1. Cell Biology
  2. Neuroscience

Intact Drosophila central nervous system cellular quantitation reveals sexual dimorphism

  1. Wei Jiao
  2. Gard Spreemann
  3. Evelyne Ruchti
  4. Soumya Banerjee
  5. Samuel Vernon
  6. Ying Shi
  7. R Steven Stowers
  8. Kathryn Hess
  9. Brian D McCabe  Is a corresponding author
  1. Brain Mind Institute, EPFL - Swiss Federal Institute of Technology, Switzerland
  2. Department of Microbiology and Cell Biology, Montana State University, United States
https://doi.org/10.7554/eLife.74968
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Cite this article
  1. Wei Jiao
  2. Gard Spreemann
  3. Evelyne Ruchti
  4. Soumya Banerjee
  5. Samuel Vernon
  6. Ying Shi
  7. R Steven Stowers
  8. Kathryn Hess
  9. Brian D McCabe
(2022)
Intact Drosophila central nervous system cellular quantitation reveals sexual dimorphism
eLife 11:e74968.
https://doi.org/10.7554/eLife.74968
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Abstract

Establishing with precision the quantity and identity of the cell types of the brain is a prerequisite for a detailed compendium of gene and protein expression in the central nervous system (CNS). Currently, however, strict quantitation of cell numbers has been achieved only for the nervous system of Caenorhabditis elegans. Here, we describe the development of a synergistic pipeline of molecular genetic, imaging, and computational technologies designed to allow high-throughput, precise quantitation with cellular resolution of reporters of gene expression in intact whole tissues with complex cellular constitutions such as the brain. We have deployed the approach to determine with exactitude the number of functional neurons and glia in the entire intact larval Drosophila CNS, revealing fewer neurons and more glial cells than previously predicted. We also discover an unexpected divergence between the sexes at this juvenile developmental stage, with the female CNS having significantly more neurons than that of males. Topological analysis of our data establishes that this sexual dimorphism extends to deeper features of CNS organisation. We additionally extended our analysis to quantitate the expression of voltage-gated potassium channel family genes throughout the CNS and uncover substantial differences in abundance. Our methodology enables robust and accurate quantification of the number and positioning of cells within intact organs, facilitating sophisticated analysis of cellular identity, diversity, and gene expression characteristics.

Editor's evaluation

This manuscript describes a pipeline involving whole brain imaging, automated neuronal segmentation, and topographical analysis, to assess the number of specific cell types in the larval Drosophila brain. The authors uncover unexpected sexual dimorphism at this early stage. This paper will be of interest to neuroscientists – from those who use larval Drosophila as their study model to others who are generally interested in connectomics and transcriptomics.

https://doi.org/10.7554/eLife.74968.sa0

Introduction

Establishing the precise number of cells in the brain is essential to create organ-wide catalogues of cell types and their gene expression (Lent et al., 2012; Devor et al., 2013). However, apart from the nervous system of the nematode Caenorhabditis elegans (302 neurons, 56 glia) (White et al., 1986), the exact numbers of cells within the central nervous system (CNS) of model organisms or that of humans is currently unknown, with estimates, including those based on extrapolation from direct quantification of brain sub-regions, varying widely (Silbereis et al., 2016; Keller et al., 2018; von Bartheld et al., 2016).

Studies of the CNS of Drosophila melanogaster, which in scale and behavioural repertoire has been viewed as intermediate between nematodes and rodents (Bellen et al., 2010; Alivisatos et al., 2012), currently include large-scale efforts to establish both a neuronal connectome and a cell atlas (Scheffer and Meinertzhagen, 2019; Allen et al., 2020; Li et al., 2022). Nonetheless, the precise number of cells (neurons or glia) in either the smaller larval or larger adult Drosophila CNS, comprised of both a brain and ventral nerve cord (VNC), remain unknown, though several approximations have been suggested. For the larval CNS, a range of 10,000–15,000 active neurons has been proposed (Scott et al., 2001; Meinertzhagen, 2018; Eschbach and Zlatic, 2020) across developmental time points. For adult Drosophila, approximations have been suggested in the range of 100,000–199,000 neurons in the brain (Simpson, 2009; Chiang et al., 2011; Kaiser, 2015; Scheffer and Meinertzhagen, 2019; Raji and Potter, 2021) together with a range of 10,000–20,000 cells in the VNC (Birkholz et al., 2015; Lacin et al., 2019; Bates et al., 2019; Allen et al., 2020). The other major CNS cell type, glia, has been estimated to be approximately 10% of the number of neurons (Kremer et al., 2017; Meinertzhagen, 2018; Raji and Potter, 2021). Given the large diversity of these estimates, precise quantification of the numbers of Drosophila neurons and glia would seem a desirable goal, beginning with the smaller larval CNS, which enables the wide compendium of larval Drosophila behaviours (Gerber et al., 2009; Neckameyer and Bhatt, 2016; Eschbach and Zlatic, 2020; Louis, 2020; Gowda et al., 2021).

Complicating the aspiration to quantitate the Drosophila larval CNS, in addition to the general problem of separating and quantifying primary cell types such as neurons and glia, are two specific confounding factors that limit simple total cell quantification approaches. First, encompassed within and surrounding the larval CNS are dividing neuroblasts, which will give rise to adult neurons (Doe, 2017). Relatedly, imbedded within the larval CNS are substantial numbers of immature adult neurons, observed from electron micrograph reconstructions as having few or no dendrites and axons that terminate in filopodia lacking synapses (Eichler et al., 2017). These immature neurons are unlikely to contribute to larval CNS function and are generally excluded when considering larval neuronal circuit architecture (Eichler et al., 2017; Scheffer and Meinertzhagen, 2019). It has been suggested that only a small fraction of the total number of larval CNS cells may actually contribute to CNS function (Ravenscroft et al., 2020).

Here, we have sought to develop a synergistic molecular genetic, imaging, and computational pipeline designed de novo to allow automated neuron, glia, or other gene expression features to be precisely quantitated with cellular resolution in an intact whole CNS. Central to the approach are high signal-to-noise gene expression reporters that produce a punctate, nucleus-localised output, facilitating downstream automated computational measurements and analysis. Exploiting multiple genetic reagents designed to selectively identify only functional neurons with active synaptic protein expression, we identify substantially fewer neurons than most previous estimates in the Drosophila larval CNS and, in addition, substantially more glia. We also discover a previously unsuspected sexual dimorphism in the numbers of both cell types at larval stages. The generation of whole CNS point clouds from our data enables us to apply the tools of topological data analysis (TDA) to summarise the CNS in terms of multiscale topological structures. Utilisation of these topological summaries in a support vector machine also supports that sexual dimorphism extends to deeper features of CNS organisation. Finally, we applied our pipeline to quantitate the whole CNS expression frequency of the Drosophila family of voltage-gated potassium channels, which revealed divergent channel expression frequencies throughout the CNS. We envision that our method can be employed to allow precise quantitation of gene expression characteristics of the constituent cells of the brain, and potentially other intact whole organs, in a format suitable for sophisticated downstream analysis.

Results

Genetic and imaging tools designed to facilitate automated whole CNS cellular quantitation

To establish a robust quantitative method to measure gene expression frequency and quantify the number of cells that contribute to Drosophila larval CNS function, we sought to develop a pipeline utilising genetic reporters designed to expediate automated neuron and glia quantitation from three-dimensional intact organ images. While membrane-associated reporters are generally employed to label Drosophila neurons (Pfeiffer et al., 2008; Jenett et al., 2012; Ravenscroft et al., 2020), we generated UAS-driven (Brand and Perrimon, 1993; Wang et al., 2012) fluorescent reporters fused to histone proteins (Sherer et al., 2020) to target fluorescence only to the nucleus, in order to facilitate subsequent automated segmentation and counting. Through empirical selection of transgene genomic integration sites, we established a set of reporter lines that produced a strong and specific punctate nucleus signal when expression was induced, with little to no unwanted background expression. We then developed a procedure to capture the entire microdissected larval CNS volume by light sheet microscopy at multiple angles and with high resolution, imaging only animals within the ~2 hr developmental time window of the wandering third instar larval stage (Ainsley et al., 2008). These multiview datasets were then processed to register, fuse, and deconvolve the entire larval CNS volume. The volume was then segmented and cell numbers were automatically quantified (Figure 1a–d).

