in Orco mutant ORNs might ae ff ct neural responses in Orco mutant at the circuit level, which in turn modulate the animal behavior upon ORN activation. ScIentIfIc REPO R Ts | (2018) 8:8580 | DOI:10.1038/s41598-018-26825-3 7 www.nature.com/scientificreports/ Figure 6. Temporal dynamics of ORN response to continuous stimulations are altered in Orco mutant larvae. (a) Expression of ChR2 and RGECO1.0 in ORNs. (b) Average ∆F/F to blue light stimulation in WT (blue; n = 31) and Orco mutants (red; n = 33). Means ± SEM. (c and d) Representative traces of ∆F/F of a single ORN in WT (c) and Orco mutant (d). ORNs are stimulated with the blue light for 18 s. Genotypes: WT, w ;Orco- Gal4,UAS-RGECO1/Orco-Gal4,UAS-hChR2 [H134R]. Orco, Orco-Gal4,UAS-RGECO1/Orco-Gal4,UAS- 1 1 hChR2[H134R];orco /orco . Figure 7. PNs respond to continuous stimulations of ORNs in Orco mutant larvae. (a) Expression of ChR2 in ORNs and RGECO1.0 in PNs. (b) Average ∆F/F of PNs to blue light stimulation of ORNs in wild-type (blue; n = 56) and Orco mutants (red; n = 70). Means ± SEM. Genotypes: WT, w ;GH146-Gal4,Orco-ChR2/UAS- 1118 1 1 RGECO1,Orco-ChR2. Orco, w ;GH146-Gal4,Orco-ChR2/UAS-RGECO1,Orco-ChR2;orco /orco . It is also feasible that the prior activity might play a role in inactivation of ORNs, as Orco mutant larvae failed to turn at the boundary specifically when larvae moved from illuminated areas in which ORNs were optogeneti- 2+ cally activated to dark areas (Fig. 4). Ca imaging data indicate that optogenetically-evoked activity in wild-type ORNs was quickly suppressed to the basal level once larvae passed the boundary from illuminated areas to the dark areas, whereas Orco mutant ORNs required longer times for evoked activity to return to the basal level (Fig. 6). Considering the results of the behavioral assay, these observations indicate that the turning behavior at the boundary may be induced by the transition of the response amplitude from a certain level to below the baseline. Consistent with this possibility, larvae expressing CsChrimson in Or42a ORNs demonstrated increased run-to-turn transitions when optogenetic activation was reduced . Based on this notion, prior activity might, at ScIentIfIc REPO R Ts | (2018) 8:8580 | DOI:10.1038/s41598-018-26825-3 8 www.nature.com/scientificreports/ least in part, contribute to the reduction of neural response of ORNs. u Th s, the prior activity might be one of the critical factors for suppression of neural responses. In summary, by the use of a combined optogenetic and ex vivo imaging technique in Drosophila larval ORNs, we have revealed a potential role for prior activity in control of olfactory behavior evoked by ORN activation. Given its relative simplicity, combined with the powerful genetic tools in Drosophila, our system could contribute to elu- cidation of the molecular and circuit-based mechanisms of how prior activity in ORNs regulates animal behavior. Materials and Methods Drosophila strains. Fly strains used in the present study were as follows: Orco-Gal4 (Bloomington − + 1 #26818), UAS-GCaMP6f (Bloomington #42747), w ;; w , orco (null allele, Bloomington #23129), Or42a-Gal4 (Bloomington #9970), Or42b-Gal4 (Bloomington #9972), UAS-Orco (second, this study), UAS-CsChrimson (Bloomington #55135), Tsh-Gal80 (second, kindly gifted by Dr. Miesenböck), UAS-RGECO1 (our stock) , UAS- 43 44 hChR2[H134R] (our stock) , Orco-ChR2 (Bloomington #63041) , GH146-Gal4 (Bloomington #30026). Transgenic strain. The Orco cDNA was PCR amplified from a plasmid (kindly provided by