Metabolic regulation of cytoskeleton functions by HDAC6-catalyzed α-tubulin lactylation

doi:10.21203/rs.3.rs-3917945/v1

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Metabolic regulation of cytoskeleton functions by HDAC6-catalyzed α-tubulin lactylation

https://doi.org/10.21203/rs.3.rs-3917945/v1

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published 27 Sep, 2024

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Posttranslational modifications (PTMs) of tubulin, termed as the "tubulin code", play important roles in regulating microtubule functions within subcellular compartments for specialized cellular activities. While numerous tubulin PTMs have been identified, a comprehensive understanding of the complete repertoire is still underway. In this study, we report that α-tubulin lactylation catalyzed by HDAC6 by using lactate to increase microtubule dynamics in neurons. We identified lactylation on lysine 40 of α-tubulin in the soluble tubulin dimers. Notably, lactylated α-tubulin enhanced microtubule dynamics and facilitated neurite outgrowth and branching in cultured hippocampal neurons. Moreover, we discovered a novel function of HDAC6, acting as the primary “writer” for α-tubulin lactylation. HDAC6-catalyzed lactylation was a reversible process, dependent on lactate concentrations. Intracellular lactate concentration triggered HDAC6 to lactylate α-tubulin, a process dependent on its deacetylase activity. Additionally, the catalytic activity for lactylation was conserved in HDAC family proteins. Our study reveals the primary role of HDAC6 in regulating α-tubulin lactylation, establishing a link between cell metabolism and cytoskeleton functions.

Biological sciences/Cell biology/Cytoskeleton/Microtubules

Biological sciences/Neuroscience/Cellular neuroscience

Microtubules, a major component of cytoskeletons are comprised of α/β-tubulin heterodimers that form a tubular structure in eukaryotic cells. Microtubules are highly dynamic and constantly undergo polymerization and depolymerization to perform their diverse functions, including intracellular transport, cell division and cell migration ^1,2. For example, during neurite growth, dynamic microtubules within the growth cone facilitate the growth of new neurites, while stable microtubules in neurite shafts serve as the structural framework, supporting axonal transport and neurite elongation ^3,4. Posttranslational modifications (PTMs) of tubulin subunits, enriched in specialized microtubule structures, regulate microtubule dynamics at these specific sites ^5,6. The majority of these PTMs occur on the exterior of microtubules, but acetylation on α-tubulin Lys40 (K40) is found in the microtubule lumen to mark stable microtubules, particularly in cilia, flagella, and long-lived cytoplasmic microtubules with slow dynamics ^7–9. Stabilization of cellular microtubules by Taxol or microtubule-associated proteins (MAPs) increases α-tubulin acetylation ^9,10. Moreover, structural studies have revealed that α-tubulin acetylation may impair the lateral interaction among the protofilaments and increase microtubule stability during mechanical aging ^11,12.

Acetylation of α-tubulin is regulated by the acetyltransferase MEC-17/α-TAT1 and the deacetylase HDAC6 or Sirt2 ^13–15. α-Tubulin acetylation serves as the stable microtubule marker, probably results from the distinct preference of MEC-17 and HDAC6 for microtubule and tubulin heterodimers, respectively ^16,17. Moreover, α-tubulin acetylation enhances the binding of motor proteins and plays an important role in early polarization events in neurons ^18,19. Deficiency of α-tubulin acetylation is related to impaired axonal transport ^19,20, neuronal migration ²¹ and axonal growth ²². Furthermore, α-tubulin acetylation may also play roles in neurogenerative disorders, including Huntington’s disease, Parkinson’s disease, and Charcot-Marie-Tooth disease ^20,23,24. Moreover, α-tubulin K40 undergoes trimethylation to regulate cell division and neuronal migration during cortical development ^25,26. Although many PTMs of microtubules have been identified, there remains a need for further exploration to uncover the new PTMs of microtubules.

Recent studies have discovered a new post-translational modification named protein lactylation, targeting lysine residues in both histones and non-histone proteins ^27–30. Acetyltransferases such as p300 or TIP60 have been shown to lactylate proteins by using lactyl-coenzyme A (Lac-CoA) as donor ^27,31,32. Additionally, HDAC proteins and Sirtuins have been found to remove protein lactylation ^29,32–34. Moreover, hypoxia and increase glycolysis have been demonstrated to elevate protein lactylation levels in various cell types ^27,35,36. However, the regulation mechanism of protein lactylation remains unclear.

In this study, we identify lactylation on K40 of α-tubulin, competing the same residue with acetylation. α-Tubulin lactylation distributes in the soluble tubulin dimers and increases microtubule dynamics. Interestingly, the α-tubulin deacetylase HDAC6 plays a primary role in regulating α-tubulin lactylation through directly lactylating α-tubulin in high lactate concentration. Finally, α-tubulin lactylation may enhance neurite outgrowth and branching in cultured neurons. Our study identifies α-tubulin lactylation, competing with acetylation in regulating microtubule dynamics, which links cell metabolism and cytoskeleton functions.

Identification of α-tubulin lactylation on K40

To analyze lactylated proteins in cortical neurons, we extracted proteins from cultured neurons and digested them into peptides by trypsin. The lactylated peptides were purified using an anti-lysine lactylation (lac-K) antibody ²⁷, and lysine lactylation was identified through high-performance liquid chromatography (HPLC)-tandem mass spectrometry (MS/MS) analysis (Fig. 1a). The standard for lysine lactylation identification was a mass shift of 72.021 Da on the lysine residue, indicative of the addition of a lactyl group. The mass spectrometry results revealed that 285 peptides had been modified by lactylation (Supplementary Table 1). These lactylated proteins are involved in various biological processes, including transcriptional regulation and cytoskeleton organization (Fig. 1b). Previous studies have investigated the lactylation regulation of histones and metabolic enzymes ^27,37,38. Our specific focus was on investigating lactylation on microtubules and microtubule-associated proteins, particularly α-tubulin.

The mass shift of 72.021 Da on the lysine residue in the peptide (HGIQPDGQMPSDKTIG) from α-tubulin and the cyclic immonium (CycIm) ion of lactyllysine formed during tandem mass spectrum ³⁹ were identified through mass spectrometry analysis (Fig. 1c), suggesting α-tubulin may undergo lactylation on Lys40 (K40). To further validate lactylation of α-tubulin, we transfected HEK293T cells with HA-tagged α-tubulins encoded by different α-tubulin genes. Subsequently, the α-tubulins were immunoprecipitated, and lysine lactylation was revealed by the anti-Lac-K antibody. The immunoblot results revealed lactylation in α-tubulins encoded by TUBA1A, TUBA1C, TUBA3B, and TUBA4A. However, both lactylation and acetylation were absent in the α-tubulin encoded by TUBA8 (Fig. 1d, e), probably due to the lack of K40 in TUBA8-encoded α-tubulin (Fig. 1d, e). We then generated a lysine to alanine mutation on the K40 residue of TUBA1A-encoded α-tubulin (α-tubulin^K40A), and found that lactylation was abolished in the mutant α-tubulin (Fig. 1f, g). Together, these results indicate that K40 is the major lactylation site of α-tubulin.

