In vivo impact of tubulin polymerization promoting protein (Tppp) knockout to the airway inflammatory response

Endres, Tori; Duesler, Lori; Corey, Deborah A.; Kelley, Thomas J.

doi:10.1038/s41598-023-39443-5

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Published: 28 July 2023

In vivo impact of tubulin polymerization promoting protein (Tppp) knockout to the airway inflammatory response

Tori Endres^1,3,
Lori Duesler²,
Deborah A. Corey² &
…
Thomas J. Kelley²

Scientific Reports volume 13, Article number: 12272 (2023) Cite this article

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Abstract

Microtubule dysfunction has been implicated as a mediator of inflammation in multiple diseases such as disorders of the cardiovascular and neurologic systems. Tubulin polymerization promoting protein (Tppp) facilitates microtubule elongation and regulates tubulin acetylation through inhibition of cytosolic deacetylase enzymes. Pathologic alterations in microtubule structure and dynamics have been described in cystic fibrosis (CF) and associated with inflammation, however the causality and mechanism remain unclear. Likewise, Tppp has been identified as a potential modifier of CF airway disease severity. Here we directly assess the impact of microtubule dysfunction on infection and inflammation by interrogating wild type and a Tppp knockout mouse model (Tppp − / −). Mice are challenged with a clinical isolate of Pseudomonas aeruginosa-laden agarose beads and assessed for bacterial clearance and inflammatory markers. Tppp − / − mouse model demonstrate impaired bacterial clearance and an elevated inflammatory response compared to control mice. These data are consistent with the hypothesis microtubule dysregulation is sufficient to lead to CF-like airway responses in mice.

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Introduction

Microtubule stability is tightly regulated through post translational modifications including acetylation and deacetylation¹. A hyper-inflammatory state has been described in a variety of genetic, cardiovascular, and neurologic conditions^2,3,4. Specifically, microtubule dysfunction has been implicated as a mediator of the hyper-inflammatory response^5,6. Cystic fibrosis (CF), an autosomal recessive genetic condition resulting from dysfunction of the cystic fibrosis transmembrane conductance regulator (CFTR), is associated with a hyperinflammatory state with elevated pro-inflammatory cytokines and neutrophilic predominant infiltrates⁷. Microtubule dynamics in CF have been well characterized and suggest a link between microtubule dysfunction and inflammation^8,9,10. Structural defects in CF microtubules, including decreased acetylation and impairment of microtubule dynamic instability, result in functional impairment as evidenced by decreased intracellular endosomal trafficking¹¹. Microtubule structural and functional deficits improve with restoration of microtubule acetylation, achieved through inhibition of a microtubule modifying protein, histone deacetylase 6 (HDAC6) or through stimulation of exchange protein activated by cAMP^5,12. The inflammatory cytokine Mip-2, a cytokine produced by monocytes and epithelial cells, is reduced to WT levels in HDAC6 depleted mice. This observation is suggestive of a causal relationship between microtubule dysfunction and inflammation.

Functional outcomes of microtubule disruption have also been assessed in vivo. A mouse model of HDAC6 depletion shows attenuation of the negative sequelae of CFTR dysfunction following bacterial challenge with Pseudomonas aeruginosa⁵. Weight loss in response to bacterial challenge is lessened, bacterial levels are reduced at a faster rate, and percent neutrophils in bronchial alveolar lavage fluid are returned to WT levels in HDAC6 depleted mice. It has also been shown that anti-inflammatory therapies are able to correct microtubule stability in CF cells further linking the microtubule phenotype with inflammatory control. Ibuprofen has been shown to restore microtubule reformation rates, microtubule extension into the cell periphery, and restore intracellular trafficking as measured by cholesterol transport through and AMP-activated kinase-dependent mechanism⁹. Similarly, resveratrol, a known anti-inflammatory molecule, was shown to restore microtubule dynamics and intracellular trafficking partially through pan inhibition of histone deacetylases¹³.

