Axon regeneration after injury is an important and conserved biological process in many animals, involving a large number of genes and pathways (He and Jin, 2016; Mahar and Cavalli, 2018; Tedeschi and Bradke, 2017). Upon axonal injury, distal axon segments degenerate and segments proximal to the cell body remain alive and can in certain cases regenerate (Chen et al., 2007; McQuarrie and Grafstein, 1973; Neumann and Woolf, 1999). Axon regeneration after injury requires rapid sealing of the damaged plasma membrane (PM) and subsequent formation of growth cones, leading to regrowth and extension from damaged proximal axons. These cellular changes involve numerous molecular pathways, starting with rapid calcium influx at injury sites (Ghosh-Roy et al., 2010; Rishal and Fainzilber, 2014; Wolf et al., 2001), retrograde injury signaling, transcriptional reprogramming to re-structuring of the cytoskeleton and re-organization of the extracellular matrix (ECM) (Blanquie and Bradke, 2018). In the adult mammalian central nervous system (CNS), axon regeneration is limited, due to the combination of a repressive glial environment and a lower intrinsic growth capacity of CNS neurons (He and Jin, 2016). The lack of axonal regrowth after CNS injuries, therefore, impairs functional recovery.

Many approaches have been proposed and tested to promote axon regeneration over the past decades (David and Aguayo, 1981; He and Jin, 2016; Park et al., 2008). Yet, mechanistic understanding of how damaged axons regenerate in a permissive environment remains fragmented. Since the discovery of functional axon regeneration in the nematode Caenorhabditis elegans (Yanik et al., 2004), several function-based genetic screens have revealed conserved axon regeneration genes and pathways, notably the highly conserved MAPKKK DLK-1 signaling cascade (Yan et al., 2009; Chen et al., 2011; Hammarlund et al., 2009; Nix et al., 2014). We previously reported a distinct set of genes identified from a genetic screen of 654 genes in mechanosensory axon regeneration (Chen et al., 2011). For example, regulators of microtubule (MT) dynamics play a rate-limiting role in axon regrowth, consistent with findings from other animal models (Bradke et al., 2012; Hur et al., 2012). Additional studies reveal other conserved pathways include the RNA-binding protein CELF/UNC-75 (Chen et al., 2016a), the miRNA and piRNA pathway (Kim et al., 2018; Zou et al., 2013), the fusogen EFF-1 (Ghosh-Roy et al., 2010; Neumann et al., 2015), and the apoptotic pathway (Pinan-Lucarre et al., 2012). Importantly, the findings from C. elegans are echoed from similar screening in mammalian neurons (Sekine et al., 2018; Zou et al., 2015).

Here, we report our analysis of 613 additional new genes using the C. elegans mechanosensory axon regeneration assay. We find new gene classes with inhibitory roles in axon regrowth, such as the NAD⁺ salvage pathway and the conserved Kelch-domain protein IVNS-1. We also find several permissive factors, such as A Disintegrin and Metalloprotease with Thrombospondin repeats (ADAMTS) proteins, a Rab GTPase RAB-8, and the membrane transporter MFSD-6. We show that the endoplasmic reticulum (ER)-PM contact site protein Extended Synaptotagmin (ESYT-2) is sensitive to axonal injury, and that Junctophilin (JPH-1) inhibits axon-axon fusion. Our studies of genes encoding lipid or phospholipid metabolic enzymes indicate extensive functional redundancy. This expanded screen reinforces several themes from the previous study, such as the inhibitory role of ECM components and the permissive role of MT stabilization (Chen et al., 2011). Together, our findings highlight the molecular complexity of axon regeneration and provide the genetic framework for a more comprehensive understanding of axon regeneration.

