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. 2025 Apr 29;4(1):kyaf008. doi: 10.1093/discim/kyaf008

Inflammation’s impact on the interaction between oligodendrocytes and axons

Tabitha R F Green 1,, Marieke Pingen 2, Julia M Edgar 3
PMCID: PMC12239092  PMID: 40636264

Abstract

Oligodendrocytes are responsible for the myelination of axons and providing trophic and metabolic support to the myelinated axon. They also interact with immune effector cells, including microglia and T cells, hence, are involved in central nervous system immune regulation. Given the crucial roles for oligodendrocytes and myelin in axonal function and maintenance, dysfunction, whether through cell death, myelin injury and loss, or failure in normal myelin formation, impairs neurological function. In diseases such as multiple sclerosis, the leukodystrophies, and viral infection, neuroinflammation is an important effector of myelin injury, having secondary consequences for the myelinated axon. In this review, we discuss the role of oligodendrocytes in health and inflammatory disease, with a focus on the interplay between inflammation and oligodendrocyte-axon interactions.

Keywords: microglia, T cells, neurodegeneration, myelin, oligodendrocytes

Graphical Abstract

Graphical Abstract.

Graphical Abstract

Introduction

In the central nervous system (CNS), axons, the electrically excitable ‘cable-like’ processes of neurons, carry information from one nerve cell soma to another. Most CNS axons are surrounded segmentally by myelin, which is produced by oligodendrocytes. Myelin speeds up the propagation of neuronal signalling and likely helps establish and modify neuronal circuitry [1–4]. However, the role of oligodendrocytes extends beyond their crucial ability to myelinate axons, as described in detail below.

Oligodendrocyte cell death and subsequent myelin loss, myelin injury, or failure in normal myelination can each impair neurological function. Neuroinflammation is an important effector of oligodendroglial and myelin injury, both as a primary and secondary insult. In this review, we describe some diseases of CNS myelin and how the associated neuroinflammation affects the oligodendroglial-axonal unit. We also briefly describe the recent evidence that oligodendrocytes themselves can act as immune effector cells.

Functions of oligodendrocytes

In the white matter of the CNS, myelin sheaths segment the axon into long (~20-200 μm) myelinated ‘internodes’ separated by short (~1 μm) unmyelinated nodes of Ranvier (Figure 1) where ion channels enable the ion flux required for action potential generation and transduction. In the grey matter, some axons are sparsely myelinated [6, 7] (Figure 1), and the function of this sparse myelin is less well understood and unlikely to be related to conduction velocity. Notwithstanding, a recent study showed that the sparse myelin on parvalbumin-positive γ-aminobutyric acid interneurons is crucial for effective inhibition of pyramidal neurons and enabling behavioural state-dependent modulation of local circuit synchronization in mice [2].

Figure 1.

Figure 1.

Grey and white matter myelin in the CNS. In the grey matter, some axons (purple, upper right) are intermittently myelinated (green). In white matter, most of the axon is sequestered beneath myelin, and myelin sheaths are separated only by short unmyelinated regions called nodes of Ranvier. In general, each oligodendrocyte (OL) myelinates multiple axons. The paranodes (P), where the paranodal loops of myelin attach to the axon through septate-like junctions, flank the node of Ranvier (N). Both grey and white matter harbour blood vessels (BV), astrocytes (blue), microglia (turquoise), and oligodendrocyte progenitor cells (OPCs). The last helps maintain immune homeostasis by downregulating microglial C-X3-C motif chemokine receptor 1 (CX3CR1) expression and suppressing microglial activation [5].

To understand how neuroinflammation impacts the oligodendroglial-axonal unit, it is important to highlight that the function of myelinating oligodendrocytes extends far beyond the insulation or modulation of neuronal circuits. Throughout life, oligodendrocytes deliver energy substrates and trophic factors to myelinated axons for axon energy homeostasis and survival (reviewed recently in Stassart et al. and Duncan et al. [8, 9]. At least in white matter tracts, this energy support function of oligodendrocytes overcomes the fact that myelin limits the capacity for such axons to receive energy substrates from the extracellular milieu, from which they are almost completely insulated [10, 11]. Myelinated axons require oligodendroglial-funnelled energy substrates, be they glucose, pyruvate, or lactate [12–14], for processes such as motor protein-dependent transport over long distances and to restore intracellular ion concentrations after action potential generation. The latter is particularly relevant as demonstrated by the relationship between ATP levels and compound action potential generation in an electrically stimulated ex vivo mouse optic nerve preparation [15].

Besides funnelling energy substrates, oligodendrocytes also buffer iron and extracellular potassium. For example, preventing the release of oligodendrocyte ferritin heavy chain-containing extracellular vesicles led to increased neuronal loss, through iron-mediated ferroptotic axonal damage, in mice [16]. Thus, oligodendrocytes have a crucial antioxidant defence function [16]. Conversely, Kir4.1 channels on the inner myelin membrane, facing the axon, sequester K+ released by firing axons, thus preventing seizure activity and maintaining axon health [17, 18]. Of note, activation of Kir4.1 channels by axon-derived K+ ions couples oligodendroglial metabolic support with axonal firing rate [19], a surrogate of axon energy consumption. Thus, periaxonal K+ ion concentration signals to the oligodendrocyte to match the axon’s fluctuating demands for energy substrates.

Oligodendrocytes also influence the structure of the myelinated axon. For example, they locally modulate neurofilament transport rates and phosphorylation, thus influencing local axon calibre, albeit to a lesser extent than in the peripheral nervous system [20–26]. Intriguingly, in grey matter, myelin clusters axonal mitochondria beneath the sparse myelin sheaths on interneuron axons [27]. However, in the optic nerve, a white matter tract that is continuously myelinated except at the optic nerve head, axonal mitochondria are most enriched at the unmyelinated region [27]. This latter pattern is seen also following white matter demyelination, where denuded axon segments have increased mitochondrial abundance compared to myelinated regions [28].

Together these data demonstrate the importance of oligodendrocytes for the function and health of myelinated CNS axons.

Oligodendroglia as immune effectors and modulators

Neuroinflammation is an important effector of myelin and axon injury, both as a primary and secondary insult. Indeed, oligodendrocytes themselves can possess an ‘immune’ phenotype that could, in principle, actively contribute to disease pathogenesis, including axonal injury (reviewed in Castelo-Branco et al. [29]).

Oligodendrocytes express Toll-like receptors 2 and 3 which sense pathogen-associated molecular patterns and damage-associated molecular patterns such as dsRNAs, bacterial surface proteins, and high mobility group box1 protein [30, 31]. They also sense and secrete many immune-related chemokines and cytokines (reviewed in Kirby and Castelo-Branco [32]) and in some circumstances, express major histocompatibility complex (MHC)-I and/or -II [33, 34]. The major histocompatibility complex (MHC) is a large locus on vertebrate DNA that encodes various MHC proteins responsible for presenting antigen to T cells. MHC-I is displayed on all nucleated cells and presents mainly endogenous peptides, while MHC-II expression is largely restricted to thymic epithelial cells and antigen-presenting cells and presents mainly exogenous antigens. Intriguingly, bulk and single-cell RNA-sequencing of neural cells demonstrated induced expression of MHC-I and -II genes in mouse oligodendroglia (including myelinating oligodendrocytes; Figure 2) in experimental autoimmune encephalomyelitis (EAE) and/or cuprizone-induced demyelination [41]. As in various stromal cells [42], interferon-γ is sufficient to induce MHC-II protein expression in oligodendrocytes and their progenitors (OPCs) and oligodendrocytes in vitro [34]. Thus, antigen presentation by oligodendroglia in neuroinflammatory conditions represents a potential direct route of interaction between oligodendrocytes and T cells (Figure 2), having implications for myelin degeneration and axonal injury [34, 43, 44].

Figure 2.

Figure 2.