Previous data demonstrate clearly that HDAC6 inhibition corrects inflammatory signaling in immortalized epithelial cell models of CF and in CF mouse models^5,8,14,15,16. Though microtubule dysfunction in CF is corrected by HDAC6 inhibition, it is not clear that microtubule function is responsible for inflammation in CF since HDAC6 does have other targets^17,18,19. Tubulin polymerization-promoting protein (Tppp) is a regulator of microtubule polymerization and promotes acetylation of alpha tubulin by binding to and inhibiting HDAC6²⁰. We have previously shown that knocking down expression of Tppp in a human tracheal epithelial cell line increases inflammatory signaling consistent with what is seen in CF cells¹². However, it is unclear how an in vivo depletion of Tppp expression will impact airway inflammatory responses to infection. Observing the phenotype of a mouse lacking expression of Tppp (Tppp − / − model) investigates the role of microtubule dysregulation in inflammation by directly affecting a protein known to be responsible for microtubule stabilization independently of other pathology. Previous studies have shown that Tppp − / − cells have WT levels of CFTR activity²¹. The hypothesis of this study is that disruption of microtubule stability through knockout of the Tppp gene will result in a hyperinflammatory state. Tppp − / − mice offer the opportunity to study a mouse model of microtubule instability and the effects of microtubule instability on inflammation in the absence of other disease processes.

Results

Evaluation of response to airway infection challenge with P. aeruginosa in Tppp − / − mice

Previous work demonstrated that inflammatory responses in CF mice (mice homozygous for the F508del mutation on CF57Bl/6 background) could me normalized by depleting expression of histone deacetylase 6 (HDAC6)⁵. HDAC6 deacetylates tubulin impacting stability and microtubule-dependent transport^22,23. However, HDAC6 also has other substrates so it is unclear whether microtubule regulation is responsible for the inflammatory regulation in CF mice. To test the hypothesis that microtubule function is key to inflammatory regulation, we tested in vivo inflammatory responses in a mouse model of microtubule disruption, Tppp − / − mice. Mice were inoculated with 25,000 CFU of the clinical isolate of P. aeruginosa labeled with mCherry (mCH PA M57-15) as described in “Methods”.

Weight changes

Weight loss is a general measure of the severity of reaction to infection in mice. Control (Tppp + / + and Tppp − / −) and Tppp − / − mice were exposed to P. aeruginosa via trans-tracheal inoculation as described in Methods and weight loss determined over three days. No significant differences are observed between control and Tppp − / − mice (Fig. 1A). Responses were further broken down to compare male and female mouse response, and there were still no significant differences between control and Tppp − / − groups (Fig. 1B,C). Female mice in both groups, however, did lose more weight than male counterparts. These data demonstrate that depletion of Tppp expression has no gross adverse effects on the health of mice in response to airway bacterial challenge.

Bacterial clearance

Previous work demonstrated that HDAC6 depletion in CF mice improved the rates of bacterial clearance compared to CF mice suggesting that correction of the microtubule defect in CF mice had a direct influence on immune response and infection control⁵. To test whether microtubule dysregulation could influence bacterial clearance independently of CFTR function, we examine the levels of recovered CFU 3 days post infection. To address the rate of bacterial clearance in mice, total bacteria (CFU/mL) recovered from both bronchoalveolar lavage (BAL) fluid and lung homogenate at 3 days post infection was assessed. Day 3 was chosen as previous studies have shown that this time point is the peak inflammatory response⁵. In Tppp − / − mice, a mean of 7613 + / − 2182 CFU/mL were recovered compared to 1133 + / − 503 CFU/mL for Tppp + / + mice and 2333 + / − 1467 CFU/mL for Tppp + / − mice (Fig. 2A). Isolating female and male responses (Fig. 2B) show the same reduced clearance in Tppp − / − mice regardless of gender. These results demonstrate a reduced rate of bacterial clearance in Tppp − / − mice compared to WT mice suggesting a notably reduced ability to handle acute bacterial infection.

