Satish Bodakuntla
Hana Nedozralova
Nirakar Basnet
Naoko Mizuno- 1Laboratory of Structural Cell Biology, National Heart, Lung, and Blood Institute, National Institutes of Health, Bethesda, MD, United States
- 2National Institute of Arthritis and Musculoskeletal and Skin Diseases, National Institutes of Health, Bethesda, MD, United States
Axon branching is a critical process ensuring a high degree of interconnectivity for neural network formation. As branching occurs at sites distant from the soma, it is necessary that axons have a local system to dynamically control and regulate axonal growth. This machinery depends on the orchestration of cellular functions such as cytoskeleton, subcellular transport, energy production, protein- and membrane synthesis that are adapted for branch formation. Compared to the axon shaft, branching sites show a distinct and dynamic arrangement of cytoskeleton components, endoplasmic reticulum and mitochondria. This review discusses the regulation of axon branching in the context of cytoskeleton and membrane remodeling.
Introduction
The brain function depends on a vast number of intricate connections between neurons to process and transmit information. To fulfill the scale and complexity of these connections, it is critical for the neurons to develop properly and maintain neuronal homeostasis over the life span of the organism. To achieve this arduous task, the primary step for neurons is to undergo a polarity establishment process with two main compartments, the somato-dendritic and the axonal compartments, which are distinct in their morphology, molecular composition and subcellular functions. In addition to establishing neuronal polarity, axon outgrowth and branching are vital steps to ensure proper connectivity and development of the brain. While axonal outgrowth is mainly linked to axon guidance and pathfinding (McCormick and Gupton, 2020), branching of axons is crucial for the intertwining of neuronal circuits through synaptic contacts (Kalil and Dent, 2013; Hoersting and Schmucker, 2021). The axonal branching process is balanced by the ability of axons on the one hand to make collateral protrusions establishing synaptic connections but also to retract protrusions eliminating synapses, a process called synaptic pruning (discussed in Gibson and Ma, 2011).
Early studies have shown that the primary growth cone dynamics is linked to the formation of axon branches. Axons do not continuously grow, but rather pause intermittently between growth phases (Harris et al., 1987; Yamamoto et al., 1997). These paused points contain remnants of growth cone components, which act as precursors for axon branching sites (Szebenyi et al., 1998). Axonal branches are formed in two major ways: (1) splitting of the growth cone to create Y- or T-shaped structures with two growing axonal paths, (2) de novo branching from the axon shaft, called collateral branch formation. Although both possibilities exist, the latter mechanism of collateral branch formation appears to be the major mechanism (Harris et al., 1987; O’Leary et al., 1990). Understanding axon branching is a challenging task as several pathways have to work together in a highly coordinated fashion on an intracellular as well as intercellular level. Moreover, neuronal cells are extremely sensitive to stress and environmental cues, which impedes many cell biological and biochemical approaches. There are several key questions in axon branching: What determines the position of a branch on the axon shaft? Which mechanisms stabilize axonal branches and allow them to grow further? Which actions are required within a cell as well as on the plasma membrane? How are these actions coordinated in space and time? How do axon guidance cues interconnect with the branching system? Given the paramount importance of axon branching in brain homeostasis, answering these questions is crucial and it will be instrumental for identifying therapeutic targets to alleviate pathological conditions like neurodegenerative diseases. We are only beginning to answer these questions and this review discusses recent advances in obtaining a better picture of the cellular organization of processes governing axon branching with an emphasis on cytoskeleton and membrane trafficking.
Cytoskeleton Organization and Dynamics at the Axonal Branch
One of the important early events in the formation of axon branches is the extensive reorganization of cytoskeletal elements (Gallo, 2011). The first observed event during branch formation is the extension of plasma membrane protrusions filled with actin-based components, either finger-like filopodia or sheet-like lamellipodia (Figure 1). The actin-rich protrusions originate from the local accumulation of short pieces of actin filaments along the axonal shaft, called actin patches (Spillane et al., 2011). Several actin-associated signaling proteins like Rho GTPases (Hall, 1998; Hall and Lalli, 2010) and actin remodeling proteins, such as ENA/VASP (enabled/vasodilator-stimulated phosphoprotein) and nucleator complexes like ARP2/3 (actin-related protein 2/3), play important roles in filopodia dynamics resulting in axon development and branch formation (Dwivedy et al., 2007). The activation of Rho in slice cultures of the upper cortical layer results in increased activity-dependent branching (Ohnami et al., 2008). A similar result is observed in cultured hippocampal neurons (Ahnert-Hilger et al., 2004). The reduction of ENA/VASP proteins in the retinal ganglion neurons leads to diminished filopodia formation and axon branching, and the deletion of ARP2/3 in hippocampal neurons reduces the frequency of filopodia (Strasser et al., 2004). ARP2/3 is also required for growth factor-induced branching of sensory axons (Spillane et al., 2011). The duration and frequency of filopodia are shown to affect the number of axonal branches (Sainath et al., 2017). However, while these studies shed light on the importance of the actin cytoskeleton for the initiation of branch formation, their maturation process is not fully understood due to the dynamic nature of actin. The extension of protrusions alone, referred to as premature branches, is not sufficient to stabilize the transformation into a mature axon branch.
Figure 1. Cellular processes during the maturation of axon branches. (A) Premature branch: Actin patches form along the axon and push the plasma membrane to initiate the formation of a filopodium. Mitochondria stall at branch sites and the translation machinery accumulates to locally synthetize new cytoskeletal proteins (Spillane et al., 2013; Armijo-Weingart and Gallo, 2017). (B) Mature branch: Dispersed actin filaments reorient and form actin bundles. Microtubules and ER can co-migrate into the growing branch to stabilize it and vesicles supply membrane components. Intracellular organelles such as mitochondria, endoplasmic reticulum, synaptic and dense-core vesicles redistribute and accumulate at the branch site to support the high demand for energy, proteins, lipid- and membrane components.