Figure 1
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Intact whole CNS quantitation pipeline schematic and validation.

(a–d) Illustration of an intact whole central nervous system (CNS) genetic, imaging and computational pipeline. (a) Genetic reagents: GAL4 is introduced into the exons of genes encoding synaptic proteins (e.g. bruchpilot [brp]) to capture their expression pattern with high fidelity. GAL4 expression regulates the production of UAS fluorescent-histone reporters, which target to the nucleus of cells, producing a punctate signal. (b) Imaging: the intact CNS is imaged at high resolution using light-sheet microscopy. Images are captured at five different angles at 72° intervals. (c) Assembly: multiview light sheet images are registered, fused, and deconvolved. (d) Quantitation: the volume is segmented, and the nucleus number and relative position are measured. Three-dimensional coordinates of the geometric centre of every nucleus can be calculated to produce a point cloud of nuclei positions.(e–h) Pipeline validation. Three-dimensional images before segmentation (above) and subsequent to segmentation (below) of (e) dopaminergic (TH-GAL4) neurons, (f) serotonergic neurons (Trh-GAL4) and (g) dopa decarboxylase expressing (Ddc-GAL4) neurons. (h) Manual or automated quantification of nuclei numbers in these volumes are similar. Scale squares in (e) and (g) are 100 μm and in (f) is 50 μm. (h) Bars indicate minimum and maximum values.

Figure 1—source data 1

Source Data for Figure 1.

https://cdn.elifesciences.org/articles/74968/elife-74968-fig1-data1-v1.xlsx

To evaluate the reliability of the procedure, we began by comparing automated counts of distinct neuronal subtypes with manual counting. We separately labelled all dopaminergic neurons (Figure 1e, TH-GAL4, Video 1; Friggi-Grelin et al., 2003a; Mao and Davis, 2009), serotonergic neurons (Figure 1f, Trh-GAL4, Video 2; Alekseyenko et al., 2010) and neurons that produce both types of neurotransmitter (Figure 1g, Ddc-GAL4, Video 3; Lundell and Hirsh, 1994) in the larval CNS. Quantification revealed a high level of concordance (Figure 1h, +/-0.21%, n=5 for TH-GAL4, +/-1%, n=5 for Trh-GAL4, +/-0.38%, n=6 for Ddc-GAL4, Figure 1—source data 1) between automated and manual measurements of these neuronal subtypes establishing confidence in the procedure.

Video 1
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Larval CNS labelled with TH-GAL4.
Video 2
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Larval CNS labelled with Trh-GAL4.
Video 3
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Larval CNS labelled with Ddc-GAL4.

Number of neurons and glia in the female larval CNS

Encouraged by our neuronal subset quantitation results, we next sought to generate GAL4 lines for genes likely to be expressed only in active larval neurons with synaptic connections but not by neuroblasts or by immature neurons (Figure 2—figure supplement 1). We biased towards generating GAL4 insertions within endogenous genomic loci in order to reproduce endogenous patterns of gene expression with high fidelity.

Bruchpilot (Brp) is a critical presynaptic active zone component widely used to label Drosophila synapses, including for large-scale circuit analyses (Wagh et al., 2006). We employed CRISPR/Cas9 genome editing to insert GAL4 within exon 2 of the brp gene, utilising a T2A self-cleaving peptide sequence (Diao et al., 2015) to efficiently release GAL4. While this exonic insertion generated a hypomorphic allele of brp (data not shown) when homozygous, the line was employed in heterozygotes to capture Brp protein expression with high fidelity. To complement this line, we used the Trojan/MiMIC technique (Diao et al., 2015), to generate a GAL4 insertion in the Syt1 gene, which encodes Synaptotagmin 1 (Littleton et al., 1994), the fast calcium sensor for synaptic neurotransmitter release (Quiñones-Frías and Littleton, 2021). Lastly, we examined a transgenic line where an enhancer of nSyb (neuronal Synaptobrevin) (Deitcher et al., 1998), which encodes an essential presynaptic vSNARE (Südhof and Rothman, 2009), is used to control GAL4 expression (Aso et al., 2014). All three lines were expressed in a similar pattern, labelling a substantial fraction but not all of the total cells in the larval CNS (Figure 2a–c, brp-GAL4 female Video 4, Syt1-GAL4 female Video 5, nSyb-GAL4 female Video 6). These lines contrasted with the widely used elav-GAL4 (Lin and Goodman, 1994), which was expressed in larval neurons, but also apparently in some immature neurons and potentially in some glia as well (Berger et al., 2007; Figure 2—figure supplement 1). To characterise our lines, we examined their expression throughout development, beginning with embryogenesis. We detected no expression from any of the three lines prior to embryonic stage 16 (Figure 2—figure supplement 2a). However, beginning at stage 17 of embryonic development, when synaptic activity begins (Baines and Bate, 1998), all three lines displayed expression in both the CNS and peripheral nervous system (Figure 2—figure supplement 2a). We also examined if these lines were expressed in neural stem cells during larval stages by co-labelling the larval CNS with the transcription factor Deadpan, a neuroblast marker (Bier et al., 1992). We found that labelling by all three lines did not overlap with Deadpan expression (Figure 2—figure supplement 2b), suggesting these lines are not expressed in neuroblasts. We also examined expression of all three lines in the adult brain and, as in the larval CNS, observed labelling of a large fraction but not all of the total cells in the adult brain (Figure 2—figure supplement 2c). Lastly, to ensure that the cells labelled by our lines were exclusively neurons, we compared their expression to that of glial cells labelled by glial specific transcription factor Repo (Xiong et al., 1994; Lin and Potter, 2016) using independent and mutually exclusive QF2 dependent labelling. We found complete exclusion of cells labelled by brp, Syt1 and nSyb GAL4 lines from cells labelled by repo (Figure 2d, brp-GAL4 & repo-QF2 Video 7, Syt1-GAL4 & repo-QF2 Video 8, nSyb-GAL4 & repo-QF2 Video 9), consistent with the brp, Syt1 and nSyb GAL4 lines labelling only neurons that express synaptic protein genes and not glial cells.

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Quantitation of neurons and glia in the whole female larval CNS.

(a–d) Multiview deconvolved images (left) and z-stack projections (right) (colours represent z position) of the central nervous system (CNS) of (a) brp-GAL4, (b) Syt1-GAL4, (c)nSyb-GAL4, and (d) repo-GAL4. (e) Distribution of inter-nuclei distances for each line. (f) Quantification of the number of labelled nuclei in each line. (a–d) left; scale squares (a) and (c) = 50 μm, (b) and (d) = 100 μm; right images identical magnification, scale bar = 100 μm. (f) Bars indicate minimum and maximum values.

Figure 2—source data 1

Source Data for Figure 2.

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Video 4
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Female CNS labelled with brp-GAL4.
Video 5
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Female CNS labelled with Syt1-GAL4.
Video 6
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Female CNS labelled with nSyb-GAL4.
Video 7
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Larval CNS labelled with brp-GAL4 and repo-QF2.
Video 8
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Larval CNS labelled with Syt1-GAL4 and repo-QF2.
Video 9
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Larval CNS labelled with nSyb-GAL4 and repo-QF2.

To further compare these lines, beginning with the CNS of female animals, we calculated three-dimensional coordinates for the geometric centre of all nuclei labelled in the brp, Syt1 and nSyb GAL4 lines to generate point cloud mathematical objects and compared them to point clouds of glial nuclei labelled by the repo-GAL4 line. We then plotted and compared the distributions of inter-nuclei distances in these lines. Using this measurement, we found that the inter-nuclei distance of glial cell nuclei exhibited a unimodal distribution (Figure 2e). In contrast, all three neuronal lines exhibited a bimodal distribution of inter-nuclei distances (Figure 2e). We thus observed two patterns of labelled nuclei, one shared among neuronal lines and the other distinct for glia (Figure 2e), again consistent with these lines labelling different cell types.

