Abstract
Myelin Protein Zero (MPZ/P0) is the most abundant glycoprotein of peripheral nerve myelin. P0 is synthesized by myelinating Schwann cells, processed in the endoplasmic reticulum (ER) and delivered to myelin via the secretory pathway. The mutant P0S63del (deletion of serine 63 in the extracellular domain of P0), that causes Charcot-Marie-Tooth type 1B (CMT1B) neuropathy in humans and a similar demyelinating neuropathy in transgenic mice, is instead retained the ER where it activates an unfolded protein response. Under ER-stress conditions, protein kinase R-like endoplasmic reticulum kinase (PERK) phosphorylates eukaryotic initiation factor 2α (eIF2α) to attenuate global translation, thus reducing the misfolded protein overload in the ER. Genetic and pharmacological inactivation of Gadd34 (damage-inducible protein 34), a subunit of the PP1 phosphatase complex that promotes the dephosphorylation of eIF2α, prolonged eIF2α phosphorylation and improved motor, neurophysiological, and morphologic deficits in S63del mice. However, PERK ablation in S63del Schwann cells ameliorated, rather than worsened, S63del neuropathy despite reduced levels of phosphorylated eIF2α. These contradictory findings prompted us to genetically explore the role of eIF2α phosphorylation in P0S63del-CMT1B neuropathy through the generation of mice in which eIF2α cannot be phosphorylated specifically in Schwann cells. Morphologic and electrophysiological analysis of male and female S63del mice showed a worsening of the neuropathy in the absence of eIF2α phosphorylation. However, we did not detect significant changes in ER stress levels, but rather a dramatic increase of the MEK/ERK/c-Jun pathway accompanied by a reduction in expression of myelin genes and a delay in Schwann cell differentiation. Our results support the hypothesis that eIF2α phosphorylation is protective in CMT1B and unveil a possible cross talk between eIF2α and the MEK/ERK pathway in neuropathic nerves.
SIGNIFICANCE STATEMENT In the P0S63del (deletion of serine 63 in the extracellular domain of P0) mouse model of Charcot-Marie-Tooth type 1B (CMT1B), the genetic and pharmacological inhibition of Gadd34 (damage-inducible protein 34) prolonged eukaryotic initiation factor 2α (eIF2α) phosphorylation, leading to a proteostatic rebalance that significantly ameliorated the neuropathy. Yet, ablation of protein kinase R-like endoplasmic reticulum kinase (PERK) also ameliorated the S63del neuropathy, despite reduced levels of eIF2α phosphorylation (P-eIF2α). In this study, we provide genetic evidence that eIF2α phosphorylation has a protective role in CMT1B Schwann cells by limiting ERK/c-Jun hyperactivation. Our data support the targeting of the P-eIF2α/Gadd34 complex as a therapeutic avenue in CMT1B and also suggest that PERK may hamper myelination via mechanisms outside its role in the unfolded protein response.
Introduction
Myelin Protein Zero (MPZ/P0) is a transmembrane glycoprotein specifically expressed by myelinating Schwann cells in the peripheral nervous system (PNS), necessary for the adhesion and compaction of adjacent myelin wraps (Filbin et al., 1990; Giese et al., 1992; Shapiro et al., 1996). To date, >200 different mutations in P0 that cause the hereditary neuropathy Charcot-Marie-Tooth 1B (CMT1B) have been identified (Sanmaneechai et al., 2015; Callegari et al., 2019). The vast majority are dominantly inherited and act via gain-of-function mechanisms (Wrabetz et al., 2006). Protein misfolding, accumulation in the endoplasmic reticulum (ER) and activation of the unfolded protein response (UPR) is emerging as a relatively common pathomechanism for P0 mutations (Bai et al., 2018). One such example is the deletion of serine 63 in the extracellular domain of P0 (P0S63del), which causes a CMT1B neuropathy characterized by hypomyelination, progressive demyelination, and onion bulb formation in both humans and transgenic mice (Wrabetz et al., 2006; Pennuto et al., 2008; Miller et al., 2012).
The mammalian UPR is characterized by the activation of the following three distinct ER resident sensors: protein kinase RNA-like ER kinase (PERK) activating transcription factor 6 (ATF6) and inositol-requiring protein 1α (Ire1α), which together coordinate translational and transcriptional responses aimed at restoring cellular homeostasis (Ron and Walter, 2007). ATF6 induces the expression of ER-resident chaperones to increase the folding capacity of the cell (Haze et al., 1999; Wu et al., 2007; Yamamoto et al., 2007). IRE1α catalyzes the unconventional splicing of the mRNA for the transcription factor X-box binding protein 1 (Xbp1) to generate the active Xbp1s (Lee et al., 2002), which in turn upregulates the expression of genes involved in ER biogenesis and ER-associated degradation (ERAD; Yoshida et al., 2001; Lee et al., 2003; Acosta-Alvear et al., 2007). Finally, PERK triggers the phosphorylation of the α subunit of eukaryotic initiation factor 2 (P-eIF2α) at Ser51 to attenuate general protein synthesis (Harding et al., 2000a; Clemens, 2001). At the same time, the phosphorylation of eIF2α is also responsible for the selective translation of a series of mRNA-containing small upstream open reading frames (Harding et al., 2000b), including the mRNA for ATF4 (Lu et al., 2004), which is proposed to induce prosurvival genes involved in the antioxidant stress response, amino acid synthesis, and protein folding (Scheuner et al., 2001; Harding et al., 2003). However, in conditions of chronic stress ATF4 may lead to cell death via the activation of the proapoptotic factor CHOP (CCAAT-enhancer-binding protein homologous protein)/Gadd153 (damage-inducible protein 153) and of genes involved in protein synthesis (Novoa et al., 2001; Han et al., 2013).
In P0S63del-CMT1B mice, genetic ablation of CHOP ameliorated motor capacity and partially reduced demyelination (Pennuto et al., 2008). We identified growth arrest and DNA damage-inducible protein 34 (Gadd34) as the maladaptive effector of Chop (D'Antonio et al., 2013). Gadd34, also known as PPP1R15a, is a regulatory subunit of protein phosphatase 1 (PP1) holophosphatase that dephosphorylates eIF2α to reactivate protein translation (Novoa et al., 2001). Genetic and pharmacological inhibition of Gadd34 prolonged eIF2α phosphorylation, largely ameliorating S63del neuropathy (D'Antonio et al., 2013; Das et al., 2015). Surprisingly, PERK haploinsufficiency or the Schwann cell-specific ablation of PERK ameliorated, rather than aggravated, the S63del neuropathic phenotype, despite reduced levels of P-eIF2α (Musner et al., 2016; Sidoli et al., 2016)
We thus decided to directly investigate the role of eIF2α phosphorylation in the P0S63del-CMT1B neuropathy. In this study, we show that the phosphorylation of eIF2α in S63del Schwann cells is protective. Surprisingly, however, lack of eIF2α phosphorylation did not significantly alter UPR or oxidative stress levels, but dramatically delayed Schwann cell differentiation and myelination, possibly acting via the MEK/ERK/c-Jun pathway. These findings support the prolonging of eIF2α phosphorylation as a valid target for therapy in ER stress-related neuropathies and uncover a previously unrecognized cross talk between the UPR and the MEK/ERK pathway.