Inflammatory response to acute P. aeruginosa pulmonary infection

The hypothesis of the study is that microtubule dysfunction mediated by the lack of Tppp expression would lead to an elevated inflammatory response. To directly test this hypothesis, mice were infected with P. aeruginosa-laden agarose beads and evaluated 3-days post-infection as previously reported⁵. Total white blood cell count (WBC) was determined from bronchoalveolar lavage (BAL) fluid from the mice described in Fig. 2. Figure 3 shows representative images of hematoxylin stained (3A) and Wright-Giemsa stained (3B) lung sections at 10X magnification 3-days post P. aeruginosa-laden agarose beads in WT and Tppp − / − mice. Pathological scoring shows no gross differences in response to infection between groups (Table 1). Samples were scored in a blinded fashion by a pathologist.

Table 1 Pathology scoring of airways 3-days post-infection in WT and Tppp − / − mice.

Full size table

Neutrophil scoring scale: Neutrophilic infiltration—1, Absent to rare solitary neutrophils; 2, detectable extravasated neutrophils seen as small loose cellular aggregates in one to a few airways and/or alveoli; 3, detectable extravasated neutrophils seen as loose to compact cellular aggregates in multiple to coalescing airway and/or alveoli with some effacement of lung architecture; 4, detectable extravasated neutrophils seen as compact cellular aggregates effacing most adjacent lung architecture²⁴.

Though no gross pathological scoring difference between groups was observed at this acute infection time point, inflammatory responses were quantified by examining bronchoalveolar lavage (BAL) samples. Total white blood cell (WBC) content was found to be significantly greater in Tppp − / − compared to control mice (Fig. 4A). Breaking down responses in male and female mice demonstrate a significant increase in total WBC in female Tppp − / − mice, but not in male mice though the trend was similar (Fig. 4B).

CF airway inflammatory responses are characterized in part by excessive neutrophil recruitment²⁵. It was hypothesized that Tppp − / − mice would also exhibit a neutrophil dominant inflammatory response as well. Neutrophil counts from Tppp − / − mice was found to be significantly greater than in Tppp + / + mice (Fig. 4C). Tppp + / − did not differ from Tppp + / + mice. Male Tppp − / − mice had a significant increase in neutrophils compared to controls while female Tppp − / − mice did not, though the trends show a similar increase (Fig. 4D).

BAL levels of monocytes and lymphocytes were also examined. Monocytes do show a significant increase in Tppp − / − BAL fluid after infection compared to Tppp + / + mice consistent with a more aggressive inflammatory response (Fig. 5A). Monocytes in Tppp + / − mice did trend higher, but did not reach statistical significance compared to Tppp + / + values. Isolating male and female responses show the same trends, but statistical significance is not achieved (Fig. 5B). Lymphocytes levels were generally low in both groups with the exception of two Tppp − / − samples leading to a statistically significant change, but with great variability (Fig. 5C). Only male mice showed the elevated lymphocyte counts, but no statistical significance was found (Fig. 5D).

Together these data demonstrate a more robust inflammatory response that is neutrophil dominant in Tppp − / − mice compared to controls. Male and female responses show that patterns are the same in each group and that overall significance in the combined analyses is not due to a preferred response in one gender.

Cytokine production

Cytokine production in response to P. aeruginosa infection was examined to further characterize the inflammatory response in Tppp − / − mice. Pro-inflammatory cytokines Mip-2, IL-1β, KC, and TNF-α were measured. The production of IL-6 that can have both pro- and anti-inflammatory functions was also measured. Mip-2 and IL1-β cytokines were significantly elevated in lung homogenates from Tppp − / − mice compared to Tppp + / + mice. Tppp + / − mice were not different from Tppp + / + mice in any measure (Fig. 6). IL-6 and TNF-a trend higher but did not reach significance. These data support the hypothesis that inflammatory responses are elevated in Tppp − / − mice and are consistent with inflammatory cell recruitment data in Figs. 4 and 5. It is unexpected that KC levels are not significantly elevated in Tppp − / − mice since it is typically produced in conjunction with Mip-2 in murine epithelium and key to the recruitment of neutrophils as is Mip-2. Cytokine production in male and female mice showed the same patterns but did not reach statistical significance in any group (not shown).

