1. Neuroscience

Presynaptic inhibition of dopamine neurons controls optimistic bias

  1. Nobuhiro Yamagata  Is a corresponding author
  2. Takahiro Ezaki
  3. Takahiro Takahashi
  4. Hongyang Wu
  5. Hiromu Tanimoto  Is a corresponding author
  1. Graduate School of Life Sciences, Tohoku University, Japan
  2. Research Center for Advanced Science and Technology, The University of Tokyo, Japan
https://doi.org/10.7554/eLife.64907
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Cite this article
  1. Nobuhiro Yamagata
  2. Takahiro Ezaki
  3. Takahiro Takahashi
  4. Hongyang Wu
  5. Hiromu Tanimoto
(2021)
Presynaptic inhibition of dopamine neurons controls optimistic bias
eLife 10:e64907.
https://doi.org/10.7554/eLife.64907
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Abstract

Regulation of reward signaling in the brain is critical for appropriate judgement of the environment and self. In Drosophila, the protocerebral anterior medial (PAM) cluster dopamine neurons mediate reward signals. Here, we show that localized inhibitory input to the presynaptic terminals of the PAM neurons titrates olfactory reward memory and controls memory specificity. The inhibitory regulation was mediated by metabotropic gamma-aminobutyric acid (GABA) receptors clustered in presynaptic microdomain of the PAM boutons. Cell type-specific silencing the GABA receptors enhanced memory by augmenting internal reward signals. Strikingly, the disruption of GABA signaling reduced memory specificity to the rewarded odor by changing local odor representations in the presynaptic terminals of the PAM neurons. The inhibitory microcircuit of the dopamine neurons is thus crucial for both reward values and memory specificity. Maladaptive presynaptic regulation causes optimistic cognitive bias.

Introduction

Regulation of reward signaling in the brain is critical for maximizing positive outcomes and for avoiding futile costs of the behaviors at the same time. Across animal phyla, dopamine neurons are primarily involved in reward processing (Brembs et al., 2002; Tobler et al., 2005; Liu et al., 2012; Ichinose et al., 2017). In the fruit fly Drosophila melanogaster, a subset of dopamine neurons in the protocerebral anterior medial (PAM) cluster mediates the reinforcement property of sugar reward (Burke et al., 2012; Liu et al., 2012). In olfactory learning, dopamine input to the mushroom body (MB) causes changes in preference of a simultaneously presented odor by modulating the output of odor-representing MB intrinsic neurons, Kenyon cells (KCs) (Séjourné et al., 2011; Boto et al., 2014; Cohn et al., 2015; Owald et al., 2015; Louis et al., 2018; Hige et al., 2015; Bilz et al., 2020). Such associative presentations of odor and electric shocks were reported to change the activity of MB-projecting dopamine neurons (Riemensperger et al., 2005). Recent studies (Hattori et al., 2017; Cervantes-Sandoval et al., 2017; Takemura et al., 2017) suggest that axon terminals of the dopamine neurons locally integrate olfactory inputs to function as multiple independent units, though such subcellular reward processing has yet to be examined.

Results and discussion

To understand neuronal mechanisms for the regulation of reward processing, we here focused on gamma-aminobutyric acid (GABA) signaling in the PAM neurons. Six GABA receptor genes are identified in the fly genome. We silenced the expression of each receptor gene in the PAM cluster neurons by targeting transgenic RNAi (Ni et al., 2011) and tested their appetitive olfactory memory (Figure 1A). We found increased memory performance by downregulation of a metabotropic GABA receptor, GABA-B-R3 (Figure 1A and Figure 1—figure supplement 1A-B).

Figure 1 with 1 supplement see all
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Gamma-aminobutyric acid (GABA)-B-R3 suppresses sugar reward.

(A) Cell type-specific GABA receptor silencing in the protocerebral anterior medial (PAM) neurons directed by R58E02-GAL4, showing GABA-B-R3-specific memory increment. *q < 0.008 (Benjamini and Hochberg method, N = 8, 23). Mean ± SEM are shown hereafter. (B) Acute silencing of GABA-B-R3 in the PAM neurons using Tub-GAL80ts and heat-induced inactivation. *p<0.05 (Sidak’s test, N = 10, 12; Dunn’s multiple comparisons test, N = 7, 8). (C, D) A substack projection image and a single optical slice showing endogenous GABA-B-R3 expression in somata of PAM neurons (C) and their axon terminal profiles in the mushroom body (MB) (D) by using GABA-B-R3-T2A-GAL4. Anti-tyrosine hydroxylase (TH) antibody signal (magenta) for labeling PAM neurons. Scale bars, 100 μm (C), 20 μm (D). (E) Memory acquisition curves of knock-down and control flies. Hyperbola curve fitting and subsequent permutation tests (Figure 1—figure supplement 1E–F) reveal an altered plateau level but not the acquisition speed in knock-down flies. N = 12. (F) Superimposed and color-coded sugar-evoked calcium signal (ΔF/F0) in a subset of PAM neurons measured in R15A04-GAL4/UAS-GCaMP6s, UAS-mCD8::RFP flies. (G) Time course of the calcium transients in defined compartments of the MB in control (left) and GABA-B-R3 knock-down (right) flies. Gray shades indicate sugar stimulation for 3 s. Mean ± SEM, N = 7, 8. (H) GABA-B-R3 knock-down significantly increases sugar-evoked peak calcium transients in γ5 and α1 neurons. *p<0.05 (Holm-Sidak’s test, N = 7, 8).

Figure 1—source data 1

GABA receptor silencing in the PAM neurons and the effects on appetitive memory.

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Figure 1—source data 2

Acute suppression of GABA-B-R3.

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Figure 1—source data 3

Memory acquisition curve in control and GABA-B-R3 knock-down flies.

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Figure 1—source data 4

Sugar response in the PAM neurons in control and GABA-B-R3 knock-down flies.

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We next examined endogenous GABA-B-R3 expression in the adult brain using the intronic CRISPR-Mediated Integration Cassette (CRIMIC) insertion of T2A-GAL4 (Lee et al., 2018). The T2A self-cleaving peptide between the target protein and GAL4 allows bi-cistronic translation by a ribosome skipping mechanism (Diao and White, 2012). GABA-B-R3 was expressed broadly in the brain, including the majority of the PAM cluster neurons (Figure 1C–D), whereas the expression was weak in KCs (Figure 1D and Figure 1—figure supplement 1C). There was no notable morphological alteration in the brain of knock-down flies (data not shown). Consistently, adult stage-specific GABA-B-R3 silencing in the PAM neurons using Tub-GAL80ts (McGuire et al., 2003) similarly enhanced appetitive memory performance (Figure 1B). Without transgene induction, their appetitive memory was indistinguishable from the controls (Figure 1B).

Increased learning speed and/or performance plateau may underlie the enhanced appetitive memory in the GABA-B-R3 knock-down flies. We attempted to distinguish these possibilities by characterizing their memory acquisition (Figure 1E and Figure 1—figure supplement 1D). The performance of R58E02-GAL4/UAS-GABA-B-R3-RNAi flies reached a significantly higher asymptote than control genotypes without changing the acquisition speed (Figure 1E and Figure 1—figure supplement 1E–F). In a learning theory, the magnitude of reinforcement is the determinant for the plateau of the acquisition curve (Rescorla, 1972), suggesting that sugar reward was perceived more strongly with enhanced dopaminergic activity in the GABA-B-R3 knock-down flies. Live calcium imaging at terminal branches of the reward-related PAM neurons (i.e., PAM-γ5 and -α1) revealed the augmented sugar responses upon downregulating GABA-B-R3 (Figure 1F–H). We thus conclude that GABA-B-R3 signaling is required for negative regulation of the sugar reward.