Oligodendrocyte dysfunction and axon injury in the inflamed CNS. Axons ensheathed by dysfunctional myelin are particularly susceptible to injury whether myelin dysfunction is due to gene mutation, as in the Plp1 and Cnp1 knockout mice, autoimmunity, as in MS and EAE, or viral infection, as in PML. While chronic demyelination can render axons vulnerable to degeneration, acutely demyelinated axons can survive for some time [35]. MHC-I and -II are induced in oligodendrocytes during inflammation and can mediate interaction with T cells. At the juxtaparanode, granzyme secreted by CD8 effector T cells is thought to induce actomyosin contractility at the paranodal loops (arrowheads, inset LHS), thus compressing the axon [36]. Organelle accumulation and axonal swelling, which resolves or leads eventually to axonal transection could alternatively be caused by reactive oxygen and nitrogen species acting on axonal mitochondria [37] or through collapse of the cytoplasm-filled spaces (pale green) of myelin [38] that mediate the transport of materials to the glial-axonal junction [39, 40]. OL: oligodendrocyte; Mg: activated microglial cell; As: astrocyte; BV: blood vessel; OPC, oligodendrocyte progenitor cell.

As well as acting as immune effector cells themselves, OPCs modulate the principal immune effector cells of the CNS, microglia [45], the long-term activation of which can incite a chronic pro-inflammatory microenvironment (reviewed recently in Green and Rowe [46]. For example, in the healthy brain, OPCs help maintain immune homeostasis through the transforming growth factor (TGF)-β2-TGFβR2 axis, which downregulates microglial C-X3-C motif chemokine receptor 1 CX3CR1 expression and suppresses microglial activation [5]. Recent publications highlight the roles microglia can play in myelin development, damage, dysregulation, and repair, thereby directly influencing neuron function and survival [47–49]. Together, the immune phenotype of oligodendroglia and the bidirectional interaction with microglia highlights their role as important cellular players in neuroinflammation.

Myelin disease and neuroinflammation

As indicated in the section ‘Oligodendrocyte Function’, oligodendrocytes and myelin play a crucial role in axonal function and maintenance. In the following sections, we briefly describe some diseases of CNS myelin and how the associated neuroinflammation affects the oligodendroglial-axonal unit. Ageing is not discussed here, having been reviewed recently [50], but there is considerable evidence that inflammation contributes to injury of myelinated axons in the aged CNS [51, 52] and that age-dependent oligodendrocyte dysfunction contributes to the pathogenesis of Alzheimer’s disease [53].

The leukodystrophies

The leukodystrophies are a group of diseases that primarily affect white matter. They are caused by gene mutations leading to dys- and/or demyelination accompanied by secondary neuroinflammation. Pelizaeus Merzbacher disease (PMD) is a well-characterized hypomyelinating leukodystrophy, caused by a mutation in the proteolipid protein (PLP) gene. Although PMD is generally considered non-inflammatory, dys-and demyelinating animal models of PMD caused by gene overexpression (modelling gene duplication in patients, the most common cause of PMD) have overt microglial activation [54, 55] and small numbers of pathogenic CD8 + effector T cells in the CNS [56–58]. Crucially, these T cells are closely associated with MHC-I expressing ‘mutant’ oligodendrocytes, as revealed by confocal microscopy [57]. When in close proximity to a target cell, CD8 + T cells can excrete perforin which forms pores in the target cell, resulting in the uptake of granzymes, which induces apoptosis. Indeed, in Plp1 overexpressing mice, neural damage could be partially ameliorated by chimerizaton with bone marrow from mice deficient in perforin or granzyme B, illustrating the importance of this mechanism for neuronal injury secondary to primary genetic abnormalities in oligodendrocytes [59]. The role of CD8 + effector T cells in axonal injury is described further in the section How neuroinflammation disrupts glial-axonal interaction’.

In contrast to the Plp1 overexpressing mouse, the rumpshaker mouse (point mutation in the Plp1 gene; Ile186Thr), a model of the allelic disorder spastic paraplegia type 2, has only a mild neuroinflammatory response characterized by a slight increase in microglial abundance in white matter tracts where myelin is thinner than normal, but otherwise grossly normal in appearance. Here, Wallerian degeneration affects only the longest myelinated axons in aged mice, indicating a slowly progressing, length-dependent mechanism that could be causally related to mild neuroinflammation, failure of oligodendroglial-mediated axonal support, or both [55, 60]. Remarkably, despite the pathogenic immune response in Plp1-overexpressing mice, a ketogenic diet can ameliorate clinical outcomes and axon and myelin pathology, associated with reduced endoplasmic reticulum stress and restoration of axonal mitochondrial morphology [61]. In the same model, wild-type neural stem cells can outcompete the endogenous ‘mutant’ cells to restore normal myelin following transplantation into the juvenile brain [58]. Notably, the ketogenic diet did not reduce microgliosis or astrocytosis, suggesting it did not reduce neuroinflammation [61], whereas neural stem cell transplantation was associated with a local reduction in activated microglia/macrophages [58].

Distinct from PMD, patients with genetic metabolic leukodystrophies such as X-linked adrenoleukodystrophy (X-ALD) or metachromatic leukodystrophy (MLD), due to mutation in the ATP binding cassette subfamily D member 1 gene and the arylsulfatase A gene respectively, may present at any age with extensive gadolinium-enhancing tumefactive lesions, associated with inflammatory demyelination, neuronal loss, and blood-brain barrier leakage [62]. Significantly, although oligodendrocytes are generally considered key to the pathophysiology of X-ALD and MLD, recent data convincingly demonstrate that microglial injury and loss precedes oligodendrocyte decay and overt myelin loss in these diseases [63]. Thus, the extent of neuroinflammation associated with the leukodystrophies varies across the disorders and within allelic disorders, with overt demyelination being associated with more severe neuroinflammation than hypomyelination, and also with a greater degree of axon injury.

Intriguingly, genetic alterations that primarily affect microglial also result in white matter abnormalities in adult-onset leukoencephalopathy with axonal spheroids and pigmented glia (ALSP), a rare human neurodegenerative disorder [64]. ALSP is due to mutations in the colony-stimulating factor 1 receptor (CSF1R) gene, which encodes CSF1R, a receptor for CSF1 and interleukin 34, required for the survival of microglia. ALSP was recently modelled by specifically ablating microglia in mice through knockout of the conserved fms intronic regulatory element, Fire, from the Csf1r locus, leading to age-dependent focal demyelination through dysregulation of TGFβ1-TGFβR1 signalling [48].

Viral infection

Viral infection is one of the leading causes of demyelination in humans and animals [65], either due to the inflammatory response to infection or through direct infection of oligodendrocytes The latter is exemplified by progressive multifocal leukoencephalopathy (PML), an often-fatal demyelinating disease of humans [66] caused by human polyomavirus 2 (HPyV-2, previously known as John Cunningham or JC virus) which infects oligodendrocytes and astrocytes following the release of virus-carrying extracellular vesicles from the choroid plexus [67]. PML has become increasingly common in the last 40 years in parallel with the acquired immunodeficiency syndrome epidemic and the use of immunosuppressants for autoimmune diseases such as rheumatoid arthritis and Crohn’s disease. One such immunosuppressant is natulizumab [68], a monoclonal antibody that targets α4-integrins which are required for cell migration, for the treatment of MS and other autoimmune disorders. Approximately 80-90% of the human population is seropositive for HPyV-2 and it remains unclear whether immunosuppression allows virus replication in the periphery with subsequent spread to the brain or whether HPyV-2 is present in the brain and immune responses are overwhelmed upon immunosuppression. Demyelination in PML is accepted to result from lytic viral infection of oligodendrocytes (reviewed in Ono et al. [69]). Notably, in the preclinical and early phases of PML, HPyV-2 causes extensive neuronal damage, although it remains unknown whether this is due directly to glial cell infection, or indirectly through the immune reconstitution inflammatory syndrome [70].