We screened 613 additional genes representing nine classes of protein function and structure, selected based on their sequence conservation and the availability of viable genetic mutants with normal axon development (Figure 1A,B; Figure 1—source data 1). We tested genetic null or strong loss-of-function mutations in each gene for effects on mechanosensory PLM (Posterior Lateral Microtubule) axon regeneration. In the PLM axon regrowth model, we sever the axon ~50 μm distal from the cell body in the fourth larval (L4) stage using a femtosecond laser and measure axon regrowth 24 hr post-axotomy in at least 10 animals per strain (Wu et al., 2007). From these 613 genes, we identified 49 genes promoting PLM regrowth (i.e. showing reduced regrowth in loss-of-function mutants) and 34 genes inhibiting regrowth (i.e. increased regrowth in loss-of-function mutants) (Tables 1 and 2; Figure 1—source data 1). As in our previous screen, genes affecting axon regrowth are found across all functional and structural classes tested (Figure 1B). The percentage of genes having positive or negative effects on regrowth was similar to that reported in our previous screen (Chen et al., 2011) (Figure 1—figure supplement 1), suggesting this screen remains far from saturated. The combined analyses of >1200 genes reinforce the conclusion that regenerative axon regrowth requires many genetic pathways, most of which are not involved in developmental axon outgrowth or guidance. Below, we first focus on a set of genes with previously uncharacterized roles in axon regeneration and then summarize common themes from the expanded screen.

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List of screened genes, reference alleles, and the functional categories.

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The conserved enzyme NMNAT inhibits axon regeneration

Among genes with significant inhibitory effects on axon regrowth, we identified NMAT-2, a member of the nicotinamide mononucleotide adenylyltransferase (NMNAT) enzyme family (Figure 2A,B). NMNAT enzymes catalyze a vital step in NAD⁺ biosynthesis and confer neuroprotection in several injury models of flies and mice (Gerdts et al., 2016). In mammalian neurons increasing NMNAT activity protects against Wallerian degeneration and axon degradation following trophic factor withdrawal (Mack et al., 2001; Vohra et al., 2010). In C. elegans, overexpression of NMAT-2/NMNAT protects against neuronal degeneration caused by the toxic mutant ion channel MEC-4(d) (Calixto et al., 2012), but does not protect against distal axon degeneration after laser axotomy (Nichols et al., 2016). We found that PLM regrowth was enhanced in two independent nmat-2 null (0) mutants, tm2905 and ju1512 (Figure 2B,C). A null mutation of NMAT-1, a close paralog, did not affect PLM regrowth (Figure 2C). nmat-2(0) adult animals are sterile, while nmat-1(0) are fertile, indicating that these two NMNATs may have distinct tissue- or cell-type-specific roles.

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Each data point in Figure 2C,D.

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To address whether the observed effects of nmat-2(0) are related to NAD⁺ synthesis, we examined loss-of-function mutants of other enzymes in the invertebrate NAD⁺ salvage synthesis pathway (Figure 2A), including the glutamine-dependent NAD⁺ synthase QNS-1, nicotinamide riboside kinase (NRK) NMRK-1, nicotinate phosphoribosyltransferase (NAPRT) NPRT-1, nicotinamidase PNC-1 and PNC-2 (Magni et al., 1999; Vrablik et al., 2009). Among these, only qns-1(0) mutants showed marginally increased axon regrowth (Figure 2C). NMAT-2 and QNS-1 catalyze the terminal steps of the NAD⁺ salvage pathway. Like nmat-2(0), qns-1(0) mutants are sterile (Wang et al., 2015) (this work), while other single mutants are fertile, suggesting that NMAT-2 and QNS-1 define essential steps in the biosynthesis of NAD⁺. To address whether sterility of the animals might contribute to the observed effects on axon regrowth, we cultured animals on 5’fluoro-2’ deoxyuridine (FUdR) and found that neither wild type or nmat-1(0) grown in FUdR showed increased PLM regrowth (Figure 2—figure supplement 1). Additionally, we have previously reported that sterile animals following germline ablation do not affect PLM regrowth (Kim et al., 2018). Thus, we conclude that NMAT-2’s role in axon regrowth is independent of animal fertility.