We visualized the localization of GABA-B-R3 proteins using a GFP-tagged reporter (Sarov et al., 2016). GABA-B-R3 proteins were heavily localized to the presynaptic terminals of the PAM neurons (Figure 2A–B and Figure 2—figure supplement 1A). We thus hypothesized that presynaptic inhibition of dopamine neurons within the MB controls the gain of reward signals. A single pair of the GABAergic anterior paired lateral (APL) neurons was reported to massively innervate the entire MB and to be involved in olfactory learning (Liu and Davis, 2009). Differential labeling of the PAM and APL neurons revealed that their ramifications abut on each other (Figure 2C–D). Consistently, we found enhanced reward memory in knock-down flies for glutamic acid decarboxylase 1 (Gad1) and vesicular GABA transporter (VGAT) in the APL neuron (Figure 2E). This result not only underscores the importance of GABA metabolism in the APL neurons, but suggests the role of the inhibitory microcircuit in the MB for the gain control of the reward value. We therefore examined the local inhibition hypothesis by comparing sugar responses in the dendrites and presynaptic terminals of the PAM neurons (Figure 2F and Figure 2—figure supplement 1B–C). The enhanced calcium activity upon GABA-B-R3 knock-down was much more pronounced in the presynaptic terminals (Figure 2G–H). Therefore, GABAergic signals from the APL neurons negatively control the reward gain at the output site of the PAM neurons through GABA-B-R3 signaling in the MB.

Figure 2 with 1 supplement see all
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Presynaptic GABAergic inhibition of the protocerebral anterior medial (PAM) neurons.

(A) A schematic showing brain regions visualized in subsequent figures. (B) A substack projection image of double labeling of GFP-tagged GABA-B-R3 protein and PAM neurons using GABA-B-R3-sfGFP-TVPTBF, R58E02-GAL4/UAS-mCD8::RFP fly. Presynaptic localization of GABA-B-R3 protein in the γ5 and α1 (Figure 2—figure supplement 1A) compartments of the mushroom body (MB). Scale bar, 10 μm. (C–D) A substack projection image showing double labeling of the PAM and anterior paired lateral (APL) neurons visualized by VT43924-GAL4/UAS-mCD8::RFP, R58E02-LexA/LexAop-rCD2::GFP. These axonal profiles co-localize at close proximity in the MB. A single optical slice of the inset in C is magnified in D. Scale bars, 10 μm (C), 2 μm (D). (E) Increased appetitive memory score by shRNA-mediated silencing of GABA neurotransmission-related genes in the APL neurons. *p<0.05 (Sidak’s test, N = 11–13). (F) A cartoon depicting volumetric imaging from axon terminals and dendritic fields of PAM neurons using a z-objective piezo actuator. (G) Time course of calcium transients (ΔF/F0) near-simultaneously recorded from axon terminals and dendrites of PAM-γ5 neurons (Figure 2—figure supplement 1) of control (left) and GABA-B-R3 knock-down (right) flies. Gray shades indicate sugar stimulation for 3 s. Mean ± SEM, N = 5. (H) Significantly increased sugar-evoked peak calcium transients of GABA-B-R3 knock-down flies in axon terminals. *p<0.05 (Dunn’s test, N = 6, 7).

Figure 2—source data 1

Inhibition of GABA neurotransmission in APL neurons.

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Figure 2—source data 2

Sugar response in the axon terminals and dendrites of the PAM neurons.

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To quantify the local activity regulation in the PAM terminals, we measured calcium influx at active zones using the ratiometric calcium sensor Brp::GCaMP6s::mCherry (Kiragasi et al., 2017). This sensor is composed of GCaMP fused to calcium insensitive mCherry and targeted to active zones using the short fragment of Brp, enabling the measurement of local calcium influx at active zones (Kiragasi et al., 2017). Immunolabelling confirmed the localization of the sensor proteins to active zones of the PAM neurons in the MB (Figure 3A and Figure 3—figure supplement 1A).

Figure 3 with 1 supplement see all
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Gamma-aminobutyric acid (GABA)-B-R3 controls presynaptic activity patterns in the protocerebral anterior medial (PAM) neurons.

(A) A single optical slice showing punctate sensor localization in the mushroom body (MB) lobe of R15A04-GAL4/UAS-Brp::GCaMP6s::mCherry flies. Scale bar, 10 μm. (B) The histograms of GFP/RFP signals from nine different time points (PAM-α1 terminals) reveal a large calcium diversity among active zones and the temporal instability in the knock-down fly (right). The probability distribution of the active-zone calcium mostly followed the Gaussian distribution, characteristics of which are well represented by the mean and standard deviation (SD). Scale bar, 0.01. (C) The temporal variance of spatially averaged intensities is larger in the GABA-B-R3 knock-down PAM neurons. *p<0.001 (Mann-Whitney test, N = 24, 17). (D) Time course of odor-evoked calcium transient (mean) and the variance (SD) of PAM-α1 terminals in control (left) and GABA-B-R3 knock-down (right) flies. The blue shade indicates odor stimulation for 3 s. Mean ± SEM, N = 6–8. (E) Map of the probability distribution of active-zone calcium intensity in the PAM-α1 terminals for each individual. The abscissa and ordinate represent the mean and SD of the signal distribution, respectively. The clear inverse correlation between the mean and the variance in wild-type terminals (r = −0.82, p<10−6) may represent individually defined unique set points of activity levels. This structured individual difference is disrupted by GABA-B-R3 RNAi (r = 0.53, p=0.03). The start and end of an arrow represent the probability distribution of active-zone calcium before and during the odor stimulation, respectively. Scale bar, 0.5 in Log10(GCaMP6s/mCherry). (F) Local peaks in the PAM terminals are color-coded for their cluster sizes (right). Schematic example of the algorithm finding the cluster structure applied to a one-dimensional system (Left). Spatial distribution of calcium intensity (Left upper). Finding steepest paths from each pixel to local peaks by computing the gradient (i.e., the difference of the intensity values between neighboring pixels)(Left middle). Note that in two-dimensional systems we analyzed, each pixel had four neighboring pixels. Clustering based on the paths to local peaks (Left lower). Pixels having the same destination (i.e., local peak) are clustered together. (G) The average area per peak is significantly larger in the GABA-B-R3 knock-down flies during baseline activity (*p<0.05, Mann-Whitney test, N = 22, 17) and odor stimulation (*p<0.05, t-test, N = 15, 11).

Figure 3—source data 1

Temporal variance of spatially averaged intensities in control and GABA-B-R3 knock-down flies.

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Figure 3—source data 2

Probability distribution of active-zone calcium intensity before and during odor stimulation.

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Figure 3—source data 3

Average cluster size in control and GABA-B-R3 knock-down flies.

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As the basal activities of dopamine neurons represent physiological information (Ichinose et al., 2017), we characterized the regulation of active zone calcium in the PAM terminals without overt stimulation. Live imaging of punctate Brp::GCaMP6s::mCherry signals in the PAM terminals visualized a large heterogeneity of calcium levels among active zones (Figure 3B, Figure 3—figure supplement 1B and Figure 3—figure supplement 1C). This heterogeneity tended to increase upon silencing GABA-B-R3 (Figure 3—figure supplement 1D). Furthermore, we found that Brp::GCaMP6s::mCherry signals had temporal fluctuations, which was amplified by silencing GABA-B-R3 (Figure 3B and Figure 3C). GABA-B-R3 in the PAM terminals may thus stabilize the basal presynaptic activity. This suggests that GABA inhibition contributes to the robustness of activity against local perturbations.

System robustness is often related to refined regulation of activity patterns by which information is efficiently coded (Hesse and Gross, 2014). As active-zone calcium in the PAM terminals is likely to reflect local input in the MB (see Figure 2G and H), we hypothesized that GABA-B-R3 controls the spatial representation of odor information in the PAM terminals. In control flies, odor presentations barely changed the distribution of active-zone calcium with a marginal increase of the overall signal intensity (Figure 3D–E and Figure 3—figure supplement 1C). In contrast, sugar ingestion induced global presynaptic calcium increase and decreased the signal heterogeneity (Figure 3—figure supplement 1D). These stimulus-specific presynaptic responses are likely to reflect differential input sites of odor and sugar signals, that is, pre- and post-synaptic sites of the PAM neurons, respectively. Strikingly, GABA-B-R3 knock-down flies responded to an olfactory stimulation much more strongly (Figure 3D–E), as if in response to a global sugar stimulation (Figure 3—figure supplement 1D). These results suggest that the local control of PAM presynaptic activity by GABA-B-R3 regulates the odor responses, possibly by refining its spatial representation.