Direct viral infection of oligodendrocytes is also observed in animal models, including laboratory mice. For example, Theiler’s murine encephalomyelitis virus (TMEV), Semliki Forest virus, and Zika virus infect oligodendrocytes and other neural cells in mice [71–75]. Not only can these viral-mediated demyelinating models help us understand the pathogenesis of human disease, so too can they help us understand oligodendroglial-axonal interaction. For example, Theiler’s virus has taught us that axonal content can be transferred to the glial cell, probably at the paranodal glial axonal junction where the two cells abut each other [73, 76, 77]. Theiler’s virus represents a remarkable example of a pathogen that navigates the various cells of the organism to evade immune responses and establish a persistent infection. Infection of oligodendrocytes is crucial for Theiler’s virus to persist in the CNS, which it can achieve by transferring non-lytically from the axon [73, 77].

Demyelination following infection with neurotropic virus can alternatively be caused by aberrant immune response to the infection. For example, in some mouse models, T and B cells play a critical role in demyelination after viral infection, for instance with a neurovirulent strain of Murine Hepatitis Virus [78], TMEV [79, 80], or Semliki Forest Virus [80–82]. Intriguingly, even in the absence of detectible virus in the brain, white matter-selective reactive microglia and increased levels of cytokines/chemokines in cerebrospinal fluid accompanied a loss of oligodendrocytes and myelin in a mouse model of SARS-CoV-2 infection, possibly helping explain cognitive impairment in some survivors of COVID-19 in whom white matter-selective reactive microglia were also observed [40]. The complex balance between protective and harmful adaptive antiviral immune responses in the CNS remains incompletely understood.

Multiple sclerosis

Acquired CNS neuroinflammatory disorders are caused by immune dysfunction. Such diseases include multiple sclerosis (MS), acute disseminated encephalomyelitis, neuromyelitis optica spectrum disorder, and myelin oligodendrocyte glycoprotein-associated disorders. MS is the best-known inflammatory demyelinating disease of the CNS and the leading cause of neurological disability in young adults across many countries in the world. In most cases, MS starts as a relapsing–remitting disease that gradually transitions into a progressive phase, where symptoms gradually worsen without distinct relapses and remissions. Several recent reviews describe the pathological events thought to underlie MS [83–85].

Although the aetiology remains unconfirmed, MS is generally considered autoimmune in nature (the outside-in hypothesis), with immune cells activated in the periphery crossing the blood-brain barrier and attacking CNS myelin [86]. One putative external factor is viral infection during adolescence. Several lines of evidence suggest that infection with Epstein–Barr virus [87] triggers an autoimmune response against glial proteins through molecular mimicry [88, 89]. The alternative possibility that MS begins with a primary pathogenic event in the CNS (the inside-out hypothesis), that could, in susceptible individuals, lead to secondary pathogenic inflammation [90], remains a matter of topical debate [91].

Histopathologically, MS is characterized by extensive grey matter demyelination, especially close to the pia [92] and focally demyelinated ‘plaques’ in the white matter, as well as histological and imaging features consistent with remyelination [93–95]. T and B lymphocytes and myeloid cells infiltrated from the periphery are associated with these lesions. For more than a century, the histological features of grey and white matter lesions have been described, culminating recently in an updated histological classification system [96] which highlights the molecular and cellular changes observed at various stages of lesion development and disease progression. Aside from various pathological changes in myelin and oligodendroglia, axon injury and loss are a key feature of MS and, alongside the loss of neuronal cell bodies, the principal correlate of permanent neurological disability in progressive MS.

Restoration of myelin to demyelinated axons is widely considered crucial to protecting neurons in MS [97]. Given the topic of this review, it is worth noting that microglia have been shown to enhance (re)myelination through a variety of mechanisms including clearing myelin debris [98] secretion of Activin A [99, 100] supply of lipid and cholesterol to oligodendrocytes [101] and through fractalkine (CX3CL1; C-X3-C motif ligand 1) signalling [102]. The role of microglia in remyelination and in MS more generally is complex, and the subject matter has been reviewed recently [103, 104].

How neuroinflammation disrupts glial-axonal interaction

In the sections above, we highlighted some disease-specific examples in which primary or secondary neuroinflammation causes injury to axons through its actions on the oligodendrocyte and myelin. Publication of key manuscripts late last century reinvigorated efforts to understand how axons are injured in myelin disease including MS and the leukodystrophies [105–113]. In MS, axon injury has been attributed, singly or in combination, to soluble and cellular immune-mediated inflammatory insult, altered sodium channel function, axonal energy insufficiency, or loss of trophic/metabolic support from the oligodendrocyte. Although most current research focusses on the susceptibility of demyelinated axons in MS, data from leukodystrophy mouse models that develop axon injury while retaining (almost) normal levels of myelin [111–113] show that myelin per se does not preserve axons. These observations, in myelin gene knockout mice, highlight that molecularly impaired myelin presents a risk for axonal health. Could acute demyelination preserve axons in circumstances where oligodendroglia or myelin are impaired, for example, due to cellular or soluble inflammatory factors?

We previously showed that, in the same optic nerve, axons undergoing active, genetically induced demyelination were more susceptible to injury (focal swelling and axonal transport stasis) than regions of the same axons that were already completely demyelinated [55]. More recently, a study led by the Stassart and Nave laboratories showed that in MS, EAE, and cuprizone-induced demyelination, both demyelinated and/or non-myelinated spinal cord axons were protected from irreversible axon damage compared to their myelinated neighbouring axons, even when the two populations shared the same inflammatory milieu [114]. Simultaneously, a manuscript from the Martini laboratory showed that the efficient stripping of dysfunctional myelin (point mutation in the Plp1 gene) protected axons against T cell-driven degeneration, mechanistically related to aberrant actomyosin constriction of axons at paranodal regions [36] (Figure 2). In the last of these three studies, the importance of adaptive immune cells in axonal demise was demonstrated by crossing the Plp1 mutant mice to Rag1 knockout mice, which lack functional lymphocytes. In the double mutants, axonal loss was significantly attenuated, although not completely ameliorated [36]. Together these data demonstrate the importance of inflammation in axonal injury in the context of inflammation-induced perturbation of oligodendrocytes and myelin, whilst also confirming the importance of molecularly intact oligodendrocytes for axonal survival.

Intriguingly, in adult-onset cerebral ALD, extensive and severe acute axonal damage can be observed prior to overt demyelination in prelesional areas defined by microglia loss and relative myelin preservation [115].

These recent data expand upon previous observations demonstrating that in EAE, an animal model of inflammatory demyelination, the earliest stages of ‘focal axonal degeneration’ (FAD) are observed on axons with intact myelin sheaths [37]. FAD begins with focal swelling of the myelinated axon (Figure 2), which can either resolve or progress to fragmentation of the axon. Mechanistically, Nikić et al. [37] demonstrated that in EAE, macrophage-derived reactive oxygen and nitrogen species (ROS and RNS) could trigger pathological changes in axonal mitochondria and initiate FAD. Indeed, they found that neutralizing ROS and RNS rescued axons already entering the degenerative process. These data are compatible with an earlier report demonstrating that the application of nitric oxide to electrically active myelinated fibres led to axon degeneration in rats, highlighting that action potential generation itself contributes to the axon’s vulnerability to inflammatory factors [116], possibly by depleting energy substrates.

Together, these studies demonstrate how myelinated axons are impacted by cellular and soluble inflammatory factors that primarily target myelin, either following immunization with myelin peptide, as in EAE, or due to mutation in genes expressed in oligodendrocytes, as in the leukodystrophy models.

Conclusion

Oligodendrocytes are complex cells that have many essential homeostatic functions: myelination, axonal trophic support, and ion buffering among others. Under pathological conditions, oligodendrocytes can sense and emit cytokines and chemokines and express MHC molecules, making them key players in neuroinflammatory disease of the CNS. Direct interactions between oligodendrocytes and microglia, T cells, and/or their products, have been shown to impact directly on axonal health. Thus, besides myelin dysfunction (due to mutation in genes expressed by oligodendrocytes or chronic demyelination), inflammation-induced myelin injury itself poses a risk for axonal health in diseases like MS, the leukodystrophies, and viral infection. The findings presented in this review highlight the need for more research to understand how oligodendrocyte functions in the context of axonal support are impaired by inflammation. One putative mechanism not already mentioned in this review is through disruption of transport processes within the cytosolic spaces of myelin that are likely vital to the transfer of materials between the two cells [39, 117] (Figure 2).