We next focused on NMAT-2 to define the role of NAD⁺ pathway in axon regeneration. Using CRISPR genome editing, we generated a single copy transgene expressing nmat-2(+) under its endogenous promoter (juSi347). This transgene fully rescued the sterility of nmat-2(0) and restored the increased axon regrowth in nmat-2(0) mutants to wild-type levels (Figure 2C), confirming that the increased axon regrowth is due to loss of NMAT-2 function. We then asked in which tissues NMAT-2 acts to inhibit axon regeneration using transgenic expression of NMAT-2 in the epidermis, intestine, or mechanosensory neurons (Figure 2—source data 1). Transgenic expression of NMAT-2 in individual tissues was not able to restore axon regeneration in nmat-2(0) to normal (Figure 2D). Interestingly, the combined expression of NMAT-2 in all three tissues restored normal axon regeneration (Figure 2D), and also partially rescued sterility. We conclude that NMAT-2 may act in both neuronal and non-neuronal cells to inhibit axon regeneration.

In addition to their enzymatic roles, several NMNAT proteins function as molecular chaperones, including Drosophila NMNAT, mouse NMNAT2, and human NMNAT3 (Ali et al., 2016; Zhai et al., 2006; Zhai et al., 2008). We therefore tested whether the enzymatic properties of NMAT-2 are required for inhibition of axon regeneration. Using CRISPR genome editing, we mutated the active site motif involved in ATP recognition (Zhang et al., 2002) (Figure 2B). This mutant nmat-2(ju1514) displayed sterility and enhanced regrowth of PLM neurons (Figure 2C), indistinguishable from nmat-2(0) mutants. Therefore, the role of NMAT-2 in axon regeneration likely requires its enzymatic activity. Here, we infer that the enhanced axon regeneration in nmat-2(0) reflects sustained low levels of NAD⁺.

The neuroprotective effect of NMNAT is cell-autonomous in Drosophila and in mice (Gilley et al., 2013; Wen et al., 2011). Our finding that NMAT-2 inhibits axon regrowth via several tissues suggests that NMNAT may function via distinct mechanisms for neuroprotection vs. axon regeneration. The PLM axon is adjacent to the intestine and is enveloped by the surrounding epidermis (Emtage et al., 2004). Speculatively, NAD⁺ might activate inhibitory factors in neurons and in surrounding tissues, which act together to repress the axon regenerative response; some of these factors might regulate cell-cell interaction and signal transduction. In Drosophila, lack of NMNAT also led to enhanced sensory axon regeneration (Chen et al., 2016b). Together, these data suggest conserved roles of NMNAT in axon regeneration. Future work will be required to dissect specific mechanisms by which NMNAT inhibits axon regeneration.

Differential roles and functional redundancy of ER-PM contact site components in axon regeneration

Membrane contact sites (MCSs) are regions where membranes from two organelles or an organelle and the PM are held together by protein tethers, most of which are conserved from yeast to mammals (Phillips and Voeltz, 2016; Saheki et al., 2016). MCSs can coordinate activities such as calcium entry or lipid transfer between membranes. Calcium entry via voltage-gated Ca²⁺ channels in the PM is critical for PLM axon regeneration (Ghosh-Roy et al., 2010). Additionally, MCSs between the PM and ER might be involved in lipid addition to the PM during rapid extension of regrowing axons (Hausott and Klimaschewski, 2016). We therefore examined mutants affecting conserved ER-PM MCS components such as Junctophilin, Extended synaptotagmin (E-Syt), Anoctamins, and OxySterol Binding Proteins (OSBP).

