Large dimension, high-resolution imaging is important for neural circuit visualisation as neurons have both long- and short-range patterns: from axons and dendrites to the numerous synapses at terminal endings. Electron Microscopy (EM) is the favoured approach for synaptic resolution imaging but how such structures can be segmented from high-density images within large volume datasets remains challenging. Fluorescent probes are widely used to localise synapses, identify cell-types and in tracing studies. The equivalent EM approach would benefit visualising such labelled structures from within sub-cellular, cellular, tissue and neuroanatomical contexts. Here we developed genetically-encoded, electron-dense markers using miniSOG. We demonstrate their ability in 1) labelling cellular sub-compartments of genetically-targeted neurons, 2) generating contrast under different EM modalities, and 3) segmenting labelled structures from EM volumes using computer-assisted strategies. We also tested non-destructive X-ray imaging on whole Drosophila brains to evaluate contrast staining. This enabled us to target specific regions for EM volume acquisition.
The ability to identify individual neurons based on their molecular, physiological and connective properties is a fundamental goal in neuroscience. A major part of this effort comes from imaging neurons, from the tracing of intricately branched axons and dendrites that span 10–100s of microns, to the identification of thin neurite endings and synaptic sites that are 10–100s of nanometre in diameter. Identifying all the patterns a single neuron makes reveals not only where the synaptic connections are and what the partner neurons may be, it also gauges its contribution to the functional network it resides in. This requires a volume-imaging approach that not only encompasses millimetre-micron wide dimensions but that also features the appropriate nanometre-scale resolutions. From a functional perspective, it is also crucial that particular neuron types can be identified based on specific molecular, morphological or physiological characteristics. For experimental paradigms, it would also be ideal if they can be easily identified between image datasets for comparative analyses. In this respect, given the complex connectivity patterns within a 3D brain environment, the specific identification and tracing of individual highly interconnected neurons from highly heterogenous neuronal populations remains a very challenging task1.
Recent EM techniques are well suited for large volume and high-resolution imaging, capable of capturing every axon and dendrite, synaptic and sub-synaptic feature2,3. Various volume EM techniques are currently available2,3,4,5,6. Serial sectioning followed by transmission electron microscopy (ssTEM) was the key method used to map the C. elegans nervous system, and was subsequently used in Drosophila and mouse7,8,9. Obtaining large numbers of manually generated, serial aligned and registered images from 100–1000s of sections is technical demanding10,11,12,13,14,15. Two recent imaging techniques, using serial block face scanning electron microscopy (SBF-SEM or SBEM) and focus ion beam scanning electron microscopy (FIBSEM), offer good alternatives as tissue blocks undergo automated cycles of image acquisition and sectioning that are typically well aligned3,5.
One recurrent challenge lies in image segmentation (here also termed as reconstruction)2,16. Dense reconstruction strategies involve tracing all neurites and synaptic features from the image volume, followed by feature and identity annotations9,17,18,19. Alternatively, sparse mapping strategies reduce the analysis to fewer neurons of interest, by choosing the most relevant features from the image volume for further analysis8,20,21,22. In both cases, these manual tasks are time-consuming and error-prone, and tracing needs to be repeated and expert-supervised to generate a consensus2,23,24,25. Novel computational approaches are also being deployed26,27,28,29,30. Nonetheless, these methods also have substantial error rates that preclude fully automated global solutions2. In practice, while no single procedure is perfect, multiple approaches can work in a complementary manner2,17,24,30,31.
EM-visible protein tags that generate electron-dense contrast can help in this effort. Acting as guides, molecularly defined neurons, synaptic sites or targets of choice can be highlighted to map circuits of interest. Such probes include enzyme peroxidases (such as HRP or APEX)32,33,34,35, photo-sensitiser proteins (such as miniSOG)36, and photosensitive dyes that associate with proteins37, or short peptides, such as ReASH38. These provide genetic solutions where cells can express these probes in situ, which are then processed for EM contrast. To date, while there have been some success, further improvements must be made to extend their targeting capabilities, labelling properties and contrast detection on the neuronal ultrastructure32,33,36,39.
Given the existing challenges in visualising the nervous system, we explored ways by which genetically encoded electron-dense probes can be used to visualise labelled neurons under various volume EM modalities. As EM projects are typically time and labour-intensive we investigated the conditions for optimal labelling, contrast staining, and sample preparation of fly brains. This was also motivated from personal experience: we find that image quality tends to be variable in terms of ultrastructure and contrast staining. Selecting specimens for EM imaging is somewhat error-prone. Without prior knowledge, sub-optimal samples are often used, resulting in wasted efforts. We investigated micro-Computed Tomography (micro-CT, also known as X-ray microscopy or XRM) as a means to assess specimen quality. While biological micro-CT/XRM is typically associated with low contrast detection in soft tissues, heavy metal and osmium-based contrast can be detected, deriving useful cell biological and neuroanatomical information40,41,42,43,44. With recent improvements and the availability of laboratory-based scanners, biological materials can be routinely scanned, yielding sub-micron resolutions43,44. Knowing which area to acquire EM images from is paramount as the field dimension is typically restricted, especially for TEM and FIBSEM, to about 10–20 µm3. This cannot be judged easily by visual inspection of the sample alone. We found that XRM could be used for this purpose. Given that this is a non-destructive process, this allows for subsequent targeted EM image acquisition.
While several electron-dense probe types are available, we focused on miniSOG36 and for proof-of-principle studies, labelled olfactory neurons in the Drosophila adult brain. We find that miniSOG labels can be targeted to distinct neuronal sub-compartments, such as membranes, cytosol, synapses and mitochondria. Through modifications in osmium and heavy metal staining, contrast introduced by the genetic label and on membrane boundaries, organelles and synaptic features can be further enhanced. The miniSOG label can be detected under TEM, SBEM or FIBSEM modalities. We explored the use of computer-based strategies to segment labelled structures throughout the volume and reveal some of the cellular and neuronal features that can be identified using these methods. Given the compatibility in contrast detection, we explored a new imaging technique, micro-computed tomography (micro-CT or X-Ray Microscopy/XRM). This allowed us to perform non-destructive X-ray imaging on intact brain samples to screen for optimally stained specimens. At submicron resolutions, macro- and micro-scale features, such as neuropil regions, axon tracts and individual cell somata could also be distinguished from these scans. This was followed with targeted volume EM acquisition to investigate features of interest at nanometre-scale resolutions.