Acknowledgements

We are grateful to Professor Ruth Stassart for helpful comments on the manuscript. The Editor-in-Chief, Simon Milling, and handling editor, Francisco Quintana would like to thank the following reviewers, Janos Groh, Juana Pasquini, and an anonymous reviewer, for their contribution to the publication of this article.

Contributor Information

Tabitha R F Green, School of Infection and Immunity, College of Medical, Veterinary and Life Science, University of Glasgow, Glasgow, UK.

Marieke Pingen, School of Infection and Immunity, College of Medical, Veterinary and Life Science, University of Glasgow, Glasgow, UK.

Julia M Edgar, School of Infection and Immunity, College of Medical, Veterinary and Life Science, University of Glasgow, Glasgow, UK.

Author contributions

Tabitha R.F. Green (Conceptualization, Writing—original draft, Writing—review & editing), Marieke Pingen (Writing—review & editing), and Julia M. Edgar (Conceptualization, Funding acquisition, Writing—original draft, Writing—review & editing, Visualization)

Conflict of interest

The authors declare no conflict of interest.

Funding

This work was supported by the UK MS Society (grant 171), NC3Rs Studentship (grant NC/T002247/1), and the Wellcome Trust (grant 217093/Z/19/Z).

Data availability

Not applicable.

Ethical approval

Not applicable.