Junctophilins are multi-pass transmembrane proteins that are localized to ER-PM contacts in excitable cells, where they couple PM- and ER-localized calcium channels (Landstrom et al., 2014). JPH-1 is the sole Junctophilin in C. elegans (Yoshida et al., 2001) (Figure 3A). We observed that jph-1(ok2823) mutants, likely null, exhibited a significantly increased rate of reconnection or fusion between the regrowing axon and distal fragment (Figure 3B). Axons that did not reconnect in jph-1 mutants exhibited reduced axon regeneration, compared to controls (Figure 3C). As reconnected axons were not measured for regrowth analysis, the reduced regrowth in jph-1 mutants might be due to an overrepresentation of poorly growing axons. Axon-axon fusion requires the fusogen EFF-1 (Ghosh-Roy et al., 2010; Pérez-Vargas et al., 2014) and a phosphoserine-mediated apoptotic cell engulfment pathway (Neumann et al., 2015). We analyzed eff-1; jph-1 double mutants and found that the enhanced reconnection in jph-1 was greatly reduced (Figure 3B). Drosophila Junctophilin-like molecule functions in apoptotic cell removal (Gronski et al., 2009). These observations suggest JPH-1-mediated contacts may restrict axon-axon fusion, dependent on eff-1.

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Extended synaptotagmins (E-Syt) are a family of proteins containing multiple C2 domains (Figure 3D) that have been shown to tether the ER to the PM (Giordano et al., 2013) and are implicated in membrane lipid transfer (Saheki et al., 2016; Yu et al., 2016). ESYT-2 is the sole E-Syt in C. elegans and is most closely related to human E-Syt2 and E-Syt3 (Figure 3D). We found that esyt-2 showed wide expression in the nervous system (Figure 3—figure supplement 1). In the mechanosensory neuron cell body, full-length GFP-ESYT-2 showed a punctate pattern, colocalizing with an ER marker PISY-1 (Rolls et al., 2002) at the peripheral ER (Figure 3E). In uninjured axons, ESYT-2 was distributed intermittently (Figure 3F; upper panel). Strikingly, upon axon injury, axonal ESYT-2 condensed into small puncta almost immediately (<1 s) (Figure 3F; lower panel). As axon injury triggers a rapid rise in axonal calcium (Ghosh-Roy et al., 2010), we speculate that the injury-induced Ca²⁺ transient triggers ESYT-2 relocalization to axonal ER-PM contact sites. This is consistent with the observation that vertebrate E-Syt1 can localize to ER-PM contact sites following an increase in cytosolic calcium (Giordano et al., 2013; Idevall-Hagren et al., 2015). We generated esyt-2 null mutants by genome editing (Figure 3D). These mutant animals were indistinguishable from wild-type animals in growth rate, body morphology, and exhibited normal axon development and regrowth (Figure 3C). Thus, while ESYT-2 undergoes temporal changes in response to axon injury, it does not appear to be essential for axon regrowth.

The Anoctamin protein family function as tethers at ER-PM contact sites in yeast (Manford et al., 2012; Wolf et al., 2012). C. elegans has two orthologs, ANOH-1 and ANOH-2. ANOH-1 is expressed in mechanosensory neurons and acts together with the apoptotic factor CED-7 to promote phosphatidylserine exposure in the removal of necrotic cells (Li et al., 2015). ced-7(0) reduces PLM axon regrowth (Neumann et al., 2015). However, we found that loss of function in anoh-1 or anoh-2, or the anoh-1; anoh-2 double mutant, did not affect PLM axon regeneration (Figure 3C).

The eukaryotic OSBP and OSBP-related (ORP) family of MCS-localized lipid transfer proteins includes multiple members. ORP5/8 act as tethers at ER-PM MCSs where they mediate PI4P/Phosphatidylserine counter-transport, while OSBP and the other ORPs function at different MCSs (Chung et al., 2015). We tested the four C. elegans homologs individually as well as a quadruple mutant. Each obr single mutant displayed normal regeneration, and the quadruple mutant displayed a significant decrease in axon regrowth (Figure 3C). While the expression pattern and action site of these OBR proteins remain to be determined, our finding is consistent with the known redundancy within the OBR family (Kobuna et al., 2010).