Design, expression and label detection of miniSOG probes
In our EM labelling strategy, we wanted to develop protein-based probes that can be selectively expressed in discrete neurons, such as through the UAS-GAL4 binary expression system45. The probe should also be flexible enough to label any localised region within the cell. As we aim for probe detection under electron-dense detection modality, the contrasting procedures (probe expression, localised targeting and contrast staining) must also be sufficiently robust and discernable over the surrounding cellular ultrastructure, throughout the image volume. The surrounding region should also be sufficiently contrasted for features of interest, such as synapses, organelles and the plasma membrane.
We cloned miniSOG DNA into Drosophila UAS expression vectors that are controllable using GAL4 drivers and initially analysed these probes in cultured Drosophila S2 cells under fluorescence microscopy (Fig. 1a–c; Methods). We found that miniSOG fluorescence photobleached quickly under wide-field fluorescence illumination. To circumvent this, bright, photostable FPs (tagRFP or mKate2) fusions were incorporated. Our aim in probe design was to ensure miniSOG labels can be detected using fluorescence microscopy and that its expression did not cause morphological artefacts in the neurons they were expressed in. Several probes were tested in this way, targeting miniSOG to the plasma membrane, synapse, cytosol or mitochondria. Using the Drosophila UAS-GAL4 system45, their expression in olfactory neurons in the adult brain were monitored by confocal microscopy detecting either for miniSOG or FP fluorescence or by immunostainings (Fig. 1e–i). Based on light-level analysis, we verified that their expression did not cause any gross axonal or dendritic targeting defects.
As previously reported, miniSOG labelling is based on photo-oxidation36 where blue light illumination is used to oxidise the substrate, Diaminobenzidine (DAB). This results in a brownish, osmophillic stain, visible in brain regions where miniSOG was expressed (Supplementary Figure 1), serving as a useful indicator of the photo-conversion process. In our tests, specimens that expressed multi-copy versions of miniSOG, either as tandem motifs within a single fusion protein or multicopy transgenes showed stronger DAB labelling. Hence, the use of tandem motifs and multicopy transgenes helps to promote DAB labelling. However, careful considerations must also be taken to determine how much DAB labelling is sufficient for EM-level visualisation and ultrastructure preservation (see Discussion).
Effect of contrasting agents on miniSOG-DAB labelling under EM
Having successfully introduced these probes into specific neurons by genetic targeting, we next determined whether miniSOG contrast could be detected under EM. Photo-oxidised samples were initially processed using standard osmium staining, followed by epoxy resin embedding. Ultrathin sections from brain samples that express membrane-targeted miniSOG (myr-miniSOG) in Mushroom body (MB) neurons (also known as Kenyon cells or KCs) or projection neurons (PNs) were imaged under TEM (Fig. 2b–f). Label contrast was visible in superficial (vertical lobe tip, <10 µm from brain surface) and deeper layers (peduncle, ~100 µm from surface; mid-brain) of the brain (Fig. 2b,c). Consistent with membrane localisation, the miniSOG-DAB label was localised to the membrane and proximal regions of the cytoplasmic space.
Given that the miniSOG and cellular contrast using standard osmium staining appeared weak in these samples, we next explored ways to enhance the contrast in brain tissue. Differences in osmium and heavy metal staining lead to variations in the labelling of cellular and tissue structures, affecting contrast and image detection on the electron microscope used46,47,48,49. Cytoplasm, membrane boundaries, organelles and synaptic densities can be enhanced by contrast stains. While on-section treatments (uranyl acetate and Reynold’s lead citrate) for TEM is routine, this procedure is highly labile46. For volume imaging, this needs to be tightly controlled so that all sections achieve consistency. For fly brain samples, while on-section stains enhanced the miniSOG contrast, the use of en bloc (bulk) stains provided a good alternative as contrast on the miniSOG-DAB and the surrounding ultrastructure was also enhanced (Fig. 2d–f). Furthermore, en bloc procedures are not only applicable for block-face imaging (SBEM and FIBSEM), but they also help to reduce charging effects by grounding the sample with heavy metals47. Even by Reduced Osmium-Thicarbohydrazide-Osmium (ROTO) staining alone, good levels of contrast can be detected when imaged under TEM, SBEM and FIBSEM (Fig. 2g; also Figs 3 and 4).
miniSOG contrast detection in other neuronal sub-compartments
When visualised under TEM or SBEM, we found the miniSOG probes we had designed to target to cytosol, synapses or mitochondria were also correctly localised and DAB labelling produced a good level of contrast in these subcellular compartments (Fig. 2g–j). These probes are useful in several ways. First, synapses and mitochondria are highly relevant to neuronal function and are best studied at nm-resolution: genetic labels can be used to visualise them with cell-targeted precision. Second, large numbers of labelled structures can be selectively visualised in very large volumes (see Fig. 3). Third, some probes can act as proximity markers, by labelling relevant neurons or associated structures without obstructing other relevant ultrastructures. As illustrated in Fig. 2i and j, putative chemical synapses and gap junctions can be distinguished close to mitochondria-labelled miniSOG. Last, acting as a whole cell tracer, the cytosol-targeted miniSOG has been useful in outlining labelled neurons (see Fig. 3 below).
Enhanced contrast based segmentation from miniSOG-labelled EM volumes
We next generated EM volumes from miniSOG-labelled samples. Different acquisition and segmentation strategies were explored to see how to best visualise the label from image stacks. From the Drosophila brain, images were collected from the different regions of olfactory processing centres50, such as the lateral horn (LH, or lateral protocerebrum) that is a higher order olfactory processing centre and target site of PN axons, and the Antennal Lobe (AL), which is the olfactory information processing site between olfactory sensory axons and projection neuron dendrites. These image stacks were acquired on SBEM microscopes that have different sensitivities and configurations (see Methods). From both image volumes, robust contrast on miniSOG and the surrounding ultrastructure (membranes, organelles and synaptic compartments) was visible (Fig. 3, see Videos 2 and 3).
Given the enhanced contrast, segmenting miniSOG-DAB labelled structures should be straightforward. While manual segmentation is the most direct, we focussed on automating segmentation for several reasons. First, computational tools can readily identify labelled structures from the image stack by thresholding. This was the case when bulk segmentation was applied to a SBEM volume that had mitochondria-targeted miniSOG (Fig. 3a and b, Video 2). Second, once defined, such regions of interest can be further interrogated computationally for desired features of interest. For instance, we can determine pixel values, volume, aspect ratio and orientation properties of the segmented objects (Fig. 3a; Video 2). Third, we find computer-assisted visualisation is able to detect subtle differences in the contrast due to miniSOG labelling. This was particularly useful when applied to low contrast-low signal SBEM images, as shown in the seed segmentation example, thus achieving greater accuracy in neural tracing (Fig. 3c and d, Videos 3 and 4). Fourth, and related to the above, computational tools will have a robust record of the selection criteria used. This is useful if the procedure needs to be replicated across datasets, or altered to define, correct or specify for new or existing features or sub-features. Last, computational tools can readily exploit 3D segmentation tools in the first instance. This aids quicker review over the objects identified (Fig. 3).