Referenes

  • 1. Dutta  DJ, Woo  DH, Lee  PR, Pajevic  S, Bukalo  O, Huffman  WC, et al.  Regulation of myelin structure and conduction velocity by perinodal astrocytes. Proc Natl Acad Sci USA  2018, 115, 11832–7. doi: https://doi.org/ 10.1073/pnas.1811013115 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 2. Dubey  M, Pascual-Garcia  M, Helmes  K, Wever  DD, Hamada  MS, Kushner  SA, et al.  Myelination synchronizes cortical oscillations by consolidating parvalbumin-mediated phasic inhibition. eLife  2022, 11. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 3. Arancibia-Cárcamo  IL, Ford  MC, Cossell  L, Ishida  K, Tohyama  K, Attwell  D.  Node of Ranvier length as a potential regulator of myelinated axon conduction speed. eLife  2017, 6, e23329. doi: https://doi.org/ 10.7554/eLife.23329 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 4. Yang  SM, Michel  K, Jokhi  V, Nedivi  E, Arlotta  P.  Neuron class-specific responses govern adaptive myelin remodeling in the neocortex. Science  2020, 370, eabd2109. doi: https://doi.org/ 10.1126/science.abd2109 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 5. Zhang  S-Z, Wang  Q-Q, Yang  Q-Q, Gu  H-Y, Yin  Y-Q, Li  Y-D, et al.  NG2 glia regulate brain innate immunity via TGF-β2/TGFBR2 axis. BMC Med  2019, 17, 204. doi: https://doi.org/ 10.1186/s12916-019-1439-x [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 6. Micheva  KD, Wolman  D, Mensh  BD, Pax  E, Buchanan  J, Smith  SJ, et al.  A large fraction of neocortical myelin ensheathes axons of local inhibitory neurons. eLife  2016, 5, e15784. doi: https://doi.org/ 10.7554/eLife.15784 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 7. Tomassy  GS, Berger  DR, Chen  H-H, Kasthuri  N, Hayworth  KJ, Vercelli  A, et al.  Distinct profiles of myelin distribution along single axons of pyramidal neurons in the neocortex. Science  2014, 344, 319–24. doi: https://doi.org/ 10.1126/science.1249766 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 8. Stassart  RM, Möbius  W, Nave  K-A, Edgar  JM.  The axon-myelin unit in development and degenerative disease. Front Neurosci  2018, 12, 467. doi: https://doi.org/ 10.3389/fnins.2018.00467 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 9. Duncan  GJ, Simkins  TJ, Emery  B.  Neuron-oligodendrocyte interactions in the structure and integrity of axons. Front Cell Dev Biol  2021, 9, 653101. doi: https://doi.org/ 10.3389/fcell.2021.653101 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 10. Nave  K-A.  Myelination and the trophic support of long axons. Nat Rev Neurosci  2010, 11, 275–83. doi: https://doi.org/ 10.1038/nrn2797 [DOI] [PubMed] [Google Scholar]
  • 11. Nave  K-A.  Myelination and support of axonal integrity by glia. Nature  2010, 468, 244–52. doi: https://doi.org/ 10.1038/nature09614 [DOI] [PubMed] [Google Scholar]
  • 12. Meyer  N, Richter  N, Fan  Z, Siemonsmeier  G, Pivneva  T, Jordan  P, et al.  Oligodendrocytes in the mouse corpus callosum maintain axonal function by delivery of glucose. Cell Rep  2018, 22, 2383–94. doi: https://doi.org/ 10.1016/j.celrep.2018.02.022 [DOI] [PubMed] [Google Scholar]
  • 13. Späte  E, Zhou  B, Sun  T, Kusch  K, Asadollahi  E, Siems  SB, et al.  Downregulated expression of lactate dehydrogenase in adult oligodendrocytes and its implication for the transfer of glycolysis products to axons. Glia  2024, 72, 1374–91. doi: https://doi.org/ 10.1002/glia.24533 [DOI] [PubMed] [Google Scholar]
  • 14. Brown  AM, Wender  R, Ransom  BR.  Metabolic substrates other than glucose support axon function in central white matter. J Neurosci Res  2001, 66, 839–43. doi: https://doi.org/ 10.1002/jnr.10081 [DOI] [PubMed] [Google Scholar]
  • 15. Trevisiol  A, Saab  AS, Winkler  U, Marx  G, Imamura  H, Möbius  W, et al.  Monitoring ATP dynamics in electrically active white matter tracts. eLife  2017, 6, e24241. doi: https://doi.org/ 10.7554/eLife.24241 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 16. Mukherjee  C, Kling  T, Russo  B, Miebach  K, Kess  E, Schifferer  M, et al.  Oligodendrocytes provide antioxidant defense function for neurons by secreting ferritin heavy chain. Cell Metab  2020, 32, 259–72.e10. doi: https://doi.org/ 10.1016/j.cmet.2020.05.019 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 17. Larson  VA, Mironova  Y, Vanderpool  KG, Waisman  A, Rash  JE, Agarwal  A, et al.  Oligodendrocytes control potassium accumulation in white matter and seizure susceptibility. eLife  2018, 7, e34829. doi: https://doi.org/ 10.7554/eLife.34829 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 18. Schirmer  L, Möbius  W, Zhao  C, Cruz-Herranz  A, Ben Haim  L, Cordano  C, et al.  Oligodendrocyte-encoded Kir4.1 function is required for axonal integrity. eLife  2018, 7, e36428. doi: https://doi.org/ 10.7554/eLife.36428 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 19. Looser  ZJ, Faik  Z, Ravotto  L, Zanker  HS, Jung  RB, Werner  HB, et al.  Oligodendrocyte-axon metabolic coupling is mediated by extracellular K+ and maintains axonal health. Nat Neurosci  2024, 27, 433–48. doi: https://doi.org/ 10.1038/s41593-023-01558-3 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 20. Monsma  PC, Li  Y, Fenn  JD, Jung  P, Brown  A.  Local regulation of neurofilament transport by myelinating cells. J Neurosci  2014, 34, 2979–88. doi: https://doi.org/ 10.1523/JNEUROSCI.4502-13.2014 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 21. Hoffman  PN, Griffin  JW, Gold  BG, Price  DL.  Slowing of neurofilament transport and the radial growth of developing nerve fibers. J Neurosci  1985, 5, 2920–9. doi: https://doi.org/ 10.1523/JNEUROSCI.05-11-02920.1985 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 22. Walker  CL, Uchida  A, Li  Y, Trivedi  N, Fenn  JD, Monsma  PC, et al.  Local acceleration of neurofilament transport at nodes of ranvier. J Neurosci  2019, 39, 663–77. doi: https://doi.org/ 10.1523/JNEUROSCI.2272-18.2018 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 23. Nixon  RA, Paskevich  PA, Sihag  RK, Thayer  CY.  Phosphorylation on carboxyl terminus domains of neurofilament proteins in retinal ganglion cell neurons in vivo: influences on regional neurofilament accumulation, interneurofilament spacing, and axon caliber. J Cell Biol  1994, 126, 1031–46. doi: https://doi.org/ 10.1083/jcb.126.4.1031 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 24. Sánchez  I, Hassinger  L, Sihag  RK, Cleveland  DW, Mohan  P, Nixon  RA.  Local control of neurofilament accumulation during radial growth of myelinating axons in vivo. Selective role of site-specific phosphorylation. J Cell Biol  2000, 151, 1013–24. doi: https://doi.org/ 10.1083/jcb.151.5.1013 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 25. Jia  Z, Li  Y.  A possible mechanism for neurofilament slowing down in myelinated axon: phosphorylation-induced variation of NF kinetics. PLoS One  2021, 16, e0247656. doi: https://doi.org/ 10.1371/journal.pone.0247656 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 26. Bin  JM, Emberley  K, Buscham  TJ, Eichel-Vogel  MA, Doan  RA, Steyer  AM, et al.  Developmental axon diameter growth of central nervous system axons does not depend on ensheathment or myelination by oligodendrocytes. bioRxiv  2025, 2025.01.10.632348. doi: https://doi.org/ 10.1101/2025.01.10.632348 [DOI] [Google Scholar]
  • 27. Bristow  EA, Griffiths  PG, Andrews  RM, Johnson  MA, Turnbull  DM.  The distribution of mitochondrial activity in relation to optic nerve structure. Arch Ophthalmol  2002, 120, 791–6. doi: https://doi.org/ 10.1001/archopht.120.6.791 [DOI] [PubMed] [Google Scholar]
  • 28. Licht-Mayer  S, Campbell  GR, Canizares  M, Mehta  AR, Gane  AB, McGill  K, et al.  Enhanced axonal response of mitochondria to demyelination offers neuroprotection: implications for multiple sclerosis. Acta Neuropathol  2020, 140, 143–67. doi: https://doi.org/ 10.1007/s00401-020-02179-x [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 29. Castelo-Branco  G, Kukanja  P, Guerreiro-Cacais  AO, Rubio Rodríguez-Kirby  LA.  Disease-associated oligodendroglia: a putative nexus in neurodegeneration. Trends Immunol  2024, 45, 750–9. doi: https://doi.org/ 10.1016/j.it.2024.08.003 [DOI] [PubMed] [Google Scholar]