HDAC6 functions as a primary “writer” for α-tubulin lactylation

Previous studies have indicated that acetyltransferases may also catalyze protein lactylation ^27,29,32. To identify the protein responsible for α-tubulin lactylation, we transfected various acetyltransferases into HEK293T cells and assessed α-tubulin lactylation levels. As expected, overexpression of the α-tubulin acetyltransferase MEC-17 led to a significant increase in α-tubulin lactylation (Extended Data Fig. 1a, b), suggesting that MEC-17 may function as an α-tubulin lactyltransferase. This lactylation was specifically on the K40 residue, as demonstrated by the abolition of α-tubulin lactylation in the α-tubulin^K40A mutant (Extended Data Fig. 1c, d). We next conducted an in vitro lactylation assay using GST-MEC-17 protein purified from E. coli and tubulins purified from the mouse brain. In the presence of Lac-CoA, MEC-17 catalyzed α-tubulin lactylation in a dose-dependent manner (Extended Data Fig. 1e, f). Interestingly, MEC-17 exhibited a preference for microtubules over tubulin dimers in catalyzing α-tubulin lactylation (Extended Data Fig. 1g, h), similar to its catalytic preference as acetyltransferase.

We next generated a polyclonal antibody against lactylated K40 peptide of α-tubulin by using the peptide containing lactylated K40 (Extended Data Fig. 2a). The antibody underwent negative screening with acetylated and un-modified peptides to eliminate nonspecific binding (Extended Data Fig. 2b) and exhibited no detectable cross-reactivity with acetylated or un-modified K40 peptides (Extended Data Fig. 2c). It specifically recognized lactylated α-tubulin in HEK293T cells, but not the α-tubulin^K40A mutant (Extended Data Fig. 2d). Taking advantage of this antibody, we compared α-tubulin lactylation levels in wildtype (WT) and MEC-17 knockout (KO) HEK293T cells. Despite the complete loss of α-tubulin acetylation, there was a slight and statistically nonsignificant reduction in α-tubulin lactylation in MEC-17-deficient cells (Extended Data Fig. 1i, j). These results suggest that α-tubulin acetyltransferase MEC-17 plays a minor role in regulating α-tubulin lactylation in cells.

Intriguingly, when we expressed HDAC family proteins in HEK293T cells, none of the HDACs exhibited delactylase activity for α-tubulin; however, HDAC6 overexpression significantly increased α-tubulin lactylation (Fig. 2a, b). Consistently, HDAC6 KO mice showed a substantial reduction in α-tubulin lactylation in the cortex (Fig. 2c, d). HDAC6-induced α-tubulin lactylation occurred on K40 residue, as the α-tubulin^K40A mutant abolished HDAC6’s effect (Fig. 2e, f). Given that HDAC6 is known as an α-tubulin deacetylase, it is possible that HDAC6-induced α-tubulin lactylation results from reduced α-tubulin acetylation, making K40 available for lactylation. However, HDAC6 overexpression in MEC-17 KO cells, lacking α-tubulin acetylation, still increased α-tubulin lactylation (Fig. 2g, h), suggesting HDAC6 causes α-tubulin lactylation independently of α-tubulin acetylation.

To compare the contribution of MEC-17 and HDAC6 to α-tubulin lactylation, we generated MEC-17 KO, HDAC6 KO and MEC-17, HDAC6 double KO (dKO) mice. Analysis of α-tubulin lactylation levels in the cortex revealed a reduction in MEC-17 KO cortex compared to WT cortex (Fig. 2i, j). Furthermore, α-tubulin lactylation was further decreased in HDAC6 KO cortex compared with MEC-17 KO cortex, indicating that HDAC6 plays a major role in regulating α-tubulin lactylation. Intriguingly, α-tubulin lactylation was completely undetectable in MEC-17 and HDAC6 double KO cortex (Fig. 2i, j). These results indicate that both MEC-17 and HDAC6 contribute to α-tubulin lactylation with HDAC6 potentially acting as the primary "writer" for α-tubulin lactylation.

HDAC6 catalyzes α-tubulin lactylation through a reversible reaction dependent on lactate concentration

While HDAC family proteins have been shown to remove protein lactylation to form lactate in the in vitro assay ³³, HDAC6 overexpression led to increased α-tubulin lactylation (Fig. 2a). Considering the relative high lactate concentration (range from about 2–30 mM) in cells ^40–42, we speculated that HDAC6-catalyzed α-tubulin delactylation is a reversible reaction and intracellular lactate concentration may trigger this reaction from delactylation to lactylation. To test this, we purified Flag-HDAC6 and incubated Flag-HDAC6 with tubulins in the presence of various lactate concentrations. HDAC6 displayed the delactylase activity at lactate concentrations below 1 mM but promoted α-tubulin lactylation at concentrations above 1 mM (Fig. 3a, b). Moreover, HDAC6 dose-dependently catalyzed α-tubulin lactylation in the presence of 10 mM lactate (Fig. 3c, d), with a preference for tubulin dimers over microtubules (Fig. 3e, f). These results demonstrate that HDAC6 lactylates α-tubulin through a reversible reaction dependent on lactate concentration.

The deacetylase activity of HDAC6 is critical for its lactylation activity

To determine whether HDAC6 deacetylase activity is required for lactylation, we applied HDAC inhibitors to impair the deacetylase activity. The HDAC inhibitor TSA effectively abolished HDAC6 catalytic activity for α-tubulin lactylation in the in vitro assay (Fig. 3g, h). Furthermore, HDAC6-induced α-tubulin lactylation was attenuated in cells treated with TSA or the HDAC6 inhibitor Tubastatin (TST) (Fig. 3i, j). HDAC6 contains two deacetylase domains, with the second deacetylase domain being crucial for α-tubulin deacetylation ⁴³. We generated mutations in two critical residues for deacetylase activity, Histidine (H)216 and H611, within the first and second deacetylase domain, respectively. Mutation of H611 but not H216 disrupted the lactylation activity for α-tubulin (Fig. 3k, l). These results indicate that HDAC6 deacetylase activity is crucial for its lactylation activity.