Discussion

Microtubule disruption is implicated in various disease states as a mechanism of comorbid inflammation in genetic, cardiovascular, and neurologic diseases^2,3,4. Previous work of ours demonstrates distinct changes to microtubule regulation in CF cells consisting of reduced tubulin acetylation and slower rates of microtubule reformation^8,9. We have also demonstrated that knocking down expression of Tppp in an immortalized epithelial cell line reproduced these microtubule phenotoypes, consistent with the function of Tppp as an enhancer of microtubule elongation and as an HDAC6 inhibitor^12,20. Inhibition of HDAC6 has been shown to have significant benefit in addressing multiple CF phenotypes^5,21,26. Tppp has also been identified as a candidate modifier gene associating with CF airway disease severity in GWAS studies²⁷. These GWAS studies directly implicate the Tppp/HDAC6 pathway in CF pathogenesis. The Tppp − / − mouse offers a model system to understand the consequences of a CFTR-independent perturbation in this pathway and to test directly the impact of a potential modifier of CF airway disease severity on airway inflammation in response to infection.

The hypothesis of this study was that depletion of Tppp expression in a mouse model would lead to elevated inflammation in response to airway bacterial challenge. This hypothesis stems from previous observations that Hdac6 depletion from CF mice normalized responses to this challenge suggesting a microtubule-related mechanism⁵. We have also recently demonstrated that Tppp − / − mice effectively replicate another phenotype of CF mice, circadian timing dysregulation^21,28. To determine if the Tppp/HDAC6 pathway could be responsible for CF-related airway inflammation, we examined Tppp − / − mice. We have previously shown that Tppp − / − MNE cells have WT levels of CFTR function so we can conclude that any CF-like phenotypes in these mice are not due to a secondary impact on CFTR activity²¹.

Consistent with the hypothesis, the Tppp − / − mice show hypercellular neutrophilic predominant BAL fluids following inoculation with P. aeruginosa. Bacterial clearance is impaired in the presence of the hyperinflammatory response, and there are increased CFU cultured in Tppp − / − BAL fluids and lung homogenates following inoculation compared to control mice. Mip-2 and IL-1b cytokine production is also increased in BAL fluid of Tppp − / − mice. These data are consistent with what is seen in CF mice and demonstrate that disruption of the Tppp/HDAC6 pathway can lead to CF-like inflammatory responses in the presence of WT CFTR function.

Though Tppp + / + and Tppp + / − groups were not statistically different in any comparison, it was noteworthy that Tppp + / − mice did have monocyte levels that trended higher than Tppp + / + mice and were similar to Tppp − / − mice. This trend towards elevated monocytes in Tppp + / − mice may be statistical variability or reflect a more sensitive outcome measure of innate changes in Tppp expression. Little is known about Tppp and inflammation, so it is difficult to speculate as to why monocytes are trending towards elevated in Tppp + / − mice. The trend seems similar in male and female mice, so a gender impact seems unlikely. In our previous work showing circadian disruptions in CF (F508del) mice and Tppp − / − mice, we did not examine the impact of Tppp heterozygosity on circadian regulation^21,28. It is well known that sleep disruption can increase inflammation, so it is possible that Tppp + / − mice have a level of sleep disruption that is sufficient to impact monocyte recruitment²⁹.

In conclusion, these studies demonstrate in an in vivo model that depletion of the microtubule regulatory protein Tppp leads to a CF-like airway inflammatory response. Though these studies do not establish directly that CF inflammation is solely due to microtubule alterations, these studies in conjunction with previous work showing microtubule alterations in CF cells and the efficacy of HDAC6 depletion in reversing CF inflammation help support targeting microtubule regulation as an anti-inflammatory therapeutic target. Since Tppp is an HDAC6 inhibitor, it is possible that the impact of Tppp knockout is independent of microtubule regulation and due to other aspects of HDAC6 signaling. We have previously shown that reducing Tppp expression in epithelial cells recapitulates CF-like inflammatory signaling¹², therefore future studies will focus on the Tppp/HDAC6 pathway in macrophages and neutrophils function in modulating in vivo inflammatory responses.