To further characterize how GABA-B-R3 regulates the structure of presynaptic activity in PAM terminals, we examined the patterns of local peaks of Brp::GCaMP6s::mCherry signals by introducing a spatial measure. We found that the average peak area (i.e., cluster size) became larger upon knocking down GABA-B-R3 both before and during the odor stimulation (Figure 3F–G). Note that we did not observe a clear correlation between the cluster size and intensity of pixels in the cluster (data not shown), suggesting that the cluster size measure provides information orthogonal to the intensity value of calcium signals. We also quantified the size of high-intensity pixels using another measure, which we call peak size (see Materials and methods; Figure 3—figure supplement 1F). We further found that intense Brp::GCaMP6s::mCherry signals are more spatially clustered in the knock-down PAM terminals, further corroborating the fine spatial regulation of calcium signals by GABA-B-R3. Since KC and PAM terminals form mutual synapses in the MB lobe (Takemura et al., 2017; Cervantes-Sandoval et al., 2017), the overall disinhibition in the knock-down terminals may impair the selective delivery of dopaminergic reward signals to odor-activated KCs.

To test if presynaptic GABA-B-R3 signaling controls odor representations, we examined the specificity of memory using odor generalization. Conditioned odor approach of wild-type flies drops by increasing the blend ratio of a contaminant odor to the trained odor (Ichinose et al., 2015; Chen et al., 2017). Strikingly, the downregulation of GABA-B-R3 in the PAM neurons resulted in a broader generalization profile, indicating that reward memory in the knock-down flies is less specific to the learned odor (Figure 4A–B). Moreover, we found similarly broadened generalization profiles by downregulating GAD1 expression in the APL neurons (Figure 4C–D). We altogether conclude that local GABAergic inhibition of the PAM neurons regulates the intensity and specificity of reward memory (Figure 4E).

Figure 4
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Compromised odor specificity in the rewarded memory by attenuating local gamma-aminobutyric acid (GABA) signaling in the mushroom body.

(A–D) Olfactory generalization of appetitive memory depends on the blend ratio of a contaminant to a trained odor 4-methylcyclohexanol (4MCH) (A, C) or octan-3-ol (3OCT) (B, D). Significantly broader generalization in R58E02-GAL4/UAS-GABA-B-R3-RNAi flies (A, B) and VT43924-GAL4/UAS-Gad1-RNAi flies (C, D) compared to the respective parental controls. *p<0.05; ***p<0.001 (Sidak’s test across genotypes at each blend ratio, N = 8–20 [A, B], N = 9–12 [C, D]). (E) A model for dual behavioral roles of GABA-B-R3 in the protocerebral anterior medial (PAM) terminal in the mushroom body (MB). GABA-B-R3 controls the overall gain (left) and localization (right) of sugar- and odor-evoked terminal activity of PAM neurons, respectively. Note that input sources of sugar and odor response are different. In an odor response, reciprocal PAM-KC (Kenyon cell) synapses serve as KC activity-dependent local enhancers for reward signaling from the PAM synapses. In wild-type flies, this local modulation is restricted to the PAM synapses onto the odor-activated KCs, which laterally inhibit activities of surrounding ones via KC-APL (anterior paired lateral) feedback. GABA-B-R3 knock-down in the PAM neurons eliminates this negative feedback from the APL, reducing the activity contrast within presynaptic terminals of the PAM neurons and the selectivity of memory to the rewarded odor.

Figure 4—source data 1

Olfactory generalization of appetitive memory in control and GABA-B-R3 knock-down flies (4MCH).

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Figure 4—source data 2

Olfactory generalization of appetitive memory in control and GABA-B-R3 knock-down flies (3OCT).

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Figure 4—source data 3

Olfactory generalization of appetitive memory in control and Gad1 knock-down flies (4MCH).

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Figure 4—source data 4

Olfactory generalization of appetitive memory in control and Gad1 knock-down flies (3OCT).

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Our results indicate that presynaptic modulation of the PAM neurons is a critical component for determining the magnitude of dopaminergic reward signals. Notably, abolition of the local GABAergic input to the PAM terminals not only enhanced the internal reward intensity but compromised memory specificity (Figures 1 and 4). These behavioral alterations can be explained by a dual physiological role of GABA-B-R3, that is, the gain control and the spatial segmentation of dopaminergic reward signals in the PAM terminals (Figure 4E). As the behavioral traits caused by the downregulation of GABA-B-R3 are characteristic in optimism (Carver et al., 2010; Solvi et al., 2016), presynaptic control of reward signals may underlie such a cognitive bias. It would be fruitful to examine if a similar subcellular modulation of punishment-mediating neurons conversely leads to the pessimistic bias (Sharot et al., 2009; Bateson et al., 2011; Sharot et al., 2012; Kregiel et al., 2016; Solvi et al., 2016; Zidar et al., 2018).

Materials and methods

Key resources table
Reagent type (species) or resourceDesignationSource or referenceIdentifiersAdditional information
Genetic reagent (Drosophila melanogaster)GMR58E02-GAL4Bloomington Drosophila Stock CenterBDSC: 41347; FLYB: FBal0253714; RRID:BDSC_41347
Genetic reagent (Drosophila melanogaster)GMR15A04-GAL4Bloomington Drosophila Stock CenterBDSC: 48671; FLYB: FBtp0057752; RRID:BDSC_48671
Genetic reagent (Drosophila melanogaster)VT043924-GAL4Vienna Drosophila Resource CenterVDRC: v201194; FLYB: FBtp0105273;
Genetic reagent (Drosophila melanogaster)UAS-GABA-B-R3-RNAiBloomington Drosophila Stock CenterBDSC: 50622; FLYB: FBti0157477; RRID:BDSC_50622FlyBase symbol:P{TRiP.HMC02989}attP40
Genetic reagent (Drosophila melanogaster)UAS-mCD8::GFPBloomington Drosophila Stock CenterBDSC: 32194; FLYB: FBti0131936; RRID:BDSC_32194FlyBase symbol: P{20XUAS-IVS-mCD8::GFP}
Genetic reagent (Drosophila melanogaster)UAS-GCaMP6sBloomington Drosophila Stock CenterBDSC: 42746; FLYB: FBti0151344; RRID:BDSC_42746FlyBase symbol: P{20XUAS-IVS-GCaMP6s}
Genetic reagent (Drosophila melanogaster)GABA-B-R3-sfGFP-TVPTBFBloomington Drosophila Stock CenterVDRC: v318614; FLYB: FBst0491638;FlyBase symbol: PBac{fTRG00613.sfGFP-TVPTBF}
Genetic reagent (Drosophila melanogaster)UAS-GCaMP6s.brpS.mCherryBloomington Drosophila Stock CenterBDSC: 77131; FLYB: FBtp0125966;
RRID:BDSC_77131
Antibody(Rabbit polyclonal) anti-GFPInvitrogenCat# A11122; RRID:AB_221569(1:1000)
Antibody(Mouse monoclonal) anti-THImmunoStarCat# 22941; RRID:AB_1267100(1:100)
Antibody(Rabbit polyclonal) anti-DsRedClontechCat# 632496; RRID:AB_10013483(1:200)
Antibody(Mouse monoclonal) anti-BrpDevelopmental Studies Hybridoma BankCat# nc82; RRID:AB_2314866(1:20)
Software, algorithmGraphPad Prism 5GraphPad Software, San Diego, CA, 2007https://www.graphpad.com/
Software, algorithmFijiMPI-CBGhttps://fiji.sc/