Note however that while initial results from such segmentation strategies can be obtained relatively quickly, cell biological and neuroanatomical expertise is necessary to review the identified objects. Following initial review, iterative segmentation steps help to refine the desired objects (Fig. 3, see Discussion). As these probes can also be visualised under fluorescence microscopy, EM traces can be cross-validated with the light-based images. Cross-validation can also be performed using Micro-CT/XRM, see below.
Micro-CT/XRM visualisation and correlation to brain regions for targeted volume EM acquisition
We were motivated to test micro-CT/XRM as an application to, 1) select optimally stained samples for EM data acquisition (prior to lengthy EM volume imaging), 2) for its ability to image whole brains non-destructively and, 3) to obtain cell biological and neuroanatomical information across very large volumes at sub-micron resolutions (Fig. 4a). Osmium-treated and epoxy-embedded fly brains were imaged on a Zeiss Xradia Versa 520 lab-based scanner. From these scans, many features were recognisable. Images were similar to those obtained from light microscopy and from scans using synchrotron-based X-ray sources51,52, respectively (Fig. 4b). In addition, our XRM images also highlighted individual cell somata from the cortical rind (perikaya) surrounding the brain, as well as axon tracts. Both appear negatively stained. Surrounding cell membranes and densely packed neuropil regions such as the antennal lobe (AL), mushroom body peduncle (MBped) and calyx (MBCA) and optic lobe lamina and medulla layers showed higher levels of staining (appearing white or light grey in Fig. 4b, see also Video 5).
A recent study showed miniSOG generated contrast in mouse brain tissue can be detected using XRM43. When miniSOG labelled Drosophila brains were scanned, contrast from labelled PN neurons clearly highlighted axon tracts and terminal boutons (appearing white in Fig. 4c; Video 6). However, labelling from within the AL glomeruli was not seen. One possible reason for this is the high level of native contrast in this densely innervated region makes any genetically introduced contrast less likely to stand out.
As part of the EM workflow, we transferred the miniSOG labelled sample to a FIBSEM microscope. From the initial XRM scan, we noticed that the bilateral miniSOG+ PN axonal structures were unevenly labelled within the specimen, with the left side having lower signal at the PN terminals in the MBCA (Fig. 4c). The reason for this is unclear, it may have occurred during the photo-oxidation or the post-staining process. Nonetheless, the XRM scan allows us to select the right MBCA as the ideal region of interest from which to acquire a FIB image sub-volume, which was approximately 0.075% of the total brain volume.
We established a correlation between FIBSEM and XRM by registering the SEM field image on the sample surface to virtual slices from the XRM volume, enabling the precise targeting to the region of interest. Using FIBSEM, we acquired image stacks from the mushroom body calyx (Ref volume: 150915-R2/5; volume dimensions: 40 × 20 × 18 µm; voxel dimension: approx. 10 × 10 × 10 nm; z-slices: 1800). Here we find the overall contrast and of the level of miniSOG labelling of the cytosol of PN axon terminals were very high. Comparisons between the XRM and FIBSEM tomograms showed the label contrast closely matched each other (Fig. 4d; Video 7). We are interested in the Mushroom Body calyx (MBCA) as it is a higher order olfactory processing region where PN axon terminals synapse with Kenyon cell (KC) dendrites50. Indeed, closer inspection of the FIBSEM images revealed very fine diameter KC dendrites surrounding the PN boutons (Fig. 4e), similar to previous reports53,54.
In summary, using XRM, we were able to screen candidate samples for optimal labelling characteristics and perform site-specific volume image acquisitions using FIBSEM. Having whole brain XRM images also provides many cell and neuroanatomical relevant features that are useful for subsequent reconstruction and analysis.
Probe labelling is a key method in biological imaging. The ability to highlight specified structures helps decipher how macromolecular complexes, cellular components, cells and tissues are organized, giving insight into their function. In neuroscience, given the diversity of molecular, cellular and physiological substrates, fluorescent probes have been used extensively in cell biological, neuroanatomical and neurophysiological studies55,56,57. Yet adopting them for the purpose of light-based neural circuit reconstruction has limitations as it is unclear how segmentation can be implemented on densely labelled neurites across large dimensions and at high resolution. Volume EM techniques are therefore favoured, with acquisition volumes of >6,000,000 μm3 and 4–50 nm voxel resolution already reported5. However, given the large amount of high-density data, working out how individual axon, dendrites and synapses are represented as neural network-based entities requires substantial reconstruction time2.
In this study, we have focused on EM-visible probes, which are genetically-encoded, highly compatible with sample preparation methods and capable of high resolution visualisation. These criteria facilitate the ease of labelling, promote ultrastructure preservation and contrast generation. This allows for a single EM modality to detect the genetically introduced label and discriminate cellular ultrastructure and both are acquired at identical nm-scale resolutions. Our feasibility study acquired volume datasets from olfactory centres in the Drosophila adult brain that are densely innervated. From these studies, several observations were made, which are discussed below.
When expressed in Drosophila neurons, we find that miniSOG works effectively when targeted to distinct cellular sub-compartments. This is a marked improvement over other EM probes such as HRP, which have limited targeting capabilities32,33,39, or ReASH, which necessitates cell-toxic conditions for probe introduction58. One initial concern was whether the inaccessibility of blue light in deeper tissue regions might hamper the labelling process34. With protocols used here, DAB label was visible in the mid-brain, ∼100 µm depth. One protocol adaptation was to perform photo-oxidation using blue-light LEDs (see Methods).
One area of continued development will be to gauge how much DAB label is sufficient for image detection. This is delicate balance, avoiding under- and over-labelling the sample, and multiple parameters, such as probe expression level, localised targeting, labelling density, DAB photo-oxidation, fixation conditions, heavy metal staining and microscope settings play a role in the EM visualisation of the labelled product. Thus, our current approach is based on multiple trials, where many samples are collected over the course of the DAB photo-oxidation step. The tandemisation approach, by attaching multiple miniSOG probes to a single targeting motif, together with multi-copy transgene expression, helps not only to promote DAB labelling, but also provides a broader array of labelled samples, increasing the chance of finding the optimal specimen. While this does not impact on the study’s conclusions, ideal probes ought to be small and minimally expressed in order to reduce the possibility of disrupting cell function. Related to this, our fluorescence imaging tests suggest that not all probes tested are currently optimal. For example, while the mitochondrial-targeted miniSOG does not perturb PN axon or dendrite targeting, as judged by light microscopy, mitochondria labelled miniSOG appeared aggregated at the cell body and less frequently in distal axon termini. Closer EM-level examination shows some mitochondria appear smaller and fragmented. Axon fragmentation was also prevalent in the LH in the specimen of a 7-day old adult fly. This suggests high levels of mitochondria-miniSOG expression may lead to neurotoxicity over time. Perhaps related to the above, we find expressing high-levels of mitochondria resident proteins, whether untagged or tagged with miniSOG, also resulted in similar aggregation, loss (or partial loss) of neurons and neurite segment phenotypes (unpublished observations). In C.elegans, high levels of miniSOG expression in the mitochondria also caused neurotoxicity and cell death59. Nonetheless, given that label contrast can be detected in mitochondria and serve an important purpose, refined probes will facilitate further improved use. Further improvements will also come from re-engineered probes60,61 and by tuning their expression close to wild-type levels, while providing sufficient levels of discrimination under EM and XRM.