Dr. Vosshall) and then subcloned into the pJFRC-MUH-20xUAS vector . The plasmid was injected into flies carrying the attP40 docking site (BestGene Inc.). Calcium imaging. Ex vivo calcium imaging was performed as previously described . Larvae were raised with the standard fly food at 25°C under 12-h light/dark conditions. Third instar larvae were washed in 1 × PBS and transferred to adult hemolymph-like (AHL) saline . To expose the larval brain, each larva was dissected, and the larval head was isolated by removing the fat body, the salivary gland, and the digestive system. The nose tip of the larval head was inserted into the hole of 22 mm × 22 mm plastic cover slip (Thermo Fisher Scientific) that was punched with 23 G needle (Terumo Corporation). To fix the brain position, the brain was covered with low-melting agarose (1.0%; LowMelt Agarose, GeneMate) in AHL and coverglass. For odor stimulation, 10 µ l −3 ethyl acetate at 10 dilution was applied manually. Calcium imaging was performed using an Olympus BX51WI (UPlanSApo objective, 40×, NA = 0.75, Olympus), with a Yokogawa CSU10 (Yokogawa, Tokyo, Japan) spinning disk confocal system and an electron-multiplying charge-coupled device (EM-CCD) digital camera (Evolve, Photometrics) . The GCaMP6f −1 signal was obtained at about 20 frames s (exposure time, 50 msec). Motion correction of the obtained mov- ies was performed using Metamorph (Molecular Devices). For calculation of the signal intensities, a region of interest (ROI) was manually selected using Image J software (http://rsb.info.nih.gov/ij/). F was computed as the mean of the 25th percentile of signal intensities in each ROI. ∆F/F was calculated according to (F-F )/F . For 0 0 0 peak detection, σ was calculated from a ΔF/F time series. Peaks were then detected as events that deviated 2σ from the baseline. Peaks were detected and the power spectrum was calculated using MATLAB (http://www. mathworks.com/). For statistical analysis of the frequency of prior activities, Wilcoxon’s rank-sum test, followed by Bonferroni correction, was applied. Optogenetic choice assay. Larvae were raised with the standard fly food containing 1 mM all-trans-retinal at 25 °C in the dark. Third instar larvae were washed in water and transferred into 10-cm diameter agarose gel (Nippon gene) plates. Ten larvae were placed at the center of the plate. This plate was put in the dark experimental chamber. In this chamber, the agarose plate was illuminated by red light. Larvae expressing CsChrimson were allowed to move between two dark quadrants and two illuminated quadrants on the plate. For optogenetic stimulation, larvae on the plate were exposed to light (617 nm, ~35 μW/mm ; M617L3, THORLABS). e Th larval behaviors were recorded −1 at about 1 frame s for 5 min by means of a CCD Camera (1500M-GE, THORLABS). The positions of larvae on the plate were analyzed using Image J sowa ft re. The performance index (PI) was calculated as the number of larval positions detected in the illuminated area, minus the number of larval positions detected in the dark area, divided by the total number of larvae, over a period of 5 min. For statistical analysis of PIs, Wilcoxon’s rank-sum test, followed by Bonferroni correction, was applied. Entering and turning behaviors at the boundary were counted manually. e p Th robability of entering illuminated quadrants from dark quadrants was calculated as the number of larvae that entered illuminated quadrants, divided by the total number of larvae that crossed the boundary from dark quad- rants