The stabilization of transient, premature branches is thought to be mediated by the insertion of axonal microtubules, as the disruption of microtubules causes a reduction in axon branching (Dent and Kalil, 2001). However, the entry of the microtubules into premature protrusions does not necessarily ensure the establishment of a mature branch. It has been shown that longer, microtubule-containing axon branches can regress (Kalil et al., 2000), presumably because microtubules themselves display dynamic instability (Mitchison and Kirschner, 1984; Mitchison, 1993)-switching between phases of microtubule polymerization and depolymerization. Thus, an additional mechanism likely plays a role in facilitating branch maturation (Figure 1). One possibility is the stabilization of microtubules by an interaction with already organized actin filaments in axonal protrusions (Dent and Kalil, 2001; Kalil and Dent, 2014; Sainath and Gallo, 2015). For instance, it has been shown that the actin-binding protein drebrin localizes at branch regions and promotes the entry of microtubules into filopodia, eventually ensuring the formation of mature axon branches (Ketschek et al., 2016). Interestingly, the treatment of neurons with nerve growth factor (NGF) promotes axonal branches (Diamond et al., 1987, 1992; Gallo and Letourneau, 1998; Ketschek and Gallo, 2010; Armijo-Weingart and Gallo, 2017) and also increases the levels of axonal drebrin (Ketschek et al., 2016), suggesting these mechanisms are responsible for changes in extracellular signaling. Septins have also been shown to localize at actin patches during the initiation of axon branching and to regulate the interactions of microtubules and actin in filopodia (Hu et al., 2012). Together, the coordination of microtubule- and actin networks play a crucial role in the formation of axon branches. The relative contribution of these mechanisms to axon branching as well as their coordination in space and time must be further explored.
Moreover, several neuronal microtubule-associated proteins (MAPs) contribute to the maturation of branches by promoting microtubule polymerization or by stabilizing the microtubules at branch sites (Kalil and Dent, 2014; Figure 2). For example, MAP7 (ensconsin or E-MAP-115) promotes microtubule polymerization in vitro and it has been shown to accumulate at newly forming axon branches, and to increase the number of axonal branches (Tymanskyj et al., 2017). MAP7 has been shown to enter the branch with a delay and colocalize with stable microtubules, suggesting a specific role in the maturation of branches by microtubule stabilization (Tymanskyj et al., 2017, 2018). Interestingly, MAP7 has been shown to enhance the recruitment of kinesin-1 to microtubules (Tymanskyj et al., 2018; Hooikaas et al., 2019), possibly related to the accumulation of organelles at the axonal branch (discussed below). Similar to MAP7, SSNA1 (Sjoegren syndrome nuclear autoantigen 1, also known as NA14), a microtubule nucleation factor, also accumulates at axon branching sites (Basnet et al., 2018) and its overexpression induces axon branching (Goyal et al., 2014). Interestingly, SSNA1 induces not only microtubule nucleation but also a unique microtubule branching in vitro (Basnet et al., 2018).
Figure 2. Remodeling of cytoskeleton and plasma membrane at axon branches. (A) Schematic representation of a mature, growing axon branch. Mitochondria increase in numbers through fission mediated by mitochondria fission factors or via constriction by the wrapping of endoplasmic reticulum. (B) Mechanisms to regulate membrane expansion (1) and retraction (2) at axon branches. Membrane expansion in response to attraction guidance cues is mediated by the fusion of synaptic vesicles with the plasma membrane or by exocytosis using SNARE proteins. The retraction of membranes is initiated by repulsion guidance cues and facilitated by endocytosis of membrane material. (C) Mechanisms for the reorganization of the cytoskeleton at axon branches. Bundled microtubule arrays are fragmented by microtubule-severing enzymes such as spastin and katanin to increase the local microtubule/tubulin pool available for polymerization. Tubulin-nucleation factors like MAP7 and SSNA1 promote and stabilize microtubule growth at axonal branches. Actin-microtubule crosslinking factors like drebrins and septins are suggested to promote the entry of microtubules into actin-rich filopodia. Note that processes at the primary growth cone and axon branch formation have similar cellular mechanisms for cytoskeletal rearrangements and responses to attractive or repulsive signaling through exocytosis and endocytosis (discussed in Dent et al., 2003; Winkle et al., 2016).
Early studies have suggested that microtubules undergo destabilization in axons during branch formation, and fragmented microtubules are transported to or generated at newly forming branches (Gallo and Letourneau, 1999; Kalil and Dent, 2014; Armijo-Weingart et al., 2019; Figure 2C), enabling their growth. It appears that microtubule fragmentation at localized areas along the axon shaft would increase the amount of available tubulin molecules or short microtubule fragments for microtubule remodeling, which eventually stabilizes and promotes the formation of mature axon branches (Yu et al., 1994; Kalil et al., 2000). Indeed, overexpression of the microtubule-severing enzymes spastin and katanin increases the localized microtubule mass (Kuo et al., 2019), leading to an increased number of axon branches (Yu et al., 2008). Agreeing with these notions, the destabilization of microtubules by an increase of the local calcium concentration along the axon was also shown to induce new collateral branches (Ziv and Spira, 1997). On the other hand, when exposed to the microtubule-stabilizing drug taxol, neurons show a reduction in the invasion of microtubules into early filopodia and consequently, decreased branch formation (Dent and Kalil, 2001; Dent et al., 2007).
Apart from the physical modulation of microtubule dynamics, the post-translational modifications of tubulin including acetylation and polyglutamylation (Janke and Magiera, 2020) can adapt the growth dynamics of microtubules to regulate axonal branches. Particularly, tubulin acetylation controls axonal branching by regulating microtubule dynamics (Dan et al., 2018). Further, it is critical that the dynamic behavior of microtubules occurs under spatial and temporal coordination. The branch specific destabilization of microtubules by the enzyme spastin at neuromuscular synapses can actually mediate the loss of branches (Brill et al., 2016) instead of their induction. Altogether, these observations highlight a key role of microtubule dynamics in axon branching.
Organelle Positioning at the Axonal Branch
While cytoskeleton re-organization unambiguously plays a crucial role in the structural support of axon branch formation, there are other cellular actions facilitating the process of branch formation and maintenance. Selective localization of cellular factors such as synaptic vesicles and mitochondria are observed (Courchet et al., 2013; Greif et al., 2013; Spillane et al., 2013; Tao et al., 2014; Figure 2A). In the next section, we will discuss the current understanding of the redistribution and potential role of these organelles at axon branch sites.