Materials and Methods
Transgenic mice
All experiments involving animals were performed in accord with experimental protocols approved by the San Raffaele Scientific Institute Animal Care and Use Committee. P0Cre and S63del mice with relative genotyping procedures have been previously described (Feltri et al., 1999; Wrabetz et al., 2006). Mice carrying a eIF2α Ser51Ala mutation (herein S/A if heterozygous and A/A if homozygous) and a loxP-flanked wild-type (WT) eIF2α transgene (fTg) in all tissues (S/A or A/A//fTg mice), were previously described (Scheuner et al., 2005; Back et al., 2009). We first crossed A/A//fTg transgenic mice with P0Cre mice to generate S/A//P0Cre mice (eIF2αSC-SA mice). In parallel, we crossed the A/A//fTg with the neuropathic S63del mice to generate S/A//fTg//S63del mice. We then crossed eIF2αSC-SA mice with S/A//fTg//S63del mice to obtain the experimental mice in which eIF2α cannot be phosphorylated in Schwann cells (in either wild-type eIF2αSC-AA or neuropathic S63del/eIF2αSC-AA background; Fig. 1). In all experiments, A/A//fTg [herein control (CTR)] and A/A//fTg//S63del (herein S63del) littermates were used as controls since morphologically indistinguishable from original WT and S63del mice, respectively (data not shown). S63del mice were maintained on the FVB/N background, whereas both P0Cre and A/A//fTg were on the C57BL/6 genetic background. The analysis of all four experimental genotypes was performed in F1 hybrid background FVB//C57BL6. Mice of either sex were used throughout the study.
Morphologic analysis
Transgenic mice were killed at the indicated time points and sciatic nerves were dissected. Semi-thin section and electron microscope analyses of sciatic nerves, were performed as described (Ferri et al., 2018). The number of amyelinated or demyelinated axons and onion bulbs were counted blind to genotype from postnatal day 21 (P21) or 5-month-old sciatic nerve semi-thin sections (0.5–1 μm thick) stained with toluidine blue, in images taken with a 100× objective. We analyzed 1000–1800 fibers from a total of 10–20 fields/nerve (five nerves). Ultrathin sections (90 nm thick) from P10 and P21 transgenic and control sciatic nerves were cut using an ultracut ultramicrotome, stained with uranyl acetate and lead citrate, and were examined by electron microscopy (EM; Leo 912 Omega). G-ratio analysis (axonal diameter/fiber diameter) and the size distribution of myelinated fibers (based on axon diameter) were measured on digitalized nonoverlapping electron micrograph images. Twenty to 25 microscopic fields, randomly chosen, from nerves of three to four animals per genotype were analyzed.
TaqMan quantitative PCR analysis
Sciatic nerves from transgenic mice were frozen in liquid nitrogen after dissection. Total RNA from at least three sciatic nerves for each genotype was extracted using TRIzol (Roche Diagnostic) and reverse transcription was performed as described previously (D'Antonio et al., 2006). Quantitative RT-PCR was performed according to manufacturer instructions (TaqMan, Thermo Fisher Scientific) on an ABI PRISM 7700 sequence detection system (Thermo Fisher Scientific). Normalization was performed using 18S rRNA as reference gene. Target and reference gene PCR amplification was performed in separate tubes with Assay on Demand (Thermo Fisher Scientific): 18S assay Hs99999901_s1; MPZ assay Mm00485141_m1; PMP22 assay Mm01333393_m1; myelin basic protein (MBP) assay Rn00690431_m1; Ddit3/Chop, Mm00492097_m1; Xbp-1u assay, Mm00457357_m1; Xbp-1s assay, Mm03464496_m1; Hspa5/BiP (Ig binding protein) assay, Mm00517691_m1; Egr2/Krox20 assay, ATF4 assay, Mm00515324_m1; Id2 assay, Mm00711781_m1; Sox2 assay, Mm00488369_m1; JUN assay, Mm00495062_m1; POU3F1/Oct6 assay, Mm00843534_m1; Hmox1 assay, Mm00516005_m1; Gpx1 assay, Mm00656767_g1; and Gss assay, Mm00515065_m1.
Protein extraction and Western blotting
Sciatic nerves from transgenic mice, at the indicated time points, were dissected and frozen in liquid nitrogen. Protein extraction and protein content analysis were previously described (Wrabetz et al., 2006). The following rabbit polyclonal antibodies were used: Grp78/Bip (1:1000; catalog #NB300-520, Novus Biologicals; RRID:AB_10011084); phospho-Akt (Ser473; 1:1000; catalog #9271, Cell Signaling Technology; RRID:AB_329825) and AKT (1:1000; catalog #9272, Cell Signaling Technology; RRID:AB_329827); and phospho-ERK1/2 (Thr202/Tyr204) and ERK1 (1:1000; catalog #9101, Cell Signaling Technology; RRID:AB_331646), and ERK2 (1:1000; catalog #9102, Cell Signaling Technology; RRID:AB_330744, respectively). Rabbit monoclonal antibodies recognized P-eIF2α (Ser51; D9G8) XPTM (1:2000; catalog #3398, Cell Signaling Technology; RRID:AB_2096481; and eIF2α (D7D3) XPTM (catalog #5324, Cell Signaling Technology; RRID:AB_10692650); and c-Jun (1:1000; catalog #9165, Cell Signaling Technology; RRID:AB_2130165). Mouse monoclonal antibody recognized ATF4/Creb2 (B-3; 1:100, Santa Cruz Biotechnology, sc-390063), EGFP (1:2000, Abcam, ab127417, RRID:AB_11129790) and β-tubulin (1:2000; Sigma, T4026, RRID:AB_477577). Peroxidase-conjugated secondary antibodies anti-mouse horseradish peroxidase (HRP; catalog # P0260, DAKO; RRID:AB_2636929) and anti-rabbit HRP (catalog #P0448, DAKO; RRID:AB_2617138) were diluted 1:3000, and results were visualized using GE Healthcare ECL or ECL Prime 225 reagent (GE Healthcare) for high-sensitivity chemiluminescent protein detection with UVItec gel analysis systems. Densitometric quantification was performed with ImageJ.