into illuminated quadrants. e p Th robability of turning back into illuminated quadrants was calculated as the number of larvae that turned back into the illuminated quadrants, divided by the total number of larvae that crossed the boundary from the illuminated quadrants into the dark quadrants. For statistical analysis of these probabilities, Fisher’s exact test, followed by Benjamini−Hochberg correction , was applied. Optical stimulation. Larvae were raised with the standard fly food containing 1 mM all-trans-retinal at 25 °C in the dark. The dissection of larvae and the sample preparation were described in the calcium imaging sec- tion. The stimulation and recording were performed with an Olympus BX51WI upright microscope (UPlanSApo objective, 40×, NA = 0.75, Olympus). For stimulation of ORNs, blue light was illuminated by pE-100 (CoolLED). −1 GCaMP6f and RGECO1 signals were obtained at about 5 frames s (exposure time, 200 ms). Obtained images were essentially analyzed as described in the calcium imaging section. In addition, background correction was performed to reduce the background noise by light stimulation. The images were mean-filtered (radius: 2 pixels) and then the background was subtracted using the rolling ball method (rolling ball radius: 50 pixels). For cal- culation of the fluorescence intensities, a region of interest (ROI) was manually selected using Image J software (http://rsb.info.nih.gov/ij/). F was computed as the mean intensity of nine frames from stimulation onset in each ROI. ∆F/F was calculated as (F-F )/F . 0 0 0 ScIentIfIc REPO R Ts | (2018) 8:8580 | DOI:10.1038/s41598-018-26825-3 9 www.nature.com/scientificreports/ References 1. Saha, D. et al. A spatiotemporal coding mechanism for background-invariant odor recognition. Nat. Neurosci. 16, 1830–1839 (2013). 2. Motokizawa, F. & Ogawa, Y. Discharge properties of mitral/tufted cells in the olfactory bulb of cats. Brain Res. 763, 285–287 (1997). 3. Leng, G., Hashimoto, H., Tsuji, C., Sabatier, N. & Ludwig, M. Discharge patterning in rat olfactory bulb mitral cells in vivo. Physiol. Rep. 2, (2014). 4. Arieli, A., Shoham, D., Hildesheim, R. & Grinvald, A. Coherent spatiotemporal patterns of ongoing activity revealed by real-time optical imaging coupled with single-unit recording in the cat visual cortex. J. Neurophysiol. 73 (1995). 5. Romano, S. A. et al. Spontaneous neuronal network dynamics reveal circuit’s functional adaptations for behavior. Neuron 85, 1070–85 (2015). 6. Luczak, A., Bartho, P. & Harris, K. D. Gating of Sensory Input by Spontaneous Cortical Activity. J. Neurosci. 33 (2013). 7. Hallem, E. A., Ho, M. G. & Carlson, J. R. The molecular basis of odor coding in the Drosophila antenna. Cell 117, 965–79 (2004). 8. Larsson, M. C. et al. Or83b encodes a broadly expressed odorant receptor essential for Drosophila olfaction. Neuron 43, 703–14 (2004). 9. Kreher, S. A., Mathew, D., Kim, J. & Carlson, J. R. Translation of sensory input into behavioral output via an olfactory system. Neuron 59, 110–24 (2008). 10. Hallem, E. A. & Carlson, J. R. Coding of odors by a receptor repertoire. Cell 125, 143–60 (2006). 11. Hoare, D. J., McCrohan, C. R. & Cobb, M. Precise and Fuzzy Coding by Olfactory Sensory Neurons. J. Neurosci. 28, 9710–9722 (2008). 12. Fishilevich, E. et al. Chemotaxis behavior mediated by single larval olfactory neurons in Drosophila. Curr. Biol. 15, 2086–96 (2005). 13. Bellmann, D. et al. Optogenetically induced olfactory stimulation in Drosophila larvae reveales the neuronal basis of odor-aversion behavior. Front. Behav. Neurosci. 