Altogether, the above analysis echoes a recent study in yeast where elimination of multiple MCS components did not impair ER-PM sterol exchange (Quon et al., 2018), highlighting the challenge to tease apart the functional redundancy of MCS proteins in biological processes.

Lipid metabolic enzymes likely have extensive functional redundancy in axon regrowth

Lipids are essential components of membranes and regulate many biological functions including energy storage and lipid signaling. In C. elegans, the majority of triglyceride is obtained from the diet, and lipogenesis accounts for less than 10% of stored body fat (Srinivasan, 2015). Lipolysis is required for cellular uptake or release of fatty acids and glycerol (Zechner et al., 2012). Classical ‘neutral’ lipolysis involves at least three different lipases: ATGL (adipose triglyceride lipase), HSL (hormone sensitive lipase), and MGL (monoglyceride lipase). ATGL requires a coactivator protein, CGI-58/ABHD5. C. elegans encodes a single ATGL (ATGL-1), three CGI-58/ABHD5 (ABHD-5.2, ABHD-5.3, and LID-1), a single HSL (HOSL-1), but lacks MGL by sequence homology (Zechner et al., 2012). We tested single mutants for all these genes and double or triple mutants for ABHD (α/β hydrolase domain) genes and observed no detectable effects in PLM axon regrowth (Figure 4A).

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Each data point in Figure 4A,B,D.

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Triglycerides can also be hydrolyzed through autophagy-mediated degradation of lipid droplets by some lysosomal acid lipases, termed lipophagy or ‘acid’ lipolysis (Singh et al., 2009). C. elegans lysosomal lipases (LIPL-1, LIPL-3, and LIPL-4), autophagy proteins (LGG-1 and LGG-2), and transcription factors (HLH-30/TFEB and MXL-3/MXL) act in lipophagy (Folick et al., 2015; O'Rourke and Ruvkun, 2013). Two nuclear hormone receptors NHR-49/PPARα and NHR-80/HNF4α are reported to regulate LIPL-4 (Folick et al., 2015). We found that single mutants for all these genes showed normal PLM regrowth (Figure 4B), suggesting that lipolysis may not play an essential role in PLM axon regeneration.

The Kennedy pathway synthesizes the most abundant phospholipids in eukaryotic membranes, phosphatidylcholine (PC) and phosphatidylethanolamine (PE) (Gibellini and Smith, 2010), and involves conserved enzymes catalyzing a series of consecutive reactions (Figure 4C). Of all mutants affecting individual enzymes in the Kennedy pathway, we found that cept-2 null mutants showed a significant reduction in axon regrowth (Figure 4D). In testing functional redundancy between cept-1 and cept-2, we found double mutants to be embryonic or larval lethal (data not shown), preventing further analysis. Definitive conclusions will require tissue-specific and temporal manipulation of this pathway. Overall, our analysis suggests that the Kennedy pathway may affect axon regeneration.

The conserved NS1A-BP ortholog IVNS-1 inhibits axon regrowth

Among other conserved proteins, we identified the BTB-Kelch family protein IVNS-1 (Influenza Virus NS1A binding protein/NS1A-BP) as an inhibitor of axon regrowth. BTB/POZ (Broad-Complex, Tramtrack, and Bric-a-Brac/Poxvirus and Zinc finger) domain and Kelch repeats function in a wide variety of biological processes including gene expression, protein ubiquitination, and cytoskeleton binding (Dhanoa et al., 2013). Human NS1A-BP was originally identified based on interaction with the influenza A virus via its Kelch domain (Wolff et al., 1998) (Figure 5A) and was later found to interact with actin filaments (Perconti et al., 2007) and RNA binding proteins, including heterogeneous nuclear ribonucleoprotein and splicing factors (hnRNPs) and RNA helicase (Tsai et al., 2013). C. elegans IVNS-1 has the same overall domain organization as NS1A-BP (Figure 5A).

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Each data point in Figure 5B,C.