HDAC6 is required for metabolic regulation of α-tubulin lactylation

Given that high lactate concentration triggers HDAC6 to lactylate α-tubulin, the glycolysis pathway, which produces lactate, may increase α-tubulin lactylation. Indeed, HEK293T cells treated with various concentrations of lactate showed a dose-dependent induction of α-tubulin lactylation (Extended Data Fig. 3a, b), consistent with previous reports indicating that lactate enhances protein lactylation ^27,32,35,44. Similarly, GSKA, an inhibitor of lactate dehydrogenase (LDH) designed to prevent lactate production, reduced α-tubulin lactylation (Extended Data Fig. 3c, d). Next, HEK293T cells were exposed to various concentrations of glucose exhibited a dose-dependent increase in α-tubulin lactylation levels (Extended Data Fig. 3e, f). Conversely, the non-metabolizable glucose analogue 2-deoxy-D-glucose (2-DG), which inhibits glycolysis, decreased α-tubulin lactylation levels (Extended Data Fig. 3g, h), indicating that glycolysis increases α-tubulin lactylation. Intracellular glucose metabolism is balanced by glycolysis and mitochondrial metabolism ^45,46. We treated HEK293T cells with rotenone, an inhibitor of mitochondrial respiratory chain complex I, to enhance glycolysis. Immunoblot revealed that rotenone treatment increased α-tubulin lactylation levels (Extended Data Fig. 3i, j). These results demonstrate that α-tubulin lactylation is regulated by glycose metabolism, particularly glycolysis.

To determine whether lactate-induced α-tubulin lactylation is dependent on HDAC6, we generated HDAC6 KO HEK293T cells and treated the cells with lactate. Immunoblot revealed that lactate-induced α-tubulin lactylation was abolished in HDAC6-deficient cells (Extended Data Fig. 3k, l), suggesting the requirement of HDAC6 in lactate-induced α-tubulin lactylation. Furthermore, HDAC6-induced α-tubulin lactylation was significantly reduced with the LDH inhibitor GSKA treatment (Extended Data Fig. 3m, n). Together, these results indicate that glycolysis modulates α-tubulin lactylation through HDAC6-catalyzed lactylation reaction.

Sirt2 is an α-tubulin delactylase

Sirtuin family proteins have been shown to remove protein lactylation ^32,34. Subsequently, we screened the Sirtuin family proteins and observed that overexpression of Sirt2 resulted in decreased α-tubulin lactylation (Extended Data Fig. 4a, b). To further validate Sirt2 as an α-tubulin delactylase, we conducted an in vitro assay. The purified GST-Sirt2 catalyzed α-tubulin delactylation in a dose-dependent manner, and Sirt2 delactylase activity was found to be dependent on NAD+ (Extended Data Fig. 4c, d). Consistently, α-tubulin lactylation levels increased in Sirt2-deficient cells (Extended Data Fig. 4e, f), indicating that Sirt2 serves as an α-tubulin delactylase in vivo. Moreover, the in vitro assay revealed a significant reduction in α-tubulin lactylation levels when Sirt2 was incubated with microtubules rather than tubulin dimers (Extended Data Fig. 4g, h), suggesting that Sirt2 catalyzes α-tubulin delactylation with the preference for microtubules.

Localization of lactylated α-tubulin in soluble tubulin dimers

Microtubules undergo dynamic polymerization and depolymerization, and tubulins may exist in polymerized microtubules or as soluble tubulin dimers ^1,2. To determine the localization of lactylated α-tubulin, we separated soluble tubulin dimers (S) and polymerized microtubules (P) in HEK293T cells. The results revealed that lactylated α-tubulin was predominantly present in the soluble fraction (Fig. 4a, b), probably resulting from the catalytic preference of HDAC6 for tubulin dimers. In contrast, acetylated α-tubulin was found in polymerized microtubules, as previously reported ^8,9. We next used microtubule-targeting agents to manipulate the balance between tubulin dimers and polymerized microtubules. Nocodazole (Noco), an inhibitor of microtubule assembly, resulted in reduced α-tubulin acetylation and increased α-tubulin lactylation (Fig. 4c, d). Conversely, Taxol, which stabilizes microtubules, led to increased α-tubulin acetylation and decreased α-tubulin lactylation (Fig. 4c, d). These findings indicate that α-tubulin lactylation marks soluble tubulin dimers, while acetylation on the same residue marks stable microtubules. Immunostaining using the anti-lactylated α-tubulin antibody was performed to examine the spatial distribution of lactylated α-tubulin in cultured hippocampal neurons. Lactylated α-tubulin was notably presented in the growth cone (Fig. 4e-h), where dynamic microtubules were enriched for neurite extension. In contrast, acetylated α-tubulin accumulated in the neurite shaft rather than the growth cone (Fig. 4e-f).

Increased microtubule dynamics by α-tubulin lactylation

To determine whether lactylated α-tubulin modulates microtubule dynamics, we purified microtubules from mouse brains and conducted the in vitro lactylation assay to obtain highly lactylated α-tubulin (Extended Data Fig. 5a-c). Microtubule formation is proposed to involve two key steps: tubulin nucleation and microtubule elongation ^47,48. In the analysis of tubulin nucleation, an early step in generating short microtubule seeds for assembly ¹¹, we observed a significant increase in the number of short microtubules in chambers incubated with lactylated α-tubulin compared to native α-tubulin (Fig. 5a, b), suggesting α-tubulin lactylation enhances the tubulin nucleation process.

We next performed the in vitro microtubule reconstitution assay (Extended Data Fig. 5d) to assess the impact of α-tubulin lactylation on microtubule elongation. The time-lapse total internal reflection fluorescence (TIRF) imaging revealed a significant increase in both the growth rate and shrinkage rate, without a notable alteration in catastrophe frequency (Fig. 5c-f), These changes resulted in an increased maximum microtubule length in the chamber incubated with lactylated α-tubulin (Fig. 5g). Taken together, these results indicate that lactylated α-tubulin promotes tubulin nucleation and enhances microtubule dynamics.

α-Tubulin lactylation enhances neurite outgrowth and branching

We further examined whether α-tubulin lactylation regulates microtubule dynamics in cultured neurons. Microtubule plus ends were labeled by EB3-tdTomato and time-lapse imaging was performed to determine the microtubule dynamics in hippocampal neurons at day in vitro (DIV) 3. Quantitative analysis revealed a significant increase in the number of EB3 comets in axons treated with lactate, and this increase was restored by expressing the α-tubulin^K40A mutant (Fig. 5h, i), suggesting that α-tubulin lactylation may increase the growing microtubule numbers probably through enhanced tubulin nucleation in neurons. Additionally, lactate treatment increased the velocity of EB3 comets in axons (Fig. 5h, i), indicating that α-tubulin lactylation may increase microtubule dynamics in cultured neurons.