Mitochondria
Mitochondria undergo bidirectional transport in axons, i.e., from the cell body to the synaptic terminal and vice versa; and their transport and redistribution along the axon is controlled by the coordinated action of the motor proteins kinesin and dynein, mitochondria adapter proteins such as TRAKs (Trafficking Kinesin Proteins)/Milton, and the anchoring protein, syntaphilin (Sheng and Cai, 2012). The perturbations of mitochondria-transport processes have been well studied in the context of neurodegenerative diseases, including Alzheimer’s disease, Huntington’s disease or amyotrophic lateral sclerosis (ALS) (Johri and Beal, 2012; Magiera et al., 2018; Guo et al., 2020). In healthy neurons, mitochondria are enriched in areas, which have high demands for energy production including synapses, growth cones and axon branch points (Sheng, 2017). The active transport of mitochondria into branching axons (Ruthel and Hollenbeck, 2003) suggests their role during branch formation. However, stalled mitochondria alone inside axons are not sufficient to induce a branch, as notably about 70% of mitochondria are stalled along axons at a given time (Cai et al., 2009). Nevertheless, evidence points toward the requirement of additional coordination of mitochondria by signaling and adapter proteins during branch formation. In cortical neurons, the depletion of liver kinase B1 (LKB1) or the anchoring protein syntaphilin leads to a decrease in the number of stalled mitochondria in axons and diminished axon branches, while the overexpression of these proteins leads to an increase of stalled mitochondria as well as associated axon branches (Courchet et al., 2013). Similar results are obtained by manipulating adenosine monophosphate-activated protein kinase AMPK signaling (Tao et al., 2014). The deletion of the mitochondria adaptor protein TRAK1 leads to a reduction of axon growth and branching (van Spronsen et al., 2013). Interestingly, studies have shown that fission and fusion events of mitochondria may control axon branching as well. For example, mitochondrial fission factor (MFF) has been shown to regulate the size and number of axonal mitochondria at presynaptic sites and show a correlation with axon branching (Lewis et al., 2018). Furthermore, neurotrophins, which promote axon branching, also induce the fission of mitochondria along sensory neurons (Armijo-Weingart et al., 2019). These studies suggest a role of mitochondria fission and the resulting increase in the number of mitochondria during branch formation.
Endoplasmic Reticulum
The endoplasmic reticulum (ER) is a continuous network of sheets and tubes present in many cell types and organisms with diverse functions such as lipid synthesis, a platform for secretory protein synthesis, maintenance of calcium homeostasis and redistribution of membrane-associated proteins (Schwarz and Blower, 2016). In immature neurons before polarity formation, ER displays perinuclear cisternae and peripheral tubules that form a dense network (Nixon-Abell et al., 2016). In mature neurons, ER mostly shows a tubular morphology along the axon while it forms both tubular and planar network in dendrites (Wu et al., 2017). ER interacts with microtubules as well as different cellular organelles including mitochondria (Spillane et al., 2013; Wu et al., 2017). While ER has been implicated to play a role in establishing neuronal polarity and dendrite arborization (Renvoise and Blackstone, 2010), its role in axon branching is unknown. In less specialized mammalian cell lines such as Cos-7 and U2OS, ER has also been shown to mark the fission sites for mitochondria (Friedman et al., 2011) in an actin-dependent manner (Korobova et al., 2013). These observations raise the question whether there is an active role of ER in axonal branch formation by controling the fission process of mitochondria, to be addressed in the future.
It is not completely understood which ER-interacting proteins play a role in mediating the ER-mitochondria interactions in neurons. In HeLa cells, PDZD8 is present at ER-mitochondria contacts, and its deletion leads to decrease in the contact points (Hirabayashi et al., 2017). Within the axon shaft, ER protein p180 (also known as ribosome binding protein 1 homolog 180-kDa, RRBP1) interacts with both ER and microtubules, and contributes to the determination of the axon from neurites during the initial stage of the neuronal polarity formation (Farias et al., 2019). Furthermore, microtubules and ER stabilize each other to promote the growth of neurites. It is plausible that the co-migration of ER and microtubules occurs at the branch and is necessary for the stabilization of dynamic microtubules in a similar mechanism as the elongation of the axon shaft. Other ER-associated proteins that also interact with microtubules include CLIMP63, kinectin (KTN1) (Shibata et al., 2010), and atlastin-1. Particularly, atlastin-1 is enriched in vesicular structures at growth cones and branch points of cortical neurons in rats. Depletion of atlastin-1 results in compromised neuronal development (Zhu et al., 2006). Interestingly, atlastin-1 regulates the number of mitochondria at branching points in dendrites of sensory neurons (Liu et al., 2019), raising the possibility that atlastin-1 may have a similar function at axon branches. These studies strengthen the notion that ER is involved in the fission process of mitochondria. Together with mitochondria, ER and its interacting proteins appear to support the cytoskeleton and other organelles to promote axon branching.
Whether axons contain rough ER has been an open question. The presence of mRNAs coding for plasma membrane proteins and components of the secretory machinery gives the first indication of their existence and local translation in axons (Willis et al., 2007; Merianda et al., 2009). Conventional electron microscopic approaches show densities resembling rough ER at axonal tips (Jin et al., 2016). However, direct evidence for the presence of rough ER at the axonal branch is still lacking. Future studies will investigate how local translation is regulated at axon branching sites and growth cones, and how rough ER might participate in branching homeostasis.
Membrane Remodeling at Axon Branches
The Role of Synaptic Vesicles and Membrane Fusion in the Expansion of Axon Branches
Membrane extension at axonal branches and growth cones requires a plethora of proteins and lipid components (Figure 2B). They are mainly supplied by accumulated synaptic vesicles, dense-core vesicles, and ER membranes. Along the axon and branching sites, synaptic vesicles are reported to be present in high numbers (Winkle et al., 2016). These vesicles deliver membrane materials to the expanding plasma membrane by simple fusing or exocytosis via SNARE (soluble N-ethylmaleimide-sensitive factor-attached protein receptor) complexes (Sollner et al., 1993; Winkle and Gupton, 2016). While the fusion-mediated maintenance of membrane- and secretory materials at synapses of mature neurons is well known for signal transduction between neurons and neuromuscular junctions, it is not clear if such a fusion mechanism is utilized in axon development. Indeed, the presence of clustered synaptic vesicles and the accompanying exocytosis machinery has been shown in developing axons even before synaptogenesis (Kraszewski et al., 1995; Verderio et al., 1999). Moreover, the overexpression of these components in neurons enhances the number of branches (Perin et al., 1990; Alsina et al., 2001; Greif et al., 2013). Imaging of GFP-tagged synaptic vesicle components in neurons reveals insights into the potential function of these accumulated vesicles. Synaptobrevin II, a synaptic vesicle marker, is enriched at branching sites of retinal ganglion cells, and most of the new branches emerged from GFP-labeled sites (Alsina et al., 2001). When exposing neurons to brain-derived neurotrophic factor (BDNF), not only axon branching is increased, but also the density of GFP-synaptobrevin at branch points, showing the response of synaptic vesicles to extracellular stimuli. On the other hand, when the effective BDNF levels are reduced by neutralizing antibodies, a reduction in synaptobrevin levels and axonal branches occurs (Hu et al., 2005). These results together emphasize the importance of the accumulation of synaptic vesicles prior to axon branching as a resource for creating a new branching path. Importantly, these studies also point out that the use of synaptic vesicles can be dynamically adapted to the physiological needs during the development, maintenance and communication of neurons.