We next counted the number of nuclei labelled by these neuronal and glial lines, again beginning with females (Figure 2f). We found that the CNS labelled by brp-GAL4 had 10,776 (±2.65%, n=6) neurons, Syt1-GAL4 had 10,097 (±5.96%, n=5) neurons, and nSyb-GAL4 had 9971 (±1.35%, n=5) neurons (Figure 2f). We tested the statistical difference in the numbers of neurons labelled by these lines and found that while nSyb-GAL4 and Syt1-GAL4 were not statistically different from each other, brp-GAL4 did label significantly more neurons than either Syt1 or nSyb GAL4 lines (brp-GAL4 vs Syt1-GAL4+6.72%, p=0.03, brp-GAL4 vs nSyb-GAL4 +8.07%, p=0.01). Averaging across the lines, we found that the female third instar larval CNS had 10,312 ±5.03%, n=16, neurons (Figure 2—source data 1). To ensure that our method did not introduce bias in dense datasets, we also manually counted a brp-GAL4 labelled CNS and compared it to the automated count. Similar to our experiments with sparse neuronal labelling, we found good agreement between manual and automated quantification with a difference of just 14 neurons (9430 nuclei manual vs 9444 nuclei automated for this individual CNS).

We next counted the number of glia labelled by the repo-GAL4 line (Figure 2d and f, repo-GAL4 female, Video 10). We measured 3860 ±3.37%, n=7, glia in the female CNS (Figure 2—source data 1). This amounted to 37% of the number of neurons, far more than previously estimated (Meinertzhagen, 2018; Raji and Potter, 2021). In sum, we found that the female Drosophila larval CNS had 10,312 neurons, fewer than most previous predictions, and several fold more glia than previously thought.

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Female CNS labelled with repo-GAL4.

Males have fewer neurons and more glia than females

We next carried out a similar analysis on the CNS of male larvae (Figure 3a–c). We found that brp-GAL4 labelled 9888 (±3.15%, n=5) neurons, Syt1-GAL4 labelled 9012 (±3.8%, n=5) neurons, and nSyb-GAL4 labelled 9286 (±5.38%, n=5) neurons in male larvae (Figure 3e, Figure 3—source data 1). In males, brp-GAL4 did not label significantly more neurons than nSyb-GAL4 but did label more than Syt1-GAL4 (brp-GAL4 vs Syt1-GAL4 +9.72%, p=0.01), while the number of neurons labelled by nSyb-GAL4 was not significantly different from Syt1-GAL4, similar to what we had found in females. Averaging across the lines, we found that the male third instar larval CNS had 9396 ±5.59%, n=15 neurons, significantly fewer than those of females (–9.75%, p<0.0001). This difference was also consistent within individual genotypes with brp-GAL4 labelling (–8.98%, p=0.0008), Syt1-GAL4 labelling (–12.04%, p=0.008) and nSyb-GAL4 labelling (–7.38%, p=0.0182) less neurons in males than in females.

Figure 3
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Quantitation of neurons and glia in the male larval CNS and topological comparison of sex differences.

(a–d) Example z-stack projections (colours represent z position) of male larval central nervous system (CNS) of (a) brp-GAL4, (b) Syt1-GAL4, (c) nSyb-GAL4, and (d) repo-GAL4. (e) Quantification of the number of labelled nuclei in each line. (f) The distribution of correlations between the ground truth and the prediction made by the support vector machine (SVM) using topological features is indicative of sexual dimorphism of the higher order structure of neuron point clouds (g) Simpler point cloud features such as properties of the distributions of inter-nuclei distances are not indicative of this. (a–d): identical magnification, scale bar = 100 μm. (e) Bars indicate minimum and maximum values.

Figure 3—source data 1

Source Data for Figure 3.

https://cdn.elifesciences.org/articles/74968/elife-74968-fig3-data1-v1.xlsx

We also counted the number of glia labelled by repo-GAL4 in males (Figure 3d and e). We found that males had 4015 ±1.98%, n=6, glia far more than previous estimates (Figure 3—source data 1). The number of glia in the male larval CNS was significantly more than in females (+3.86%, p=0.0284). In summary, male Drosophila larva have significantly fewer CNS neurons than females but more glia.

Topological analysis detects CNS structural differences between males and females

We next wished to determine if the differences between point clouds derived from the positions of neuronal nuclei of the male and female CNS went beyond simple numerics. To do this, we applied the tools of TDA (Rabadán and Blumberg, 2019; Chazal and Michel, 2021) to summarise the CNS in terms of multiscale topological structures (Expert et al., 2019). These topological summaries, the construction of which is described in the methods, can be thought of as multiscale descriptions of the shape of the dataset. Topological summaries, which can be compared by standard methods despite the lack of common reference points, could then be used as the classification features in a support vector machine (SVM). Since the total number of point clouds was relatively small for this type of analysis (Supplementary file 1), we down-sampled each whole CNS point cloud randomly to 8000 points 100 times, producing a total of 3100 point clouds, for each of which we then computed a certain topological summary, called the degree-1 persistence diagram of its alpha complex (Edelsbrunner and Mücke, 1994).

After fixing the necessary hyperparameters, sex classification experiments were run across 5000 random train/test splits of the topological summaries. In each split, the summaries derived from subsamplings of a single CNS point cloud were either all in the training set or all in the testing set, to avoid leaking information. Each time, the SVM was trained once with the animal’s true sex as the target class and once with a randomly assigned sex as the target as a control. We then computed the Pearson’s correlation between the classifier’s output on the testing set and the true (respectively randomised) sex of the animal.

The 5000 splits were used to produce 5000 correlations with the true sex and 5000 correlations with a randomly assigned sex. The distribution of these correlations (Figure 3f), exhibiting clearly that the SVM is able to extract the sex of the animal reliably: only about 1.9% of the splits result in a higher correlation in the control set than in the true data. Moreover, repeating the procedure with simpler point cloud features, like properties of the distributions of inter-nuclei distances, did not produce a significant signal (Figure 3g). Thus, the pattern, which seems hard to describe concisely, is not revealed through simpler descriptors of the neuron configurations, leading us to suspect that CNS sexual dimorphism extends to deeper features of organisation that are both subtle and widely distributed. These results, in addition to the differences in total cell numbers, support sexual dimorphism of the male and female Drosophila CNS at the larval stage.

Potassium channel family member gene expression density in the CNS

Having established a baseline of total numbers of neurons in the larval CNS, we next sought to deploy the quantification pipeline to measure the expression frequency of key neuronal function genes throughout the CNS. We chose to examine the family of voltage-gated potassium channels, which are essential for many aspects of neuronal function and for which Drosophila studies defined the founding members (McCormack, 2003). We generated GAL4 insertions in the Shaker (Sh) (Kv1 family), Shab (Shab) (Kv 2 family), Shaw (Shaw) (Kv3 family), and Shal (Shal) (Kv4 family) (McCormack, 2003) genes using the Trojan/Mimic technique (Diao et al., 2015). As the Sh gene is x-linked, we carried out our quantitation analysis in the male CNS only to avoid potential gene dosage effects. To determine whether our GAL4 reporter lines had patterns of expression consistent with the known properties of these channels, we examined the expression of all four lines in motor neurons, where functional activity for Shaker, Shab, Shaw, and Shal had previously been demonstrated by electrophysiological measurements (Covarrubias et al., 1991; Ryglewski and Duch, 2009). We found that the GAL4 reporters for all 4 channels were expressed as expected in motor neurons (Figure 4—figure supplement 1), consistent with accurate reproduction of the established expression of these proteins.