To explore the functional roles of α-tubulin lactylation in neurite outgrowth, we investigated the neurite outgrowth in cultured hippocampal neurons. Control hippocampal neurons at DIV3 typically displayed a polarized morphology with one SMI-312-positive axon and several dendrites. However, the polarization percentage was reduced in lactate-treated neurons, which displayed multipolar morphologies (Fig. 6a, b). Furthermore, lactate treatment increased the number of neurite tips and branching (Fig. 6a, b). These alterations induced by lactate could be restored by the α-tubulin^K40A mutant (Fig. 6a, b). These results suggest that α-tubulin lactylation plays important roles in regulating neuronal development and nerite outgrowth.

To assess the potential impact of α-tubulin lactylation on axonal regrowth after injury, cortical neurons were plated on one-half part of the dish to separate extended axons from cell bodies. After 7 days of culture, axons extended into the other half of the dish. We severed axons without affecting cell bodies and measured axon extension to assess regrowth after injury. Our results revealed significantly increased regrowth in the lactate-treated neurons, and the α-tubulin^K40A mutant abolished the lactate-induced increment (Fig. 6c, d).

The conservation of lactylation catalytic activity among HDACs

Finally, we wanted to determine whether the lactylation activity is conserved among HDAC family proteins. We examined several microtubule-associated proteins (MAPs) previously identified as lactylated in mass spectrum analysis (Fig. 1b). When these proteins were transfected into HEK293T cells along with HDAC family proteins, we observed distinct patterns of lactylation. Specifically, HDAC3 increased lactylation of EB3 (Extended Data Fig. 6a). To further validate this, we generated HDAC3 KO cells and observed a substantial reduction in overall protein lactylation in the cell lysate (Extended Data Fig. 6b, c), with a significant decrease in EB3 lactylation levels (Extended Data Fig. 6d, e). Moreover, DCX lactylation was regulated by HDAC3 and HDAC6 (Extended Data Fig. 6f-h). In contrast, MAP2 lactylation was increased by HDAC3 and HDAC8 (Extended Data Fig. 6i), and STMN2 lactylation was increased by HDAC6 (Extended Data Fig. 6j). These findings support the conservation of lactylation activity within HDAC family proteins.

In summary, our results support a model in which glycolysis regulates cytoskeleton functions by α-tubulin lactylation (Fig. 7). The intracellular glycolysis, which produces lactate, enhances α-tubulin lactylation catalyzed by HDAC6. This modification competes with α-tubulin acetylation to enhance microtubule dynamics. Furthermore, the MAPs are also catalyzed by HDAC family proteins, especially HDAC3, HDAC6 and HDAC8. Lactylation on MAPs might regulate their binding affinity to microtubules, thereby influencing cytoskeleton functions (Fig. 7). Our findings establish a link between cell metabolism to cytoskeleton functions.

Protein lactylation has been shown to be mediated by acetyltransferases and reversed by deacetylases ^45,49. Acetyltransferases such as p300 or TIP60 catalyze protein lactylation by using Lac-CoA as the lactyl donor ^27,32, while histone deacetylases and Sirtuins have been implicated in the removal of protein lactylation ^33,34. In this study, we identified a novel function of HDAC6 as a “writer” for α-tubulin lactylation, which is supported by several pieces of evidence: First, HDAC6 overexpression led to increased α-tubulin lactylation (Fig. 2a), and HDAC6 deficiency caused a dramatic reduction in α-tubulin lactylation (Fig. 2c). Second, in vitro experiments revealed that HDAC6-catalyzed α-tubulin lactylation was a reversible reaction, indicating that high concentration of lactate drives the reaction from delactylation to lactylation (Fig. 3a). Third, the second catalytic domain of HDAC6 is critical for lactylation writer’s activity, and the residues involved in deacetylase activity are critical for catalyzing α-tubulin lactylation (Fig. 3k, l). Finally, we tested several MAPs identified in the mass spectrometry results and found that HDAC3 and HDAC8 also serve as lactylation “writers” for MAPs (Extended Data Fig. 6). Notably, it is possible that other HDAC family proteins may also possess the lactylation “writer” activity, especially considering that the proteins examined in this study were exclusively cytosolic. This suggests a potential conserved function among HDAC proteins in acting as lactylation “writers” to control protein lactylation.

Protein posttranslational modifications are dynamically regulated by the metabolic state in cells. The metabolites often function as modification donors to covalently conjugate to protein substrates. For example, acetyl-coenzyme A (Ac-CoA) and S-adenosylmethionine (SAM) can be catalyzed by acetyltransferases for lysine acetylation and by methyltransferases for lysine methylation, respectively ^50,51. The Lac-CoA is believed to be the lactyl donor catalyzed by acetyltransferases to increase protein lactylation ⁴⁵. Moreover, lactylglutathione (LGSH), an intermediate in the glyoxalase pathway, can serve as a lactyl donor by reacting nonenzymatically to promote lysine lactylation on glycolytic enzymes ³⁷. However, the Lac-CoA concentration is about 10 nM compared to 10 µM Ac-CoA in the cytosol ³¹. Therefore, the acetyltransferases mainly regulate protein acetylation instead of lactylation, due to much higher Ac-CoA concentration in cells. Indeed, the deficiency of MEC-17 resulted in the elimination of α-tubulin acetylation, although it had a relatively minor impact on α-tubulin lactylation (Extended Data Fig. 1i, j), suggesting acetyltransferases and Lac-CoA may not play a primary role in regulating protein lactylation.

It is believed that lactate is converted into Lac-CoA to promote protein lactylation ^27,45. However, our study discovered that lactate could directly conjugated onto lysine residues catalyzed by HDAC6. In vitro experiments showed that high lactate concentration triggered HDAC6 to lactylate α-tubulin (Fig. 3a). This notion was further supported by the observation that lactate treatment increased α-tubulin lactylation in WT cells and MEC-17-deficient cells (Extended Data Fig. 1i), but not in HDAC6-deficient cells (Extended Data Fig. 3k). Moreover, the intracellular lactate concentration can range from about 2 mM to 30 mM ^40–42, much higher than Lac-CoA, and this concentration is enough to trigger HDAC6-catalyzed α-tubulin lactylation reaction (Fig. 3a). Importantly, HDAC6 plays a major role in regulating α-tubulin lactylation because HDAC6 deficiency led to a large reduction in α-tubulin lactylation (Fig. 2c, i). Together, these results demonstrate that lactate may be the major lactyl-group donor in regulating protein lactylation, catalyzed by HDAC proteins.