Similar to BDNF, Netrin-1, another extracellular signaling molecule, increases the number of axonal branches in cultured cortical neurons (Dent et al., 2004). A higher local concentration of Netrin-1 induces an increase in calcium transients in neurons (Hutchins and Kalil, 2008), possibly leading to the modulation of synaptic exocytosis and stimulated branch formation. Using cortical neurons, the involvement of synaptic vesicle fusion in increased branch formation has also been shown in response to Netrin-1 (Winkle et al., 2014). Terminal branches emerge from sites displaying high fluorescence intensity using fluorescently labeled synaptic-vesicle protein synaptophysin in live cell imaging in zebrafish and Xenopus retinotectal projections (Ruthazer et al., 2006). Notably, branches emerging from only faintly labeled puncta retract themselves, suggesting that the critical accumulation of synaptic vesicle components and their fusion with the plasma membrane (Winkle et al., 2014) is required for the maturation of axonal branches (Meyer and Smith, 2006; Ruthazer et al., 2006). Furthermore, the overexpression of syntaxin1-binding protein Sec1, which is involved in the formation of SNARE complexes (Jahn, 2000; Waters and Hughson, 2000), leads to a higher number of collateral axon branches in hippocampal neurons (Steiner et al., 2002). Altogether, these studies demonstrate that synaptic vesicles and their fusion with the plasma membrane is important for axonal branch formation.
The Role of ER and Its Associated Proteins in the Expansion of Axon Branches
The ER in axons is in contact with the plasma membrane, which suggests that it provides necessary lipids for membrane expansion (Fowler et al., 2019; Figure 2B). ER and its associated proteins at axon branches contribute to membrane remodeling by regulating membrane fusion and the pool of synaptic vesicles. In Drosophila motor neurons, changing the levels of the ER-associated protein atlastin perturbs the release of synaptic vesicles along axons (De Gregorio et al., 2017). In contrast, overexpression of protrudin, an ER-resident protein, leads to membrane deformation and the formation of long neurites (Shirane and Nakayama, 2006), likely mediated by the interaction with the GDP-form of Rab11 and Kinesin-1. Both regulate the anterograde transport of recycling endosomes to the plasma membrane at growing axons (Shirane and Nakayama, 2006; Matsuzaki et al., 2011; Raiborg et al., 2015). A similar mechanism is found for protrudin in cultured cortical neurons as well as in injured optic nerves in vivo (Petrova et al., 2020). A recent study shows that protrudin interacts with ER via PDZD8, which has a lipid transferring activity at the contact sites of ER and endosomes (Shirane et al., 2020) and possibly at the ER-mitochondria interface (Hirabayashi et al., 2017). These point toward a role of protrudin as part of the lipid shuttling machinery to control the membrane expansion and shrinkage.
Endocytosis for the Control of Membrane Retraction
Accumulating observations suggest that membrane expansion and retraction are controlled by membrane trafficking events. Considering the similarity of branching axons to growth cones, it is plausible that the expansion of membranes at branching axons is mediated by exocytosis, while the retraction of branched axons may be controlled by an intake of membrane through endocytosis (Figure 2B). The inhibition of endocytic pathways has been shown to increase the number of branches in different types of neurons (Zhou et al., 2007; Hausott et al., 2011; Kanamori et al., 2015), presumably due to the accumulation of branching signaling elements like NGFs and FGFR1. Furthermore, it has been shown that the membrane-curvature forming F-BAR (FER/CIP4 Homology Bin-Amphiphysin-RVS) family proteins, involved in endocytosis, negatively regulate axon branch formation (reviewed in Winkle et al., 2016). GFP-labeled Rab5 vesicles, that mark early endosomes, accumulate at axon branching sites (Ponomareva et al., 2014). This series of experiments shows that endocytic trafficking itself may regulate axon branching negatively, while exocytosis of synaptic vesicles correlates with the promotion of axon branching. In addition to these classical models of membrane retraction, Bishop et al. (2004) reported that axon branches at neuromuscular junctions are removed by a shedding of membrane-bound remnants, which contain mitochondria and synaptic vesicles. This particular mechanism could be advantageous for rapidly retracting axonal branches, especially for the axon pruning process. However, its regulation mechanism has yet to be shown.
Concluding Remarks
Axon branching is a dynamic process that modulates the axonal architecture and fosters various cellular activities to ensure interconnections with neighboring neurons. It requires a highly coordinated and controlled organization of numerous cellular machineries. While many cellular processes at axon branches resemble those found in non-neuronal cells, some functions and regulatory features have been specifically adapted to axon branching. Despite a wealth of in-depth information on the axon branching process unveiled in recent years, many key questions are still open and part of active research: How are initial branching sites selected? What is the hierarchical sequence of molecular actions from the initiation of branching to a stabilized, mature branch site? How is the crosstalk of membranes and cytoskeleton components mediated? How are cellular components like synaptic vesicles and mitochondria shuttled to and stationed at branching sites? How is the assembly of the building blocks coordinated to achieve the formation of axon branches? Do all types of neurons share similar mechanisms, considering the diversity of different neurons and their morphologies? Answering these questions in the future will help to understand how neuronal circuit formation is facilitated on a molecular level.
Author Contributions
SB and NM collected, analyzed the relevant literature, and wrote the review manuscript. HN prepared the figures with the help of the other authors. NB commented on and reviewed the manuscript prior to submission. All authors read and approved the submitted version.
Funding
The Mizuno lab was supported by the Intramural Research Program of the National Heart Lung and Blood Institute and NM was jointly supported by the National Institute of Arthritis and Musculoskeletal and Skin Diseases of National Institutes of Health, United States.
Conflict of Interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
Publisher’s Note
All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors and the reviewers. Any product that may be evaluated in this article, or claim that may be made by its manufacturer, is not guaranteed or endorsed by the publisher.
Acknowledgments
We thank members of the Mizuno lab and Dr. Christian Biertümpfel for helpful discussions.
References
Ahnert-Hilger, G., Holtje, M., Grosse, G., Pickert, G., Mucke, C., Nixdorf-Bergweiler, B., et al. (2004). Differential effects of Rho GTPases on axonal and dendritic development in hippocampal neurones. J. Neurochem. 90, 9–18. doi: 10.1111/j.1471-4159.2004.02475.x
Alsina, B., Vu, T., and Cohen-Cory, S. (2001). Visualizing synapse formation in arborizing optic axons in vivo: dynamics and modulation by BDNF. Nat. Neurosci. 4, 1093–1101. doi: 10.1038/nn735
Armijo-Weingart, L., and Gallo, G. (2017). It takes a village to raise a branch: cellular mechanisms of the initiation of axon collateral branches. Mol. Cell. Neurosci. 84, 36–47. doi: 10.1016/j.mcn.2017.03.007
Armijo-Weingart, L., Ketschek, A., Sainath, R., Pacheco, A., Smith, G. M., and Gallo, G. (2019). Neurotrophins induce fission of mitochondria along embryonic sensory axons. Elife 8:e49494.