We next examined the expression frequency of these genes in the entire CNS (Figure 4a–d, Sh-GAL4 Video 11, Shal-GAL4 Video 12, Shab-GAL4 Video 13, Shaw-GAL4 Video 14). We found that Sh and Shal were expressed in large numbers of neurons 8204 ±5.67%, n=10 and 8261 ±3.1%, n=5 respectively, though significantly less (–12.7% and −12.1%, p<0.0001) than the average number of all male neurons (Figure 4a, b and e, Figure 4—source data 1). In contrast, Shab (3057 ±8.21%, n=10) and Shaw (1737 ±4.3%, n=11) were expressed in smaller numbers of neurons (Figure 4c–e), with expression observed in only 32.5% or 18.5% of total male neurons respectively, suggesting more discrete functions within CNS neurons, contrasting with the collective expression of all four genes within motor neurons (Figure 4—figure supplement 1). In particular, Shab and Shaw had very reduced expression in the brain lobes of larva (Figure 4c and d) compared with Sh and Shal (Figure 4a and b). These results establish that our genetic-imaging pipeline can enable quantitation of the expression frequency of families of genes essential for neuronal properties across the entire CNS.

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Quantitation of the number of neurons expressing voltage-gated potassium channel genes.

(a–d) Multiview deconvolved images (left) and z-stack projections (right) (colours represent z position) of potassium channel family members: (a) Sh-GAL4, (b) Shal-GAL4, (c) Shab-GAL4, and (d) Shaw-GAL4. (e) Quantification of the number of labelled nuclei in each line. (a–d) left, scale squares = 50 μm, right, identical magnification, scale bar = 50 μm. (e) Bars indicate minimum and maximum values.

Figure 4—source data 1

Source Data for Figure 4.

https://cdn.elifesciences.org/articles/74968/elife-74968-fig4-data1-v1.xlsx
Video 11
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Larval CNS labelled with Sh-GAL4.
Video 12
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Larval CNS labelled with Shal-GAL4.
Video 13
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Larval CNS labelled with Shab-GAL4.
Video 14
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Larval CNS labelled with Shaw-GAL4.

Discussion

Establishing the number and identity of cells in the CNS is a foundational metric upon which to construct molecular, developmental, connectomic, and evolutionary atlases of central nervous systems across species (Lent et al., 2012; Devor et al., 2013). Here, we develop and deploy a methodological pipeline to label discrete cell types in the intact Drosophila CNS with genetic reporters designed to facilitate the subsequent segmentation and automated quantification of cell types, in addition to capturing positional coordinates of relative nucleus positions throughout the organ. Using this toolset, we find fewer active neurons, as defined by expression of synaptic protein genes, in the Drosophila larval CNS than most previous predictions and also substantially more glia. We additionally discover previously unsuspected differences in both neuron and glial density and CNS topology between the sexes at the larval stage, when external sex organs are absent, with females possessing both more neurons and fewer glia than males. Topological analysis of point clouds derived from neuronal nucleus position, which can detect potentially subtle and complex geometric structure in the data, also strongly support the existence of differences between the male and female CNS. In addition, deploying these tools, we find that while all members of the Drosophila voltage-gated potassium channel family are expressed in motor neurons, consistent with prior mutant analyses, the Kv2 channel Shab and Kv3 channel Shaw are expressed in a much smaller number of neurons in the CNS than the Kv1 channel Shaker and the Kv4 channel Shal, suggesting conclusions drawn about the coordinated activity of these channels from studies of motor neurons may not be broadly applicable across the CNS, where the genes encoding these channels are frequently not co-expressed.

A number of semiquantitative methods have been employed to estimate the number of neurons in the brains of humans and model organisms, including Drosophila (Lent et al., 2012; Keller et al., 2018). For example, the number of neurons or other cells in the brain has been estimated using stereological counting of subregions. A major limitation of this approach is the assumption of homogenous cell density across the organ or within subregions, which is not supported by the high variability of counts even between samples of similar regions, and thus likely introduces large errors (von Bartheld et al., 2016; Keller et al., 2018). Rough extrapolation of neuronal counts of electron microscope volumes of regions of the Drosophila larval CNS had suggested an estimate of ~15,000 neurons (Meinertzhagen, 2018; Eschbach and Zlatic, 2020). An alternate approach is isotropic fractionation, where all cells in large regions or the entire CNS are dissociated to produce a homogeneous single-cell suspension. Nuclei in the suspension can then be labelled by immunohistochemistry and cells in a subvolume counted in a Neubauer chamber to estimate the total number of cells present. Limitations of the approach include the necessity to ensure complete dissociation of cells while avoiding tissue loss, the requirement for homogenous antibody labelling, and highly accurate dilution (Deniz et al., 2018). This approach has recently been used to estimate the total number of neurons and glia in the adult Drosophila brain and suggested a number of 199,000 neurons (Raji and Potter, 2021), twice prior estimates (Scheffer and Meinertzhagen, 2019; Allen et al., 2020). In contrast to our results in the larval CNS, this study found no significant differences in the number of neurons between the sexes and also found that ‘non-neuronal’ cells, which should include glia, accounted for less than 9% of the total cells counted. In addition to the inherent inaccuracy of the isotropic fractionation technique, which the authors both observed and acknowledge (Raji and Potter, 2021), their use of anti-Elav antibody labelling, which can label some glia in addition to neurons (Berger et al., 2007), or perhaps differences in life stage, may explain some of the discrepancies between our results.

An unpredicted result from our whole CNS neuron quantitation was substantial differences in neuron and glial numbers between the sexes in larva. In adult Drosophila, sexually dimorphic neural circuitry has been observed in the olfactory system (Kimura et al., 2005), and human females have also been reported to have more olfactory bulb neurons and glia than males (Oliveira-Pinto et al., 2014). While sex-specific behavioural differences are obvious in adult Drosophila (Jazin and Cahill, 2010), few sexually dimorphic behavioural differences have been reported in larva (Aleman-Meza et al., 2015). However, male and female larva do differ in nutritional preference (Rodrigues et al., 2015; Davies et al., 2018), which could potentially account for some aspects of the dimorphism we observe. In addition to differences in total cell numbers, our topological methods, which take into account multiscale structure, suggest that differences in CNS structure between the sexes are both subtle (in the mathematical sense) and non-localised in nature, and indeed are not observable with simpler methods of analysis of CNS organisation.

In addition to enabling precise counting of genetically labelled cells, our method allows the relative measurement of discrete cell types or gene expression frequencies throughout the CNS. For example, the relative frequency of glial cells to neurons in the human brain has been long debated (von Bartheld et al., 2016) and in the adult Drosophila brain it has been suggested there are 0.1 glial per neuron (Kremer et al., 2017; Scheffer and Meinertzhagen, 2019; Raji and Potter, 2021). In the larval Drosophila CNS, we found closer to 0.4 glial cells per neuron on average, more similar to the glial-neuron ratios reported for rodents or rabbits (Verkhratsky and Butt, 2018). An important potential caveat, however, is that the large relative ratio of glia we observe in the third instar larva could conceivably be glia produced in advance of adult CNS development. As adult specific neuron numbers expand during pupation, the relative ratio of glia could potentially decline. Additional glial-neuron ratio measurements in the adult CNS will be required to examine this possibility.

Our approach may also allow the assignment of potential functional classes of neurons. For example, from our examination of voltage-gated potassium channel family gene expression, all these channels are collectively expressed in motor neurons; however, the Shab and Shaw genes have more discrete expression patterns in other CNS neuron classes, potentially imbuing these neurons with unique functional characteristics (Chow and Leung, 2020). Future multiplexing of binary genetic expression systems and reporters (Simpson, 2009; del Valle Rodríguez et al., 2011; Diao et al., 2015) should enable neurons or glia to be further quantitively subclassified by gene expression features throughout the entire intact CNS.