Flies

Canton-S was used as a wild-type strain. w;;R58E02-GAL4, w;R58E02-LexA, and w;;R15A04-GAL4 (Jenett et al., 2012; Liu et al., 2012), yv;UAS-Grd-RNAi (#58175), yv;UAS-Lcch3-RNAi (#50668), yv;UAS-Rdl-RNAi (#52903), yv;UAS-GABA-B-R1-RNAi (#51817), yv;UAS-GABA-B-R2-RNAi (#50608), yv;UAS-GABA-B-R3-RNAi (#50622), UAS-Gad1-RNAi (#51794), and UAS-VGAT-RNAi (#41958) (Ni et al., 2011), yw;GABA-B-R3-T2A-GAL4 (#78976) (Lee et al., 2018), w;;UAS-mCD8::GFP (#32194) (Pfeiffer et al., 2010), Tub-GAL80ts (McGuire et al., 2003), w;UAS-GCaMP6s (#42746) (Chen et al., 2013), w;;LexAop-rCD2::GFP (Miyamoto et al., 2012), w;;VT043924-GAL4 (v201194) (Wu et al., 2013), GABA-B-R3-sfGFP-TVPTBF (v318614) (Sarov et al., 2016), and UAS-GCaMP6s.brpS.mCherry (#77131) (Kiragasi et al., 2017) were previously described. w;UAS-mCD8::RFP is a gift from Dr Ilona Kadow. Flies were raised at 24°C with 12:12 LD cycle. Knock-down flies were prepared as the F1 progeny of the crosses between females of w;;R58E02-GAL4 or w;UAS-Tub-GAL80ts;R58E02-GAL4 or w and males of UAS effectors or CS (Figures 1A–B, E and 4A–B and Figure 1—figure supplement 1A–B), or females of UAS effectors or w and males of w;;VT043924-GAL4 or w (Figures 2E and 4C–D). The F1 progeny was raised at 24°C, aged to 6–12 days after eclosion before experiments. For the adult-specific knock-down experiment (Figure 1B), the F1 progeny was raised at 18°C and aged to 9–14 days after eclosion. For immunohistochemistry, a female reporter strain w;;UAS-mCD8::GFP (Figure 1C–D) or w;UAS-mCD8::RFP;LexAop-rCD2::GFP (Figure 2C–D) or w;UAS-mCD8::RFP;R58E02-GAL4 (Figure 2B) or UAS-GCaMP6s.brpS.mCherry (Figure 3A and Figure 3—figure supplement 1A) was crossed to male GAL4 drivers or a reporter strain, yw;GABA-B-R3-T2A-GAL4, w;R58E02-LexA;VT043924-GAL4, GABA-B-R3-sfGFP-TVPTBF, or w;;R15A04-GAL4. Flies used for whole-mount immunohistochemistry were aged to 3–10 days after eclosion. For calcium imaging experiments, males of w;UAS-GCaMP6s,UAS-mCD8::RFP (Figures 1F–H and 2F–H) or UAS-GCaMP6s.brpS.mCherry (Figure 3B–G) were crossed to w;;R15A04-GAL4 or w;UAS-GABA-B-R3-RNAi;R15A04-GAL4 females and raised at 24°C, aged to 3–8 days after eclosion, typically. For detailed fly genotypes used for experiments, see supplementary file 1.

Behavioral assays

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The conditioning and testing protocols were as described previously (Yamagata et al., 2015; Yamagata et al., 2016). Briefly, for a normal sugar learning experiment (Figures 1A–B and 2E and Figure 1—figure supplement 1A–B), a group of approximately 50 flies in a training tube alternately received octan-3-ol (3OCT; Merck) and 4-methylcyclohexanol (4MCH; Sigma-Aldrich) for 1 min in a constant air stream with or without dried 2 M sucrose paper. For varied training duration protocol (Figure 1E and Figure 1—figure supplement 1D), flies received two odors and dried sugar alternately for defined duration (10–120 s) with an interval of 1 min between two odors. For odor generalization protocol (Figure 4A–D), flies were trained with an odor, that is, they alternately received 4MCH and paraffin oil (Sigma-Aldrich), or 3OCT and paraffin oil, for 1 min in a constant air stream with or without dried 2 M sucrose paper. Then the conditioned response of the trained flies was measured. For the normal protocol (Figures 1A–B, E and 2E, Figure 1—figure supplement 1A-B, D), flies were given a choice between CS+ and CS- for 2 min in a T maze. For generalization protocol (Figure 4A–D), flies were given a choice between a ‘trained’ odor with a respective mixture ratio of a contaminant odor (2-methylcyclohexanol [2MCH]; Sigma-Aldrich or 1-octen-3-ol [1OCT]; Sigma-Aldrich) and the solvent for 2 min in a T maze. All odors were diluted to 10% in the paraffin oil and placed in a cup with a diameter of 3 mm (OCT) or 5 mm (MCH). The memories were tested immediately after training unless otherwise stated. A learning index was then calculated by taking the mean preference of the two reciprocally trained groups. A half of the trained groups received reinforcement together with the first presented odor, and the other half with the second odor to cancel the effect of the order of reinforcement.

Brain dissection, immunohistochemistry, and sample mounting

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Dissection of fly brains was performed as previously described (Kondo et al., 2020) with minor modifications. Brains of female (Figures 1C–D, 2B–D and 3A, Figure 2—figure supplement 1A–B and Figure 3—figure supplement 1A) flies were dissected in PBS, pre-fixed in 1% paraformaldehyde (PFA) in PBS on ice up to 30 min, then fixed in 2% PFA in PBS for 1 hr at room temperature. Fixed brains were washed in PBT (0.1% Triton X-100 in PBS) for 3 × 10 min. Immunostaining was performed as previously described (Kondo et al., 2020). The following primary antibodies were used at the indicated dilution: rabbit anti-GFP (1:1000; Invitrogen; A11122), mouse anti-TH (1:100; ImmunoStar Inc; 22941), rabbit anti-DsRed (1:200; Clontech, 632496), or mouse anti-Brp (1:20; DSHB; nc82). The following secondary antibodies were used at the indicated dilution: AlexaFluor-488 goat anti-rabbit (1:1000; Invitrogen; A11034), Cy3 goat anti-rabbit (1:200; Jackson Labs), AlexaFluor-568 goat anti-mouse (1:1000; Invitrogen; 11004), AlexaFluor-568 goat anti-rabbit (1:250; Invitrogen; A11036), AlexaFluor-633 goat anti-mouse (1:200; Invitrogen; A21052). In Figure 1C and D and Figure 2—figure supplements 1B, 86% glycerol was used as a mounting medium, and the native GFP fluorescence was imaged without immunohistochemistry. In Figures 2B–D and 3A, Figure 2—figure supplement 1A and Figure 3—figure supplement 1A, SeeDB2 (Ke et al., 2016) was used as mounting medium and either native or immunostained fluorescence was imaged.

Confocal imaging

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Imaging was performed on the Olympus FV1200 confocal microscope with GaAsP sensors. A 30×/1.05 silicone immersion objective (UPLSAPO30XS, Olympus) (Figure 1C–D and Figure 2—figure supplement 1B), or a 60×/1.42 oil immersion objective (PLAPON60XO, Olympus) (Figures 2B–D and 3A, Figure 2—figure supplement 1A and Figure 3—figure supplement 1A) was used for scanning specific regions of interest (ROIs). A final voxel size of the image was 0.17 × 0.17 × 0.76 μm3 (Figure 1C–D), 0.11 × 0.11 × 0.45 μm3 (Figure 2B and Figure 2—figure supplement 1A), 0.21 × 0.21 × 0.43 μm3 (Figure 2C–D), 0.10 × 0.10 × 0.45 μm3 (Figure 3A), 0.51 × 0.51 × 0.68 μm3 (Figure 2—figure supplement 1B), and 0.79 × 0.79 × 0.37 μm3 (Figure 3—figure supplement 1A), respectively. Confocal stacks were analyzed with the open-source software ImageJ (National Institute of Health) and Fiji (Schindelin et al., 2012). Where appropriate, 2D/3D image deconvolution was applied using Diffraction PSF 3D and Parallel Iterative Deconvolution plugins in ImageJ.