  • 30. Bsibsi  M, Nomden  A, van Noort  JM, Baron  W.  Toll-like receptors 2 and 3 agonists differentially affect oligodendrocyte survival, differentiation, and myelin membrane formation. J Neurosci Res  2012, 90, 388–98. doi: https://doi.org/ 10.1002/jnr.22767 [DOI] [PubMed] [Google Scholar]
  • 31. Frederiksen  HR, Haukedal  H, Freude  K.  Cell type specific expression of Toll-like receptors in human brains and implications in Alzheimer’s disease. Biomed Res Int  2019, 2019, 7420189. doi: https://doi.org/ 10.1155/2019/7420189 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 32. Kirby  L, Castelo-Branco  G.  Crossing boundaries: interplay between the immune system and oligodendrocyte lineage cells. Semin Cell Dev Biol  2021, 116, 45–52. doi: https://doi.org/ 10.1016/j.semcdb.2020.10.013 [DOI] [PubMed] [Google Scholar]
  • 33. Abdelwahab  T, Stadler  D, Knöpper  K, Arampatzi  P, Saliba  A-E, Kastenmüller  W, et al.  Cytotoxic CNS-associated T cells drive axon degeneration by targeting perturbed oligodendrocytes in PLP1 mutant mice. iScience  2023, 26, 106698. doi: https://doi.org/ 10.1016/j.isci.2023.106698 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 34. Falcão  AM, van Bruggen  D, Marques  S, Meijer  M, Jäkel  S, Agirre  E, et al.  Disease-specific oligodendrocyte lineage cells arise in multiple sclerosis. Nat Med  2018, 24, 1837–44. doi: https://doi.org/ 10.1038/s41591-018-0236-y [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 35. Sarrazin  N, Chavret-Reculon  E, Bachelin  C, Felfli  M, Arab  R, Gilardeau  S, et al.  Failed remyelination of the nonhuman primate optic nerve leads to axon degeneration, retinal damages, and visual dysfunction. Proc Natl Acad Sci USA  2022, 119, e2115973119. doi: https://doi.org/ 10.1073/pnas.2115973119 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 36. Groh  J, Abdelwahab  T, Kattimani  Y, Hörner  M, Loserth  S, Gudi  V, et al.  Microglia-mediated demyelination protects against CD8+ T cell-driven axon degeneration in mice carrying PLP defects. Nat Commun  2023, 14, 6911. doi: https://doi.org/ 10.1038/s41467-023-42570-2 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 37. Nikić  I, Merkler  D, Sorbara  C, Brinkoetter  M, Kreutzfeldt  M, Bareyre  FM, et al.  A reversible form of axon damage in experimental autoimmune encephalomyelitis and multiple sclerosis. Nat Med  2011, 17, 495–9. doi: https://doi.org/ 10.1038/nm.2324 [DOI] [PubMed] [Google Scholar]
  • 38. Snaidero  N, Velte  C, Myllykoski  M, Raasakka  A, Ignatev  A, Werner  HB, et al.  Antagonistic functions of MBP and CNP establish cytosolic channels in CNS myelin. Cell Rep  2017, 18, 314–23. doi: https://doi.org/ 10.1016/j.celrep.2016.12.053 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 39. Chapple  KJ, Wirth  S, Chen  Y-H, Green  TRF, Gerwig  U, Aicher  ML, et al.  A myelinic channel system for motor-driven organelle transport. bioRxiv  2024. [Google Scholar]
  • 40. Fernández-Castañeda  A, Lu  P, Geraghty  AC, Song  E, Lee  M-H, Wood  J, et al.  Mild respiratory COVID can cause multi-lineage neural cell and myelin dysregulation. Cell  2022, 185, 2452–68.e16. doi: https://doi.org/ 10.1016/j.cell.2022.06.008 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 41. Harrington  EP, Catenacci  RB, Smith  MD, Heo  D, Miller  CE, Meyers  KR, et al.  MHC class I and MHC class II reporter mice enable analysis of immune oligodendroglia in mouse models of multiple sclerosis. eLife  2023, 12, e82938. doi: https://doi.org/ 10.7554/eLife.82938 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 42. Reith  W, LeibundGut-Landmann  S, Waldburger  J-M.  Regulation of MHC class II gene expression by the class II transactivator. Nat Rev Immunol  2005, 5, 793–806. doi: https://doi.org/ 10.1038/nri1708 [DOI] [PubMed] [Google Scholar]
  • 43. Fernández-Castañeda  A, Chappell  MS, Rosen  DA, Seki  SM, Beiter  RM, Johanson  DM, et al.  The active contribution of OPCs to neuroinflammation is mediated by LRP1. Acta Neuropathol  2020, 139, 365–82. doi: https://doi.org/ 10.1007/s00401-019-02073-1 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 44. Kirby  L, Jin  J, Cardona  JG, Smith  MD, Martin  KA, Wang  J, et al.  Oligodendrocyte precursor cells present antigen and are cytotoxic targets in inflammatory demyelination. Nat Commun  2019, 10, 3887. doi: https://doi.org/ 10.1038/s41467-019-11638-3 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 45. Wang  W-Y, Tan  M-S, Yu  J-T, Tan  L.  Role of pro-inflammatory cytokines released from microglia in Alzheimer’s disease. Ann Transl Med.  2015, 3, 136. doi: https://doi.org/ 10.3978/j.issn.2305-5839.2015.03.49 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 46. Green  TRF, Rowe  RK.  Quantifying microglial morphology: an insight into function. Clin Exp Immunol  2024, 216, 221–9. doi: https://doi.org/ 10.1093/cei/uxae023 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 47. Lombardi  M, Parolisi  R, Scaroni  F, Bonfanti  E, Gualerzi  A, Gabrielli  M, et al.  Detrimental and protective action of microglial extracellular vesicles on myelin lesions: astrocyte involvement in remyelination failure. Acta Neuropathol  2019, 138, 987–1012. doi: https://doi.org/ 10.1007/s00401-019-02049-1 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 48. McNamara  NB, Munro  DAD, Bestard-Cuche  N, Uyeda  A, Bogie  JFJ, Hoffmann  A, et al.  Microglia regulate central nervous system myelin growth and integrity. Nature  2023, 613, 120–9. doi: https://doi.org/ 10.1038/s41586-022-05534-y [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 49. Kalafatakis  I, Karagogeos  D.  Oligodendrocytes and microglia: key players in myelin development, damage and repair. Biomolecules  2021, 11, 1058. doi: https://doi.org/ 10.3390/biom11071058 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 50. Groh  J, Simons  M.  White matter aging and its impact on brain function. Neuron  2025, 113, 127–39. doi: https://doi.org/ 10.1016/j.neuron.2024.10.019 [DOI] [PubMed] [Google Scholar]
  • 51. Groh  J, Knöpper  K, Arampatzi  P, Yuan  X, Lößlein  L, Saliba  A-E, et al.  Accumulation of cytotoxic T cells in the aged CNS leads to axon degeneration and contributes to cognitive and motor decline. Nat Aging  2021, 1, 357–67. doi: https://doi.org/ 10.1038/s43587-021-00049-z [DOI] [PubMed] [Google Scholar]
  • 52. Kaya  T, Mattugini  N, Liu  L, Ji  H, Cantuti-Castelvetri  L, Wu  J, et al.  CD8+ T cells induce interferon-responsive oligodendrocytes and microglia in white matter aging. Nat Neurosci  2022, 25, 1446–57. doi: https://doi.org/ 10.1038/s41593-022-01183-6 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 53. Depp  C, Sun  T, Sasmita  AO, Spieth  L, Berghoff  SA, Nazarenko  T, et al.  Myelin dysfunction drives amyloid-β deposition in models of Alzheimer’s disease. Nature  2023, 618, 349–57. doi: https://doi.org/ 10.1038/s41586-023-06120-6 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 54. Tatar  CL, Appikatla  S, Bessert  DA, Paintlia  AS, Singh  I, Skoff  RP.  Increased Plp1 gene expression leads to massive microglial cell activation and inflammation throughout the brain. ASN Neuro  2010, 2, e00043. doi: https://doi.org/ 10.1042/AN20100016 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 55. Edgar  JM, McCulloch  MC, Montague  P, Brown  AM, Thilemann  S, Pratola  L, et al.  Demyelination and axonal preservation in a transgenic mouse model of Pelizaeus-Merzbacher disease. EMBO Mol Med  2010, 2, 42–50. doi: https://doi.org/ 10.1002/emmm.200900057 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 56. Ip  CW, Kroner  A, Groh  J, Huber  M, Klein  D, Spahn  I, et al.  Neuroinflammation by cytotoxic T-lymphocytes impairs retrograde axonal transport in an oligodendrocyte mutant mouse. PLoS One  2012, 7, e42554. doi: https://doi.org/ 10.1371/journal.pone.0042554 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 57. Ip  CW, Kroner  A, Bendszus  M, Leder  C, Kobsar  I, Fischer  S, et al.  Immune cells contribute to myelin degeneration and axonopathic changes in mice overexpressing proteolipid protein in oligodendrocytes. J Neurosci  2006, 26, 8206–16. doi: https://doi.org/ 10.1523/JNEUROSCI.1921-06.2006 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 58. Gruenenfelder  FI, McLaughlin  M, Griffiths  IR, Garbern  J, Thomson  G, Kuzman  P, et al.  Neural stem cells restore myelin in a demyelinating model of Pelizaeus-Merzbacher disease. Brain  2020, 143, 1383–99. doi: https://doi.org/ 10.1093/brain/awaa080 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 59. Kroner  A, Ip  CW, Thalhammer  J, Nave  K-A, Martini  R.  Ectopic T-cell specificity and absence of perforin and granzyme B alleviate neural damage in oligodendrocyte mutant mice. Am J Pathol  2010, 176, 549–55. doi: https://doi.org/ 10.2353/ajpath.2010.090722 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 60. Schneider  A, Montague  P, Griffiths  I, Fanarraga  M, Kennedy  P, Brophy  P, et al.  Uncoupling of hypomyelination and glial cell death by a mutation in the proteolipid protein gene. Nature  1992, 358, 758–61. doi: https://doi.org/ 10.1038/358758a0 [DOI] [PubMed] [Google Scholar]