Basnet, N., Nedozralova, H., Crevenna, A. H., Bodakuntla, S., Schlichthaerle, T., Taschner, M., et al. (2018). Direct induction of microtubule branching by microtubule nucleation factor SSNA1. Nat. Cell Biol. 20, 1172–1180. doi: 10.1038/s41556-018-0199-8
Bishop, D. L., Misgeld, T., Walsh, M. K., Gan, W. B., and Lichtman, J. W. (2004). Axon branch removal at developing synapses by axosome shedding. Neuron 44, 651–661. doi: 10.1016/j.neuron.2004.10.026
Brill, M. S., Kleele, T., Ruschkies, L., Wang, M., Marahori, N. A., Reuter, M. S., et al. (2016). Branch-specific microtubule destabilization mediates axon branch loss during neuromuscular synapse elimination. Neuron 92, 845–856. doi: 10.1016/j.neuron.2016.09.049
Cai, S., Weaver, L. N., Ems-Mcclung, S. C., and Walczak, C. E. (2009). Kinesin-14 family proteins HSET/XCTK2 control spindle length by cross-linking and sliding microtubules. Mol. Biol. Cell 20, 1348–1359. doi: 10.1091/mbc.e08-09-0971
Courchet, J., Lewis, T. L. Jr., Lee, S., Courchet, V., Liou, D. Y., Aizawa, S., et al. (2013). Terminal axon branching is regulated by the LKB1-NUAK1 kinase pathway via presynaptic mitochondrial capture. Cell 153, 1510–1525. doi: 10.1016/j.cell.2013.05.021
Dan, W., Gao, N., Li, L., Zhu, J. X., Diao, L., Huang, J., et al. (2018). alpha-tubulin acetylation restricts axon overbranching by dampening microtubule plus-end dynamics in neurons. Cereb. Cortex 28, 3332–3346. doi: 10.1093/cercor/bhx225
De Gregorio, C., Delgado, R., Ibacache, A., Sierralta, J., and Couve, A. (2017). Drosophila atlastin in motor neurons is required for locomotion and presynaptic function. J. Cell Sci. 130, 3507–3516.
Dent, E. W., Barnes, A. M., Tang, F., and Kalil, K. (2004). Netrin-1 and semaphorin 3A promote or inhibit cortical axon branching, respectively, by reorganization of the cytoskeleton. J. Neurosci. 24, 3002–3012. doi: 10.1523/jneurosci.4963-03.2004
Dent, E. W., and Kalil, K. (2001). Axon branching requires interactions between dynamic microtubules and actin filaments. J. Neurosci. 21, 9757–9769. doi: 10.1523/jneurosci.21-24-09757.2001
Dent, E. W., Kwiatkowski, A. V., Mebane, L. M., Philippar, U., Barzik, M., Rubinson, D. A., et al. (2007). Filopodia are required for cortical neurite initiation. Nat. Cell Biol. 9, 1347–1359. doi: 10.1038/ncb1654
Dent, E. W., Tang, F., and Kalil, K. (2003). Axon guidance by growth cones and branches: common cytoskeletal and signaling mechanisms. Neuroscientist 9, 343–353. doi: 10.1177/1073858403252683
Diamond, J., Coughlin, M., Macintyre, L., Holmes, M., and Visheau, B. (1987). Evidence that endogenous beta nerve growth factor is responsible for the collateral sprouting, but not the regeneration, of nociceptive axons in adult rats. Proc. Natl. Acad. Sci. U. S. A. 84, 6596–6600. doi: 10.1073/pnas.84.18.6596
Diamond, J., Holmes, M., and Coughlin, M. (1992). Endogenous NGF and nerve impulses regulate the collateral sprouting of sensory axons in the skin of the adult rat. J. Neurosci. 12, 1454–1466. doi: 10.1523/jneurosci.12-04-01454.1992
Dwivedy, A., Gertler, F. B., Miller, J., Holt, C. E., and Lebrand, C. (2007). Ena/VASP function in retinal axons is required for terminal arborization but not pathway navigation. Development 134, 2137–2146. doi: 10.1242/dev.002345
Farias, G. G., Freal, A., Tortosa, E., Stucchi, R., Pan, X., Portegies, S., et al. (2019). Feedback-driven mechanisms between microtubules and the endoplasmic reticulum instruct neuronal polarity. Neuron 102, e188.
Fowler, P. C., Garcia-Pardo, M. E., Simpson, J. C., and O’sullivan, N. C. (2019). NeurodegenERation: the central role for ER contacts in neuronal function and axonopathy, lessons from hereditary spastic paraplegias and related diseases. Front. Neurosci. 13:1051. doi: 10.3389/fnins.2019.01051
Friedman, J. R., Lackner, L. L., West, M., Dibenedetto, J. R., Nunnari, J., and Voeltz, G. K. (2011). ER tubules mark sites of mitochondrial division. Science 334, 358–362. doi: 10.1126/science.1207385
Gallo, G. (2011). The cytoskeletal and signaling mechanisms of axon collateral branching. Dev. Neurobiol. 71, 201–220. doi: 10.1002/dneu.20852
Gallo, G., and Letourneau, P. C. (1998). Localized sources of neurotrophins initiate axon collateral sprouting. J. Neurosci. 18, 5403–5414. doi: 10.1523/jneurosci.18-14-05403.1998
Gallo, G., and Letourneau, P. C. (1999). Different contributions of microtubule dynamics and transport to the growth of axons and collateral sprouts. J. Neurosci. 19, 3860–3873. doi: 10.1523/jneurosci.19-10-03860.1999
Gibson, D. A., and Ma, L. (2011). Developmental regulation of axon branching in the vertebrate nervous system. Development 138, 183–195. doi: 10.1242/dev.046441
Goyal, U., Renvoise, B., Chang, J., and Blackstone, C. (2014). Spastin-interacting protein NA14/SSNA1 functions in cytokinesis and axon development. PLoS One 9:e112428. doi: 10.1371/journal.pone.0112428
Greif, K. F., Asabere, N., Lutz, G. J., and Gallo, G. (2013). Synaptotagmin-1 promotes the formation of axonal filopodia and branches along the developing axons of forebrain neurons. Dev. Neurobiol. 73, 27–44. doi: 10.1002/dneu.22033
Guo, W., Stoklund Dittlau, K., and Van Den Bosch, L. (2020). Axonal transport defects and neurodegeneration: molecular mechanisms and therapeutic implications. Semin. Cell Dev. Biol. 99, 133–150. doi: 10.1016/j.semcdb.2019.07.010
Hall, A. (1998). Rho GTPases and the actin cytoskeleton. Science 279, 509–514. doi: 10.1126/science.279.5350.509