Fly preparation and in vivo calcium imaging

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Flies were treated as described in Hiroi et al., 2013; Shiozaki and Kazama, 2017 with some modifications. The fly was briefly (<1 min) anesthetized on ice and placed in a custom-made holding device on a Peltier plate (CP-085, Scinics) held at 4°C. The head capsule was fixed to the dish by UV curing optical adhesives (NOA68, Thorlabs). The proboscis was glued onto the capsule to eliminate brain movement. Forelegs interfering sugar feeding during recordings were removed. A small window on the top of the head capsule was opened using sharp forceps in Drosophila saline (103 mM NaCl [31320–05, Nacalai tesque], 3 mM KCl [28514–75, Nacalai tesque], 5 mM TES [32810–55, Nacalai tesque], 8 mM Trehalose [Tokyo kasei kogyo], 10 mM D-glucose [16806–25, Nacalai tesque], 26 mM NaHCO3 [31213–15, Nacalai tesque], 1 mM NaH2PO4 [A0110846 010, Merch], 1.5 mM CaCl2 [C5080, Sigma-Aldrich], 4 mM MgCl2 [M2670, Sigma-Aldrich], ~270 mol/kg, pH ~7.2). Air sacs and fat bodies covering the brain surface were carefully removed.

A laser scanning confocal microscope (A1R, Nikon) equipped with a 30×/1.1 water immersion objective (Apo LWD 25×, Nikon) and a Piezo nanopositioner (Nano-F450, MCL Inc) combined with a Nano-Driveone controller (MCL Inc) was used for live imaging. GCaMP6s and mCD8::RFP or mCherry were sequentially excited at 488 and 561 nm, respectively. The emission light was collected onto GaAsP detectors using dichroic mirrors and emission filters (BP500–550 and BP570-620). Transverse sections of the MB lobes and the superior medial protocerebrum were scanned at a resolution of 0.5 μm/pixel (512 × 128 pixels) at 333 ms/frame (Figure 1F–H), 0.5 μm/pixel (512 × 256 pixels) at 1 s/frame (Figure 2G–H and Figure 2—figure supplement 1C), or 0.33 μm/pixel (512 × 128 pixels) at 1 s/frame (Figure 3B–E and Figure 3—figure supplement 1A–D) with line scans with 4× (Figures 1F–H and 2G–H and Figure 2—figure supplement 1C) or 16× (Figure 3B–E and Figure 3—figure supplement 1) averages using the resonant scanning mode. The pinhole was set to 2.5 AU (561 nm). For 3D imaging, two z sections (ca. 100 μm interval) were scanned using a piezoelectric motor. To record calcium responses to sugar and odors, images were acquired for 20 or 30 s and saved for later image processing. For sugar stimulation, a droplet of 500 mM sucrose deposited on a tip of Microloader pipette tip (Eppendorf) was presented to the proboscis for 3 s using a micromanipulator (UN-3C, Narishige). Sugar stimulation to flies was monitored with a USB camera (Grasshopper3, FLIR) mounted with a zoom lens (MACRO ZOOM 0.3×−1 × 1:4.5, Computar) and captured by FlyCapture2 (FLIR). Odor stimulation has been made manually using a 50 ml syringe containing a piece of filter paper (1 × 2 cm2) soaked with pure or 10 times diluted 4MCH and 3OCT. For each stimulation, ~15 ml odor contained air was delivered to a fly in 3 s through a 4 mm silicon tube placed ca. 10 mm away from the fly head.

Data analyses

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All the acquired images were first processed with Fiji. An object in each recording was stabilized by TurboReg plugin (Thévenaz et al., 1998) using mCD8::RFP or mCherry signal. ROIs to be involved in later calculations were defined by mCD8::RFP signal in the left or right hemisphere. In Figures 1F–H and 2F–H and Figure 2—figure supplement 1C, GCaMP6s signal was used as a fluorescent F value. The ΔF/F0 was calculated as:

ΔF/F0=Ft−F0F0,

where Ft and F0 denote fluorescent values at time frame t and baseline (i.e., ~7 frames before stimulation), respectively. To highlight MB compartments that responded to stimulations (Figure 1F), a time series projection of the ΔF/F0 during stimulation (for 3 s) was thresholded and superimposed on a projection image of mCD8::RFP signal at respective frames.

After XY registration, the Brp::GCaMP6s signal was divided by mCherry (GCaMP6s/mCherry) to normalize the calcium signal by Bruchpilot abundance. An ROI for the α1 compartment of the MB was defined by mCherry signal. Pixels devoid of an mCherry fluorescence value were censored. The image stacks were then imported to Matlab (MathWorks) and log-transformed.

To evaluate the spatial pattern of the calcium intensity in the PAM-α1 terminals, we computed the size of the area of each peak (Figure 3F) in the following manner: (i) For each pixel in an image, the pixel with the largest intensity value among the four neighboring pixels was identified. If the given pixel had a larger intensity value than those of the neighboring pixels, we recorded the pixel as a local peak. We ignored pixels that had the background intensity value. This procedure yielded the steepest path to a local peak from each pixel. (ii) We clustered the pixels based on the local peak connected by the paths. Note that this simple algorithm is a discrete version of the gradient ascent algorithm and used for clustering with height information elsewhere (Ezaki et al., 2017). (iii) We counted the number of pixels belonging to the same cluster and computed the average cluster size for each fly based on nine frames before stimulation (or three frames during the stimulation). Because the average cluster size may be affected by the size and shape of the PAM-α1 terminals in the recorded images, we normalized it by a null model. The average cluster size for the null model was obtained as follows. (iv) For each image, we shuffled the intensity values across the pixels. (v) We computed the average cluster size for the shuffled image by performing (i)–(iii). (vi) We repeated (iv) and (v) for 1000 runs. (vii) Finally, we calculated the average cluster size for the null model by averaging the results over the 1000 runs and nine frames before stimulation (or three frames during the stimulation). This value was used for normalization in Figure 3F.

In addition to the cluster size analysis above, we used another measure (i.e., peak size) to quantify the spatial structure of the calcium intensity. The peak size was computed for each image as follows. First, we collected the pixels that had an intensity value larger than 95 percentile of the entire pixels in each image. Then, we identified the clusters of these selected pixels by checking if multiple pixels (peaks) were adjacent to each other at the top, bottom, left, or right. Finally, we counted the number of pixels in each cluster and computed the average. Similarly to the cluster size measure above, we normalized this value by using a null model. We computed the peak size for 1000 randomized images that were obtained by shuffling the intensity values in the pixels in the original image. The results were averaged over the 1000 null data, which we used for the normalization.

Statistics

Statistics were performed by Eclipse (Eclipse foundation) and Prism5 (Graphpad). For the data points that did not violate the assumption of normality and homogeneity of variance (D’Agostino and Brown-Forsythe test), parametric statistics were applied. The data points that were significantly different from the normal distribution were analyzed with nonparametric statistics. The significance level of statistical tests was set to 0.05. For details, see Supplementary file 1. 

To estimate the acquisition curve dynamics (Figure 1E), hyperbola curve fitting was applied:

LI=AtB+t

where A and B are constants, t is the training duration, and LI is learning index. ‘A’ denotes the theoretical maximum value of LI (i.e., plateau) and ‘B’ the training duration required to reach the half of the maximum (i.e., acquisition speed). To test the statistical significance of observed differences in A and B (ΔAobs. and ΔBobs.) between genotypes, we performed permutation tests (Knijnenburg et al., 2009); we randomly shuffled the experimental dataset by reassigning the group labels and fitted a hyperbola function to the data to calculate the differences in A and B between groups (ΔAperm. and ΔBperm.). The procedure was repeated over 2000 runs to generate the null distributions of ΔAperm. and ΔBperm. for testing the statistical significance of ΔAobs. and ΔBobs.