To aid segmentation, labelling probes should fulfil several key criteria. Exhibiting highly localised contrast is critical. The label needs to be detected uniformly throughout the regions and structure of interest targeted. Label generation needs to be minimally disruptive for image detection; any background artefact introduced has to be minimal. Several aspects were addressed in this study. Highly localized miniSOG contrast was consistently observed. Segmentation throughout the volume suggests artefacts and background effect were minimal. In any imaging paradigm, there are always concerns regarding the extent of targeting and labelling density any probe can achieve. In the course of neurite tracing using cytosolic miniSOG, we found that segmentation errors can result from signal drop-off, particularly at dendritic branch points and at large axonal segments where it was more difficult to achieve high or uniform levels of labelling. Such errors are easily detected when imaging at nanometre-scale resolutions. Nonetheless, with expert knowledge of projection patterns and by looking at the underlying ultrastructure, such errors can be easily rectified (see Video 8 for examples). Thus, one area of continued development will be to determine how each designed probe can achieve optimal labelling at targeted sites of interest. One easy way is to allow for more DAB label to develop. However, overdevelopment can generate labelling artefacts and result in the loss of resolution (Supplementary Figure 2). Masking, where the underlying ultrastructure is obscured by DAB labelling, is also another concern.
Labelling approaches provide a simple way to extract information from complex biological images. As we have shown using miniSOG, labelled neuronal components can be easily segmented from high-density EM images. Computational tools work well in this respect as discrete pixel-based criteria can be applied to the entire volume. As low- and high-order features become attributed to each segmented object, this forms a valuable way of linking them within the volume, facilitating large-scale, comparative and interpretive analysis. Future work will explore how such tools work best and the types of information that can be obtained with each probe. More tools will inevitably be needed to complement and complete the reconstruction process. This might include semi-automated and rules-based segmentation algorithms that reflect neuronal morphologies and cellular structures. While this manuscript was being finalised, we were encouraged to find similar approaches were also being developed to exploit genetically encoded EM marker based neural tracing in mouse neurons35. Similar approaches to adopt unsupervised segmentation of labelled neurons will be useful in our future work.
One interesting property of computer-assisted segmentation is the high degree of morphological complexity found in the dendritic arbours of labelled PNs, particularly in the lateral regions (Example 3 in Fig. 4d). The organisational significance of these intricate branch protrusions is unclear. Interestingly, high-resolution analysis in the AL of silkmoth Bombyx mori also show similar dense protrusions from the dendritic shafts of PNs62. These features are also reminiscent of the ‘twig-like’ or ‘spine-like’ structures recently found throughout Drosophila neurons analysed, where thin actin-rich and microtubule-free terminal neurites show high levels of synaptic input63. Future work will determine whether these tufted protrusions on PN dendrites carry specific molecular and regional identities or synaptic patterns required for AL connectivity.
Many aspects of fixation, labelling and contrast generation are not well understood and have led researchers to reinvestigate EM sample preparation methods to achieve better consistency47,48,49,64,65. The inability to predict if EM specimens are optimal leads to wasted efforts, which on any given microscope incurs days-weeks of acquisition time. If sub-optimal image volumes become incorporated into the segmentation workflow, this adds to further waste. This prompted us to investigate XRM as a method for checking sample quality. Our initial testing has shown it to be critical prior to EM volume acquisition. In addition, XRM has become an invaluable imaging tool, revealing cell body and long-range projections patterns as well as discrete brain regions. Future work will explore how the XRM can be used as a part of a reconstruction workflow to trace neurons across scales of whole brains, brain regions, axon and dendrite projections and ultimately leading to synaptic connectivity patterns under EM.
In summary, our study explores the implementation of EM-based reporters to label neurons in a whole brain setting. We propose a set of tools that uses genetically-encoded probes, enhanced contrast staining, automated image volume acquisition and computer-assisted segmentation for the dissection of complex neural circuits. By combining genetic labelling with the structural analysis of molecularly defined components, such targeted approaches help uncover local network motifs and synaptic connectivity patterns. They are especially valuable in identifying targeted neurons even within a restricted EM volume (which can be acquired in shorter periods of days) that does not include enough of the neuronal arbour for cell type identification by morphology. With these approaches, we can contemplate scaling towards comparative analyses, to determine how circuit properties are altered under the influence of genetic, environmental and physiological cues. With enough examples from different samples and brain regions, their insights can contribute to wider EM neural reconstruction efforts that are taking place across larger regions and to the general understanding of the nervous system organization.
Although our own research focuses on neural circuitry, these tools will also be very useful in cell and developmental biology and disease model studies. With a focus on large dimension, high-resolution based imaging, EM probes can be used to identify rare features (e.g. transient structures or cell types that arise from morphogenetic or pathological events), or to acquire large datasets for ultrastructural studies of specific cellular components.
Drosophila stocks and immunohistochemistry
Brain samples were dissected from 3–7 day old adult males. GAL4 drivers used have been previously described66,67,68. Immunostaining was performed as previously described69. miniSOG antibodies were generated in guinea pigs (Eurogentec S.A., Seraing, Belgium).
miniSOG design, vector construction and Drosophila transgenesis
miniSOG DNA was custom synthesised (GeneArt, Life Technologies) for optimal codon expression in Drosophila, with the addition of restriction sites at the 5′ and 3′ ends to facilitate in-frame fusion cloning. To make tandem versions, several fragments were mixed together during restriction cloning into Drosophila expression vectors70. Probes were targeted to the plasma membrane using a Src myristoylation tag70. miniSOG fusion to the Drosophila Eb1 protein resulted in cytoplasm localisation. Eb1 DNA (Eb1-PE; Flybase ID: FBpp0089088) was made synthetically, as above. Synaptic targeting was achieved by fusing miniSOG to Synaptotagmin, similar to previous strategies69. Mitochondria-localisation was based on miniSOG fusion to a Drosophila gene product (CG18769; Isoform PG; Flybase ID: FBpp0300165), based on its sequence homology to the Mitochondria Calcium Uniporter gene (MCU). Its labelling characteristics in Drosophila neurons (Figs 2i and 3b) are very similar to previous studies34. All miniSOG fusions were incorporated at the COOH-terminal to the above-targeted proteins. Drosophila transgenic lines were derived from germline transformations (Bestgene Inc., CA, USA) using the ΦC31/attP system71.