Dynamic instability is the key feature of microtubules that modulates microtubule properties and functions. The combinations of tubulin posttranslational modifications and tubulin isotypes could control microtubule dynamics and functions ¹. In this study, we discovered lactylation on K40 of α-tubulin, the same residue modified by acetylation (Fig. 1f). Interestingly, acetylated α-tubulin is enriched in the stable microtubules with longer lifetime, while lactylated α-tubulin is distributed in soluble tubulin dimers (Fig. 4a) Moreover, lactylated α-tubulin promotes tubulin nucleation and increases both the growth and shrinkage rates of microtubules (Fig. 5c-e). These observations demonstrate that lactylation modulate tubulin properties but in the opposite way to acetylation, making K40 residue on α-tubulin a molecular switch to alter microtubule dynamic instability.

α-Tubulin acetylation is a well-studied modification in the microtubule lumen and labels stable microtubules. Stable microtubules marked by acetylation probably result from the catalytic preference of the “writer” MEC-17 for microtubules and the “eraser” HDAC6’s preference for tubulin dimers ^16,17. In contrast, the distribution of lactylated α-tubulin in tubulin dimers may also arise from the distinct substrate preference of the “writer” and “eraser”. The primary “writer” HDAC6 preferred tubulin dimers over microtubules (Fig. 3e), whereas the eraser Sirt2 catalyzed α-tubulin delactylation in microtubules (Extended Data Fig. 4g) resulting in enriched α-tubulin lactylation in soluble tubulin dimers. Previous studies have demonstrated that α-tubulin acetylation reduces the lateral interactions between protofilaments and protects microtubules from repeated mechanical stress ^11,12. However, the mechanism by which α-tubulin lactylation regulates microtubule dynamics needs to be further studied.

In summary, our results support a model in which glycolysis regulates cytoskeleton functions by glycolysis (Fig. 7). The intracellular glycolysis, which produces lactate, enhances α-tubulin lactylation catalyzed by HDAC6. This modification competes with α-tubulin acetylation to enhance microtubule dynamics. Furthermore, the MAPs are also catalyzed by HDAC family proteins, especially HDAC3, HDAC6 and HDAC8. Lactylation on MAPs might regulate their binding affinity to microtubules, thereby influencing cytoskeleton functions (Fig. 7). Our findings establish a link between cell metabolism to cytoskeleton functions.

Acknowledgment

We thank X. Li, C. Fan, R. Wang and Z. Yang from the Molecular Imaging Core Facility (MICF); P. Hao, Z. Shi and C. Zhang from the Multi-Omics Core Facility (MOCF); and Y. Xiong, X. Ren, and J. Li from the Molecular and Cell Biology Core Facility (MCBCF); J. Wang from the Animal Core Facility at the School of Life Science and Technology, ShanghaiTech University for providing technical support. We thank Dr. Lei Diao and Dr. Lan Bao from CAS Center for Excellence in Molecular Cell Science, Zhihao Gu and Dr. Fang Bai from ShanghaiTech University for discussions and technical support. This study was supported by grants from the National Natural Science Foundation of China (91949117, 31871044 to L.L.).

Author contributions

L.L., S.S. and Z.X. designed the experiments and wrote the manuscript. S.S. and Z.X. performed and analyzed most of the experiments; L.H. performed and analyzed Mass spectrometry experiment. X.L. and Y.S. contributed to protein purification. Y.Q., Y.Z. and Y.H.S. contributed to data analyses.

Competing interests

The authors declare no competing interests.

Data availability

All data associated with this study are available in the main text or the Supplementary Materials. All requests for reagents should be made to the corresponding authors upon reasonable request. They will be made available through appropriate administrative channels (MTA).

Additional information

Supplementary Information is available for this paper.

Correspondence and requests for materials should be addressed to L.L.

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Materials

Pan anti-Kla (PTM-bio, Cat# PTM-1401), anti-acetylated tubulin (Sigma, Cat# T7451), anti-HA tag (Abmart, Cat# M20003), anti-HA tag (Sigma, Cat# H6908), anti-Flag tag (Abmart, Cat# M20008), anti-Flag tag (Sigma, Cat# F7425), anti-GFP (Thermo Fisher Scientific, Cat# A-11122), anti-α-tubulin (Santa Cruz, Cat# sc-32293), anti-α-tubulin (Proteintech, Cat# 11224-1-AP), anti-HDAC6 (Proteintech, Cat# 12834-1-AP), anti-β3-Tubulin (Cell Signaling technology, Cat# 5568), anti-β3-Tubulin (Merck/Millipore, Cat# MAB1637), Purified anti-Neurofilament Marker (SMI-312, BioLegend, Cat# 837904), anti-Sirt2 (PTM-bio, Cat# PTM-6318), anti-HDAC3 (PTM-bio, Cat# PTM-5183), Phalloidin-iFluor 633 Reagent (Abcam, Cat# ab176758), Sodium L-lactate (Sigma, Cat# 71718), Lactyl coenzyme A (Chemsoon, Cat# FM120), GSK2837808A (GSKA, TargetMol, Cat# T15435), D-(+)-Glucose (Sigma, G7021), 2-Deoxy-D-glucose (APExBIO, Cat# B1027), Rotenone (TargetMol, Cat# T2970), Nocodazole (APExBIO, Cat# A8487), Paclitaxel (Taxol) (APExBIO, Cat# A4393), NAD+ (Santa Cruz, Cat# sc-208084B), Trichostatin A (TSA) (APExBIO, Cat# A8183), Tubastatin A (TST) (Selleck, Cat# S8049), Biotin-tubulin (Cytoskeleton, Cat# T333P-A), Rhodamine-tubulin (Cytoskeleton, Cat# TL590M-A), HiLyte-488-tubulin (Cytoskeleton, Cat# TL488M-A), GMPCPP (Jena Biosciences, Cat# NU-405S).

Plasmids

Flag-p300, Flag-HDAC1, Flag-HDAC2, Flag-HDAC3, Flag-HDAC5, Flag-HDAC7, Flag-HDAC9 were acquired from BIO-RESEARCH INNOVATION CENTER SUZHOU. Flag-Sirtuins were gifts from Dr. Gaofeng Fan in Shanghaitech University. Plasmid HA-α-tubulin-1A/1C/3B/4A/8, GFP-MEC-17, GST-MEC-17 and EB3-tdTomato were gifts from Dr. Lan Bao in CAS Center for Excellence in Molecular Cell Science, Chinese Academy of Sciences.

Cell culture and transfection

HEK293T cells were cultured in Dulbecco’s Modified Eagle Medium (DMEM, Gibco) supplemented with 10% fetal bovine serum (Gibco) and antibiotics (ABCONE). Transient transfection was performed using PEI 40000 (Yeasen), and subsequent assays were conducted 36 h after transfection.