Materials and methods

Drosophila stocks

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The following stocks were employed - y[1] w[*]; Mi{y[+mDint2]=MIC}Syt1[MI02197] (BDSC#35973) (Venken et al., 2011), y(1) w(*) Mi(y[+mDint2]=MIC) Sh(MI10885) (BDSC#56260), y(1) w(*);Mi(y[+mDint2]=MIC)Shal(MI10881) (BDSC#56089) (Venken et al., 2011), y(1) w(*); Mi(y[+mDint2]=MIC) Shab(MI00848) (BDSC#34115) (Venken et al., 2011), nSyb-GAL4(GMR57C10)(BDSC#39171) (Pfeiffer et al., 2008), repo-GAL4 (BDSC#7415) (Sepp et al., 2001), repo-QF2 (BDSC#66477) (Lin and Potter, 2016), Shaw-GAL4 (BDSC#60325) (Venken et al., 2011; Li-Kroeger et al., 2018), Ddc-GAL4(BDSC#7009) (Feany and Bender, 2000), TH-GAL4(BDSC#8848) (Friggi-Grelin et al., 2003b), Trh-GAL4(BDSC#38389) (Alekseyenko et al., 2010), UAS_H2A-GFP (Sherer et al., 2020), QUAS_H2B-mCherry (Sherer et al., 2020), brp-GAL4 (this manuscript), UAS_H2A::GFP-T2A-mKok::Caax (this manuscript). All lines were raised on standard media at 25°C, 50% RH.

Generation of brp-GAL4 exon 2 insertion line

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A GAL4.2 sequence was inserted in genome, immediately after the start codon of the Brp-RD isoform using CRISPR based gene editing employing the following constructs. brp gRNA pCDF3: two gRNA sequences targeting each side of the insertion location in exon 2 of brp, were selected using the FlyCRISPR algorithm (http://flycrispr.molbio.wisc.edu/), consisting of 20 nucleotides each (PAM excluded), and predicted to have minimal off-targets. Each individual 20-nucleotide gRNA sequence were inserted into pCFD3 plasmid (Addgene #49,410) using the KLD enzyme mix (New England Biolabs). brp-GAL4 insertion construct: the seven following PCR amplified fragments were assembled using HIFI technology: (1) 1198 bp homology arm covering 5’ UTR until 5’ target site; (2) the region between 5’ target site and the start codon were amplified from Drosophila nos-cas9 (attp2) genomic DNA (a modified Pam sequence was inserted using overlapping primers); (3) Linker-T2A-GAL4.2 sequence was amplified from pBID-DSCP-G-GAL4 (Wang et al., 2012) (the linker-T2A sequence was added upstream of the forward primer); (4) P10-3’UTR was amplified from pJFRC81-10XUAS-IVS-Syn21-GFP-p10 (Addgene 36432); (5) 3xP3-Hsp70pro-dsRed2-SV40polyA selection cassette, flanked by two LoxP sites, was amplified from pHD-sfGFP scareless dsRed (Addgene 80811); (6) The region covering the end of DsRed cassette until 3’ target site; and (7) the 1079 bp homology arm two covering from the 3’ target site to exon 2, were amplified from Drosophila nos-cas9 (attp2) genomic DNA. Full length assembly was topo cloned in zero-blunt end pCR4 vector (Invitrogen), all constructs have been verified by sequencing (Microsynth AG, Switzerland) and injections were carried out into a nos-cas9 (attp2) strain (Ren et al., 2013). Correct insertion of GAL4 was verified by genome sequencing. All primer sequences are included in Appendix 1—key resources table.

Construction of UAS_H2A::GFP-T2A-mKok::Caax

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PCR amplifications were performed using Platinium Superfi polymerase (Invitrogen). The three PCR fragments were assembled together using Hifi technology (Invitrogen): (1) Histone2A (H2A) cDNA was amplified from pDESTP10 LexO-H2A-GFP template (Gift from Steve Stowers) with a synthetic 5’UTR sequence (syn21) added upstream to H2A on the forward primer; (2) sfGFP was amplified from template pHD-sfGFP Scareless dsRed (Addgene 80811); and (3) mKok amplified from pCS2 +ChMermaid S188 (Addgene 53617) with the CAAX membrane tag sequence (Sutcliffe et al., 2017) added at the 3’ end of the protein using the reverse primer. A Thosea asigna virus 2 A(T2A) self-cleaving peptide sequence (Diao et al., 2015), was inserted between sfGFP and mKok, using sfGFP reverse and mKok forward overlapping primers. The full length assembly was TOPO cloned into pCR8GW-TOPO vector (Invitrogen) generating pCR8GW-H2A::GFP-T2A-mKok::Caax. The insert, H2A::GFP-T2A-mKok::Caax was, then, transferred to pBID_UASC_G destination vector (Wang et al., 2012) using LR II clonase kit (Invitrogen) to generate pBID_UAS-H2A::GFP-T2A-mKok::Caax. The transgene was generated by injection into the JK66B landing site. All primer sequences are included in Appendix 1—key resources table.

Generation of novel Trojan GAL4 lines

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MiMIC lines generated by the group of Hugo Bellen (Venken et al., 2011) were acquired from the Bloomington Stock Center. Conversion of Mimic lines to Trojan GAL4 lines was performed as described previously (Diao et al., 2015).

Larval CNS preparation and image acquisition

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Wandering third instar larvae were dissected in 1 × PBS (Mediatech) and fixed with 4% formaldehyde (Sigma-Aldrich) for 20 mins. 1 × PBS were added to remove the fixative, and then the CNS was dissected (Hafer and Schedl, 2006) and rinsed with 1 × PBS with 4% Triton-X 100 for 2 days at 4°C. After rinses, the CNS was embedded in 1% low melting temperature agarose (Peq gold) mixed with 200 nm red fluorescent beads (1:50,000), then introduced into a glass capillary and positioned well separated from each other. After solidification of the agarose, the capillary was mounted to sample holder, transferred to a Zeiss Lightsheet Z.1 microscope and the samples were extruded from the capillary for imaging. CNS images were acquired with a 20 ×/1.0 Apochromat immersion detection objective and two 10 ×/0.2 illumination objectives at five different views, with 1 µm z-intervals. Voxel resolution was 0.317 um.

Image processing and data analysis

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Collected multiview datasets were registered and fused with the Fiji Multiview Reconstruction plugin (Preibisch et al., 2010; Schindelin et al., 2012). Image datasets after multiview deconvolution were analysed with Vision4D 3.0.0 (Arivis AG). A curvature flow filter was first used to denoise the image dataset. Subsequently, a Blob Finder algorithm (Najman and Couprie, 2003) was applied to detect and segment bright rounded three-dimensional sphere-like structures in the images with 4.5 µm set as the diameter. Segmented objects with volume less than 15 µm3 were removed from analysis by segmentation filter to avoid unspecific signals. Subsequently, the number of nuclei and the x, y, z coordinates of the geometric center of each nucleus were output from Vision4D. Where manual counting was employed (Figure 1 and a randomly selected brp-GAL4 labelled CNS), Vision4D was used to visualise and iteratively proceed through and manually annotate the dataset. Example whole CNS datasets where functional neurons or glia are labelled are available (Jiao and McCabe, 2021a; Jiao and McCabe, 2021b). Raw coordinates of the centre of geometry for the nuclei for whole male and female CNS are available in Supplementary file 1. In two-dimensional representations, Z position is indicated by colour coding using the scheme below.

Scheme 1
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Z-position colour code employed in 2D representations.

Mathematical analysis

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The topological summaries methods employed have previously been introduced (Edelsbrunner and Harer, 2010; Ghrist, 2014; Rabadán and Blumberg, 2019; Chazal and Michel, 2021). For a motivating example of the principles underlying topological summaries, one could think of pearls forming a necklace. Topological summaries express the global structure of the necklace formed by the relationships between the positions of the individual pearls, but are invariant under translation and rotation of the necklace overall. Two such necklaces have topological summaries that are comparable even if the pearls in one have no relationship to the pearls in the other. It is the global structures—such as its circular shape on a large scale, or bulges on a smaller scale—formed by the relationships of the individual pearls of each one that matter.