  • 61. Stumpf  SK, Berghoff  SA, Trevisiol  A, Spieth  L, Düking  T, Schneider  LV, et al.  Ketogenic diet ameliorates axonal defects and promotes myelination in Pelizaeus-Merzbacher disease. Acta Neuropathol  2019, 138, 147–61. doi: https://doi.org/ 10.1007/s00401-019-01985-2 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 62. Ayrignac  X, Carra-Dallière  C, Marelli  C, Taïeb  G, Labauge  P.  Adult-onset genetic central nervous system disorders masquerading as acquired neuroinflammatory disorders: a review. JAMA Neurol  2022, 79, 1069–78. doi: https://doi.org/ 10.1001/jamaneurol.2022.2141 [DOI] [PubMed] [Google Scholar]
  • 63. Bergner  CG, van der Meer  F, Winkler  A, Wrzos  C, Türkmen  M, Valizada  E, et al.  Microglia damage precedes major myelin breakdown in X-linked adrenoleukodystrophy and metachromatic leukodystrophy. Glia  2019, 67, 1196–209. doi: https://doi.org/ 10.1002/glia.23598 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 64. Papapetropoulos  S, Pontius  A, Finger  E, Karrenbauer  V, Lynch  DS, Brennan  M, et al.  Adult-onset leukoencephalopathy with axonal spheroids and pigmented glia: review of clinical manifestations as foundations for therapeutic development. Front Neurol  2021, 12, 788168. doi: https://doi.org/ 10.3389/fneur.2021.788168 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 65. Fazakerley  JK, Walker  R.  Virus demyelination. J Neurovirol  2003, 9, 148–64. doi: https://doi.org/ 10.1080/13550280390194046 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 66. Ferenczy  MW, Marshall  LJ, Nelson  CDS, Atwood  WJ, Nath  A, Khalili  K, et al.  Molecular biology, epidemiology, and pathogenesis of progressive multifocal leukoencephalopathy, the JC virus-induced demyelinating disease of the human brain. Clin Microbiol Rev  2012, 25, 471–506. doi: https://doi.org/ 10.1128/CMR.05031-11 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 67. O’Hara  BA, Morris-Love  J, Gee  GV, Haley  SA, Atwood  WJ.  JC Virus infected choroid plexus epithelial cells produce extracellular vesicles that infect glial cells independently of the virus attachment receptor. PLoS Pathog  2020, 16, e1008371. doi: https://doi.org/ 10.1371/journal.ppat.1008371 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 68. Langer-Gould  A, Atlas  SW, Green  AJ, Bollen  AW, Pelletier  D.  Progressive multifocal leukoencephalopathy in a patient treated with natalizumab. N Engl J Med  2005, 353, 375–81. doi: https://doi.org/ 10.1056/NEJMoa051847 [DOI] [PubMed] [Google Scholar]
  • 69. Ono  D, Shishido-Hara  Y, Mizutani  S, Mori  Y, Ichinose  K, Watanabe  M, et al.  Development of demyelinating lesions in progressive multifocal leukoencephalopathy (PML): comparison of magnetic resonance images and neuropathology of post-mortem brain. Neuropathology.  2019, 39, 294–306. doi: https://doi.org/ 10.1111/neup.12562 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 70. Dalla Costa  G, Leocani  L, Pisa  M, Croese  T, Martinelli  V, Moiola  L, et al.  Neuroaxonal damage in natalizumab-treated MS patients: the role of JCV antibody titres. Mult Scler  2024, 30, 1561–5. doi: https://doi.org/ 10.1177/13524585241260977 [DOI] [PubMed] [Google Scholar]
  • 71. Cumberworth  SL, Barrie  JA, Cunningham  ME, de Figueiredo  DPG, Schultz  V, Wilder-Smith  AJ, et al.  Zika virus tropism and interactions in myelinating neural cell cultures: CNS cells and myelin are preferentially affected. Acta Neuropathol Commun  2017, 5, 50. doi: https://doi.org/ 10.1186/s40478-017-0450-8 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 72. Schultz  V, Barrie  JA, Donald  CL, Crawford  CL, Mullin  M, Anderson  TJ, et al.  Oligodendrocytes are susceptible to Zika virus infection in a mouse model of perinatal exposure: implications for CNS complications. Glia  2021, 69, 2023–36. doi: https://doi.org/ 10.1002/glia.24010 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 73. Roussarie  J-P, Ruffié  C, Edgar  JM, Griffiths  I, Brahic  M.  Axon myelin transfer of a non-enveloped virus. PLoS One  2007, 2, e1331. doi: https://doi.org/ 10.1371/journal.pone.0001331 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 74. Dal Canto  MC, Melvold  RW, Kim  BS, Miller  SD.  Two models of multiple sclerosis: experimental allergic encephalomyelitis (EAE) and Theiler’s murine encephalomyelitis virus (TMEV) infection. A pathological and immunological comparison. Microsc Res Tech  1995, 32, 215–29. doi: https://doi.org/ 10.1002/jemt.1070320305 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 75. Fragkoudis  R, Tamberg  N, Siu  R, Kiiver  K, Kohl  A, Merits  A, et al.  Neurons and oligodendrocytes in the mouse brain differ in their ability to replicate Semliki Forest virus. J Neurovirol  2009, 15, 57–70. doi: https://doi.org/ 10.1080/13550280802482583 [DOI] [PubMed] [Google Scholar]
  • 76. Brahic  M, Roussarie  J-P, Roussarie  J-P.  Axon-myelin interactions during a viral infection of the central nervous system. PLoS Pathog  2009, 5, e1000519. doi: https://doi.org/ 10.1371/journal.ppat.1000519 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 77. Roussarie  J-P, Ruffié  C, Brahic  M.  The role of myelin in Theiler’s virus persistence in the central nervous system. PLoS Pathog  2007, 3, e23. doi: https://doi.org/ 10.1371/journal.ppat.0030023 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 78. Wu  GF, Dandekar  AA, Pewe  L, Perlman  S.  CD4 and CD8 T cells have redundant but not identical roles in virus-induced demyelination. J Immunol  2000, 165, 2278–86. doi: https://doi.org/ 10.4049/jimmunol.165.4.2278 [DOI] [PubMed] [Google Scholar]
  • 79. Miller  SD, Vanderlugt  CL, Begolka  WS, Pao  W, Yauch  RL, Neville  KL, et al.  Persistent infection with Theiler’s virus leads to CNS autoimmunity via epitope spreading. Nat Med  1997, 3, 1133–6. doi: https://doi.org/ 10.1038/nm1097-1133 [DOI] [PubMed] [Google Scholar]
  • 80. Wannemacher  R, Reiß  A, Rohn  K, Lühder  F, Flügel  A, Baumgärtner  W, et al.  Ovalbumin-specific CD4+ and CD8+ T cells contribute to different susceptibility for Theiler’s murine encephalomyelitis virus persistence. Front Immunol  2023, 14, 1194842. doi: https://doi.org/ 10.3389/fimmu.2023.1194842 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 81. Safavi  F, Feliberti  JP, Raine  CS, Mokhtarian  F.  Role of γδ T cells in antibody production and recovery from SFV demyelinating disease. J Neuroimmunol  2011, 235, 18–26. doi: https://doi.org/ 10.1016/j.jneuroim.2011.02.013 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 82. Mokhtarian  F, Huan  C, Roman  C, Raine  CS.  Semliki forest virus-induced demyelination and remyelination--involvement of B cells and anti-myelin antibodies. J Neuroimmunol  2003, 137, 19–31. doi: https://doi.org/ 10.1016/s0165-5728(03)00039-0 [DOI] [PubMed] [Google Scholar]
  • 83. Filippi  M, Bar-Or  A, Piehl  F, Preziosa  P, Solari  A, Vukusic  S, et al.  Multiple sclerosis. Nat Rev Dis Primers  2018, 4, 43. doi: https://doi.org/ 10.1038/s41572-018-0041-4 [DOI] [PubMed] [Google Scholar]
  • 84. Garton  T, Gadani  SP, Gill  AJ, Calabresi  PA.  Neurodegeneration and demyelination in multiple sclerosis. Neuron  2024, 112, 3231–51. doi: https://doi.org/ 10.1016/j.neuron.2024.05.025 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 85. Reich  DS, Lucchinetti  CF, Calabresi  PA.  Multiple sclerosis. N Engl J Med  2018, 378, 169–80. doi: https://doi.org/ 10.1056/NEJMra1401483 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 86. Compston  A, Coles  A.  Multiple sclerosis. Lancet  2008, 372, 1502–17. doi: https://doi.org/ 10.1016/S0140-6736(08)61620-7 [DOI] [PubMed] [Google Scholar]