Primary neurons were cultured as previously described ⁵². The mouse hippocampus and cortex were dissected at postnatal day (P0) in Hank’s balanced salt solution (HBSS, CellGro) and digested with 0.25% trypsin (Gibco) for 15 min at 37°C. After digestion, the tissues were washed three times in DMEM and dissociated by repeated passaging through a 1 ml pipette. The neurons were then plated on poly-D-lysine (Sigma) coated dishes with DMEM containing 10% fetal bovine serum. After 2 h, the medium was replaced by Neurobasal medium (Gibco) containing 2% B-27 supplement (Gibco) and 2 mM GlutaMAX-I (Gibco). Half media changes were performed every 3 days. For neuron growth experiment, lentivirus was added to hippocampal neurons 2 h after plating and removed after 12 h treatment. For EB3 time-lapse imaging, the indicated plasmids were transfected into hippocampal neurons by Lipofectamine LTX (Thermo) 12 h after plating and removed after 12 h treatment. The neurons were used for immunostaining or time-lapse imaging at DIV3.

Peptide Immunoprecipitation

Primary cortical neurons obtained from C57/BL6J mice at P0 were lysed directly with 8 M urea. The supernatant was diluted with 50 mM NH₄HCO₃ buffer to decrease the urea concentration to 1 M. Subsequently, the proteins were digested into peptides by trypsin overnight at 37°C. The peptides were incubated with protein A/G agarose beads (Abmart) immobilized with Pan lactylated-lysine antibody for 4 h at 4°C. Peptides were eluted from the beads with 0.1% TFA, followed by desalting on a Sep-pak C18 cartridges column and subsequent vacuum lyophilization. The vacuum-dried samples were resuspended in 0.1% FA for liquid chromatography (LC)-MS/ MS analysis.

HPLC/MS/MS analysis

The peptide samples were loaded and separated by a C18 analytical column (75 μm ID×15 cm, 1.9 μm, self-pack). The separation and analysis of peptides were carried out using an Easy-nLC 1200 system coupled to a Q-Exactive HF Hybrid Quadrupole-Orbirap Mass spectrometer system (Thermo Fisher Scientific). A 60-min gradient was established using mobile phase A (0.1% formic acid) and mobile phase B (0.1% formic acid in 98% ACN), consisting of 51 min of 2-28% B, 1 min of 28-38% B, 1 min of 38-90% B, and 7 min of 90% B, at a constant flow rate of 300 nL/min at 45°C. Electrospray ionization at 2.2 kV was employed for peptide ionization. Full scan MS spectra (from m/z 375 to 1500) were acquired in the Orbitrap at a high resolution of 60,000 with an automatic gain control (AGC) of 5e5 and a maximum fill time of 50 ms. The twenty most intense ions were sequentially isolated and fragmented in the HCD collision cell with normalized collision energy of 25%. Fragmentation spectra were acquired in the Orbitrap analyzer with a resolution of 15,000. Ions selected for MS/MS were dynamically excluded for a duration of 10 s.

Immunoblotting and immunoprecipitation

Immunoblotting was performed as described previously ^43,52. Cells were lysed in common RIPA buffer (50 mM Tris-HCl pH 7.5, 150 mM NaCl, 1% Triton X-100, 10% glycerol and protease inhibitor Cocktail (APExBIO)) and the brain tissues were lysed in RIPA Lysis Buffer (Beyotime) (50 mM Tris pH 7.4, 150 mM NaCl, 1% Triton X-100, 1% sodium deoxycholate, 0.1% SDS). Protein samples were separated by SDS-PAGE, transferred to the nitrocellulose membrane (Cytiva), blocked by 5% skim milk for 30 min at room temperature, probed with specific antibodies and then visualized with Omni-ECL™ Femto Light Chemiluminescence Kit (Epizyme). Images were captured with Tanon 5200 and analyzed using ImageJ software.

For dot blotting, indicated peptides were spotted onto the nitrocellulose membrane. The membrane was blocked with 5% skim milk after air-drying and then incubated indicated antibodies.

For the co-immunoprecipitation experiment, cells were lysed in RIPA buffer. Following centrifugation, the supernatant was incubated with anti-HA IP resin (Genescript) at 4°C for 2 h and directly eluted with 1x loading buffer (2.5 mM Tris-HCl pH 6.8, 2% SDS, 0.1% Bromophenol blue, 10% glycerol, 8% 2-Hydroxy-1-ethanethiol in ddH₂O). The immunoprecipitated samples were analyzed by immunoblotting.

Protein expression and purification

GST-tagged proteins were purified as previously described ⁵³. The mouse MEC-17 containing residues 1-193 or the full-length human Sirt2 was subcloned into pGEX-2T expression vector and expressed in E. coli BL21 at 37°C for 4 h. Subsequently, induction was carried out with 0.1 mM IPTG (ABCONE) at 16°C for 16 h. Cells were collected by centrifugation at 6,000 x g for 10 min, and cell pellets were resuspended with lysis buffer (PBS pH 7.4, 1 mM DTT (ABCONE), Cocktail) followed by sonication at 4°C. Cell fragments were removed by centrifugation at 12,000 x g for 20 min at 4°C. The lysates were then incubated with GST-tag purification resin (Beyotime) for 4 h and rinsed with PBS (pH 7.4). Proteins were collected in the elution buffer (50 mM Tris-HCl pH 8.0, 150 mM NaCl, 20 mM reduced L-glutathione (Sigma)), which was subsequently replaced by PBS. The proteins were concentrated, quantitatively analyzed, frozen by liquid nitrogen and stored at -80°C.

For Flag-HDAC6, the purification was performed as previously described ⁵⁴. The full-length human HDAC6 was expressed in 293S cells. The cell pellet was re-suspended in 100 ml buffer containing PBS pH 7.4, 300 mM NaCl, 10 mM MgCl₂, 10% glycerol, and 1 ml protease inhibitor cocktail (EDTA-Free, 100x in DMSO; ApexBio), followed by sonication for cell lysis. The cell lysate was then centrifuged at 24,300 x g for 40 min at 4°C. The supernatant obtained was incubated with Flag beads (Smart-Lifesciences) for 2 hours at 4°C. The beads were then washed 4 times with 50 bed volumes of wash buffer (PBS pH 7.4, 463 mM NaCl, 1 mM DTT) and eluted with a buffer containing 50 mM HEPES pH 7.5 and 150 mM NaCl. The protein was further purified by chromatography using a HiLoad 16/600 Superdex 200 pg column (Cytivia) (AKTA). The collected peak fraction was concentrated, quantitatively analyzed, frozen by liquid nitrogen and stored at -80°C.