Hall, A., and Lalli, G. (2010). Rho and Ras GTPases in axon growth, guidance, and branching. Cold Spring Harb. Perspect. Biol. 2:a001818. doi: 10.1101/cshperspect.a001818
Harris, W. A., Holt, C. E., and Bonhoeffer, F. (1987). Retinal axons with and without their somata, growing to and arborizing in the tectum of Xenopus embryos: a time-lapse video study of single fibres in vivo. Development 101, 123–133. doi: 10.1242/dev.101.1.123
Hausott, B., Rietzler, A., Vallant, N., Auer, M., Haller, I., Perkhofer, S., et al. (2011). Inhibition of fibroblast growth factor receptor 1 endocytosis promotes axonal branching of adult sensory neurons. Neuroscience 188, 13–22. doi: 10.1016/j.neuroscience.2011.04.064
Hirabayashi, Y., Kwon, S. K., Paek, H., Pernice, W. M., Paul, M. A., Lee, J., et al. (2017). ER-mitochondria tethering by PDZD8 regulates Ca(2+) dynamics in mammalian neurons. Science 358, 623–630. doi: 10.1126/science.aan6009
Hoersting, A. K., and Schmucker, D. (2021). Axonal branch patterning and neuronal shape diversity: roles in developmental circuit assembly: axonal branch patterning and neuronal shape diversity in developmental circuit assembly. Curr. Opin. Neurobiol. 66, 158–165. doi: 10.1016/j.conb.2020.10.019
Hooikaas, P. J., Martin, M., Muhlethaler, T., Kuijntjes, G.-J., Peeters, C. A. E., Katrukha, E. A., et al. (2019). MAP7 family proteins regulate kinesin-1 recruitment and activation. J. Cell Biol. 218, 1298–1318. doi: 10.1083/jcb.201808065
Hu, B., Nikolakopoulou, A. M., and Cohen-Cory, S. (2005). BDNF stabilizes synapses and maintains the structural complexity of optic axons in vivo. Development 132, 4285–4298. doi: 10.1242/dev.02017
Hu, J., Bai, X., Bowen, J. R., Dolat, L., Korobova, F., Yu, W., et al. (2012). Septin-driven coordination of actin and microtubule remodeling regulates the collateral branching of axons. Curr. Biol. 22, 1109–1115. doi: 10.1016/j.cub.2012.04.019
Hutchins, B. I., and Kalil, K. (2008). Differential outgrowth of axons and their branches is regulated by localized calcium transients. J. Neurosci. 28, 143–153. doi: 10.1523/jneurosci.4548-07.2008
Jahn, R. (2000). Sec1/Munc18 proteins: mediators of membrane fusion moving to center stage. Neuron 27, 201–204. doi: 10.1016/s0896-6273(00)00029-5
Janke, C., and Magiera, M. M. (2020). The tubulin code and its role in controlling microtubule properties and functions. Nat. Rev. Mol. Cell Biol. 21, 307–326. doi: 10.1038/s41580-020-0214-3
Jin, L. Q., Pennise, C. R., Rodemer, W., Jahn, K. S., and Selzer, M. E. (2016). Protein synthetic machinery and mRNA in regenerating tips of spinal cord axons in lamprey. J. Comp. Neurol. 524, 3614–3640. doi: 10.1002/cne.24020
Johri, A., and Beal, M. F. (2012). Mitochondrial dysfunction in neurodegenerative diseases. J. Pharmacol. Exp. Ther. 342, 619–630.
Kalil, K., and Dent, E. W. (2013). Branch management: mechanisms of axon branching in the developing vertebrate CNS. Nat. Rev. Neurosci. 15, 7–18.
Kalil, K., and Dent, E. W. (2014). Branch management: mechanisms of axon branching in the developing vertebrate CNS. Nat. Rev. Neurosci. 15, 7–18. doi: 10.1038/nrn3650
Kalil, K., Szebenyi, G., and Dent, E. W. (2000). Common mechanisms underlying growth cone guidance and axon branching. J. Neurobiol. 44, 145–158. doi: 10.1002/1097-4695(200008)44:2<145::aid-neu5>3.0.co;2-x
Kanamori, T., Yoshino, J., Yasunaga, K., Dairyo, Y., and Emoto, K. (2015). Local endocytosis triggers dendritic thinning and pruning in Drosophila sensory neurons. Nat. Commun. 6:6515.
Ketschek, A., and Gallo, G. (2010). Nerve growth factor induces axonal filopodia through localized microdomains of phosphoinositide 3-kinase activity that drive the formation of cytoskeletal precursors to filopodia. J. Neurosci. 30, 12185–12197. doi: 10.1523/jneurosci.1740-10.2010
Ketschek, A., Spillane, M., Dun, X. P., Hardy, H., Chilton, J., and Gallo, G. (2016). Drebrin coordinates the actin and microtubule cytoskeleton during the initiation of axon collateral branches. Dev. Neurobiol. 76, 1092–1110. doi: 10.1002/dneu.22377
Korobova, F., Ramabhadran, V., and Higgs, H. N. (2013). An actin-dependent step in mitochondrial fission mediated by the ER-associated formin INF2. Science 339, 464–467. doi: 10.1126/science.1228360
Kraszewski, K., Mundigl, O., Daniell, L., Verderio, C., Matteoli, M., and De Camilli, P. (1995). Synaptic vesicle dynamics in living cultured hippocampal neurons visualized with CY3-conjugated antibodies directed against the lumenal domain of synaptotagmin. J. Neurosci. 15, 4328–4342. doi: 10.1523/jneurosci.15-06-04328.1995
Kuo, Y.-W., Trottier, O., Mahamdeh, M., and Howard, J. (2019). Spastin is a dual-function enzyme that severs microtubules and promotes their regrowth to increase the number and mass of microtubules. Proc. Natl. Acad. Sci. U. S. A. 116, 5533–5541. doi: 10.1073/pnas.1818824116
Lewis, T. L. Jr., Kwon, S. K., Lee, A., Shaw, R., and Polleux, F. (2018). MFF-dependent mitochondrial fission regulates presynaptic release and axon branching by limiting axonal mitochondria size. Nat. Commun. 9:5008.
Liu, X., Guo, X., Niu, L., Li, X., Sun, F., Hu, J., et al. (2019). Atlastin-1 regulates morphology and function of endoplasmic reticulum in dendrites. Nat. Commun. 10:568.
Magiera, M. M., Bodakuntla, S., Ziak, J., Lacomme, S., Marques Sousa, P., Leboucher, S., et al. (2018). Excessive tubulin polyglutamylation causes neurodegeneration and perturbs neuronal transport. EMBO J. 37:e100440.