Methods

Mice

Mice were cared for in accordance with Case Western Reserve University Institutional Animal Care and Use Committee guidelines by the CF Animal Core Facility. The Animal Care and Use Committee of Case Western Reserve University approved all animal procedures. The mouse strain used for this research project, C57BL/6N-Tppp^{tm1.1(KOMP)Vlcg}/JMmucd, RRID:MMRRC_050196-UCD, was obtained from the Mutant Mouse Resource and Research Center (MMRRC) at University of California at Davis, an NIH-funded strain repository, and was donated to the MMRRC by The KOMP Repository, University of California, Davis; Originating from Stephen Murray, The Jackson Laboratory. The mutation is a deletion described at http://velocigene.com/komp/detail/12652.

Preparation of P. aeruginosa-laden agarose beads

P. aeruginosa labeled with mCherry (mCH PA M57-15) was streaked on a 0.3 mg/ml gentamycin/LB agar plate and incubated at 37 °C overnight. The clinical isolate was obtained from the CF Center Biorepository at Rainbow Babies and Children’s Hospital. Five colonies of mCH PA M57-15 were collected and added to 25 ml of LB broth and incubated at 37 °C, 200 rpm, for 18–20 h. After 20 h, the optical density at 600 nm of the mCH PA M57-15 was measured to obtain an absorbance of ~ 0.3 for a tenfold dilution. Bacteria were stored on ice until ready to use.

Two 600-mL beakers containing 250 mL sterile mineral oil and stir bars and a flask of sterile 2% agarose in PBS were warmed in a 50 °C water bath for 30 min. The 2 beakers of mineral oil were placed in ~ 6 × 10 inch plastic container and then placed on magnetic stir plates and set at a medium–high stir to form a vortex. 23 mL of warm, dissolved agarose/PBS was pipetted into one of the beaker of mineral oil to form sterile beads. 5 mL of mCH PAM57-15 was pipetted into the remaining agarose/PBS and mixed and then 23 mL of the mCH PAM57-15/agarose/PBS mixture was pipetted into the other beaker of mineral oil. After 6 min of stirring, 20 g of ice was added to the plastic container every minute for 10 min while monitoring the stirring to ensure a constant vortex. After 10 min, the bead/oil mixture was poured into 50 mL conical tubes containing 15 mL of pre-warmed 0.5% SDC/PBS and spun at 4 °C, 3000 g, for 15 min to separate the beads on the bottom from the top layer of oil. The oil was removed and the top half layer of beads were pipetted into 50 ml conical tubes containing 20 mL of pre-warmed 0.25% SDC/PBS and spun under same conditions. After the second wash, any oil/PBS was removed to ~ 15 mL and the beads were pipetted into 50 ml conical tubes containing 20 mL of PBS and washed 4 ×. After the final wash, the PBS was removed to a 3:4 volume of beads to PBS. A 100 ul aliquot of the bead mixture was used to image and measure the size of beads, which should be ~ 20–600 µm. The beads were viewed under the red channel to ensure sterile beads are sterile and bacterial-laden beads have mCH PA M57-15. A 1:50 dilution of the beads was homogenized on highest speed for 1 min and serial diluted tenfold 10 times. The dilutions were plated on a 0.3 mg/mL gentamycin/LB agar plate and incubated at 37 °C overnight. The following day, the CFU/mL were calculated the bead/PBS mixture was diluted to a concentration of 25,000 CFU/50 µL.

Inoculation of mouse airway with agarose beads

All animal studies were approved by the CWRU IACUC committee, and all experiments were performed in accordance with relevant guidelines and regulations. The mice receiving sterile bead treatment were used first to avoid cross contamination. The mouse was anesthetized with isoflurane via inhalation with a nosecone. Ophthalmic ointment was applied the eyes and the thorax was sterilized with isopropanol. A ~ 1 cm midline median incision was made using surgical scissors in the tracheal region. The tracheal muscles were gently teased apart to expose the trachea and a ~ 1 mm transverse incision was made between the tracheal cartilage. A 1 mL syringe fitted with a 22G × 1″ flexible catheter was used to mix and draw up the bead/PBS mixture leaving no dead space in catheter. The catheter/syringe was immediately inserted into the tracheal incision and 50 mL of the bead/PBS mixture was injected into the lungs of the mouse to administer 25,000 CFU per mouse. The mouse was placed into a clean, sterile cage on top of a warming pad and monitored until out of anesthesia. The weight and condition of inoculated mice were monitored until the day of harvest.