We trained a machine learning classifier, specifically an SVM, on the CNS nuclei positions in order to evaluate its power in determining characteristics of the animal from which it was derived. The data encompassed all point clouds generated from all CNS lines (brp-GAL4, Syt1-GAL4, nSyb-GAL4, repo-GAL4, Supplementary file 1). Correlation significance (classification power) is determined by comparing the performance of the SVM on the actual classification task to one where each larva is randomly assigned a class.

Mathematically speaking, the nuclei positions from a single CNS form a point cloud, a finite set of points in R3. A possible, naive approach to SVM feature selection for point clouds would be to consider the mean, variance, or other modes of the distribution of pairwise distances within the cloud. These real-valued features could then be passed through, for example, radial basis function kernels for use in SVMs. We focused on very different kind of features, namely ones obtained from the topology of the point clouds. When the point cloud is of low dimension, such as the three-dimensional point clouds arising from nuclei position data, the following approach is relevant. Let X be a finite point cloud in R3. For any r≥0, we let Xr denote the same point cloud, but with each point replaced by a ball of radius r. As r increases, the sequence formed by the Xr expresses different topological features of X. By topological features, we here mean the presence or absence of multiple connected components, unfilled loops, and unfilled cavities.

The figure below illustrates this process in the case of a synthetic two-dimensional point cloud, but the idea extends to any dimension including whole CNS point clouds. When r is small, Xr is topologically very similar to X=X0, and is essentially a collection of disjoint points. When r is very large, Xr is topologically very similar to X∞, i.e., one giant, featureless blob. As the sequence Xr progresses through the continuum of scales between these two trivial extremes, it undergoes non-trivial topological changes: components merge, and loops form and later get filled. In higher dimensions, cavities of various dimensions likewise form and get filled in.

Scheme 2
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Illustrative 2-dimensional synthetic point cloud.

A small two-dimensional point cloud X viewed at four different scales 0<a<b<c, forming the filtration X=X0⊂ Xa⊂ Xb⊂ Xc.

In the parlance of TDA, we refer to this appearance and disappearance of topological structures as the birth and death of homology classes in various degrees. We capture the whole life cycle with a mathematical object called the persistent homology of the point cloud, which can be fully described by its persistence diagram, a planar collection of points (labelled by multiplicity), whose coordinates encode the birth and death of homological features. For the filtration in the figure above, the persistence diagram that tracks one-dimensional features (i.e. unfilled loops) contains only a single point with coordinates (x, y). Here, the first coordinate, x, is the radius at which the loop is first formed, and the second coordinate, y, is the radius at which the loop has just been filled in. In the example it is clear that a<x<b<y< c.

As multisets of points in the plane, persistence diagrams are not immediately usable as features for SVMs. One way to vectorise persistence diagrams and thus render them digestible by SVMs is to define kernels based on the diagrams, with the heat kernel (Reininghaus et al., 2015) being an oft-used candidate with nice properties. For persistence diagrams P and Q, the heat kernel can informally be defined by the inner product of two solutions of the heat equation—one with an initial condition defined by P, and the other one defined by Q.

In this analysis, we calculated the persistent homology of the alpha complex (Edelsbrunner and Mücke, 1994) of the point clouds, using GUDHI (The GUDHI Editorial Board, 2019). The heat kernels were computed using RFPKOG (Spreemann, 2021). Only the persistence diagrams in degree 1 were used. Since the number of whole CNS point clouds was relatively small, we subsampled each one randomly to 8000 points 100 times, producing a total of 3100 point clouds. This was done both in order to test the stability of the method and to ensure that the variability in the number of points in each cloud is not the source of any signal.

The hyperparameters involved, i.e., the SVM regulariser and the heat kernel bandwidth, were determined by a parameter search in the following way. Six point clouds from males and six from females were randomly selected. All 100 subsampled versions of each of these 12 constituted a training set, for a total of 1200 training point clouds. The remaining 1900 subsampled point clouds constituted the testing set. The Pearson’s correlation between the gender predicted by the SVM on the testing set and the ground truth was computed for each choice of hyperparameters, and a choice in a stable region with high correlation was selected: a regularisation parameter c=10 in the notation of Pedregosa et al., 2011 and a bandwidth of σ=1/100 in the notation of Reininghaus et al., 2015. For the simple distance distribution features, a similar parameter selection process yielded c=10 and a radial kernel bandwidth of 10^5.

Immunofluorescence and confocal microscopy

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Embryos were collected and staged at 25°C on apple agar plates supplemented with yeast paste. Standard methods were used for dechorionation, removal of the vitelline membrane and fixation (Bashaw, 2010). Embryos were stored in 100% ethanol at –20°C before IHC labelling. Embryos were stained with mouse anti-myc9EH10 (1:100, DSHB), visualised with goat anti mouse Alexa Fluor 488 (1:400, Jackson ImmunoResearch) together with conjugated goat anti HRP Alexa Fluor 647 (1:200, Jackson ImmunoResearch) and mounted in VectaShield (Vector Laboratories). Duel colour Z-stack images of stage 15/16 and late stage 17 embryos were obtained on a CSU-W1 Confocal Scanner Unit (Yokogowa, Japan) using two prime BSI express cameras (Teledyne Photometrics). For motor neuron and adult brain preparations, larval fillets from the third instar larvae, or brains from adults were dissected and fixed with 4% formaldehyde (Sigma-Aldrich) for 20 mins. After fixation, samples were rinsed with 1 × PBS and were washed in PBT overnight at 4°C, and then mounted in Vectashield antifade mounting medium. Z-stack images were obtained with a Leica SP8 upright confocal microscope.

For Deadpan staining, the CNS from the third instar larvae were dissected out and fixed with 4% PFA for 20 mins. After fixation, samples were rinsed with 1 × PBS, and permealised with PBT (1 × PBS + 4% Triton-X 100). Antibody stainings were done in PBT +5% normal goat serum. The dilution for chicken anti-GFP (Abcam) was 1:500, for rat anti-Deadpan (Abcam) was 1:50. Goat anti-chicken Alexa Fluor 488, and goat anti-rat Alexa Fluor 594 secondary antibodies were obtained from ThermoFisher and used at the 1:500 dilutions. The CNS were mounted in VectaShield antifade mounting medium, and imaged using a Leica SP8 upright confocal microscope.

Statistical analysis

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Column statistics analyses were performed using GraphPad Prism 9 (GraphPad Software). For Figure 1, statistical significance was determined by unpaired t-test. For Figures 2—4, statistical significances were determined by ordinary one-way ANOVA, followed by a Tukey’s honestly significant difference test when multiple comparisons were required. The distribution analysis in Figure 2 were performed using matlab (MathWorks). Distances between nuclei coordinates were calculated in matlab using code available at https://doi.org/10.5281/zenodo.6574838 and plotted as a histogram of distance distribution.