Tubulin purification and lactylated tubulin preparation

Tubulin purification from the brain of C57/BL6J mice involved two cycles of polymerization/depolymerization as previously described ⁵⁵. The tubulin was firstly deacetylated by purified GST-Sirt2 with 5 mM NAD+ in the depolymerization buffer (DB, 50 mM MES pH 6.6, 1 mM CaCl₂) at 4°C for 30 min for depolymerization, and then at 37°C for 1 h for deacetylation, followed by another 4°C for 30 min for depolymerization for the next cycle. The low acetylated tubulin obtained was polymerized in HMPB (1 M PIPES/KOH pH 6.9, 10 mM MgCl₂, 20 mM EGTA, 50% glycerol, 1.5 mM ATP (Sigma), 0.5 mM GTP (Sigma)) at 37°C for 30 min to remove Sirt2 by centrifugation. Subsequently, GST-MEC-17 (1-193) protein and 10 μM Lac-CoA were added to the depolymerization buffer for α-tubulin lactylation at 37°C for 1 h and removed through two cycles. The lactylated tubulin was dissolved in cold BRB80 buffer (80 mM PIPES-KOH pH 6.8, 1 mM EGTA, 1 mM MgCl₂) and frozen by liquid nitrogen and stored at -80°C.

In vitro α-tubulin lactylation and delactylation assays

The MEC-17 lactyltransferase assays were performed in a buffer that was used for histone acetyltransferase assays, containing 50 mM Tris-HCl pH 8.0, 10% glycerol, 0.1 mM EDTA, 1 mM DTT. The reaction mixture included 10 μM Lac-CoA, purified GST-MEC-17, 1 mM GTP and tubulins from brain. The reaction lasted for 1 h or the indicated time at 37°C. The HDAC6 lactylation assays were performed in BRB80 buffer containing 80 mM PIPES-KOH pH 7.4, 1 mM MgCl₂, 1 mM EGTA. The reaction mixture included purified Flag-HDAC6, tubulins from brain and lactate with indicated concentrations. The reaction lasted for 1 h or the indicated time at 37°C. The Sirt2 delactylation assays were performed in BRB80 buffer (pH 6.8). The reaction mixture included purified GST-Sirt2 and tubulins from brain or 1 mM NAD+. The reaction lasted for 1 h or the indicated time at 37°C.

All the reactions were stopped by adding 2x or 4x loading buffer, followed by heating for 7 min at 98°C, and subjected to immunoblotting.

Preparation of tubulin polymers

To obtain Taxol-stabilized microtubules (MTs), tubulins at a concentration of 6 mg/ml was polymerized for 30 min at 37°C in BRB80 buffer (pH 6.8) supplemented with 4.8% DMSO, 1 mM GTP and 20 µM Taxol. Following polymerization, the polymers were pelleted at 30,000 x g for 40 min at 37°C, and the resulting pellet was suspended in warm BRB80 (pH 6.8) with 20 µM Taxol to achieve the required concentration and stored at room temperature.

Cell line gene editing

CRISPR-Cas9 gene-modified cells were generated as previously described ⁵³. Briefly, the guidance RNAs were inserted into BbsI site of PX330-GFP construct and verified by sequencing. The constructs were transfected into HEK293T cells by PEI 40000. After 48 hours, the GFP-positive cells were sorted by FACS and seeded into the 96-well plate, with each well containing a single cell. The cloned cells derived from an individual cell were verified by genomic DNA sequencing and Immunoblotting. The sequence of sgRNAs is as follows, MEC-17 sgRNA 5′-CCGACCCGGAACCACAACGC-3′ and HDAC6 sgRNA 5′-ACAACCAGGCAGCGAAGAAGT-3′, Sirt2 sgRNA 5′-CTACTTCATGCGCCTGCTGA-3′ and HDAC3 sgRNA 5′-ACGGTGTCCTTCCACAAATA-3′.

Generation of the antibody against α-tubulin K40 lactylation

The antibody against α-tubulin K40 lactylation was custom-designed and generated by HUA BIO, Zhejiang, China. The control peptide (DGQMPSDKTIGGGDDC), the acetylated peptide [DGQMPSDK(Ac)TIGGGDDC] and the lactylated peptide [DGQMPSDK(Lac)TIGGGDDC] were synthesized. The lactylated peptide served as the immunogen for raising the specific antibody in rabbits. Initial purification of α-tubulin K40 lactylation-specific antibody involved negative screening using serial columns with control and acetylated peptides. Subsequently, specific affinity purification was carried out using lactylated peptides.

Measurement of the soluble and polymerized tubulin fractions

HEK293T cells were lysed with pre-warmed BRB80 (pH 6.8) supplemented with 0.5% Triton X-100 for 5 min, followed by centrifugation at 17,400 x g for 10 min at room temperature. The supernatant, denatured with 4 x loading buffer, used as soluble tubulin fraction (S). The pellet, containing microtubules, was reconstituted with cold BRB80 buffer and kept on ice for 15 min to include microtubule depolymerization. After centrifugation at 5,000 x g for 10 min, the supernatant was denatured and used as the polymerized microtubule fraction (P).

Immunostaining

Immunostaining was performed as described previously ⁵². The cultured neurons were fixed with 4% paraformaldehyde (PFA) for 20 min at room temperature, blocked by the immunostaining buffer (1% BSA, 0.5% Triton X-100 in PBS) for 15 min at room temperature, and subsequently incubated with primary antibodies diluted in the immunostaining buffer overnight at 4°C. Following washing steps, samples were incubated with the Alexa-Fluor-conjugated secondary antibodies for 45 min at 37°C, followed by staining with Hoechst (Meilune) for 10 min at room temperature.

For growth cone staining, cultured neurons were fixed with 2% glutaraldehyde in PHEM buffer (60 mM PIPES pH 6.9, 25 mM HEPES, 10 mM EGTA, 2 mM MgCl₂and 1 mg/ml sodium borohyride) for 15 min. To facilitate permeabilized labeling, 1% Triton X-100 was added into the fixative to remove the membranes and soluble substances, allowing the retention of cytoskeletal components and their associated proteins. Subsequently, the cultured neurons were immunostained with primary antibodies for 48 h at 4°C. Following washing steps, phalloidin-staining was performed by incubating with phalloidin-633 (Abcam) at 37°C for 60 min.

Fluorescent images were acquired using the Zeiss 980 Upright microscope and analyzed using ImageJ software.