Matsuzaki, F., Shirane, M., Matsumoto, M., and Nakayama, K. I. (2011). Protrudin serves as an adaptor molecule that connects KIF5 and its cargoes in vesicular transport during process formation. Mol. Biol. Cell 22, 4602–4620. doi: 10.1091/mbc.e11-01-0068
McCormick, L. E., and Gupton, S. L. (2020). Mechanistic advances in axon pathfinding. Curr. Opin. Cell Biol. 63, 11–19. doi: 10.1016/j.ceb.2019.12.003
Merianda, T. T., Lin, A. C., Lam, J. S., Vuppalanchi, D., Willis, D. E., Karin, N., et al. (2009). A functional equivalent of endoplasmic reticulum and Golgi in axons for secretion of locally synthesized proteins. Mol. Cell Neurosci. 40, 128–142. doi: 10.1016/j.mcn.2008.09.008
Meyer, M. P., and Smith, S. J. (2006). Evidence from in vivo imaging that synaptogenesis guides the growth and branching of axonal arbors by two distinct mechanisms. J. Neurosci. 26, 3604–3614. doi: 10.1523/jneurosci.0223-06.2006
Mitchison, T., and Kirschner, M. (1984). Dynamic instability of microtubule growth. Nature 312, 237–242. doi: 10.1038/312237a0
Mitchison, T. J. (1993). Localization of an exchangeable GTP binding site at the plus end of microtubules. Science 261, 1044–1047. doi: 10.1126/science.8102497
Nixon-Abell, J., Obara, C. J., Weigel, A. V., Li, D., Legant, W. R., Xu, C. S., et al. (2016). Increased spatiotemporal resolution reveals highly dynamic dense tubular matrices in the peripheral ER. Science 354:aaf3928. doi: 10.1126/science.aaf3928
O’Leary, D. D., Bicknese, A. R., De Carlos, J. A., Heffner, C. D., Koester, S. E., Kutka, L. J., et al. (1990). Target selection by cortical axons: alternative mechanisms to establish axonal connections in the developing brain. Cold Spring Harb. Symp. Quant. Biol. 55, 453–468. doi: 10.1101/sqb.1990.055.01.045
Ohnami, S., Endo, M., Hirai, S., Uesaka, N., Hatanaka, Y., Yamashita, T., et al. (2008). Role of RhoA in activity-dependent cortical axon branching. J. Neurosci. 28, 9117–9121. doi: 10.1523/jneurosci.1731-08.2008
Perin, M. S., Fried, V. A., Mignery, G. A., Jahn, R., and Sudhof, T. C. (1990). Phospholipid binding by a synaptic vesicle protein homologous to the regulatory region of protein kinase C. Nature 345, 260–263. doi: 10.1038/345260a0
Petrova, V., Pearson, C. S., Ching, J., Tribble, J. R., Solano, A. G., Yang, Y., et al. (2020). Protrudin functions from the endoplasmic reticulum to support axon regeneration in the adult CNS. Nat. Commun. 11:5614.
Ponomareva, O. Y., Holmen, I. C., Sperry, A. J., Eliceiri, K. W., and Halloran, M. C. (2014). Calsyntenin-1 regulates axon branching and endosomal trafficking during sensory neuron development in vivo. J. Neurosci. 34, 9235–9248. doi: 10.1523/jneurosci.0561-14.2014
Raiborg, C., Wenzel, E. M., Pedersen, N. M., Olsvik, H., Schink, K. O., Schultz, S. W., et al. (2015). Repeated ER-endosome contacts promote endosome translocation and neurite outgrowth. Nature 520, 234–238. doi: 10.1038/nature14359
Renvoise, B., and Blackstone, C. (2010). Emerging themes of ER organization in the development and maintenance of axons. Curr. Opin. Neurobiol. 20, 531–537. doi: 10.1016/j.conb.2010.07.001
Ruthazer, E. S., Li, J., and Cline, H. T. (2006). Stabilization of axon branch dynamics by synaptic maturation. J. Neurosci. 26, 3594–3603. doi: 10.1523/jneurosci.0069-06.2006
Ruthel, G., and Hollenbeck, P. J. (2003). Response of mitochondrial traffic to axon determination and differential branch growth. J. Neurosci. 23, 8618–8624. doi: 10.1523/jneurosci.23-24-08618.2003
Sainath, R., and Gallo, G. (2015). Cytoskeletal and signaling mechanisms of neurite formation. Cell Tissue Res. 359, 267–278. doi: 10.1007/s00441-014-1955-0
Sainath, R., Ketschek, A., Grandi, L., and Gallo, G. (2017). CSPGs inhibit axon branching by impairing mitochondria-dependent regulation of actin dynamics and axonal translation. Dev. Neurobiol. 77, 454–473. doi: 10.1002/dneu.22420
Schwarz, D. S., and Blower, M. D. (2016). The endoplasmic reticulum: structure, function and response to cellular signaling. Cell. Mol. Life Sci. 73, 79–94. doi: 10.1007/s00018-015-2052-6
Sheng, Z. H. (2017). The interplay of axonal energy homeostasis and mitochondrial trafficking and anchoring. Trends Cell Biol. 27, 403–416. doi: 10.1016/j.tcb.2017.01.005
Sheng, Z. H., and Cai, Q. (2012). Mitochondrial transport in neurons: impact on synaptic homeostasis and neurodegeneration. Nat. Rev. Neurosci. 13, 77–93.
Shibata, Y., Shemesh, T., Prinz, W. A., Palazzo, A. F., Kozlov, M. M., and Rapoport, T. A. (2010). Mechanisms determining the morphology of the peripheral ER. Cell 143, 774–788. doi: 10.1016/j.cell.2010.11.007
Shirane, M., and Nakayama, K. I. (2006). Protrudin induces neurite formation by directional membrane trafficking. Science 314, 818–821. doi: 10.1126/science.1134027
Shirane, M., Wada, M., Morita, K., Hayashi, N., Kunimatsu, R., Matsumoto, Y., et al. (2020). Protrudin and PDZD8 contribute to neuronal integrity by promoting lipid extraction required for endosome maturation. Nat. Commun. 11:4576.