Appendix 1

Key resources table

Appendix 1—key resources table
Reagent type (species) or resourceDesignationSource or referenceIdentifiersAdditional information
strain, strain background (Escherichia Coli)One shot top10InvitrogenCat#: C404010
genetic reagent (D. melanogaster)y[1] w[*]; Mi{y[+mDint2]=
MIC}Syt1[MI02197]		Bloomington Drosophila Stock CenterPMID: 21985007BDSC:35973FLYB: FBal0314405
RRID:BDSC_35973		FlyBase symbol: Mi{y[+mDint2]=
MIC}Syt1[MI02197]
genetic reagent (D. melanogaster)y[1] w[*] Mi{y[+mDint2]=
MIC}Sh[MI10885]		Bloomington Drosophila Stock CenterPMID: 21985007BDSC:56260FLYB:
FBal0297530
RRID:BDSC_56260		FlyBase symbol: Mi{MIC}ShMI10885
genetic reagent (D. melanogaster)y[1] w[*];Mi{y[+mDint2]=
MIC}Shal[MI10881]		Bloomington Drosophila Stock CenterPMID: 21985007BDSC:56089FLYB: FBal0295200
RRID:BDSC_56089		FlyBase symbol: Mi{MIC}ShalMI10881
genetic reagent (D. melanogaster)y[1] w[*]; Mi{y[+mDint2]=MIC} Shab[MI00848]Bloomington Drosophila Stock CenterPMID: 21985007BDSC:34115FLYB: FBal0249123
RRID:BDSC_34115		FlyBase symbol:
Mi{MIC}ShabMI00848
genetic reagent (D. melanogaster)nSyb-GAL4Bloomington Drosophila
Stock CenterPMID: 18621688		BDSC: 39171FBgn0013342
RRID:BDSC_39171		Flybase symbol:
P{GMR57C10-GAL4}
genetic reagent (D. melanogaster)repo-GAL4Bloomington Drosophila
Stock Center PMID: 7926782		BDSC:7415FLYB: FBal0127275
RRID:BDSC_7415		FlyBase symbol: P{GAL4}repo
genetic reagent (D. melanogaster)repo-QF2Bloomington Drosophila Stock Centerdoi:10.1534/
genetics.116.191783		BDSC:66477FLYB: FBal0322908
RRID:BDSC_66477		FlyBase symbol: P{ET-QF2.GU}repo
genetic reagent (D. melanogaster)Shaw-GAL4Bloomington Drosophila
Stock CenterPMID: 21985007		BDSC:60325FLYB: FBal0304243
RRID:BDSC_60325		FlyBase symbol:
GAL4Shaw-
MI01735-TG4.1
genetic reagent (D. melanogaster)Ddc-GAL4Bloomington Drosophila Stock Center
doi:10.1006/
dbio.1994.1261		BDSC:7009FLYB: FBtp0012451
RRID:BDSC_7009		FlyBase symbol:
P{Ddc-GAL4.L}
genetic reagent (D. melanogaster)TH-GAL4Bloomington Drosophila Stock CenterPMID: 12555273BDSC:8848FLYB: FBtp0114847
RRID:BDSC_8848		FlyBase symbol:
P{ple-GAL4.F}3
genetic reagent (D. melanogaster)Trh-GAL4Bloomington Drosophila Stock Centerdoi:10.1371/journal.
pone.0010806		BDSC:38389FLYB:
FBtp0055412
RRID:BDSC_38389		FlyBase symbol:
P{Trh-GAL4.long}
genetic reagent (D. melanogaster)UAS_H2A-GFPSteve Stowers (Montana SU)doi:10.1371/journal.
pgen.1008609		FLYB: FBgn0001196
genetic reagent (D. melanogaster)QUAS_H2A-mCherrySteve Stowers(Montana SU)doi:10.1371/journal.
pgen.1008609		FLYB: FBgn0001196
genetic reagent (D. melanogaster)brp-GAL4This paper, available
upon request, https://www.epfl.ch/labs/mccabelab/resources/		FLYB:FBgn0259246See Materials and
Methods, Section 2
genetic reagent (D. melanogaster)Syt1-Gal4This paper, available
upon request, https://www.epfl.ch/labs/mccabelab/resources/		FLYB: FBal0314405See Materials and
Methods, Section 4
genetic reagent (D. melanogaster)Sh-Gal4This paper, available
upon request,https://www.epfl.ch/labs/mccabelab/resources/		FLYB: FBal0297530See Materials and
Methods, Section 4
genetic reagent (D. melanogaster)Shal-Gal4This paper, available upon request,https://www.epfl.ch/labs/mccabelab/resources/FLYB: FBal0249123See Materials and
Methods, Section 4
genetic reagent (D. melanogaster)Shab-Gal4This paper, available
upon request,https://www.epfl.ch/labs/mccabelab/resources/		FLYB: FBal0249123See Materials and
Methods, Section 4
genetic reagent (D. melanogaster)UAS_H2A::GFP-
T2A-mKok::Caax		This paper, available
upon request,https://www.epfl.ch/labs/mccabelab/resources/		FLYB: FBgn0001196See Materials and
Methods, Section 3
antibodyanti-myc9EH10(Mouse monoclonal)DSHBDSHB Cat# 9E 10, RRID:AB_2266850IF(1:100)
antibodyanti-GFP(Chicken polyclonal)AbcamCat#ab13970IF(1:500)
antibodyanti-Deadpan(Rat monoclonal)AbcamCat#ab195173IF(1:50)
antibodyGoat Anti-Mouse IgG (H+L), Alexa Fluor 488 (Goat polyclonal Secondary Antibody)Jackson
ImmunoResearch		Cat#115-545-166IF(1:400)
antibodyGoat Anti-Horseradish Peroxidase,Alexa Fluor 647 (Goat polyclonal)Jackson
ImmunoResearch		Cat#123-605-021IF(1:200)
antibodyGoat anti-Chicken IgY (H+L), Alexa Fluor 488 (Goat polyclonal Secondary Antibody)ThermoFisherCat#A-11039IF(1:500)
antibodyGoat anti-Rat IgG (H+L) Cross-Adsorbed, Alexa Fluor 594 (Goat polyclonal Secondary Antibody)ThermoFisherCat#A-11007IF(1:500)
recombinant DNA reagentpBID_DSCP-G-Gal4 (plasmid)McCabe Lab,Available
upon request.https://www.epfl.ch/labs/mccabelab/resources/		Cat# #35,200
recombinant DNA reagentpJFRC81-10XUAS-IVS-
Syn21-GFP-p10 (plasmid)		AddgeneCat#: 36,432
recombinant DNA reagentpHD-sfGFP Scareless dsRed (plasmid)AddgeneCat#: 80,811
recombinant DNA reagentpCFD3 (plasmid)AddgeneCat#: 49,410
recombinant DNA reagentpCR4 brp-Gal4This paper, available
upon request, https://www.epfl.ch/labs/mccabelab/resources/		CRISPR construct inserted
in D. Melanogaster
recombinant DNA reagentpBID LexO_H2A-mCherryGift from Steve Stowers
(Montana SU),
DOI: 10.1371/journal.pgen.1008609
recombinant DNA reagentpCS2+ChMermaid S188AddgeneCat#: 53,617
recombinant DNA reagentpBID-UAS_H2A::GFP-T2A-mKok::CaaxThis paper, available
upon request, https://www.epfl.ch/labs/mccabelab/resources/		construct inserted
in D. Melanogaster
sequence-based reagentpCFD3 gRNA brp-5’This paperGuide RNA for Brp CRISPR knock inGGTGAACCGA
CCGGGACAAC
sequence-based reagentpCFD3 gRNA brp-3’This paperGuide RNA for Brp CRISPR knock inGGGAGCCCCGC
GACCGCTCC
sequence-based reagentbrp Ha1 FoThis paperPCR primerGAGAGAGCATCT
CGATTGTGCCGTGTG
sequence-based reagentbrp Pam7 ReThis paperPCR primerAATGTTGTCCCG
GTCGGTTCACCG
sequence-based reagentbrp Pam7_In1 ReThis paperPCR primerTTCTAGCGTCCAA
CGGCTCAGCTGTG
GGCCATTTTCTAGT
AATGTTGTCCCGG
TCGGTTCACCG
sequence-based reagentbrp HA_In1 FoThis paperPCR primerACTAGAAAATGGCC
CACAGCTGAGCC
sequence-based reagentbrp V5_In1 ReThis paperPCR primerTAGAATCGAGACCG
AGGAGAGGGTTAGGG
ATAGGCTTACCCATT
GCTGAAATTCACACA
CACACAGAATTCATGAG
sequence-based reagentbrp V5_ FoThis paperPCR primerGGTAAGCCTATCCC
TAACCCTCTCCTC
sequence-based reagentbrp PB5’ ReThis paperPCR primerTTAAGGGATCTTTCTA
TTAGTATAACACTGCATGC
sequence-based reagentbrp Ex2 foThis paperPCR primerAAATTGCATGCAGTGTT
ATACTAATAGAAAGATCC
CTTAATCGGCAGTCCAT
ACTACCGCGACATGGATG
sequence-based reagentbrp Pam2_ReThis paperPCR primerTCTGGAGCGGT
CGCGGGGC
sequence-based reagentbrp Pam2_Brp Ha2 ReThis paperPCR primerGCTCGTCCTCTAGGTAC
AGGCCCCGTTCGAGGGA
TCTGTCTCTGGAGC
GGTCGCGGGG
sequence-based reagentbrp Ha2 FoThis paperPCR primerGACAGATCCCTC
GAACGGGGCC
sequence-based reagentSyn21 H2A FoThis paperPCR primerAACTTAAAAAAAAAA
ATCAAAATGTCTGGA
CGTGGAAAAGGTGGC
sequence-based reagentH2A ReThis paperPCR primerCCCAAGAAGACC
GAGAAGAAGGCC
sequence-based reagentH2A-GFP FoThis paperPCR primerACAGGCTGTTCTGT
TGCCCAAGAAGACC
GAGAAGAAGGCCAT
GGTGTCCAAGGG
CGAGGAG
sequence-based reagentGFP-T2A ReThis paperPCR primerGGGTTCTCCTCCAC
ATCGCCGCAGGTCAG
CAGGCTGCCGCGGC
CCTCCTTGTACAGCT
CATCCATGCCCAGG
sequence-based reagentT2A-mKok FoThis paperPCR primerGCGGCAGCCTGCT
GACCTGCGGCGATG
TGGAGGAGAACCCC
GGGCCCATGGTGAGT
GTGATTAAACCAG
AGATGAAGATG
sequence-based reagentmKok-Caax ReThis paperPCR primerTTACATAATTACACA
CTTTGTCTTTGACTT
CTTTTTCTTCTTTTTA
CCATCTTTGCTCATGG
AATGAGCTACTGCAT
CTTCTACCTGC
chemical compound, drugFormaldehyde 37%SigmaCat#: 252,549
chemical compound, drugLow melt agarosePeq goldCat#: 35–2010
chemical compound, drugVECTASHIELD
Antifade Mounting Media		VECTOR LaboratoriesCat#: H-1000
chemical compound, drugFluoSpheres, 0.2 µm, red fluorescent (580/605)Thermo Fisher ScientificCat#: F8810
commercial assay or kitZero Blunt TOPO
PCR Cloning Kit		InvitrogenCat#: 450,245
commercial assay or kitpCR8/GW/TOPO
TA Cloning Kit		InvitrogenCat#: K250020
commercial assay or kitGateway LR Clonase
II Enzyme mix		InvitrogenCat#:11791020
commercial assay or kitNEBuilder HiFi
DNA Assembly Master Mix		New England BiolabsCat#: E2621S
commercial assay or kitKLD enzyme mixNew England BiolabsCat#:M0554S
commercial assay or kitPlatinium
Superfi polymerase		InvitrogenCat#:12359010
software, algorithmCNS nuclei distance
(code for Matlab)		https://doi.org/10.5281/zenodoThis manuscript
software, algorithmFijihttps://fiji.sc/RRID:SCR_002285
software, algorithmArivis Vision4D 3.0.0ArivisRRID:SCR_018000
software, algorithmMATLAB (R2018a)MathWorksRRID:SCR_001622
software, algorithmGraphPad Prism 9.0GraphPadRRID:SCR_002798