Data availability

All data is available in the main text or the supplementary materials, or in the following data repositories (Source Data: https://gin.g-node.org/Nobu/Yamagata_Data_Source, Source Code: https://github.com/tkEzaki/peak_size_analysis; copy archived at https://archive.softwareheritage.org/swh:1:rev:ba29c4fb5f303958286f1a2f90fe8a8b7cb3ea84).

References

    1. Ezaki T
    2. Watanabe T
    3. Ohzeki M
    4. Masuda N
    (2017) Energy landscape analysis of neuroimaging data
    Philosophical Transactions of the Royal Society A: Mathematical, Physical and Engineering Sciences 375:20160287.
    https://doi.org/10.1098/rsta.2016.0287
    1. Rescorla RA
    (1972)
    A theory of pavlovian conditioning: variations in the effectiveness of reinforcement and nonreinforcement
    Current Research and Theory 64:lp99.
  45. Conference
    1. Thévenaz P
    2. Ruttimann UE
    3. Unser M
    (1998) A pyramid approach to subpixel registration based on intensity
    IEEE Transactions on Image Processing: A Publication of the IEEE Signal Processing Society. pp. 27–41.
    https://doi.org/10.1109/83.650848

Decision letter

  1. K VijayRaghavan
    Senior and Reviewing Editor; National Centre for Biological Sciences, Tata Institute of Fundamental Research, India

In the interests of transparency, eLife publishes the most substantive revision requests and the accompanying author responses.

Acceptance summary:

Learning in this system is based on dopamine-induced synaptic plasticity. The present work demonstrates that the dopaminergic inputs can be modulated by pre-synaptic inhibition from a GABAergic neuron in the circuit. So this is one way the circuit can control the strength of the reward signal reaching the learning centers, even when the sensory inputs remain the same. It adds a new level of complexity to reward signaling pathways in the brain,

Decision letter after peer review:

Thank you for submitting your article "Presynaptic inhibition of dopamine neurons controls optimistic bias" for consideration by eLife. Your article has been reviewed by 2 peer reviewers, and the evaluation has been overseen by K VijayRaghavan as the Senior and Reviewing Editor. The reviewers have opted to remain anonymous.

The reviewers have discussed their reviews with one another, and the Reviewing Editor has drafted this to help you prepare a revised submission.

This work studies how Drosophila mushroom body dopaminergic- neurons are affected by inhibitory inputs. Learning in this system is based on dopamine-induced synaptic plasticity. The present work demonstrates that the dopaminergic inputs can be modulated by presynaptic inhibition from a GABAergic neuron in the circuit, demonstrating one way the circuit can control the strength of the reward signal reaching learning centers, even when the sensory inputs remain the same. The study adds a new level of complexity to reward signaling pathways in the brain.

There are substantial concerns that the authors are requested to address before acceptance. These are delineated in the consolidated reviews below.

Essential revisions:

1. Figure 1B is an important basis of the whole work. Considering that the temperature may significantly affect appetitive learning performance, the parental control groups at 18℃ should be completed.

2. Since the RNAi strategy might have an off-target problem, checking the efficiency of GABA-B-R3-RNAi using Q-PCR or employing another independent RNAi line of GABA-B-R3 is helpful.

3. Considerable attention needs to be given to the calcium imaging of DAN active zones in Figure 3. What, in the authors' view, is the biological significance of a larger cluster size? It is also not clear how that increase connects to the behavioral results about generalization. Given that these patterns are odor-evoked rather than reward-evoked, how can we understand their role in learning-related plasticity? They need to be clarified since on p10, lines 8-10, they write: 'These results suggest that GABA-B-R3 function at the presynaptic terminal is necessary for the fine spatial regulation of the reward signal'. However, their experiments do not examine the reward signal itself. Further, the authors need to clarify whether they think the increase in cluster size is simply a reflection of greater amplitude activity in these cells, or whether new 'active zones' are recruited when inhibition is blocked. Would they see the same increase simply using higher odor concentrations? Simply increasing DAN activity could potentially have the same effect on memory as 'blurring DAN activity', but the authors are not clear about the distinction in the text.

4. There are important technical issues with specific panels in Figure 3.

Figure 3A: There is no validation that these spots are individual active zones. There should be some co-localization with other presynaptic proteins to even begin this direction. And there is almost certainly not enough resolution to say these are individual AZs (axial resolution is at least 4 microns so there are almost certainly many AZs collapsed on one another in their images). This could be addressed with a more measured language in the text (i.e. don't write 'we measured calcium influx at individual active zones' p.5 line 20-21).

Figure 3B: How would GABAR knockdown broaden the distribution on the low end (left side of x-axis)? We can see how it would increase the mean intensity, but it seems that both ends of the distribution expand in this analysis. How robust is the effect? Is it seen with a different set of 9 frames? Why only analyze 9 frames, why not do all frames?

Figure 3D is a confusing way of representing imaging data. We would prefer to see a video or a per pixel dF/F heat map of what the stimulus responses looked like. I also don't see the biological significance of the diminished inverse correlation between mean and SD in the GABAR knockdown.

Figure 3E and F: What are the cluster sizes in microns rather than arbitrary units? In Fig3F the difference in cluster sizes +-GABAR RNAi is very small. If we go from how they calculated what 'normalized cluster size' should be, then the difference between the null distribution of sizes and their observations in WT (1.055 -1) is less than the difference +- GABAR RNAi (1.065-1.055). So is this really a significant difference? Does it make sense when expressed in physical distance?

How different are dFF values between clusters? The graphic in Fig3E is color-coded by cluster size (in pixels), not by response amplitude.

Overall it would be much more informative to simply show a zoom of the ROI displaying the dFF values they observed.

5. A general technical comment, which should be addressed: Will not increasing response amplitude naturally lead to an increase in cluster sizes, as there is more signal to poke out above the background? If the authors looked at higher odor intensities, would they also see an increase in cluster size?

Important points on the interpretation of experiments:

6. Importantly, the experiments in Figure 3 don't look at DAN responses to reward (sucrose), they look at odor responses. It is not clear what that has to do with plasticity. It will be better to look at responses to sucrose for this whole question.

Based on the text on p.10 lines 1-3 it sounds like the authors think the calcium they measure in the DAN terminals carries a representation of the odor i.e. is different for distinct odors. And the increase in cluster size is presumed to decrease the complexity of the pattern, and again presumably make patterns for different odors less distinct. However, according to p.16 line 20, these clusters are derived from analysis of 9 frames prior to stimulation. So how could they carry an odor representation (as claimed p.10 lines 1-3) if the odor has not yet been presented?

7. How consistent are these clusters? Should we be shown results from repeated odor presentations, but maybe that's not the claim? But shouldn't they at least be consistent across timepoints?

8. There is no metric for the complexity of the patterns, only the size of the clusters. How odor-specific are these patterns (how distinct for the odors in question, and how consistent across repeated presentations)?

9. The most likely explanation for their results seems to be that the reward signal gets stronger and broader (akin to increasing the concentration of sucrose). But since they're imaging odor responses here, we are not sure what they're trying to say, the text describing their overall interpretation (p.10) is not easily digestible.

10. In Figure 4: Since GABAR RNAi flies start with a higher learning score, the authors should compensate for this when evaluating whether they generalize more than controls. Generalization is evident in Figure 4A, but in 4B the red line seems to be just an upward shift of the other lines. The difference at 50:50 is perhaps not increased generalization, rather it is just a consequence of increased overall learning.

https://doi.org/10.7554/eLife.64907.sa1

Author response

Essential revisions:

1. Figure 1B is an important basis of the whole work. Considering that the temperature may significantly affect appetitive learning performance, the parental control groups at 18°C should be completed.

We agree with the reviewer’s point that temperature may significantly affect flies’ performance. We thus conducted a control learning experiment using the same genotypes raised at 18℃ to permit the GAL80[ts] suppression of transgenic RNAi. No statistical differences were observed across genotypes, suggesting a physiological rather than a developmental effect of GABA-B-R3-KD on performance enhancement. This new data is now incorporated into Figure 1B.