4, 27 (2010). 14. Sato, K. et al. Insect olfactory receptors are heteromeric ligand-gated ion channels. Nature 452, 1002–6 (2008). 15. Wicher, D. et al. Drosophila odorant receptors are both ligand-gated and cyclic-nucleotide-activated cation channels. Nature 452, 1007–11 (2008). 16. Prieto-Godino, L. L., Diegelmann, S. & Bate, M. Embryonic Origin of Olfactory Circuitry in Drosophila: Contact and Activity- Mediated Interactions Pattern Connectivity in the Antennal Lobe. PLoS Biol. 10, e1001400 (2012). 17. Cao et al. Odor-evoked inhibition of olfactory sensory neurons drives olfactory perception in Drosophila. Nat. Commun. 8, 1357 (2017). 18. Nolte et al. No Evidence for Ionotropic Pheromone Transduction in the Hawkmoth Manduca sexta. PLoS One 11, e0166060 (2016). 19. Jones, P. L., Pask, G. M., Rinker, D. C. & Zwiebel, L. J. Functional agonism of insect odorant receptor ion channels. Proc. Natl. Acad. Sci. USA 108, 8821–8825 (2011). 20. Sun et al. Identification and characterization of pheromone receptors and interplay between receptors and pheromone binding proteins in the diamondback moth, Plutella xyllostella. PLoS One 8, e62098 (2013). 21. Xia, Y. & Zwiebel, L. J. Identification and characterization of an odorant receptor from the West Nile Virus mosquito, Culex quinquefasciatus. Insect Biochem. Mol. Biol. 36, 169–176 (2006). 22. Tsai-Wen Chen et al. Ultrasensitive fluorescent proteins for imaging neuronal activity. Nature 499(7458), 295–300 (2013). 23. Brand, A. H. & Perrimon, N. Targeted gene expression as a means of altering cell fates and generating dominant phenotypes. Development 118, 401–15 (1993). 24. Asahina, K., Louis, M., Piccinotti, S. & Vosshall, L. B. A circuit supporting concentration-invariant odor perception in Drosophila. J. Biol. 8, 9 (2009). 25. Kreher, S. A., Kwon, J. Y. & Carlson, J. R. The molecular basis of odor coding in the Drosophila larva. Neuron 46, 445–56 (2005). 26. Nakagawa, T., Pellegrino, M., Sato, K., Vosshall, L. B. & Touhara, K. Amino Acid Residues Contributing to Function of the Heteromeric Insect Olfactory Receptor Complex. PLoS One 7, e32372 (2012). 27. Klapoetke, N. C. et al. Independent optical excitation of distinct neural populations. Nat. Methods 11, 338–46 (2014). 28. Zhang, F., Wang, L.-P., Boyden, E. S. & Deisseroth, K. Channelrhodopsin-2 and optical control of excitable cells. Nat. Methods 3, 785–792 (2006). 29. Bellmann, D. et al. Optogenetically Induced Olfactory Stimulation in Drosophila Larvae Reveals the Neuronal Basis of Odor- Aversion behavior. Front. Behav. Neurosci. 4, 27 (2010). 30. Stocker, R. F., Lienhard, M. C., Borst, A. & Fischbach, K. F. Neuronal architecture of the antennal lobe in Drosophila melanogaster. Cell Tissue Res. 262, 9–34 (1990). 31. Berck, M. E. et al. The wiring diagram of a glomerular olfactory system. Elife 5, e14859 (2016). 32. Wagh, D. A. et al. Bruchpilot, a Protein with Homology to ELKS/CAST, Is Required for Structural Integrity and Function of Synaptic Active Zones in Drosophila. Neuron 49, 833–844 (2006). 33. Luczak, A., Barthó, P. & Harris, K. D. Spontaneous Events Outline the Realm of Possible Sensory Responses in Neocortical Populations. Neuron 62, 413–425 (2009). 34. Arieli, A., Sterkin, A., Grinvald, A. & Aertsen, A. Dynamics of Ongoing Activity: Explanation of the Large Variability in Evoked Cortical Responses. Science (80-.). 273, 1868–1871 (1996). 35. Petersen, C. C. H., Hahn, T. T. G., Mehta, M., Grinvald, A. & Sakmann, B. Interaction of sensory responses with spontaneous depolarization in layer 2/3 barrel cortex. Proc. Natl. Acad. Sci. USA 100, 13638–43 (2003). 