miniSOG expression in S2 cells and Drosophila brain
miniSOG was initially tested in Drosophila S2 cells as described previously72 and analysed under confocal microscopy. miniSOG probes were expressed in vivo using neuronal GAL4 driver lines to express UAS-miniSOG products in mushroom body Kenyon cells (OK107-GAL466) or projection neurons (PNs) [using the GH146-GAL468 [or Mz19-GAL4, that label PN subsets innervating glomerulus DA1, VA1d and DC3)]67. Fluorescence images for miniSOG, tagRFP and mKate2 fluorescence data were acquired as previously described36 (http://evrogen.com/spectra-viewer/viewer.shtml).
Sample preparation for miniSOG photo-oxidation
Brain samples were processed similarly to previous studies36, with minor modifications. Drosophila adult whole brains were fixed overnight in 4% paraformaldehyde, 0.5% glutaraldehyde in 2 mM CaCl2, 0.1 M Cacodylate, (pH 7.4). These samples were kept cold whenever possible. Fixed brains were rinsed in chilled cacodylate buffer and were incubated in blocking buffers (in 0.1 M cacodylate) sequentially for 10–15 minutes each time in (1) 10 mM Glycine, (2) 10 mM Potassium Cyanide, (3) 5 mM 3-aminotriazole and (4) 5 mM Mersalyl acid, to reduce non-specific DAB staining. miniSOG photo-oxidations were initially performed using a 150W Xenon light source (Lambda DG-4alpha, Sutter Instruments, CA, USA) with a 20×/NA 0.75 Plan Fluor Nikon objective that was mounted on a Nikon TE2000 microscope. At 470 nm, this was approximately 1 W/cm2 with 3.8 mm2 field of view. Subsequently, a LED-based photo-oxidation unit was built (CREE; Code: 2216679; Part: XBDROY-00-0000-000000L01). This achieved illumination stability and several samples could be processed simultaneously. Samples were photo-oxidised for 2–20 minutes, being kept at 4 °C throughout. For some probes, it was possible to monitor the progress of this process due to the presence of the brownish DAB precipitation. This was not the case for mitochondria-localised miniSOGs.
Brain sample preparations for osmification, resin embedding and image acquisition
Different osmium and heavy metal stains were applied, following previous protocols46,48. The variations in osmification included the use of 1% osmium tetraoxide (standard), 1.5% potassium ferricyanide with 1% osmium tetraoxide (reduced osmium or RO) or reduced osmium-thiocarbohydrazide-osmium (ROTO; RO as above, followed by 1% thiocarbohydrazide and a second round of 1% standard osmium). For contrast stains, en bloc uranyl acetate and lead aspartate were applied to whole brain samples. On-grid staining included uranyl acetate and Reynold’s lead citrate; applied for 2–5 minutes prior to TEM imaging46. Epoxy (Durcupan ACM, Sigma Aldrich #44611) embedded samples were sectioned and visualised by TEM (Technai T12 Spirit, FEI, Hillsborough, OR, USA), using a 2 K × 2 K camera detector (BM-Orius, Gatan, Pleasanton, CA, USA). Following TEM verification, miniSOG-positive specimens were imaged using SBEM or FIBSEM. SBEM data was acquired using a 3View serial-block-face imaging unit (Gatan, Pleasanton, CA, USA) installed either with a high-vacuum Merlin or Sigma variable pressure (VP) field emission-SEM (Carl Zeiss Microscopy, Jena, Germany), equipped with either a 32 K × 32 K or a 8 K × 8 K camera detector, respectively. We noticed that SBEM operating at high vacuum will produce better contrast and resolved images than those operating under variable pressure mode. This is a direct result of the absence of gas scattering and higher surface sensitivity, enabling lower beam energies to acquire data during probe scanning. Similar results in brain tissue were recently reported elsewhere19. Apart from SBEM, volume data was also collected on an Auriga Crossbeam FIBSEM, equipped with the ATLAS 5 scan generator and software tools (Carl Zeiss Microscopy, Jena, Germany).
Image processing, visualization and segmentation analysis
Confocal microscopy data were acquired and processed as previously69. For EM images, individual TEM micrographs, single or sub-stacks of SBEM and FIBSEM images were inspected using Fiji73. Image pre-processing was applied as necessary to remove background noise, improve visualization and figure presentation. These filters included Thresholding, Smoothing, Gaussian blur, Non-Local Means and Sharpening. Image stack alignments were also performed as necessary using StackReg on Fiji. Figures are presented in 8-bit to reduce file size.
Large EM volume stacks were visualized and analysed using ORS Visual SI Advanced software (Object Research Systems Inc., Montreal, Canada; Carl Zeiss Microscopy GmbH, Jena, Germany). To facilitate better performance on the workstation, image datasets were downsampled by binning (3 × 3 × 1).
Following SBEM volume acquisition, two computer-assisted segmentation approaches were tried. For the mitochondria-miniSOG labelled volume (Ref: 140807-R04; 63 × 63 × 31 µm; voxel dimension: 6.3 × 6.3 × 50 nm; number of z-image sections: 624), given that the label was well contrasted and segregated, bulk segmentation was applied. Range values as determined from pixel probe readings and interactively setting minima and maxima threshold values. Once the selected range correlated with the labeled structure, a Region Of Interest (ROI) can then be defined. However, initially, all pixels corresponding to the desired range will be segmented from the image volume. High contrast but low volume objects were eliminated from the segmented dataset as these were corresponded to non-specific background signals (cutoff: <10 voxels; <0.0002 µm3). A further filter based on the variance intensity, eliminated larger, cell-based structures, such as highly contrasted cell membrane segments. The segmented objects were then examined in 2D and 3D, comparing them against the underlying ultrastructure. Following this, an Object Analysis function was applied. This produced an object mesh and listed all the segmented objects identified, together with their analysed features (voxel intensities, volume and orientation properties). SBEM image volume was acquired, using a 3View-Merlin SEM, from a specimen (Sample 10) that has been treated with ROTO with UA and Pb stains.