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We analyzed two independent ivns-1 mutants (gk252 and ok3171) and observed increased axon regrowth, which was restored to control levels following transgenic expression of ivns-1 driven by its own promoter (Figure 5A,B). ivns-1 mutants showed increased regrowth as early as 6 hr post-injury (Figure 5C), while growth cone formation in ivns-1 mutants was normal (Figure 5D). The effects of ivns-1 on axon regrowth appeared to be unique, as mutants in two other BTB-Kelch proteins kel-8 and kel-20 displayed normal regrowth (Figure 5B). Whether the function of IVNS-1 involves actin cytoskeleton or RNA regulation remains to be determined.

Functional screening for axon regeneration phenotypes is a powerful approach to identify novel regulators of axon regrowth after injury. C. elegans PLM axons exhibit robust response to injury, and therefore allow efficient screening of positive and negative regulators of regrowth. In this work we have nearly doubled the number of genes tested using genetic mutations and the PLM regeneration assay, taking the total number of genes screened to 1267. We expanded some gene classes previously analyzed in depth (e.g. kinases, ECM components, ion channels, and transporters) and have also specifically targeted several pathways not addressed in our earlier screen, such as NAD⁺ biosynthesis, MCS components, lipid metabolism, and actin regulators. Interestingly, both MCS components and lipid metabolism tested display a high degree of genetic redundancy, such that single mutants only occasionally display regeneration defects, and compound mutant strains are required to assess functional requirements. Nevertheless, our findings suggest that ER-PM contact sites may be regulated by axon injury and that phospholipid synthesis may be critical for axon regeneration. Further work will be required to define whether these pathways play a role in lipid addition to the regrowing axon membrane or a more general signaling role.

Several axon regeneration screens have now been reported in C. elegans and the results may be compared to assess reproducibility and generalizability of the results. The present work and our prior screen (Chen et al., 2011) analyzed the effect of genetic mutations on PLM axon regeneration. In contrast, other studies have used RNAi or genetic mutants to analyze motor neuron regeneration (Nix et al., 2014). Differing results between the two screens (e.g. the opposite requirement for nex-1 in PLM and motor neurons) may reflect cell-type-specific roles of the regulators in axon regeneration. A recent genome-wide in vitro axon regeneration screen in mouse cortical neurons revealed significant overlap with orthologous genes identified from C. elegans screen despite differences in neuron types, species, and experimental methods (Chen et al., 2011; Nix et al., 2014; Sekine et al., 2018), suggesting significant conservation of regenerative mechanisms.

Our screen approach is based on candidates and not random mutagenesis, and thus classical estimates of genetic saturation do not apply. However, it is notable that the frequency of positive and negative hits in the current screen does not differ from our previous screen. Our prior screen included many previously well-studied axon guidance and outgrowth pathways and thus might have been enriched for functionally important factors, but the present analysis suggests many genes not previously associated with the nervous system (e.g. ptps-1, tep-1, brap-2) also have functionally important roles in regrowth. One trend is that fewer mutants with dramatically reduced regrowth (<30% of wild type, such as dlk-1, unc-75, sdn-1) were identified, and thus the number of genes essential for initiation of regrowth may be limited. On the other hand, the present screen identified new mutants with drastically enhanced regrowth (>140% of wild type, such as efa-6 and pxn-2 from previous screen and nmat-2 and drag-1 from this screen). Interestingly, a recent genome-wide screen for enhanced regrowth in mouse cortical neurons reported a positive hit rate of 3% (Sekine et al., 2018), whereas we find 3.9% of genes displayed significantly elevated axon regrowth. The frequency of axon regrowth phenotypes may therefore be consistent across screening platforms.

All data generated or analysed during this study are included in the manuscript and supporting files.