Detection of oxidized proteins
Protein concentration of sciatic nerve extracts was measured using the BCA Protein Assay Kit (Thermo Fisher Scientific). A reducing agent (1%, 2-mercaptoethanol) was added to the extracts to prevent the oxidation of proteins that may occur after cell lysis. A total amount of 15 μg of protein per sample, was derivatized with a twofold volume of 2,4-dinitrophenylhydrazine (DNPH) solution or derivatization control solution (Oxyblot Protein Oxidation Detection Kit, EMD Millipore) as described in the protocol. Proteins were separated by SDS-PAGE. The gels containing DNPH-derivatized proteins were transferred to a nitrocellulose membrane (250 mA for 2 h) and subsequently blocked for 1 h with 1% BSA in PBS-T buffer (PBS with 0.5% Tween-20). Oxyblots were incubated with a rabbit anti-dinitrophenyl primary antibody (1:150) overnight at 4°C Membranes were washed three times with PBS-T buffer and incubated for 1 h with an anti-rabbit IgG2a HRP-conjugated secondary antibody diluted 1:300 (both 1° and 2° antibodies from Oxyblot Protein Oxidation Detection Kit, EMD Millipore) and developed using the ECL method, as described above.
Immunofluorescence
Sciatic nerves from P21 transgenic mice were dissected, embedded in optimal cutting temperature compound, and frozen in liquid nitrogen. Eight-micrometer-thick transverse sections (model CM1850_UV Cryostat, Leica) were fixed for 10 min in 4% PFA, rinsed and permeabilized with cold methanol; samples were then blocked with antibody blocking solution [ADS (10% NGS, 1% BSA in PBS 1×)] for 1 h. The following primary antibodies were diluted in ADS and incubated overnight at 4°C: rat anti-MBP (1:10 culture medium 233 of hybridoma cells; a gift from Judith Grinspan Department of Neurology, The Children's Hospital of Philadelphia, Philadelphia, Pennsylvania); and rabbit anti-EGFP (1:100; catalog #A11122, Thermo Fisher Scientific; RRID:AB_221569). Goat anti rat Cy3TM-coniugated (catalog #112166062, Jackson ImmunoResearch; RRID:AB_2338254) and donkey anti rabbit Alexa Fluor 488-coniugated (catalog #711545152, Jackson ImmunoResearch; RRID:AB_2313584) were used 1:200 as secondary antibodies. The samples were viewed with a Leica DM5000 microscope, and images were acquired with a Leica DFC480 digital camera and processed with Adobe Photoshop CS4 (Adobe Systems).
Electrophysiological analyses
The electrophysiological evaluation was performed on five to nine mice/genotype at 5 months of age with a specific EMG system (Neuro-Mep-Micro, Neurosoft), as previously described (Biffi et al., 2004). Mice were anesthetized with trichloroethanol 0.02 ml/g body weight (25–30 g) and placed under a heating lamp to maintain constant body temperature. Sciatic nerve conduction velocity (NCV) was obtained by stimulating the nerve with steel monopolar needle electrodes. A pair of stimulating electrodes was inserted subcutaneously near the nerve at the ankle. A second pair of electrodes was placed at the sciatic notch to obtain two distinct sites of stimulation, proximal and distal along the nerve. Compound motor action potential was recorded with a pair of needle electrodes; the active electrode was inserted in muscles in the middle of the paw, whereas the reference was placed in the skin between the first and second digit. Sciatic nerve F-wave latency (FWL) measurement was obtained by stimulating the nerve at the ankle and recording the responses in the paw muscle, with the same electrodes used for the NCV study.
Experimental design and statistical analysis
No statistical methods were used to predetermine sample sized, but our sample sizes are similar to those generally used in the field. Graphs and data were generated and analyzed using GraphPad Prism Software. Data show the mean ± SEM. Student's t test (two tailed, unpaired) or one-way ANOVA with Bonferroni's multiple-comparison post hoc test were used as indicated. Significance levels were marked on figures as follows: *p ≤ 0.05, **p ≤ 0.01, ***p ≤ 0.001.
Results
P0Cre-driven deletion of the floxed WT eIF2α transgene impedes eIF2α phosphorylation in Schwann cells
To directly study the effects of the inactivation of eIF2α phosphorylation in Schwann cells, we crossed mice in which eIF2α cannot be phosphorylated because of a conditional homozygous eIF2αSer51Ala mutation (AA//fTg mice; Back et al., 2009) with P0Cre mice (Feltri et al., 1999). The resulting mice (eIF2αSC-AA) were then crossed with P0S63del-CMT1B mutant mice (S63del; Wrabetz et al., 2006) to generate S63del/eIF2αSC-AA mice for testing the role of eIF2α phosphorylation in neuropathic nerves with activated UPR (Fig. 1A). The floxed WT eIF2α transgene (fTg) was designed to induce green fluorescence protein (EGFP) expression on Cre-mediated deletion of the eIF2α coding region (Back et al., 2009; Fig. 1B). Immunostaining analysis for MBP and EGFP on P21 sciatic nerve transverse sections confirmed the specificity of the P0Cre-mediated excision of the fTg transgene followed by induction of EGFP expression in the Schwann cells of both eIF2αSC-AA and S63del/eIF2αSC-AA mice (Fig. 2A). The S63del/eIF2αSC-AA nerve sections appeared compromised, as shown by reduced and disorganized myelinated fibers compared with S63del and WT (CTR) controls (Fig. 2A). Western blot (WB) analysis on P21 sciatic nerve lysates confirmed that EGFP expression was confined to Cre-expressing nerves (Fig. 2B) and that P-eIF2α, which as expected was strongly increased in S63del nerves compared with WT (D'Antonio et al., 2013), was almost completely impeded in S63del/eIF2αSC-AA mice (Fig. 2C). The weak P-eIF2α signal still visible in the eIF2αSC-AA and S63del/eIF2αSC-AA samples was probably because of the presence of cell types other than Schwann cells (e.g., fibroblasts, endothelial cells, resident macrophages) in the sciatic nerve, that do not undergo recombination.
Diagram depicting the breeding strategy used to obtain the experimental genotypes. A, Mice homozygous for the eIF2α Ser51Ala (S/A) mutation and carrying the fTg transgene (floxed eIF2α wild-type transgene; A/A/fTg mice; Back et al., 2009) were crossed with the P0Cre mice (a), which express a Schwann cell-specific Cre (Feltri et al., 1999), or with the S63del-CMT1B neuropathic mice (b; Wrabetz et al., 2006). These crossings generated S/A//P0Cre (a′) and S/A//fTg//P0Cre (a′′), or S/A//fTg//S63del (b′) and S/A//S63del mice (b′′), respectively, which were then bred to obtain the four experimental genotypes. B, In the fTg transgene, the expression of eIF2α-WT is driven by the CMV enhancer and chicken β-actin promoter (Enh-Pro; Back et al., 2009). Lox-P sequences (black arrows) allow the P0Cre-mediated excision of the eIF2α coding sequence and coordinate the expression of EGFP in Schwann cells.