A seed-based segmentation method was applied to cytosol-miniSOG labelled PNs as that the label appeared contiguous and thus likely to have overlapping voxels (see Video 3). After defining the range values, a seed point (black pin icon) was placed at the cell body location. A Point and Click seeding function initiates the 3D segmentation process. Several trials were performed based on defined range intensities. Set to common maximum, increasingly lower range intensities were sampled (trial/ROI 1–12). Each step change represented 0.2–0.4% of the true range. This SBEM volume (Ref volume: 141127-R01; volume dimension: 86 × 86 × 13.5 µm; voxel dimension: 10.5 × 10.5 × 25 nm; z-sections: 541) was acquired using the 3View-Sigma VP SEM, from a ROTO treated specimen (E1). It was also used in TEM (Fig. 2g). The volume stack corresponds to mid - posterior location on the right AL. For segmentation analysis, the stack was image pre-processed by applying non-local means (sigma = 5).
Video editing was performed using ORS Visual SI Advanced and on iMovie (Apple Inc., Cupertino, CA, USA).
XRM/micro-CT analysis of epoxy embedded Drosophila brains
X-ray microscopy (XRM) was performed using a Zeiss Xradia Versa 520 (Carl Zeiss X-ray Microscopy, Pleasanton, CA, USA). The following settings were used to collect tomograms. The emission source was set at 70–80 kV and 6–7 W. The samples were placed 8.9 mm from RA-Source and 6.4 mm for RA-Detector. A LE1 source filter was used. A 40× optical magnification objective was used, resulting in a field image of 0.409 mm × 0.409 mm. With a 1950 × 1950 pixel image size, this translates to a 200 nm voxel size. The estimated reconstructed spatial resolution is 700 nm. The total scan time lasted 22–24 hours, based approximately on 17 sec exposure time and 360° degree rotation and step size of 0.11.
How to cite this article: Ng, J. et al. Genetically targeted 3D visualisation of Drosophila neurons under Electron Microscopy and X-Ray Microscopy using miniSOG. Sci. Rep. 6, 38863; doi: 10.1038/srep38863 (2016).
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Lichtman, J. W. & Denk, W. The big and the small: challenges of imaging the brain’s circuits. Science 334, 618–623, doi: 10.1126/science.1209168 (2011).
Helmstaedter, M. Cellular-resolution connectomics: challenges of dense neural circuit reconstruction. Nat Methods 10, 501–507, doi: 10.1038/nmeth.2476 (2013).
Briggman, K. L. & Bock, D. D. Volume electron microscopy for neuronal circuit reconstruction. Curr Opin Neurobiol 22, 154–161, doi: 10.1016/j.conb.2011.10.022 (2012).
Kuwajima, M., Mendenhall, J. M., Lindsey, L. F. & Harris, K. M. Automated transmission-mode scanning electron microscopy (tSEM) for large volume analysis at nanoscale resolution. PLoS One 8, e59573, doi: 10.1371/journal.pone.0059573 (2013).
Peddie, C. J. & Collinson, L. M. Exploring the third dimension: volume electron microscopy comes of age. Micron 61, 9–19, doi: 10.1016/j.micron.2014.01.009 (2014).
Eberle, A. L., Eberle, A. L., Mikula, S., Schalek, R. & Lichtman, J. High‐resolution, high‐throughput imaging with a multibeam scanning electron microscope. Journal of microscopy (Oxford) 259, 114–120, doi: 10.1111/jmi.12224 (2015).
White, J. G., Southgate, E., Thomson, J. N. & Brenner, S. The structure of the nervous system of the nematode Caenorhabditis elegans. Philos Trans R Soc Lond B Biol Sci 314, 1–340 (1986).
Bock, D. D. et al. Network anatomy and in vivo physiology of visual cortical neurons. Nature 471, 177–182, doi: 10.1038/nature09802 (2011).
Takemura, S. Y. et al. A visual motion detection circuit suggested by Drosophila connectomics. Nature 500, 175–181, doi: 10.1038/nature12450 (2013).
Cardona, A. et al. TrakEM2 software for neural circuit reconstruction. PLoS One 7, e38011, doi: 10.1371/journal.pone.0038011 (2012).
Saalfeld, S., Fetter, R., Cardona, A. & Tomancak, P. Elastic volume reconstruction from series of ultra-thin microscopy sections. Nat Methods 9, 717–720, doi: 10.1038/nmeth.2072 (2012).
Saalfeld, S., Cardona, A., Hartenstein, V. & Tomancak, P. As-rigid-as-possible mosaicking and serial section registration of large ssTEM datasets. Bioinformatics 26, i57–63, doi: 10.1093/bioinformatics/btq219 (2010).
Takemura, S. Y. et al. Cholinergic circuits integrate neighboring visual signals in a Drosophila motion detection pathway. Curr Biol 21, 2077–2084, doi: 10.1016/j.cub.2011.10.053 (2011).
Hayworth, K. J. et al. Imaging ATUM ultrathin section libraries with WaferMapper: a multi-scale approach to EM reconstruction of neural circuits. Front Neural Circuits 8, 68, doi: 10.3389/fncir.2014.00068 (2014).
Harris, K. M. et al. Uniform serial sectioning for transmission electron microscopy. J Neurosci 26, 12101–12103, doi: 10.1523/JNEUROSCI.3994-06.2006 (2006).
Lichtman, J. W., Pfister, H. & Shavit, N. The big data challenges of connectomics. Nat Neurosci 17, 1448–1454, doi: 10.1038/nn.3837 (2014).
Kasthuri, N. et al. Saturated Reconstruction of a Volume of Neocortex. Cell 162, 648–661, doi: 10.1016/j.cell.2015.06.054 (2015).
Helmstaedter, M. et al. Connectomic reconstruction of the inner plexiform layer in the mouse retina. Nature 500, 168–174, doi: 10.1038/nature12346 (2013).
Wanner, A. A., Genoud, C., Masudi, T., Siksou, L. & Friedrich, R. W. Dense EM-based reconstruction of the interglomerular projectome in the zebrafish olfactory bulb. Nat Neurosci 19, 816–825, doi: 10.1038/nn.4290 (2016).
Briggman, K. L., Helmstaedter, M. & Denk, W. Wiring specificity in the direction-selectivity circuit of the retina. Nature 471, 183–188, doi: 10.1038/nature09818 (2011).
Cardona, A. et al. An integrated micro- and macroarchitectural analysis of the Drosophila brain by computer-assisted serial section electron microscopy. PLoS Biol 8, doi: 10.1371/journal.pbio.1000502 (2010).
Ohyama, T. et al. A multilevel multimodal circuit enhances action selection in Drosophila. Nature 520, 633–639, doi: 10.1038/nature14297 (2015).