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Author details

1. Kyung Won Kim

   Section of Neurobiology, Division of Biological Sciences, University of California, San Diego, La Jolla, United States

   Present address

   Convergence Program of Material Science for Medicine and Pharmaceutics, Department of Life Science, Multidisciplinary Genome Institute, Hallym University, Chuncheon, Republic of Korea

   Contribution

   Conceptualization, Resources, Data curation, Formal analysis, Validation, Investigation, Visualization, Methodology, Writing—original draft, Writing—review and editing

   For correspondence

   kwkim@hallym.ac.kr

   Competing interests

   No competing interests declared

   "This ORCID iD identifies the author of this article:" 0000-0002-8252-6203

2. Ngang Heok Tang

   Section of Neurobiology, Division of Biological Sciences, University of California, San Diego, La Jolla, United States

   Contribution

   Resources, Data curation, Validation, Investigation, Visualization, Writing—original draft, Writing—review and editing

   Competing interests

   No competing interests declared

3. Christopher A Piggott

   Section of Neurobiology, Division of Biological Sciences, University of California, San Diego, La Jolla, United States

   Contribution

   Resources, Data curation, Validation, Investigation, Visualization, Writing—original draft, Writing—review and editing

   Contributed equally with

   Matthew G Andrusiak and Seungmee Park

   Competing interests

   No competing interests declared

4. Matthew G Andrusiak

   Section of Neurobiology, Division of Biological Sciences, University of California, San Diego, La Jolla, United States

   Contribution

   Resources, Data curation, Validation, Investigation, Visualization, Writing—original draft, Writing—review and editing

   Contributed equally with

   Christopher A Piggott and Seungmee Park

   Competing interests

   No competing interests declared

5. Seungmee Park

   Section of Neurobiology, Division of Biological Sciences, University of California, San Diego, La Jolla, United States

   Contribution

   Resources, Data curation, Validation, Investigation, Visualization, Writing—original draft, Writing—review and editing

   Contributed equally with

   Christopher A Piggott and Matthew G Andrusiak

   Competing interests

   No competing interests declared

6. Ming Zhu

   Section of Neurobiology, Division of Biological Sciences, University of California, San Diego, La Jolla, United States

   Contribution

   Resources, Data curation, Validation, Investigation, Writing—review and editing

   Competing interests

   No competing interests declared

7. Naina Kurup

   Section of Neurobiology, Division of Biological Sciences, University of California, San Diego, La Jolla, United States

   Contribution

   Resources, Validation, Investigation, Writing—review and editing

   Competing interests

   No competing interests declared

8. Salvatore J Cherra III

   Section of Neurobiology, Division of Biological Sciences, University of California, San Diego, La Jolla, United States

   Present address

   Department of Neuroscience, University of Kentucky College of Medicine, Lexington, United States

   Contribution

   Resources, Validation, Investigation

   Competing interests

   No competing interests declared

9. Zilu Wu

   Section of Neurobiology, Division of Biological Sciences, University of California, San Diego, La Jolla, United States

   Contribution

   Resources, Validation, Investigation

   Competing interests

   No competing interests declared

10. Andrew D Chisholm

    Section of Neurobiology, Division of Biological Sciences, University of California, San Diego, La Jolla, United States

    Contribution

    Conceptualization, Data curation, Supervision, Funding acquisition, Writing—original draft, Project administration, Writing—review and editing

    For correspondence

    adchisholm@ucsd.edu

    Competing interests

    No competing interests declared

    "This ORCID iD identifies the author of this article:" 0000-0001-5091-0537

11. Yishi Jin

    1. Section of Neurobiology, Division of Biological Sciences, University of California, San Diego, La Jolla, United States
    2. Department of Cellular and Molecular Medicine, University of California, San Diego, School of Medicine, La Jolla, United States

    Contribution

    Conceptualization, Data curation, Supervision, Funding acquisition, Writing—original draft, Project administration, Writing—review and editing

    For correspondence

    yijin@ucsd.edu

    Competing interests

    No competing interests declared

    "This ORCID iD identifies the author of this article:" 0000-0002-9371-9860

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