Conditional inactivation of eIF2α phosphorylation in Schwann cells. A, Immunofluorescence analysis on P21 sciatic nerves transversal cryosections. MBP (red) was used to visualize myelin; EGFP (green) marks the excision of the WT eIF2α coding sequence. Schwann cell nuclei are stained with DAPI (blue). Scale bar, 20 μm. B, Western blot analysis of P21 sciatic nerve lysates for EGFP; tubulin was used as a loading control. C, Western blot analysis of sciatic nerve lysates from P21 sciatic nerves to evaluate eIF2α phosphorylation. One representative blot of three (quantified in the graph) is shown. D, Western blot analysis on sciatic nerve lysates from P21 sciatic nerves for ATF4; Coomassie staining was used to show equal loading. One representative blot of four (quantified in the graph) is shown. *p ≤ 0.05, **p ≤ 0.01, ***p ≤ 0.001 by Student's t test.
Under ER stress conditions, eIF2α phosphorylation results in global translation attenuation, and in the concomitant selective translation of ATF4 mRNA (Harding et al., 2000b; Scheuner et al., 2001; Harding et al., 2003). The evaluation of translational rates in sciatic nerves in vivo is extremely difficult (D'Antonio et al., 2013). Thus, as a direct measure of the P-eIF2α downstream cascade, we assessed ATF4 protein levels. ATF4 was increased in S63del nerve extracts but returned toward control levels in S63del/eIF2αSC-AA (Fig. 2D), confirming the inactivation of the pathway. Collectively, these results affirm that the P0Cre recombination system removes the floxed eIF2α-WT fTg transgene abolishing eIF2α phosphorylation specifically in Schwann cells.
The genetic ablation of eIF2α phosphorylation in Schwann cells severely affects the dysmyelinating phenotype of S63del nerves
We previously showed that in S63del nerves the phosphorylation of eIF2α is highly induced during the active phase of myelination, between P10 and P30 (Musner et al., 2016). This therefore represents a good time frame to directly examine the effects of the absence of eIF2α phosphorylation in Schwann cells. Transverse semi-thin cross sections on P10 sciatic nerves confirmed a reduction in myelination extent in S63del nerves compared with CTR nerves (Wrabetz et al., 2006), but we could not detect any striking difference in S63del/eIF2αSC-AA compared with S63del mice (Fig. 3A). A more detailed morphometric analysis performed with EM (Fig. 3B), however, revealed a mild increase in g-ratio in S63del/eIF2αSC-AA compared with neuropathic S63del nerves (g-ratio average values: CTR, 0.625 ± 0.015; eIF2αSC-AA, 0.638 ± 0.013; S63del, 0.760 ± 0.002; S63del/eIF2αSC-AA, 0.792 ± 0.011; Fig. 2C), which was statistically significant when restricted to axon with a diameter >2 μm (Fig. 3D).
Lack of eIF2α phosphorylation in Schwann cells mildly affects S63del myelination at P10. A, B, Transverse semi-thin cross sections (scale bar, 20 μm; A) and electron microscopy tomography (EM; scale bar, 2 μm; B) of sciatic nerves at P10. C, G-ratio analysis performed on sciatic nerve EM cross sections at P10 shown as average g-ratio values (top) or scatterplot toward axon diameter (bottom); n.s., not significant; ***p ≤ 0.001 by one-way ANOVA. D, Average g-ratio plotted by axon diameter; 150 fibers/nerve were analyzed, n = 3 mice/genotype. **p ≤ 0.01, ***p ≤ 0.001 by one-way ANOVA.
We next looked at P21, a time that roughly corresponds to the peak of ER stress in S63del nerves (D'Antonio et al., 2013). At this time point, the phenotype in S63del/eIF2αSC-AA nerves appeared remarkably compromised, with a severe worsening in hypomyelination compared with S63del. Conversely, the inactivation of eIF2α phosphorylation in a wild-type background (eIF2αSC-AA) did not affect sciatic nerve morphology, at either P10 or P21, despite the highly secretory nature of Schwann cells (Figs. 3A, 4A). EM analysis confirmed the reduction in myelin thickness in S63del/eIF2αSC-AA mice, as measured by g-ratio analysis (Fig. 4B,C; g-ratio: CTR, 0.631 ± 0.011; eIF2αSC-AA, 0.645 ± 0.002; S63del, 0.709 ± 0.008; S63del/eIF2αSC-AA, 0.767 ± 0.010). This reduction appeared to be mostly restricted to axons with a diameter up to 3 μm (Fig. 4D). Moreover, we detected a threefold increase in amyelinated fibers (axons with diameter >1µm blocked in a 1:1 relationship with a Schwann cell) in S63del/eIF2αSC-AA compared with S63del sciatic nerves (Fig. 4B,E), accompanied by a small reduction in the total number of myelinated axons per nerve section (Fig. 4F). Concomitantly, the nerve section area was increased in S63del/eIF2αSC-AA compared with S63del sciatic nerves (CTR, 0.77 ± 0.045; eIF2αSC-AA, 0.84 ± 0.08; S63del, 0.98 ± 0.05; S63del/eIF2αSC-AA, 1.24 ± 0.09 mm2; Fig. 4G). As a result, the relative myelinated fiber density was significantly reduced in S63del/eIF2αSC-AA (in fibers/mm2; CTR, 4151.7 ± 127.7; eIF2αSC-AA, 3978.2 ± 238.4; S63del, 2630.3 ± 72.6; S63del/eIF2αSC-AA, 1900 ± 134.7; Fig. 4A,H).
The genetic ablation of P-eIF2α in Schwann cells leads to a severe worsening of the dysmyelinating phenotype in 3-week-old S63del nerves. A, B, Transverse semi-thin cross sections (A) and EM sections (scale bar, 2 μm; B) of P21 sciatic nerves. Arrows, Amyelinated fibers. C, G-ratio analysis performed on sciatic nerve EM cross sections at P21. Top, Average g-ratio; bottom, g-ratio scatterplot on axon diameter (scatter plot). **p ≤ 0.01, ***p ≤ 0.001 by one-way ANOVA. D, Average g-ratio plotted by axon diameter; 130–170 fibers/mouse were analyzed, n = 3 mice/genotype. ***p ≤ 0.001 by one-way ANOVA. E, Quantification of amyelinated axons per EM field (black arrows, as in B) in P21 sciatic nerves; n = 3 mice/genotype. *p ≤ 0.05 by Student's t test. F, Total number of myelinated fibers per sciatic nerve semi-thin cross sections at P21. G, Total area (in mm2) of sciatic nerves semi-thin cross sections at P21 (n.s., not significant by one-way ANOVA; n = 3 nerves/genotype). H, Quantification of myelinated fibers density; *p < 0.05, ***p < 0.001 by one-way ANOVA; n = 3 nerves/genotype.