Saalfeld, S., Cardona, A., Hartenstein, V. & Tomancak, P. CATMAID: collaborative annotation toolkit for massive amounts of image data. Bioinformatics 25, 1984–1986, doi: 10.1093/bioinformatics/btp266 (2009).
Kim, J. S. et al. Space-time wiring specificity supports direction selectivity in the retina. Nature 509, 331–336, doi: 10.1038/nature13240 (2014).
Helmstaedter, M., Briggman, K. L. & Denk, W. High-accuracy neurite reconstruction for high-throughput neuroanatomy. Nat Neurosci 14, 1081–1088, doi: 10.1038/nn.2868 (2011).
Helmstaedter, M. The mutual inspirations of machine learning and neuroscience. Neuron 86, 25–28, doi: 10.1016/j.neuron.2015.03.031 (2015).
Kaynig, V. et al. Large-scale automatic reconstruction of neuronal processes from electron microscopy images. Med Image Anal 22, 77–88, doi: 10.1016/j.media.2015.02.001 (2015).
Kreshuk, A. et al. Automated detection and segmentation of synaptic contacts in nearly isotropic serial electron microscopy images. PLoS One 6, e24899, doi: 10.1371/journal.pone.0024899 (2011).
Turaga, S. C. et al. Convolutional networks can learn to generate affinity graphs for image segmentation. Neural Comput 22, 511–538, doi: 10.1162/neco.2009.10-08-881 (2010).
Berning, M., Boergens, K. M. & Helmstaedter, M. SegEM: Efficient Image Analysis for High-Resolution Connectomics. Neuron 87, 1193–1206, doi: 10.1016/j.neuron.2015.09.003 (2015).
Plaza, S. M., Scheffer, L. K. & Saunders, M. Minimizing manual image segmentation turn-around time for neuronal reconstruction by embracing uncertainty. PLoS One 7, e44448, doi: 10.1371/journal.pone.0044448 (2012).
Watts, R. J., Schuldiner, O., Perrino, J., Larsen, C. & Luo, L. Glia engulf degenerating axons during developmental axon pruning. Curr Biol 14, 678–684, doi: 10.1016/j.cub.2004.03.035 (2004).
Li, J., Wang, Y., Chiu, S. L. & Cline, H. T. Membrane targeted horseradish peroxidase as a marker for correlative fluorescence and electron microscopy studies. Front Neural Circuits 4, 6, doi: 10.3389/neuro.04.006.2010 (2010).
Martell, J. D. et al. Engineered ascorbate peroxidase as a genetically encoded reporter for electron microscopy. Nat Biotechnol 30, 1143–1148, doi: 10.1038/nbt.2375 (2012).
Joesch, M. et al. Reconstruction of genetically identified neurons imaged by serial-section electron microscopy. Elife 5, doi: 10.7554/eLife.15015 (2016).
Shu, X. et al. A genetically encoded tag for correlated light and electron microscopy of intact cells, tissues, and organisms. PLoS Biol 9, e1001041, doi: 10.1371/journal.pbio.1001041 (2011).
Liss, V., Barlag, B., Nietschke, M. & Hensel, M. Self-labelling enzymes as universal tags for fluorescence microscopy, super-resolution microscopy and electron microscopy. Sci Rep 5, 17740, doi: 10.1038/srep17740 (2015).
Gaietta, G. et al. Multicolor and electron microscopic imaging of connexin trafficking. Science 296, 503–507, doi: 10.1126/science.1068793 (2002).
Atasoy, D. et al. A genetically specified connectomics approach applied to long-range feeding regulatory circuits. Nat Neurosci 17, 1830–1839, doi: nn.3854 (2014).
Mizutani, R., Takeuchi, A., Hara, T., Uesugi, K. & Suzuki, Y. Computed tomography imaging of the neuronal structure of Drosophila brain. J Synchrotron Radiat 14, 282–287, doi: 10.1107/S0909049507009004 (2007).
Ribi, W., Senden, T. J., Sakellariou, A., Limaye, A. & Zhang, S. Imaging honey bee brain anatomy with micro-X-ray-computed tomography. J Neurosci Methods 171, 93–97, doi: 10.1016/j.jneumeth.2008.02.010 (2008).
Metscher, B. D. MicroCT for comparative morphology: simple staining methods allow high-contrast 3D imaging of diverse non-mineralized animal tissues. BMC Physiol 9, 11, doi: 10.1186/1472-6793-9-11 (2009).
Bushong, E. A. et al. X-ray microscopy as an approach to increasing accuracy and efficiency of serial block-face imaging for correlated light and electron microscopy of biological specimens. Microsc Microanal 21, 231–238, doi: 10.1017/S1431927614013579 (2015).
Karreman, M. A. et al. Fast and precise targeting of single tumor cells in vivo by multimodal correlative microscopy. J Cell Sci 129, 444–456, doi: 10.1242/jcs.181842 (2016).
Brand, A. H. & Perrimon, N. Targeted gene expression as a means of altering cell fates and generating dominant phenotypes. Development 118, 401–415 (1993).
Hayat, M. A. Stains and cytochemical methods. (Plenum Press, 1993).
Deerinck, T. et al. Enhancing Serial Block-Face Scanning Electron Microscopy to Enable High Resolution 3-D Nanohistology of Cells and Tissues. Microscopy and Microanalysis 16, 1138–1139, doi: 10.1017/S1431927610055170 (2010).
Tapia, J. C. et al. High-contrast en bloc staining of neuronal tissue for field emission scanning electron microscopy. Nat Protoc 7, 193–206, doi: nprot.2011.439 (2012).
Hua, Y., Laserstein, P. & Helmstaedter, M. Large-volume en-bloc staining for electron microscopy-based connectomics. Nat Commun 6, 7923, doi: ncomms8923 (2015).
Masse, N. Y., Turner, G. C. & Jefferis, G. S. Olfactory information processing in Drosophila. Curr Biol 19, R700–713, doi: 10.1016/j.cub.2009.06.026 (2009).
Ito, K. et al. A systematic nomenclature for the insect brain. Neuron 81, 755–765, doi: 10.1016/j.neuron.2013.12.017 (2014).
Mizutani, R., Saiga, R., Takeuchi, A., Uesugi, K. & Suzuki, Y. Three-dimensional network of Drosophila brain hemisphere. J Struct Biol 184, 271–279, doi: 10.1016/j.jsb.2013.08.012 (2013).
Butcher, N. J., Friedrich, A. B., Lu, Z., Tanimoto, H. & Meinertzhagen, I. A. Different classes of input and output neurons reveal new features in microglomeruli of the adult Drosophila mushroom body calyx. J Comp Neurol 520, 2185–2201, doi: 10.1002/cne.23037 (2012).