Microtubule nucleation assay

The microtubule nucleation assay was performed as descripted previously²⁶ . Briefly, a mixture of 10 μM free tubulins (comprising unlabeled and HiLyte-488-tubulin at a 9:1 ratio) were incubated at 37°C for 30 min in BRB80 buffer (pH 6.8) supplemented with 1 mM GTP and 5% glycerol. Microtubules were fixed with 0.5% glutaraldehyde in BRB80 buffer (pH 6.8) for 15 min, and then centrifuged through a glycerol cushion onto a coverslip. The microtubules were imaged using Zeiss 980 Upright microscope equipped with a 63x oil immersion objective. The microtubules were counted using imageJ software.

In vitro microtubule reconstitution assay

To generate rhodamine-labeled GMPCPP-stabilized microtubule seeds through two cycles of polymerization, a mixture of unlabeled mouse brain tubulin dimers (1 mg/ml), biotin-tubulin (Cytoskeleton) at a concentration of 0.1 mg/ml and rhodamine-tubulin (Cytoskeleton) at a concentration of 0.1 mg/ml was incubated with 1 mM GMPCPP (Jena Biosciences) at 37°C for 30 min. The mixture was then subjected to centrifugation at 126,000 x g for 5 min at 37°C to remove unpolymerized tubulin. The microtubule pellet was resuspended in cold BRB80 (pH 6.8), followed by depolymerization at 4°C for 20 min and a second round of polymerization with 1 mM GMPCPP for 30 min at 37°C. Finally, microtubule seeds were obtained after centrifugation at 126,000 x g for 5 min at 37°C, resuspended using 37°C pre-warmed BRB80 (pH 6.8), frozen by liquid nitrogen and stored at −80°C.

For the assembly of sample chamber, a cleaned and silanized glass coverslip was attached onto microscopic slides by double-sided tape to create a reaction space. A mixture of control tubulin or lactylated tubulin and HiLyte-488 labeled tubulin (at a 19:1 ratio) was prepared in BRB80 (pH 6.8) reaction buffer containing 5 mM Dithiothreitol (DTT), 0.1% methylcellulose, 75 mM KCl, 0.25 mg/mL bovine serum albumin (BSA), 25 mM glucose, 25 μg/ml catalase, 50 μg/ml glucose oxidase and 1 mM GTP. For the microtubule growth assay, microtubule seeds were flowed through the channel for 8 min at 37°C before adding the reaction buffer. The sealed chamber was placed into Nikon Ti2-E TIRF Microscope with a pre-warmed 37°C temperature-controlled workstation. Microtubule growth images were acquired with a 60x oil immersion 1.49 NA TIRF objective and Prime 95B Scientific CMOS (sCMOS) camera every 3 s for 15 min. Kymographs were generated and further analyzed using ImageJ software.

Time-lapse imaging

To detect the movement of EB3 in axons, hippocampal neurons were transfected with EB3-tdTomato and either pCDH-TUBA1A-ires-copGFP or pCDH-TUBA1A^K40A-ires-copGFP after planting on glass-bottom dishes for 12 h. At DIV3, the dishes were placed on a temperature-controlled workstation (37°C, 5% CO₂) with an inverted microscope and positive neurons were captured using Zeiss LSM 980 Airyscan under 10x objective for 5 min at 2 s intervals. Kymographs were generated and further analyzed using ImageJ software.

Primary neurons axotomy and axon regeneration

Primary cortical neurons from C57/BL6J mice at P0 were densely plated onto 15 mm glass bottom cell culture dish (NEST), with half of them tightly precoated with the sterile parafilm (Bemis). After 2 h, the DMEM containing 10% fetal bovine serum medium was replaced by Neurobasal medium containing 2% B-27 supplement and 2 mM GlutaMAX-I. The parafilm was removed after 12 h of neuron plating to mechanically clear cells from the designated culture area. Lentivirus was introduced to the neurons and removed after 12 h of treatment. The axons were scratched using a 10 μl tip at the position 600-800 μm distal from the soma at DIV7 and allowed to regenerate for 24 h from pre-existing neurites before fixation by 4% PFA for regeneration quantification. The images were captured by Olympus CKX53 Microscope and analyzed using ImageJ software.

Animals

The MEC-17 KO mice were gifts from Dr. Lan Bao in CAS Center for Excellence in Molecular Cell Science, Chinese Academy of Sciences ²². Mice were genotyped using primers (MEC-17-WT-forward: 5′-GGCTGCCAGGAATGACTTACACG-3′; MEC-17-WT-reverse: 5′-CAGGGAATAATGACAGTAAGACTCACG-3′; MEC-17-KO-forward: 5′-GCAGCCTCTGTTCCACATACACTTCA-3′; MEC-17-KO-reverse: 5′-TAGACTGTTTCCTGGGTTCTACTGCC-3′). The HDAC6 KO mice (#027068) were purchased from the GemPharmatech and genotyped using primers (HDAC6-WT-forward: 5′-GATGGCAGATACTTGCCAGAATG-3′; HDAC6-WT-reverse: 5′-GTACTGGGTTGTCTCCATCAGATC-3′; HDAC6-KO-forward: 5′-GGCTGCCAGGAATGACTTACACG-3′; HDAC6-KO-reverse: 5′-CAGGGAATAATGACAGTAAGACTCACG-3′).

All animal experiments including mouse housing and breeding were executed in compliance with the ethical guidelines of the Institutional Animal Care (IACUC) and Use Committee of ShanghaiTech University. All mice were housed under a 12-h light-dark cycle in the institutional animal care facility.

Statistical analysis

All data were collected from at least 3 independent experiments and presented as the mean ± SEM. Statistical analysis was performed using Prism 8.0.2 software (GraphPad). Comparisons between two groups of immunoblots were evaluated by the student's t-test. Comparisons among multiple groups were performed with one-way ANOVA or two-way ANOVA. The p-value < 0.05 was considered significant (*p < 0.05; **p < 0.01; ***p < 0.001).

There is NO Competing Interest.

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Metabolic regulation of cytoskeleton functions by HDAC6-catalyzed α-tubulin lactylation

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Abstract

Figures

Introduction

Results

Identification of α-tubulin lactylation on K40

HDAC6 functions as a primary “writer” for α-tubulin lactylation

HDAC6 catalyzes α-tubulin lactylation through a reversible reaction dependent on lactate concentration

The deacetylase activity of HDAC6 is critical for its lactylation activity

HDAC6 is required for metabolic regulation of α-tubulin lactylation

Sirt2 is an α-tubulin delactylase

Localization of lactylated α-tubulin in soluble tubulin dimers

Increased microtubule dynamics by α-tubulin lactylation

α-Tubulin lactylation enhances neurite outgrowth and branching

The conservation of lactylation catalytic activity among HDACs

Discussion

Declarations

References

Materials And Methods

Additional Declarations

Supplementary Files

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