Collectively, these data indicate that, despite being dispensable for normal PNS myelination, the phosphorylation of eIF2α is a protective event in developing CMT1B-S63del neuropathic Schwann cells. These results corroborate previous observations showing that the inhibition of eIF2α dephosphorylation ameliorated S63del myelination (D'Antonio et al., 2013; Das et al., 2015).
Lack of eIF2α phosphorylation in Schwann cells worsens neurophysiology and demyelination in S63del mice
Adult S63del mice manifest reduced NCV, increased FWL, and progressive demyelination, similar to the alterations found in patients (Wrabetz et al., 2006; Miller et al., 2012). To test how the genetic ablation of eIF2α phosphorylation would affect these features, we performed neurophysiological analysis on mice at 5 months of age. We confirmed a significant alteration of NCV and FWL in S63del mice compared with control mice (Wrabetz et al., 2006); S63del/eIF2αSC-AA showed a further impairment of these parameters (Fig. 5A). Yet, this worsening was somehow less dramatic than we anticipated based on the severe phenotype observed in S63del/eIF2αSC-AA sciatic nerves at P21, despite the fact that also at 5 months P-eIF2α was increased in S63del nerves compared with CTR (although to a lesser extent compared with P21) and impeded in S63del/eIF2αSC-AA (Fig. 5B). We therefore performed both morphologic and morphometric analysis on adult nerves to investigate how lack of eIF2α phosphorylation was affecting myelin maintenance. Similar to what we observed at P21, 5-month-old eIF2αSC-AA nerves did not show any appreciable difference compared with control nerves, whereas S63del nerves were clearly hypomyelinated. Surprisingly, S63del/eIF2αSC-AA nerves recovered myelin thickness to levels comparable to those of S63del mice (Fig. 5C), as measured by g-ratio analysis on transverse semi-thin cross sections (CTR, 0.683 ± 0.005; eIF2αSC-AA, 0.687 ± 0.005; S63del, 0.738 ± 0.006; S63del/eIF2αSC-AA, 0.726 ± 0.009; Fig. 5D); on the other hand, S63del/eIF2αSC-AA nerves still displayed a significantly increased number of naked axons (which could represent either amyelinated or demyelinated axons) compared with S63del (Fig. 5C,E). These observations suggest that, although phosphorylation of eIF2α may be dispensable for S63del nerves to eventually reach their maximal myelin thickness, it is still necessary to promote myelination of all axons and to protect Schwann cells from demyelination. The increase in naked axons may also explain why S63del/eIF2αSC-AA still showed impaired neurophysiology compared with S63del.
The genetic ablation of P-eIF2α in Schwann cells worsens neurophysiological parameters in adult S63del mice. A, Analysis of NCV (top) and FWL (bottom) in 5-month-old mice. N = 7–10 animals/genotype. Data represent the mean ± SEM; *p ≤ 0.05, ***p ≤ 0.001 by one-way ANOVA. B, Western blot analysis of 5-month-old sciatic nerve lysates for P-eIF2α and EGFP; tubulin was used as a loading control. One representative blot of three (quantified in the graph) is shown. *p ≤ 0.05 by Student's t test. C, Sciatic nerves semi-thin cross sections from 5-month-old CTR, eIF2αSC-AA, S63del, and S63del/eIF2αSC-AA mice. White arrow and inset show a demyelinated fiber. D, G-ratio analysis, **p ≤ 0.01 by one-way ANOVA, n.s., not significant. E, Quantification of naked axons; ***p ≤ 0.001 by Student's t test. N = 3 mice/genotype.
Ablation of eIF2α phosphorylation does not exacerbate the UPR or oxidative stress in S63del nerves
Our data indicate that in S63del Schwann cells the lack of eIF2α phosphorylation is highly detrimental in particular during the phase of active myelination, when S63del nerves experience the maximal induction of the UPR (D'Antonio et al., 2013; Musner et al., 2016). We reasoned that unabated mRNA translation and lack of ATF4 downstream target activation in S63del/eIF2αSC-AA nerves might lead to excessive production and accumulation of mutant P0S63del in the ER with consequent exacerbation of the UPR. Indeed, mice that express higher levels of P0S63del (S63del-H mice; Wrabetz et al., 2006) or mice with increased accumulation of P0S6del in the ER because of ERAD inefficiency (Volpi et al., 2019) show augmented UPR and a very severe phenotype, not dissimilar from what seen in S63del/eIF2αSC-AA nerves.
We thus analyzed the activation state of the three arms of the UPR in sciatic nerves lysates from S63del/eIF2αSC-AA and littermate control mice at P21. Quantitative real-time PCR (qRT-PCR) showed that the mRNA levels of ATF4 and its downstream target CHOP (PERK/eIF2α pathway of the UPR) were significantly increased in S63del compared with WT mice (Pennuto et al., 2008; D'Antonio et al., 2013). In S63del/eIF2αSC-AA, ATF4 returned toward WT levels, whereas CHOP, although reduced compared with S63del, was still partially elevated (Fig. 6A) possibly because CHOP can be activated also through the ATF6 branch of the UPR (Li et al., 2000; Yoshida et al., 2000). As a measure of ATF6 and Ire1 pathway activation, we evaluated the levels of their targets BiP/Grp78 and spliced Xbp1 (Xbp1s), respectively (Bertolotti et al., 2000; Yoshida et al., 2001; Lee et al., 2003). BiP/Gpr78 mRNA and protein, as well as the levels of the mRNA for Xbp1s were increased in S63del nerves compared with WT controls (Wrabetz et al., 2006; Pennuto et al., 2008; D'Antonio et al., 2013), but we did not detect any significant change in the absence of eIF2α phosphorylation in Schwann cells (Fig. 6B–D, respectively). Overall, these data suggested that the genetic ablation of eIF2α phosphorylation results in worsening of the S63del-CMT1B nerve phenotype, yet without further intensifying the toxic gain of function mechanism.