Data availability

All data generated or analysed during this study are included in the manuscript and supporting files. A source data file has been provided for all figures. Raw co-ordinates of the center of geometry of CNS nuclei for all animals is attached as Supplementary file 1. Matlab code employed is available at https://doi.org/10.5281/zenodo.6574838. Example unprocessed whole CNS microscopy data is publicly available for neurons - https://doi.org/10.5281/zenodo.5585334 and for glia https://doi.org/10.5281/zenodo.5585358.

The following data sets were generated
    1. McCabe B
    2. Jiao W
    (2021) Zenodo
    Whole Brain Drosophila Larval Neurons.
    https://doi.org/10.5281/zenodo.5585334
    1. McCabe B
    2. Jiao W
    (2021) Zenodo
    Whole Brain Drosophila Larval Glia.
    https://doi.org/10.5281/zenodo.5585358

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Article and author information

Author details

  1. Wei Jiao

    Brain Mind Institute, EPFL - Swiss Federal Institute of Technology, Lausanne, Switzerland
    Contribution
    Conceptualization, Data curation, Formal analysis, Investigation, Methodology, Resources, Validation, Visualization, Writing – original draft, Writing – review and editing
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0003-1536-5937

  2. Gard Spreemann

    Brain Mind Institute, EPFL - Swiss Federal Institute of Technology, Lausanne, Switzerland
    Present address
    Telenor Research, Fornebu, Norway
    Contribution
    Conceptualization, Investigation, Methodology, Software, Validation, Visualization, Writing – original draft, Writing – review and editing
    Competing interests
    No competing interests declared

  3. Evelyne Ruchti

    Brain Mind Institute, EPFL - Swiss Federal Institute of Technology, Lausanne, Switzerland
    Contribution
    Resources, Visualization
    Competing interests
    No competing interests declared

  4. Soumya Banerjee

    Brain Mind Institute, EPFL - Swiss Federal Institute of Technology, Lausanne, Switzerland
    Contribution
    Resources
    Competing interests
    No competing interests declared

  5. Samuel Vernon

    Brain Mind Institute, EPFL - Swiss Federal Institute of Technology, Lausanne, Switzerland
    Contribution
    Investigation
    Competing interests
    No competing interests declared

  6. Ying Shi

    Brain Mind Institute, EPFL - Swiss Federal Institute of Technology, Lausanne, Switzerland
    Contribution
    Formal analysis, Methodology
    Competing interests
    No competing interests declared

  7. R Steven Stowers

    Department of Microbiology and Cell Biology, Montana State University, Bozeman, United States
    Contribution
    Resources, Writing – review and editing
    Competing interests
    No competing interests declared

  8. Kathryn Hess

    Brain Mind Institute, EPFL - Swiss Federal Institute of Technology, Lausanne, Switzerland
    Contribution
    Methodology, Supervision, Writing – original draft, Writing – review and editing
    Competing interests
    No competing interests declared

  9. Brian D McCabe

    Brain Mind Institute, EPFL - Swiss Federal Institute of Technology, Lausanne, Switzerland
    Contribution
    Conceptualization, Funding acquisition, Project administration, Supervision, Writing – original draft, Writing – review and editing
    For correspondence
    brian.mccabe@epfl.ch
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0003-1620-0501

Funding

Swiss National Science Foundation (31003A_179587)

  • Brian D McCabe

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

Acknowledgements

This work was supported in part using the resources and services of the BioImaging & Optics Platform (BIOP) Research Core Facility at the School of Life Sciences of EPFL and we are especially thankful for the assistance of Arne Seitz. We are grateful to Hugo Bellen, Benjamin White, Gerry Rubin, Vanessa Auld, Christopher Potter, Mel Feany, Serge Birman, Ed Kravitz, Chris Doe, and Pavel Tomancak for generating Drosophila stocks, software and providing advice. Stocks obtained from the Bloomington Drosophila Stock Center (NIH P40OD018537) were used in this study.

Version history

  1. Received: October 25, 2021
  2. Preprint posted: November 4, 2021 (view preprint)
  3. Accepted: June 9, 2022
  4. Version of Record published: July 8, 2022 (version 1)

Copyright

© 2022, Jiao 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. Wei Jiao
  2. Gard Spreemann
  3. Evelyne Ruchti
  4. Soumya Banerjee
  5. Samuel Vernon
  6. Ying Shi
  7. R Steven Stowers
  8. Kathryn Hess
  9. Brian D McCabe
(2022)
Intact Drosophila central nervous system cellular quantitation reveals sexual dimorphism
eLife 11:e74968.
https://doi.org/10.7554/eLife.74968

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