Leiss, F., Groh, C., Butcher, N. J., Meinertzhagen, I. A. & Tavosanis, G. Synaptic organization in the adult Drosophila mushroom body calyx. J Comp Neurol 517, 808–824, doi: 10.1002/cne.22184 (2009).
Madisen, L. et al. Transgenic mice for intersectional targeting of neural sensors and effectors with high specificity and performance. Neuron 85, 942–958, doi: 10.1016/j.neuron.2015.02.022 (2015).
Huang, Z. J. & Zeng, H. Genetic approaches to neural circuits in the mouse. Annu Rev Neurosci 36, 183–215, doi: 10.1146/annurev-neuro-062012-170307 (2013).
Lerner, T. N., Ye, L. & Deisseroth, K. Communication in Neural Circuits: Tools, Opportunities, and Challenges. Cell 164, 1136–1150, doi: 10.1016/j.cell.2016.02.027 (2016).
Boassa, D. et al. Mapping the subcellular distribution of alpha-synuclein in neurons using genetically encoded probes for correlated light and electron microscopy: implications for Parkinson’s disease pathogenesis. J Neurosci 33, 2605–2615, doi: 10.1523/JNEUROSCI.2898-12.2013 (2013).
Qi, Y. B., Garren, E. J., Shu, X., Tsien, R. Y. & Jin, Y. Photo-inducible cell ablation in Caenorhabditis elegans using the genetically encoded singlet oxygen generating protein miniSOG. Proc Natl Acad Sci USA 109, 7499–7504, doi: 10.1073/pnas.1204096109 (2012).
Westberg, M., Holmegaard, L., Pimenta, F. M., Etzerodt, M. & Ogilby, P. R. Rational design of an efficient, genetically encodable, protein-encased singlet oxygen photosensitizer. J Am Chem Soc 137, 1632–1642, doi: 10.1021/ja511940j (2015).
Lam, S. S. et al. Directed evolution of APEX2 for electron microscopy and proximity labeling. Nat Methods 12, 51–54, doi: 10.1038/nmeth.3179 (2015).
Namiki, S. & Kanzaki, R. Heterogeneity in dendritic morphology of moth antennal lobe projection neurons. J Comp Neurol 519, 3367–3386, doi: 10.1002/cne.22754 (2011).
Schneider-Mizell, C. M. et al. Quantitative neuroanatomy for connectomics in Drosophila. Elife 5, doi: 10.7554/eLife.12059 (2016).
Mikula, S. & Denk, W. High-resolution whole-brain staining for electron microscopic circuit reconstruction. Nat Methods 12, 541–546, doi: 10.1038/nmeth.3361 (2015).
Pallotto, M., Watkins, P. V., Fubara, B., Singer, J. H. & Briggman, K. L. Extracellular space preservation aids the connectomic analysis of neural circuits. Elife 4, doi: 10.7554/eLife.08206 (2015).
Connolly, J. B. et al. Associative learning disrupted by impaired Gs signaling in Drosophila mushroom bodies. Science 274, 2104–2107, doi: 10.1126/science.274.5295.2104 (1996).
Jefferis, G. S. et al. Developmental origin of wiring specificity in the olfactory system of Drosophila. Development 131, 117–130, doi: 10.1242/dev.00896 (2004).
Stocker, R. F., Heimbeck, G., Gendre, N. & de Belle, J. S. Neuroblast ablation in Drosophila P[GAL4] lines reveals origins of olfactory interneurons. J Neurobiol 32, 443–456 (1997).
Kohl, J. et al. Ultrafast tissue staining with chemical tags. Proc Natl Acad Sci USA 111, E3805–3814, doi: 10.1073/pnas.1411087111 (2014).
Pfeiffer, B. D. et al. Refinement of tools for targeted gene expression in Drosophila. Genetics 186, 735–755, doi: 10.1534/genetics.110.119917 (2010).
Groth, A. C., Fish, M., Nusse, R. & Calos, M. P. Construction of transgenic Drosophila by using the site-specific integrase from phage phiC31. Genetics 166, 1775–1782, doi: 10.1534/genetics.166.1775 (2004).
Klueg, K. M., Alvarado, D., Muskavitch, M. A. & Duffy, J. B. Creation of a GAL4/UAS-coupled inducible gene expression system for use in Drosophila cultured cell lines. Genesis 34, 119–122, doi: 10.1002/gene.10148 (2002).
Schindelin, J. et al. Fiji: an open-source platform for biological-image analysis. Nat Methods 9, 676–682, doi: 10.1038/nmeth.2019 (2012).
Ng, M. et al. Transmission of olfactory information between three populations of neurons in the antennal lobe of the fly. Neuron 36, 463–474, doi: 10.1016/S0896-6273(02)00975-3 (2002).
Mosca, T. J. & Luo, L. Synaptic organization of the Drosophila antennal lobe and its regulation by the Teneurins. Elife 3, e03726, doi: 10.7554/eLife.03726 (2014).
We thank the following for contributions: Jeremy Skepper and Lyn Carter (CAIC, University of Cambridge, UK) for training help with EM sample preparations and sectioning. Tom Deerinck and Mark Ellisman (NCMIR, University of California, San Diego) for help establishing miniSOG protocols. Martin Kyte and Steve Scotcher (MRC-LMB, Cambridge) for help in building LED photo-oxidation unit. Lucy Collinson and Chris Peddie (Francis Crick Institute, London) for help with SBEM acquisition on the 3View-SigmaVP and advice on image processing. This was acquired under the auspices of a MRC research grant awarded to the University of York (UK) and Cancer Research UK London Research Institute; The EM Core Technology Facility at Lincolns Inn Fields, London, provided services and the authors acknowledge its funding from Cancer Research UK, and from the MRC, BBSRC and EPSRC under grant award MR/K01580X/1’. Chris Guérin and Anneke Kremer (VIB Bio-Imaging Core, Ghent) helped with SBEM acquisition on the 3View-Merlin SEM. Matt Wayland (University of Cambridge) and Joe Ceremuga (Zeiss XRM, CA) for help implementing ORS. Jimena Berni, Lucy Collinson, Philip Schlegel, and members of the Jefferis and Landgraf labs provided feedback on the manuscript. This work was supported by European Research Council Starting Investigator and Consolidator grants, the European Molecular Biology Organization (EMBO) Young Investigator Programme, and Medical Research Council (MRC) Grant MC-U105188491 (G.S.X.E.J).
The authors declare no competing financial interests.
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Ng, J., Browning, A., Lechner, L. et al. Genetically targeted 3D visualisation of Drosophila neurons under Electron Microscopy and X-Ray Microscopy using miniSOG. Sci Rep 6, 38863 (2016). https://doi.org/10.1038/srep38863
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