Ablation of P-eIF2α does not alter the UPR in S63del nerves. A, B, qRT-PCR analysis of P21 sciatic nerve extracts for the UPR factors ATF4, CHOP, and BiP; n = 3–5 reverse transcriptions (RTs) from independent pools of nerves. Values are expressed as the fold change compared with WT. C, Western blot analysis on P21 sciatic nerve extracts for the ER stress marker BiP/Gpr78; one representative blot of three (quantified in the graph) is shown. D, qRT-PCR analysis on P21 sciatic nerve extracts for the UPR factor Xbp1s; n = 3–5 RTs from independent pools of nerves. Values are expressed as the fold change compared with WT. *p ≤ 0.05 and **p ≤ 0.01 by one-way ANOVA, n.s., not significant.
Studies performed in pancreatic and hepatic cells have shown how deficiency of eIF2α phosphorylation can lead to cell death induced by oxidative damage (Back et al., 2009; Choi et al., 2017), possibly because of the role of ATF4 in maintaining cellular redox homeostasis (Harding et al., 2003; Lange et al., 2008). Hence, to explore the possibility of an ROS cytotoxic effect also in S63del/eIF2αSC-AA sciatic nerves, we measured the mRNAs levels of a subset of ROS defense genes. The mRNA levels of both GPX1, a hydrogen peroxide-scavenging enzyme, and Hemy-oxygenase-1 (HO-1), a NADPH-dependent antioxidant enzyme, did not show any relevant difference in eIF2αSC-AA compared with WT mice, and Glutatione S-transferase (GSS) levels were actually significantly increased (Fig. 7A). GSS levels were also slightly increased in S63del nerves along with GPX1 levels, but we did not detect any difference in the expression of these antioxidant enzymes between S63del and S63del/eIF2αSC-AA mice (Fig. 7A). Next, we tested for the presence of carbonylated proteins, a largely used oxidative stress biomarker, via Western blot immunoassay. This analysis did not reveal differences in the general redox status among the four genotypes (Fig. 7B), overall indicating that the genetic ablation of eIF2α phosphorylation in Schwann cells does not lead to a detrimental oxidative stress.
The genetic ablation of eIF2α in Schwann cells does not affect the cell redox status. A, qRT-PCR analysis of P21 sciatic nerve extracts for the ROS defense genes GPX1, GSS, and HO-1; n = 3–5 reverse transcriptions from independent pools of nerves. Values are expressed as the fold change compared with WT. Error bars represent the SEM. **p ≤ 0.01 by Student's t test; ns, Not significant. B, Immunoblot detection of carbonyl groups in P21 sciatic nerve extracts. Coomassie staining shows equal loading of protein extracts.
The deficiency of eIF2α phosphorylation leads to a delay in Schwann cell differentiation that may involve the MEK/ERK/c-Jun pathway
Our data showed that S63del/eIF2αSC-AA Schwann cells did not experience either exacerbation of the UPR or a significant activation of oxidative stress. On the other hand, previous work on pancreatic cells had also implicated eIF2α phosphorylation in controlling cell differentiation (Back et al., 2009).
Schwann cell differentiation and myelination are regulated by a precise balancing between positive and negative transcriptional regulators (Jessen and Mirsky, 2008), and CMT1B-S63del Schwann cells are maintained in a limited differentiation state, characterized by sustained expression of a series of negative regulators that preserve their viability (D'Antonio et al., 2013; Florio et al., 2018). We thus wondered whether lack of eIF2α phosphorylation could interfere with this finely tuned equilibrium. To test this hypothesis, we first analyzed the mRNA expression of a panel of genes related to Schwann cell development. The mRNAs for the myelin proteins MBP and PMP22, which are slightly decreased in S63del compared with control, appeared further decreased in S63del/eIF2αSC-AA (Fig. 8A). Of note, the levels of MPZ mRNA also appeared to be decreased, although not significantly, in S63del/eIF2αSC-AA nerves.
The conditional ablation of eIF2α phosphorylation leads to a delay of Schwann cell differentiation. A, B, qRT-PCR analysis of P21 sciatic nerve extracts for the myelin genes MPZ, MBP, and PMP22 (A) and for the transcription factors Krox20/Egr2 and Oct6/Pou3f1 (B). C, qRT-PCR analysis of P21 sciatic nerve extracts for the negative regulators of myelination Sox2, Id2, and c-Jun. Values are expressed as the fold change compared with WT. Error bars represent the SEM; n = 5 reverse transcriptions from independent pools of nerves. *p ≤ 0.05, **p ≤ 0.01, and ***p < 0.001 by Student's t test. D, Western blot analysis on P21 sciatic nerve extracts for c-Jun. One representative blot of three (quantified in the graph) is shown. Coomassie staining was used to show equal loading. *p ≤ 0.05 by one-way ANOVA.
Next, we checked the transcript levels of Krox20/Egr2, one of the master regulators of myelination (Topilko et al., 1994; Parkinson et al., 2004), which appeared roughly unchanged between S63del and CTR sciatic nerves, but then slightly decreased in S63del/eIF2αSC-AA (Fig. 8B). Intriguingly, the levels of Oct6, a crucial transcription factor involved in the transition from promyelinating to myelinating Schwann cells (Jaegle et al., 1996), previously shown to be increased in S63del nerves (Florio et al., 2018), was further increased in S63del/eIF2αSC-AA nerves (Fig. 8B), suggesting defects in Schwann cell differentiation. We therefore examined the levels of several known negative regulators of myelination such as c-Jun, Sox2, and Id2 (Le et al., 2005; Parkinson et al., 2008; Fazal et al., 2017; Florio et al., 2018). We confirmed that all of them were upregulated in S63del sciatic nerves (D'Antonio et al., 2013; Florio et al., 2018), but, while we did not observe any further changes in Sox2 and Id2 mRNA levels (Fig. 8C), we detected a significant increase in c-Jun mRNA and protein levels in S63del/eIF2αSC-AA compared with S63del nerves (Fig. 8D). In peripheral nerves, c-Jun is a downstream target of the MEK/ERK pathway (Napoli et al., 2012), and activation of MEK/ERK signaling is sufficient to drive myelin gene downregulation, Schwann cell dedifferentiation, and demyelination in adult nerves (Harrisingh et al., 2004; Napoli et al., 2012). Indeed, WB analysis of P21 sciatic nerves detected a striking increase of ERK1/2 phosphorylation in S63del/eIF2αSC-AA nerves, whereas P-AKT(Ser473) activity, which is known to also control Schwann cell myelination (Ogata et al., 2004; Domènech-Estévez et al., 2016), was not affected (Fig. 9A). Of note, imbalance between AKT and ERK1/2 phosphorylation levels was suggested to contribute to differentiation defects during early postnatal development in neuropathic Schwann cells (Fledrich et al., 2014). Instead, at 5 months of age, phospho-ERK1/2 expression in S63del/eIF2αSC-AA nerves returned to levels comparable to those of S63del, and a similar trend was observed for c-Jun (Fig. 9B). Altogether, these data suggest a complex scenario in which, during the active phase of myelination when ER stress is at its peak, the absence of eIF2α phosphorylation in S63del Schwann cells determines a dramatic differentiation delay that is probably mediated by the hyperactivation of the MEK/ERK/c-Jun pathway. In adult S63del nerves, the overall reduction in ER stress (D'Antonio et al., 2013; Fig. 5B) drives MEK/ERK/c-Jun expression toward basal levels even in the absence of eIF2α phosphorylation, allowing S63del/eIF2αSC-AA nerves to complete myelination to a degree similar to that in S63del.