Sollner, T., Bennett, M. K., Whiteheart, S. W., Scheller, R. H., and Rothman, J. E. (1993). A protein assembly-disassembly pathway in vitro that may correspond to sequential steps of synaptic vesicle docking, activation, and fusion. Cell 75, 409–418. doi: 10.1016/0092-8674(93)90376-2
Spillane, M., Ketschek, A., Jones, S. L., Korobova, F., Marsick, B., Lanier, L., et al. (2011). The actin nucleating Arp2/3 complex contributes to the formation of axonal filopodia and branches through the regulation of actin patch precursors to filopodia. Dev. Neurobiol. 71, 747–758. doi: 10.1002/dneu.20907
Spillane, M., Ketschek, A., Merianda, T. T., Twiss, J. L., and Gallo, G. (2013). Mitochondria coordinate sites of axon branching through localized intra-axonal protein synthesis. Cell Rep. 5, 1564–1575. doi: 10.1016/j.celrep.2013.11.022
Steiner, P., Sarria, J. C., Huni, B., Marsault, R., Catsicas, S., and Hirling, H. (2002). Overexpression of neuronal Sec1 enhances axonal branching in hippocampal neurons. Neuroscience 113, 893–905. doi: 10.1016/s0306-4522(02)00225-7
Strasser, G. A., Rahim, N. A., Vanderwaal, K. E., Gertler, F. B., and Lanier, L. M. (2004). Arp2/3 is a negative regulator of growth cone translocation. Neuron 43, 81–94. doi: 10.1016/j.neuron.2004.05.015
Szebenyi, G., Callaway, J. L., Dent, E. W., and Kalil, K. (1998). Interstitial branches develop from active regions of the axon demarcated by the primary growth cone during pausing behaviors. J. Neurosci. 18, 7930–7940. doi: 10.1523/jneurosci.18-19-07930.1998
Tao, K., Matsuki, N., and Koyama, R. (2014). AMP-activated protein kinase mediates activity-dependent axon branching by recruiting mitochondria to axon. Dev. Neurobiol. 74, 557–573. doi: 10.1002/dneu.22149
Tymanskyj, S. R., Yang, B., Falnikar, A., Lepore, A. C., and Ma, L. (2017). MAP7 regulates axon collateral branch development in dorsal root ganglion neurons. J. Neurosci. 37, 1648–1661. doi: 10.1523/jneurosci.3260-16.2017
Tymanskyj, S. R., Yang, B. H., Verhey, K. J., and Ma, L. (2018). MAP7 regulates axon morphogenesis by recruiting kinesin-1 to microtubules and modulating organelle transport. Elife 7:e36374.
van Spronsen, M., Mikhaylova, M., Lipka, J., Schlager, M. A., Van Den Heuvel, D. J., Kuijpers, M., et al. (2013). TRAK/Milton motor-adaptor proteins steer mitochondrial trafficking to axons and dendrites. Neuron 77, 485–502. doi: 10.1016/j.neuron.2012.11.027
Verderio, C., Coco, S., Bacci, A., Rossetto, O., De Camilli, P., Montecucco, C., et al. (1999). Tetanus toxin blocks the exocytosis of synaptic vesicles clustered at synapses but not of synaptic vesicles in isolated axons. J. Neurosci. 19, 6723–6732. doi: 10.1523/jneurosci.19-16-06723.1999
Waters, M. G., and Hughson, F. M. (2000). Membrane tethering and fusion in the secretory and endocytic pathways. Traffic 1, 588–597. doi: 10.1034/j.1600-0854.2000.010802.x
Willis, D. E., Van Niekerk, E. A., Sasaki, Y., Mesngon, M., Merianda, T. T., Williams, G. G., et al. (2007). Extracellular stimuli specifically regulate localized levels of individual neuronal mRNAs. J. Cell Biol. 178, 965–980. doi: 10.1083/jcb.200703209
Winkle, C. C., and Gupton, S. L. (2016). Membrane trafficking in neuronal development: ins and outs of neural connectivity. Int. Rev. Cell Mol. Biol. 322, 247–280. doi: 10.1016/bs.ircmb.2015.10.003
Winkle, C. C., Mcclain, L. M., Valtschanoff, J. G., Park, C. S., Maglione, C., and Gupton, S. L. (2014). A novel Netrin-1-sensitive mechanism promotes local SNARE-mediated exocytosis during axon branching. J. Cell Biol. 205, 217–232. doi: 10.1083/jcb.201311003
Winkle, C. C., Taylor, K. L., Dent, E. W., Gallo, G., Greif, K. F., and Gupton, S. L. (2016). Beyond the cytoskeleton: the emerging role of organelles and membrane remodeling in the regulation of axon collateral branches. Dev. Neurobiol. 76, 1293–1307. doi: 10.1002/dneu.22398
Wu, Y., Whiteus, C., Xu, C. S., Hayworth, K. J., Weinberg, R. J., Hess, H. F., et al. (2017). Contacts between the endoplasmic reticulum and other membranes in neurons. Proc. Natl. Acad. Sci. U. S. A. 114, E4859–E4867.
Yamamoto, N., Higashi, S., and Toyama, K. (1997). Stop and branch behaviors of geniculocortical axons: a time-lapse study in organotypic cocultures. J. Neurosci. 17, 3653–3663. doi: 10.1523/jneurosci.17-10-03653.1997
Yu, W., Ahmad, F. J., and Baas, P. W. (1994). Microtubule fragmentation and partitioning in the axon during collateral branch formation. J. Neurosci. 14, 5872–5884. doi: 10.1523/jneurosci.14-10-05872.1994
Yu, W., Qiang, L., Solowska, J. M., Karabay, A., Korulu, S., and Baas, P. W. (2008). The microtubule-severing proteins spastin and katanin participate differently in the formation of axonal branches. Mol. Biol. Cell 19, 1485–1498. doi: 10.1091/mbc.e07-09-0878
Zhou, X., Babu, J. R., Da Silva, S., Shu, Q., Graef, I. A., Oliver, T., et al. (2007). Unc-51-like kinase 1/2-mediated endocytic processes regulate filopodia extension and branching of sensory axons. Proc. Natl. Acad. Sci. U. S. A. 104, 5842–5847. doi: 10.1073/pnas.0701402104
Zhu, P. P., Soderblom, C., Tao-Cheng, J. H., Stadler, J., and Blackstone, C. (2006). SPG3A protein atlastin-1 is enriched in growth cones and promotes axon elongation during neuronal development. Hum. Mol. Genet. 15, 1343–1353. doi: 10.1093/hmg/ddl054
Keywords: cytoskeleton, mitochondria, actin, microtubules, endoplasmic reticulum, axon branching, membraneremodeling and neurons
Citation: Bodakuntla S, Nedozralova H, Basnet N and Mizuno N (2021) Cytoskeleton and Membrane Organization at Axon Branches. Front. Cell Dev. Biol. 9:707486. doi: 10.3389/fcell.2021.707486
Received: 10 May 2021; Accepted: 06 August 2021;
Published: 01 September 2021.
Edited by:
Anna Onnis, University of Siena, ItalyReviewed by:
Nobuhiko Yamamoto, Osaka University, JapanLe Ma, Thomas Jefferson University, United States
Copyright © 2021 Bodakuntla, Nedozralova, Basnet and Mizuno. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Naoko Mizuno, naoko.mizuno@nih.gov; Satish Bodakuntla, satish.bodakuntla@nih.gov