2. Since the RNAi strategy might have an off-target problem, checking the efficiency of GABA-B-R3-RNAi using Q-PCR or employing another independent RNAi line of GABA-B-R3 is helpful.

The reviewer might have overlooked them, but we did indeed include consistent behavioral data using the ‘second’ RNAi strain in our original manuscript. They are presented in Figure 1—figure supplement 1B.

3. Considerable attention needs to be given to the calcium imaging of DAN active zones in Figure 3. What, in the authors' view, is the biological significance of a larger cluster size? It is also not clear how that increase connects to the behavioral results about generalization. Given that these patterns are odor-evoked rather than reward-evoked, how can we understand their role in learning-related plasticity? They need to be clarified since on p10, lines 8-10, they write: 'These results suggest that GABA-B-R3 function at the presynaptic terminal is necessary for the fine spatial regulation of the reward signal'. However, their experiments do not examine the reward signal itself. Further, the authors need to clarify whether they think the increase in cluster size is simply a reflection of greater amplitude activity in these cells, or whether new 'active zones' are recruited when inhibition is blocked. Would they see the same increase simply using higher odor concentrations? Simply increasing DAN activity could potentially have the same effect on memory as 'blurring DAN activity', but the authors are not clear about the distinction in the text.

We thank the reviewer for raising these important potential problems, as these explanations were indeed unclear. We made a major textual revision for Figure 3 to better explain why we characterize active-zone calcium patterns in the PAM terminals. Now it extends to 4 paragraphs (P5, L119-P12, L256).

The reviewer also raised an interesting question regarding the interpretation of increased cluster size (Figure 3F). We made a scatter plot to analyze the relationship between peak size and calcium signal intensity (Author response image 1). This revealed no clear correlation between them. Furthermore, a similar plot for GABA-B-R3 knock-down terminals, which responded to odor stimulation with larger calcium increase, did not show a greater correlation (even slightly smaller dependency on the contrary [slope of the regression: 0.0543 vs. 0.0517 in WT and GABA-B-R3-KD flies, respectively]). This suggests that the cluster size is controlled by other mechanism(s) than the amplitude (see also Author response image 2). One such possibility would be the recruitment of adjacent active zones. We now added this information in the revised text (P12. L247- P12. L249)

Author response image 1
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Scatter plots showing dependency between the size (abscissa) and intensity (ordinate) of each peak calculated by the method we described.

Each circle represents a single cluster in the 9 frames before stimulation of a single representative fly.

Author response image 2
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The cluster value map.

Each cluster is color-coded by the averaged intensity of associated pixels. Left: control, right: GABA-B-R3-KD.

4. There are important technical issues with specific panels in Figure 3.

Figure 3A: There is no validation that these spots are individual active zones. There should be some co-localization with other presynaptic proteins to even begin this direction. And there is almost certainly not enough resolution to say these are individual AZs (axial resolution is at least 4 microns so there are almost certainly many AZs collapsed on one another in their images). This could be addressed with a more measured language in the text (i.e. don't write 'we measured calcium influx at individual active zones' p.5 line 20-21).

Following the suggestion, we revised the corresponding text by providing a more factual result description (P5, L120, P8, L163-165).

We validated the localization of the sensor to the active zones in the PAM terminals. The calcium sensor is fused to brp-short (Kiragasi et al., Cell Rep 2017), a widely accepted molecular tag for the localization in the active zone. While the monoclonal antibody against Brp (nc82) does not recognize the Brpshort in the sensor (Schumid et al., Nat Neurosci, 2008), Brpshort::GCaMP6s::mCherry expressed in the PAM neurons nicely colocalized with nc82 signal, indicating sensor integration into native active zones. This proper sensor integration is consistent with the observation in the motor neurons (Kiragasi et al., Cell Rep 2017). We now present this new data in the revision (P8, L165-167, Figure 3—figure supplement 1A).

Figure 3B: How would GABAR knockdown broaden the distribution on the low end (left side of x-axis)? We can see how it would increase the mean intensity, but it seems that both ends of the distribution expand in this analysis. How robust is the effect? Is it seen with a different set of 9 frames? Why only analyze 9 frames, why not do all frames?

Since the intensity distributions in Figure 3B are representative examples, it does not make too much sense to discuss the broadened tails in this knock-down fly. The intention and the point of these Figure 3B and 3C are to show that GABA-B-R3 is required for the regulation of terminal calcium levels. We now mention the tendency of broader distributions of the Brp::GCaMP6s::mCherry signals upon knock down, in addition to increased temporal fluctuations, suggesting compromised robustness. In addition, we provide textual explanations regarding these analyses (P8. L173-180).

Figure 3D is a confusing way of representing imaging data. We would prefer to see a video or a per pixel dF/F heat map of what the stimulus responses looked like. I also don't see the biological significance of the diminished inverse correlation between mean and SD in the GABAR knockdown.

Since the mean and SD are the primary statistics that represent the Gaussian distribution, we mapped our data in the logarithm mean vs. sd space (Figure 3E). Although the biological importance of the observed inverse correlation is unclear, it suggests that each individual has a unique ‘set point’ of activity level and heterogeneity in the dopamine terminals, and such a control requires GABA-B-R3. The structure of these set points among individuals might be relevant to the “criticality” state of a system for efficient information processing (e.g., Hesse and Gross, 2014; Ezaki et al., Communications biology 2020). We mentioned this in the figure legend (P9, L194-196, P10, L202-205).

Given sample motion during measurement, pixel-wise dF/F would not be a powerful approach. To be a little more reader friendly, we added separate mean and sd traces in the main figure of the revised manuscript (Figure 3D). The original files for our analyses are also deposited online (https://gin.g-node.org/Nobu/Yamagata_Data_Source).

We would like to remind that one of the significant advantages of using the Brp::GCaMP6s::mCherry sensor is that each molecule has the mCherry reference. This makes the measurement more robust against motion artifacts and sensor expression levels (P8. L163-165).

Figure 3E and F: What are the cluster sizes in microns rather than arbitrary units? In Fig3F the difference in cluster sizes +-GABAR RNAi is very small. If we go from how they calculated what 'normalized cluster size' should be, then the difference between the null distribution of sizes and their observations in WT (1.055 -1) is less than the difference +- GABAR RNAi (1.065-1.055). So is this really a significant difference? Does it make sense when expressed in physical distance?

The lateral resolution of our images is 0.33 um/px, yielding physical cluster sizes of 0.536 and 0.544um2 for the control and GABA-B-R3 KD samples respectively. Since we normalized these values with the mean cluster size of the randomly reshuffled images, these values do not have a unit.

To further support this cluster size analysis, we examined another metrics, i.e., peak size, which quantifies the size of bright pixels (brighter than the 95 percentile of the entire pixel intensities in a given ROI). This metrics is thus independent of overall intensities but also quantifies the fineness of the pattern. This measure also supported our conclusion: GABA-B-R3 KD caused larger peak sizes. This new data is now incorporated into the text (P12 L249-254), and supplementary figure (Figure 3—figure supplement 1F).

How different are dFF values between clusters? The graphic in Fig3E is color-coded by cluster size (in pixels), not by response amplitude.

We mapped the calcium intensity of each cluster, but did not find a clear correlation with the cluster size (Author response image 2). As shown in Author response image 1, the amplitude does not well explain the cluster size.

Overall it would be much more informative to simply show a zoom of the ROI displaying the dFF values they observed.

For the reasons we already argued in our response to the comment 4 above, we mainly focus on the frame-wise spatial pattern of active-zone calcium activities.

5. A general technical comment, which should be addressed: Will not increasing response amplitude naturally lead to an increase in cluster sizes, as there is more signal to poke out above the background? If the authors looked at higher odor intensities, would they also see an increase in cluster size?

This is essentially the same concern which we addressed above (Author response images 1 and 2).