The genetic ablation of eIF2α phosphorylation in S63del nerves hyperactivates the MEK/ERK pathway. A, Western blot analysis of P21 sciatic nerves to evaluate Akt(Ser473) and Erk1/2 phosphorylation. One representative blot of three (quantified in the graph) is shown. **p < 0.01 by one-way ANOVA. Error bars represent SEM. B, Western blot analysis of 5-month-old sciatic nerves extract for Erk1/2 phosphorylation and c-Jun. One representative blot of three is shown. Densitometric quantification is shown in the graph. Coomassie staining was used to show equal loading. Error bars represent the SEM. n.s., Not significant.
Discussion
Protein misfolding and activation of the UPR is emerging as a common mechanism in CMT1B and several other myelin disorders (Volpi et al., 2017; Bai et al., 2018; Lin and Stone, 2020). Pharmacological inhibition of eIF2α dephosphorylation alleviated disease manifestations in S63del-CMT1B mice (D'Antonio et al., 2013; Das et al., 2015), making small molecules that prolong eIF2α phosphorylation appealing therapeutic candidates (Das et al., 2015; Krzyzosiak et al., 2018). Unexpectedly, the ablation of PERK also ameliorated S63del neuropathy, despite reduction in P-eIF2α (Musner et al., 2016; Sidoli et al., 2016), highlighting the need to fully understand the role of eIF2α phosphorylation in CMT1B. Here we show that P-eIF2α is required in S63del Schwann cells to preserve myelination, which appears uncoupled from exacerbated UPR or oxidative stress but may depend on the hyperactivation of the MEK/ERK/c-Jun pathway (Fig. 10).
A UPR-independent role for eIF2α phosphorylation in CMT1B Schwann cells. In condition of ER stress, PERK phosphorylates eIF2α to attenuate general protein synthesis. This also leads to the selective translation of the mRNA for the transcription factor ATF4, which in turn activates genes involved in in the antioxidant response and in amino acid metabolism. ATF4 also activates CHOP and Gadd34 (also known as PPP1R15a), which is part of the PP1 holophosphatase complex that dephosphorylates eIF2α to restart protein translation. In most cell types (here epitomized by pancreatic β-cells), impediment of eIF2α phosphorylation and lack of ATF4 translation leads to a failure to properly activate the UPR pathways governed by IRE1 and ATF6, accumulation of misfolded protein, and increased ER stress and oxidative stress, ultimately resulting in apoptosis. In S63del-CMT1B Schwann cells lacking eIF2α phosphorylation, despite reduced translation of ATF4, the IRE1 and ATF6 pathways of the UPR remain properly activated, and there is no increase in ER stress or oxidative stress. Rather, through an as yet unidentified mechanism, lack of eIF2α phosphorylation determines a hyperactivation of the P-ERK/c-Jun pathway, which in turn disrupts Schwann cell development and myelination.
The phosphorylation of eIF2α is dispensable for Schwann cell development and myelination but is adaptive in CMT1B
Several studies have highlighted the relevance of P-eIF2α in the physiology of many cell types, including mouse embryonic fibroblasts, pancreatic β-cells, hepatocytes (Scheuner et al., 2001; Harding et al., 2003; Back et al., 2009; Choi et al., 2017), Paneth cells (Cao et al., 2014), and hippocampal cells (Di Prisco et al., 2014). In these cells, a lack of eIF2α phosphorylation resulted in suboptimal induction of UPR genes and an increased susceptibility to ER stress and oxidative stress. However, whereas β-cells lacking eIF2α phosphorylation undergo apoptosis (Scheuner et al., 2001; Back et al., 2009), Paneth cells are able to proliferate and differentiate in the absence of P-eIF2α but become more susceptible to infections (Cao et al., 2014), and eIF2α phosphorylation-deficient hepatocytes can differentiate but quickly die following challenges with ER stressors (Choi et al., 2017). This indicates some cell- or context-dependent differences in the role of P-eIF2α in cell viability. Surprisingly, given their highly secretory nature, Schwann cells lacking eIF2α phosphorylation developed and myelinated normally without displaying signs of altered cellular homeostasis. This adds up to the normal developmental phenotype observed in PERK-null Schwann cells (Sidoli et al., 2016) and in Schwann cells with impaired ERAD (Volpi et al., 2019). Together, these studies suggest that Schwann cells are intrinsically capable of tolerating mild proteostatic fluctuations, presumably by virtue of efficient protein quality control systems and their remarkable plasticity, which allows them to tailor their differentiation state to different conditions (Kim et al., 2013; Volpi et al., 2017; Florio et al., 2018; Jessen and Mirsky, 2019).
However, in stark contrast with the improved phenotype observed in S63del/PERK-null mice (Sidoli et al., 2016), we found that the genetic impediment of eIF2α phosphorylation is detrimental in myelinating S63del nerves. To the best of our knowledge, this is the first time such a dichotomy in PERK versus P-eIF2α signaling has been reported. For example, deletion of PERK or the eIF2α Ser51Ala mutation have similar, although not identical, effects in fibroblasts and β-cells (Harding et al., 2001; Scheuner et al., 2001; Back et al., 2009; Rajesh et al., 2013). The reasons for this striking difference are not clear, but it should be noted that in S63del/PERK-null and S63del/eIF2α SC-AA nerves the UPR levels were unaffected, suggesting that in Schwann cells both P-eIF2α and PERK may work through pathways other than just the UPR.
The absence of eIF2α phosphorylation transiently blocks S63del Schwann cell differentiation via the MEK/ERK/c-Jun pathway
In the ER stress condition, P-eIF2α is required for translational attenuation, UPR gene induction, and cell survival (Harding et al., 2000b; Scheuner et al., 2001, 2005; Back et al., 2009). We reasoned that a lack of P-eIF2α in S63del Schwann cells could result in excessive accumulation of misfolded protein in the ER. For example, S63del-H mice, expressing higher levels of P0S63del, or S63del Schwann cells lacking the ERAD factor Derlin-2, experience higher ER stress levels and present a very severe neuropathic phenotype (Wrabetz et al., 2006; Volpi et al., 2019). Surprisingly, ER stress and UPR levels were unchanged between S63del and S63del/eIF2αSC-AA nerves. This is in contrast with what happens in β-cells, Paneth cells, and hepatocytes (Back et al., 2009; Cao et al., 2014; Choi et al., 2017), where genetic inactivation of eIF2α phosphorylation results in overall defective UPR signaling and suggests that in Schwann cells P-eIF2α is not necessary for activation of the UPR (Fig. 10).