  • 87. Bjornevik  K, Münz  C, Cohen  JI, Ascherio  A.  Epstein-Barr virus as a leading cause of multiple sclerosis: mechanisms and implications. Nat Rev Neurol  2023, 19, 160–71. doi: https://doi.org/ 10.1038/s41582-023-00775-5 [DOI] [PubMed] [Google Scholar]
  • 88. Cortese  M, Leng  Y, Bjornevik  K, Mitchell  M, Healy  BC, Mina  MJ, et al.  Serologic response to the Epstein-Barr virus peptidome and the risk for multiple sclerosis. JAMA Neurol  2024, 81, 515–24. doi: https://doi.org/ 10.1001/jamaneurol.2024.0272 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 89. Lanz  TV, Brewer  RC, Ho  PP, Moon  J-S, Jude  KM, Fernandez  D, et al.  Clonally expanded B cells in multiple sclerosis bind EBV EBNA1 and GlialCAM. Nature  2022, 603, 321–7. doi: https://doi.org/ 10.1038/s41586-022-04432-7 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 90. Stys  PK, Zamponi  GW, van Minnen  J, Geurts  JJG.  Will the real multiple sclerosis please stand up? Nat Rev Neurosci  2012, 13, 507–14. doi: https://doi.org/ 10.1038/nrn3275 [DOI] [PubMed] [Google Scholar]
  • 91. Luchicchi  A, Preziosa  P’, t Hart  B.  Editorial: “Inside-Out” vs “Outside-In” paradigms in multiple sclerosis etiopathogenesis. Front Cell Neurosci  2021, 15, 666529. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 92. Lucchinetti  CF, Popescu  BFG, Bunyan  RF, Moll  NM, Roemer  SF, Lassmann  H, et al.  Inflammatory cortical demyelination in early multiple sclerosis. N Engl J Med  2011, 365, 2188–97. doi: https://doi.org/ 10.1056/NEJMoa1100648 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 93. Patani  R, Balaratnam  M, Vora  A, Reynolds  R.  Remyelination can be extensive in multiple sclerosis despite a long disease course. Neuropathol Appl Neurobiol  2007, 33, 277–87. doi: https://doi.org/ 10.1111/j.1365-2990.2007.00805.x [DOI] [PubMed] [Google Scholar]
  • 94. Franklin  RJM, Frisén  J, Lyons  DA.  Revisiting remyelination: towards a consensus on the regeneration of CNS myelin. Semin Cell Dev Biol  2021, 116, 3–9. doi: https://doi.org/ 10.1016/j.semcdb.2020.09.009 [DOI] [PubMed] [Google Scholar]
  • 95. Hill  MFE, Cunniffe  NG, Franklin  RJM.  Seeing is believing: identifying remyelination in the central nervous system. Curr Opin Pharmacol  2022, 66, 102269. doi: https://doi.org/ 10.1016/j.coph.2022.102269 [DOI] [PubMed] [Google Scholar]
  • 96. Kuhlmann  T, Ludwin  S, Prat  A, Antel  J, Brück  W, Lassmann  H.  An updated histological classification system for multiple sclerosis lesions. Acta Neuropathol  2017, 133, 13–24. doi: https://doi.org/ 10.1007/s00401-016-1653-y [DOI] [PubMed] [Google Scholar]
  • 97. Franklin  RJM, Ffrench-Constant  C.  Regenerating CNS myelin - from mechanisms to experimental medicines. Nat Rev Neurosci  2017, 18, 753–69. doi: https://doi.org/ 10.1038/nrn.2017.136 [DOI] [PubMed] [Google Scholar]
  • 98. Neumann  H, Kotter  MR, Franklin  RJM.  Debris clearance by microglia: an essential link between degeneration and regeneration. Brain  2009, 132, 288–95. doi: https://doi.org/ 10.1093/brain/awn109 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 99. Miron  VE, Boyd  A, Zhao  J-W, Yuen  TJ, Ruckh  JM, Shadrach  JL, et al.  M2 microglia and macrophages drive oligodendrocyte differentiation during CNS remyelination. Nat Neurosci  2013, 16, 1211–8. doi: https://doi.org/ 10.1038/nn.3469 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 100. Goebbels  S, Wieser  GL, Pieper  A, Spitzer  S, Weege  B, Yan  K, et al.  A neuronal PI(3,4,5)P3-dependent program of oligodendrocyte precursor recruitment and myelination. Nat Neurosci  2017, 20, 10–5. doi: https://doi.org/ 10.1038/nn.4425 [DOI] [PubMed] [Google Scholar]
  • 101. Berghoff  SA, Spieth  L, Sun  T, Hosang  L, Schlaphoff  L, Depp  C, et al.  Microglia facilitate repair of demyelinated lesions via post-squalene sterol synthesis. Nat Neurosci  2021, 24, 47–60. doi: https://doi.org/ 10.1038/s41593-020-00757-6 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 102. de Almeida  MMA, Watson  AES, Bibi  S, Dittmann  NL, Goodkey  K, Sharafodinzadeh  P, et al.  Fractalkine enhances oligodendrocyte regeneration and remyelination in a demyelination mouse model. Stem Cell Rep  2023, 18, 519–33. doi: https://doi.org/ 10.1016/j.stemcr.2022.12.001 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 103. Guerrero  BL, Sicotte  NL.  Microglia in multiple sclerosis: friend or foe? Front Immunol  2020, 11, 374. doi: https://doi.org/ 10.3389/fimmu.2020.00374 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 104. Lloyd  AF, Miron  VE.  The pro-remyelination properties of microglia in the central nervous system. Nat Rev Neurol  2019, 15, 447–58. doi: https://doi.org/ 10.1038/s41582-019-0184-2 [DOI] [PubMed] [Google Scholar]
  • 105. Ferguson  B, Matyszak  MK, Esiri  MM, Perry  VH.  Axonal damage in acute multiple sclerosis lesions. Brain  1997, 120 ( Pt 3), 393–9. doi: https://doi.org/ 10.1093/brain/120.3.393 [DOI] [PubMed] [Google Scholar]
  • 106. Trapp  BD, Peterson  J, Ransohoff  RM, Rudick  R, Mörk  S, Bö  L.  Axonal transection in the lesions of multiple sclerosis. N Engl J Med  1998, 338, 278–85. doi: https://doi.org/ 10.1056/NEJM199801293380502 [DOI] [PubMed] [Google Scholar]
  • 107. Trapp  BD, Stys  PK.  Virtual hypoxia and chronic necrosis of demyelinated axons in multiple sclerosis. Lancet Neurol  2009, 8, 280–91. doi: https://doi.org/ 10.1016/S1474-4422(09)70043-2 [DOI] [PubMed] [Google Scholar]
  • 108. De Stefano  N, Narayanan  S, Matthews  PM, Francis  GS, Antel  JP, Arnold  DL.  In vivo evidence for axonal dysfunction remote from focal cerebral demyelination of the type seen in multiple sclerosis. Brain  1999, 122 ( Pt 10), 1933–9. doi: https://doi.org/ 10.1093/brain/122.10.1933 [DOI] [PubMed] [Google Scholar]
  • 109. Edgar  JM, McLaughlin  M, Yool  D, Zhang  S-C, Fowler  JH, Montague  P, et al.  Oligodendroglial modulation of fast axonal transport in a mouse model of hereditary spastic paraplegia. J Cell Biol  2004, 166, 121–31. doi: https://doi.org/ 10.1083/jcb.200312012 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 110. Edgar  JM, McLaughlin  M, Werner  HB, McCulloch  MC, Barrie  JA, Brown  A, et al.  Early ultrastructural defects of axons and axon-glia junctions in mice lacking expression of Cnp1. Glia  2009, 57, 1815–24. doi: https://doi.org/ 10.1002/glia.20893 [DOI] [PubMed] [Google Scholar]
  • 111. Griffiths  I, Klugmann  M, Anderson  T, Yool  D, Thomson  C, Schwab  MH, et al.  Axonal swellings and degeneration in mice lacking the major proteolipid of myelin. Science  1998, 280, 1610–3. doi: https://doi.org/ 10.1126/science.280.5369.1610 [DOI] [PubMed] [Google Scholar]
  • 112. Lappe-Siefke  C, Goebbels  S, Gravel  M, Nicksch  E, Lee  J, Braun  PE, et al.  Disruption of Cnp1 uncouples oligodendroglial functions in axonal support and myelination. Nat Genet  2003, 33, 366–74. doi: https://doi.org/ 10.1038/ng1095 [DOI] [PubMed] [Google Scholar]
  • 113. Yin  X, Crawford  TO, Griffin  JW, Tu  P, Lee  VM, Li  C, et al.  Myelin-associated glycoprotein is a myelin signal that modulates the caliber of myelinated axons. J Neurosci  1998, 18, 1953–62. doi: https://doi.org/ 10.1523/JNEUROSCI.18-06-01953.1998 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 114. Schäffner  E, Bosch-Queralt  M, Edgar  JM, Lehning  M, Strauß  J, Fleischer  N, et al.  Myelin insulation as a risk factor for axonal degeneration in autoimmune demyelinating disease. Nat Neurosci  2023, 26, 1218–28. doi: https://doi.org/ 10.1038/s41593-023-01366-9 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 115. Bergner  CG, Genc  N, Hametner  S, Franz  J, van der Meer  F, Mitkovski  M, et al.  Concurrent axon and myelin destruction differentiates X-linked adrenoleukodystrophy from multiple sclerosis. Glia  2021, 69, 2362–77. doi: https://doi.org/ 10.1002/glia.24042 [DOI] [PubMed] [Google Scholar]
  • 116. Smith  KJ, Kapoor  R, Hall  SM, Davies  M.  Electrically active axons degenerate when exposed to nitric oxide. Ann Neurol  2001, 49, 470–6. [PubMed] [Google Scholar]
  • 117. Schäffner  E, Edgar  JM, Lehning  M, Strauß  J, Bosch-Queralt  M, Wieghofer  P, et al.  Myelin insulation as a risk factor for axonal degeneration in autoimmune demyelinating disease. bioRxiv  2021. [DOI] [PMC free article] [PubMed] [Google Scholar]

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