Important points on the interpretation of experiments:

6. Importantly, the experiments in Figure 3 don't look at DAN responses to reward (sucrose), they look at odor responses. It is not clear what that has to do with plasticity. It will be better to look at responses to sucrose for this whole question.

Basically, this is the repetition of the first part of Point 3 above. These explanations were indeed unclear. We made a major textual revision for Figure 3 to better explain why we characterize active-zone calcium patterns in the PAM terminals. Now it extends to 4 paragraphs (P5, L119-P12, L256).

Based on the text on p.10 lines 1-3 it sounds like the authors think the calcium they measure in the DAN terminals carries a representation of the odor i.e. is different for distinct odors. And the increase in cluster size is presumed to decrease the complexity of the pattern, and again presumably make patterns for different odors less distinct. However, according to p.16 line 20, these clusters are derived from analysis of 9 frames prior to stimulation. So how could they carry an odor representation (as claimed p.10 lines 1-3) if the odor has not yet been presented?

The reviewer correctly understands our points. Since the local active-zone calcium influx in the PAM terminals reflects KC odor activity, it should be related to evaluating odors.

As resting-state functional connectivity predicts how the circuit operates tasks (e.g., Cole et al., Nat Neurosci, 2016), we analyzed its basal activity in the PAM terminals. In response to the reviewer’s suggestion, we now analyzed the cluster size during odor stimulation. Indeed, we found the increased cluster size in the knock-down terminals, a consistent result with baseline activity (Figure 3G left). This new data is now presented in the main figure (Figure 3G right) and text (P12. L244-247).

7. How consistent are these clusters? Should we be shown results from repeated odor presentations, but maybe that's not the claim? But shouldn't they at least be consistent across timepoints?

Following the reviewer’s request, we calculated cluster sizes for all frames before and during odor stimulation (Author response image 3). The result clearly shows consistently greater cluster size in GABA-B-R3 knock-down flies over time.

Author response image 3
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Time courses of normalized cluster size (left) and the comparison between genotypes using all frames from pre- and during-stimulation phases (frames 1-12, right).

The averaged cluster size was consistently higher in the GABA-B-R3 knock-down flies compared to wild-type flies. * P < 0.05, Mann Whitney test. N=15, 11.

8. There is no metric for the complexity of the patterns, only the size of the clusters. How odor-specific are these patterns (how distinct for the odors in question, and how consistent across repeated presentations)?

We meant the spatial ‘blurring’ as larger local cluster sizes, but replaced this word to avoid any unnecessary confusions by readers (P9, L190, P12, L255).

9. The most likely explanation for their results seems to be that the reward signal gets stronger and broader (akin to increasing the concentration of sucrose). But since they're imaging odor responses here, we are not sure what they're trying to say, the text describing their overall interpretation (p.10) is not easily digestible.

Thank you for the comment. Our model is that the sugar reward signal is globally inhibited in the PAM terminals by GABA-B-R3, and locally disinhibited by the input from odor-representing KCs to selectively enhance dopaminergic reward signals to these KCs. This has been clarified through the text revision (P12, L254-256), and revising a figure panel (Figure 4E).

10. In Figure 4: Since GABAR RNAi flies start with a higher learning score, the authors should compensate for this when evaluating whether they generalize more than controls. Generalization is evident in Figure 4A, but in 4B the red line seems to be just an upward shift of the other lines. The difference at 50:50 is perhaps not increased generalization, rather it is just a consequence of increased overall learning.

We understand the reviewer’s concern. To evaluate the generalization curve irrespective of the intensity, we normalized the data by dividing the average score of the 100:0 mixture (i.e., testing with the trained odor), and found essentially the same results (Author response image 4). Significant reduction of odor generalization at the 50:50 mixture was detected in the control groups, but not in the experimental group (Author response image 4). These results are thus consistent with our previous presentation, and indicate that GABA-B-R3 in the PAM terminals is required for the specificity of rewarded memory to the learned odor.

Author response image 4
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Normalized generalization curves using 4MCH:2MCH (left) and 3OCT:1OCT (right) mixtures.

Statistics suggest experimental group exhibit altered memory specificity to learned odors when compared with its parental control groups. (4MCH:2MCH) R58E02-GAL4/+, p = 0.030; UAS-GBR3-RNAi/+, p = 0.006; R58E02-GAL4/UAS-GBR3-RNAi, p = 0.972. N = 8-17. (3OCT:1OCT) R58E02-GAL4/+, p = 0.002; UAS-GBR3-RNAi/+, p = 0.006; R58E02-GAL4/UAS-GBR3-RNAi, p = 0.500. N = 8-20. Tukey’s multiple comparisons test.

To corroborate the result with receptor knock down, we performed a new set of generalization experiments upon silencing GABA synthesis in the APL neurons. Strikingly, APL-GAL4/UAS-GAD1-RNAi flies showed significantly broad generalization profile, very similar to the results of GABA-B-R3 knock down in the PAM neurons (Figure R9). We confirmed this broadened generalization with two different odors (Figure R9). We now added these new data in the revised text (P12. L263-264; Figures 4C, 4D).

https://doi.org/10.7554/eLife.64907.sa2

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Author details

  1. Nobuhiro Yamagata

    Graduate School of Life Sciences, Tohoku University, Sendai, Japan
    Contribution
    Conceptualization, Data curation, Formal analysis, Supervision, Funding acquisition, Validation, Investigation, Visualization, Methodology, Writing - original draft, Project administration, Writing - review and editing
    For correspondence
    nobuhiro.yamagata.a5@tohoku.ac.jp
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0003-1993-2038

  2. Takahiro Ezaki

    Research Center for Advanced Science and Technology, The University of Tokyo, Tokyo, Japan
    Contribution
    Data curation, Software, Formal analysis, Visualization, Methodology, Writing - original draft
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0003-4175-3028

  3. Takahiro Takahashi

    Graduate School of Life Sciences, Tohoku University, Sendai, Japan
    Contribution
    Investigation
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-3584-7565

  4. Hongyang Wu

    Graduate School of Life Sciences, Tohoku University, Sendai, Japan
    Contribution
    Investigation
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-7889-6941

  5. Hiromu Tanimoto

    Graduate School of Life Sciences, Tohoku University, Sendai, Japan
    Contribution
    Conceptualization, Data curation, Formal analysis, Supervision, Funding acquisition, Validation, Writing - original draft, Project administration, Writing - review and editing
    For correspondence
    hiromut@m.tohoku.ac.jp
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-5880-6064

Funding

Japan Society for the Promotion of Science (19KK0383)

  • Nobuhiro Yamagata

Japan Society for the Promotion of Science (17H04765)

  • Nobuhiro Yamagata

Japan Society for the Promotion of Science (20H05525)

  • Hiromu Tanimoto

Japan Society for the Promotion of Science (19K22577)

  • Hiromu Tanimoto

Japan Society for the Promotion of Science (17H01378)

  • Hiromu Tanimoto

The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.

Acknowledgements

We thank I Kadow, V Ruta, BDSC and VDRC for sharing fly stocks; T Hige, M Hiroi, H Kazama, HM Shiozaki, GC Turner for our setting up calcium imaging experiments; T Ichinose for helping statistics; Y Aso, S Kondo, M Tanaka, K Hamaguchi, Y Hirano for stimulating discussions and for commenting on the manuscript.

Senior and Reviewing Editor

  1. K VijayRaghavan, National Centre for Biological Sciences, Tata Institute of Fundamental Research, India

Publication history

  1. Received: November 14, 2020
  2. Accepted: May 16, 2021
  3. Version of Record published: June 1, 2021 (version 1)

Copyright

© 2021, Yamagata et al.

This article is distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use and redistribution provided that the original author and source are credited.

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  1. Nobuhiro Yamagata
  2. Takahiro Ezaki
  3. Takahiro Takahashi
  4. Hongyang Wu
  5. Hiromu Tanimoto
(2021)
Presynaptic inhibition of dopamine neurons controls optimistic bias
eLife 10:e64907.
https://doi.org/10.7554/eLife.64907

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