In many cell types, P-eIF2α, through the selective translation of ATF4, is essential to protect against oxidative stress. In fibroblasts, β-cells, and hepatocytes, unrestricted protein translation and lack of ATF4 induction determines an increase in ROS production and a concomitant decrease in antioxidant gene expression, ultimately resulting in cell death (Harding et al., 2003; Back et al., 2009; Cao and Kaufman, 2014; Choi et al., 2017). Here, however, we did not detect alterations in the redox status of eIF2αSC-AA nor S63del/eIF2αSC-AA, despite a reduction in ATF4 expression. Previous studies suggested that Schwann cells display a strong basal antioxidant capacity that allows them to withstand fluctuations in glucose concentrations or mild oxidative stress (Delaney et al., 2001; Vincent et al., 2009). Our data indicate that, most likely, the antioxidant response in Schwann cells is P-eIF2α independent (Fig. 10).
EIF2α phosphorylation is, however, necessary to promote S63del Schwann cell differentiation and myelination. In particular, Oct6/Pou3f1 and c-Jun were significantly increased in S63del/eIF2αSC-AA nerves. Downregulation of Oct6 transcription factor is crucial for the transition from premyelinating to myelinating Schwann cells (Jaegle et al., 1996). Transgenic mice that constitutively expressed Oct6 in Schwann cells were persistently hypomyelinated but showed normal levels of Krox20 mRNA and decreased expression of the major myelin proteins (Ryu et al., 2007). Hypomyelination and reduction in myelin gene expression were also shown in mice expressing high levels of c-Jun in Schwann cells (Fazal et al., 2017). In peripheral nerves, c-Jun is downstream of the ERK signaling pathway (Napoli et al., 2012), and, accordingly, we found a strong elevation of P-ERK1/2 in S63del/eIF2αSC-AA nerves. Activation of MEK/ERK/c-Jun is necessary for Schwann cell transdifferentiation to the repair Schwann cell phenotype after nerve injury (Arthur-Farraj et al., 2012), and strong induction of this pathway is sufficient to block Schwann cell differentiation in vitro or to drive dedifferentiation in adult nerves (Harrisingh et al., 2004; Napoli et al., 2012). The hyperactivation of the MEK/ERK/c-Jun signaling in developing S63del/eIF2αSC-AA nerves likely underlies the severe dysmyelination (Fig. 10).
How the inhibition of eIF2α phosphorylation triggers ERK1/2 hyperactivation is unclear. In Schwann cells, moderate ERK1/2 activation downstream of neuregulin-1 (NRG1) type III promotes differentiation and myelination (Newbern et al., 2011). The PI3K/AKT pathway, another crucial mediator of myelination (Goebbels et al., 2010; Domènech-Estévez et al., 2016), also lies downstream of NRG1 type III. Yet, PI3K/AKT is not hyperactivated in our system, making it unlikely that the lack of P-eIF2α hyperactivates ERK1/2 through NRG1. Imbalance in PI3K/AKT and ERK1/2 signaling pathways has been suggested to contribute to Schwann cell differentiation defects in neuropathy (Fledrich et al., 2014) and may therefore also play a role in our system. Several works have also suggested that during ER stress activation of the ERK1/2, mostly through IRE1, represents a prosurvival mechanism (Nguyên et al., 2004; Darling and Cook, 2014). Although we do not see an increase in P-ERK1/2 in S63del nerves, where IRE1 is activated at levels similar to S63del/eIF2αSC-AA, we cannot exclude that, in the absence of P-eIF2α, IRE1 may contribute to hyperactivate ERK1/2.
The dysmyelination of S63del/eIF2αSC-AA nerves was, however, transient. By 5 months, S63del/eIF2αSC-AA nerves had recovered myelination to levels comparable to S63del. This could potentially be explained by the returning of ERK/c-Jun toward S63del levels, which would allow S63del/eIF2αSC-AA to proceed with myelination. A similar effect was seen in mice expressing a tamoxifen-inducible Raf/MEK/ERK transgene. Strong induction of ERK led to demyelination and inflammation; once tamoxifen was withdrawn, Schwann cells rapidly redifferentiated and remyelinated axons (Napoli et al., 2012). We speculate that in conditions of strong ER stress, such as those found in myelinating P10–P30 S63del nerves, the lack of P-eIF2α leads to hyperactivation of P-ERK1/2 and c-Jun, which in turn blocks differentiation. In adult S63del mice, ER stress levels are reduced (D'Antonio et al., 2013), as also testified by the reduction in P-eIF2α at 5 months compared with P21 (compare Figs. 2C, 5B). In these conditions, even in the absence of P-eIF2α, ERK1/2 phosphorylation is no longer triggered, allowing S63del/eIF2αSC-AA to complete myelination. The generation of transgenic mice in which eIF2α phosphorylation could be impeded specifically in adulthood would help in addressing this point.
Conclusions
Our data demonstrate that eIF2α phosphorylation has a protective role in CMT1B and support its prolonging as a therapeutic option (Das et al., 2015). On the other hand, the phenotypic recovery in adult S63del/eIF2αSC-AA also hints that early intervention in CMT1B patients might be preferable. Finally, we also show that, at least in Schwann cells, PERK and P-eIF2α functions can be uncoupled. How and why the ablation of PERK improves S63del myelination (Sidoli et al., 2016) remains to be explored. The Schwann cell-specific identification of PERK substrates outside of the UPR would represent a first step in this direction.
Footnotes
This work was supported by Fondazione Telethon, Italy (Grants GGP14147 and GGP15012 to M.D.) the Italian Ministry of Health (Grant GR-2011-02346791 to M.D.), AFM-Telethon, France (Grant 19968 to M.D.), and the Umberto Veronesi Foundation (Fellowship Award 2014 to C.S.). This work was supported in part by National Institutes of Health Grants R01-CA-198103, R01-DK-113171, and R01-AG-062190 (to R.J.K.). We thank Rosa Mastrangelo, Maria Carla Panzeri, and the Alembic facility at the San Raffaele Scientific Institute for excellent technical support, and Ghjuvan'Ghjacumu Shackleford for help with the artwork.
The authors declare no competing financial interests.
- Correspondence should be addressed to Maurizio D'Antonio at dantonio.maurizio{at}hsr.it
References
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