36. Azouz, R. & Gray, C. M. Cellular Mechanisms Contributing to Response Variability of Cortical Neurons In Vivo. J. Neurosci. 19, 2209–2223 (1999). 37. Fox, M. D., Snyder, A. Z., Vincent, J. L. & Raichle, M. E. Intrinsic fluctuations within cortical systems account for intertrial variability in human behavior. Neuron 56, 171–84 (2007). 38. Bean, B. P. The action potential in mammalian central neurons. Nat. Rev. Neurosci. 8, 451–465 (2007). 39. Cho, R. W. et al. Phosphorylation of Complexin by PKA Regulates Activity-Dependent Spontaneous Neurotransmitter Release and Structural Synaptic Plasticity. Neuron 88, 749–761 (2015). 40. Flavell, S. W. et al. Activity-dependent regulation of MEF2 transcription factors suppresses excitatory synapse number. Science (80-.). 311, 1008–1012 (2006). 41. Hooks, B. M. & Chen, C. Distinct Roles for Spontaneous and Visual Activity in Remodeling of the Retinogeniculate Synapse. Neuron 52, 281–291 (2006). 42. Hernandez-Nunez, L. et al. Reverse-correlation analysis of navigation dynamics in Drosophila larva using optogenetics. Elife 4, (2015). 43. Kanamori, T. et al. Compartmentalized Calcium Transients Trigger Dendrite Pruning in Drosophila Sensory Neurons. Science 80, 340 (2013). 44. Honda, T., Lee, C.-Y., Yoshida-Kasikawa, M., Honjo, K. & Furukubo-Tokunaga, K. Induction of Associative Olfactory Memory by Targeted Activation of Single Olfactory Neurons in Drosophila Larvae. Sci. Rep. 4, 4798 (2015). 45. Wang, J. W. et al. Two-Photon Calcium Imaging Reveals an Odor-Evoked Map of Activity in the Fly Brain. Cell 112, 271–282 (2003). 46. Benjamini, Y. & Hochberg, Y. Controlling the False Discovery Rate: a Practical and Powerful Approach to MultipleTesting. J. R. Stat. Soc. 57, 289–300 (1995). ScIentIfIc REPO R Ts | (2018) 8:8580 | DOI:10.1038/s41598-018-26825-3 10 www.nature.com/scientificreports/ Acknowledgements We would like to thank G. Miesenböck, Bloomington Drosophila Stock Center, and Kyoto Stock Center for fly stocks; L.B. Vosshall for reagents; Y. Dairyo for critical comments and discussion on the experimental design; R. Taniguchi for critical comments and discussion on the manuscript; M. Miyahara and H. Itoh for technical assistance. This work is supported by MEXT Grants-in-Aid for Scientific Research on Innovative Areas “Dynamic regulation of brain function by Scrap & Build system” (KAKENHI 16H06456), JSPS (KAKENHI 16H02504), WPI-IRCN, AMED-CREST (JP18gm0610014), JST-CREST, the Strategic Research Program for Brain Sciences, Toray Foundation, Naito Foundation, Takeda Science Foundation, and Uehara Memorial Foundation to K.E. and by a grant from the National Institutes of Health (NINDS R01 NS076614) to J.P. Author Contributions N.U. and K.E. designed this study and wrote the manuscript; C.W. and J.P. assisted with RNA-Seq analysis; N.U. performed the experiments and analyzed the data. Additional Information Supplementary information accompanies this paper at https://doi.org/10.1038/s41598-018-26825-3. Competing Interests: The authors declare no competing interests. Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations. Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Cre- ative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not per- mitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/. © The Author(s) 2018 ScIentIfIc REPO R Ts | (2018) 8:8580 | DOI:10.1038/s41598-018-26825-3 11
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