Harvest

Sterile bead inoculated mice were harvest first to avoid cross contamination. The mouse was euthanized by CO2 inhalation, placed in the supine position, and disinfected with 70% ethanol. A midline, median incision was made to expose the thoracic cage and the diaphragm cut to expose the lungs. A 22G × 1″ flexible catheter was inserted between the tracheal cartilage to just before the bronchi. Surgical thread was tied around trachea and catheter. BAL fluid was collected using a syringe filled with 1 ml PBS inserted into the catheter and injected into and withdrawn from lungs. Ten microliters of BAL fluid was used to determine total white blood cell count, another 15 µL was plated on 0.3 mg/mL gentamycin/LB agar for CFU/µL count, and 200 µL of BAL fluid was used to determine cell differentials using Giemsa/Miller staining. The BAL fluid was then spun at 4 °C, 500 g, 10 min. The supernatant was used for cytokine analysis using Luminex. The lungs were removed and rinsed with PBS and placed in 2 mL tubes containing zirconium homogenization beads and homogenized and 15 µL plated on 0.3 mg/mL gentamycin/LB agar for CFU/µL count. The remaining lung homogenate was spun at 4 °C, 5000 g, 10 min and the supernatant removed. The remaining supernatant was stored at − 80 °C. For staining of lung tissue, 10 μm sections were fixed in formalin, embedded in paraffin, deparaffinized in xylene and ethanol, and stained with hematoxylin and eosin by the histology core facility at CWRU.

White blood cell differentiation and counting

Cell counts were conducted manually by a board-certified pathologist blinded to experimental group through the CF Histology Core facility at CWRU. Cells are counted manually in a Neubauer chamber and morphology determined visually. If necessary histological staining is performed to differentiate between neutrophils, lymphocytes, and leukocytes.

Statistical analysis

Statistical analyses were performed with GraphPad-Prism, Version 10.0.0. Analysis of results with Tppp + / + , Tppp + / − , and Tppp − / − groups were done by ordinary one-way ANOVA with Dunnett’s multiple comparison test to compare Tppp + / − and Tppp − / − groups to the Tppp + / + group; p ≤ 0.05 is * and p ≤ 0.01 is **. Statistical analysis of male and female groups were done with unpaired t-test comparing control group (Tppp + / + and Tppp + / − groups) to Tppp − / − groups; p ≤ 0.05 is * and p ≤ 0.01 is **.

ARRIVE guidelines

This study has been conducted and data reported in accordance with ARRIVE guidelines.

Data availability

The datasets generated during and/or analyzed during the current study are available from the corresponding author on reasonable request.

References

Bär, J., Popp, Y., Bucher, M. & Mikhaylova, M. Direct and indirect effects of tubulin post-translational modifications on microtubule stability: Insights and regulations. Biochim. Biophys. Acta Mol. Cell. Res. 1869, 119241. https://doi.org/10.1016/j.bbamcr.2022.119241 (2022).
Article CAS PubMed Google Scholar
Nichols, D., Chmiel J Fau - Berger, M. & Berger, M. Chronic inflammation in the cystic fibrosis lung: alterations in inter- and intracellular signaling. Clin Rev Allergy Immunol. 34(2), 146–62 (2008).
Kaplan, R. C. & Frishman, W. H. Systemic inflammation as a cardiovascular disease risk factor and as a potential target for drug therapy. Heart Dis. 3, 326–332. https://doi.org/10.1097/00132580-200109000-00009 (2001).
Article CAS PubMed Google Scholar
Mangalmurti, A. & Lukens, J. R. How neurons die in Alzheimer's disease: Implications for neuroinflammation. Curr Opin Neurobiol. 75, 102575 (2022).
Rosenjack, J., Hodges, C. A., Darrah, R. J. & Kelley, T. J. HDAC6 depletion improves cystic fibrosis mouse airway responses to bacterial challenge. Sci. Rep. 9, 10282. https://doi.org/10.1038/s41598-019-46555-4 (2019).
Article ADS CAS PubMed PubMed Central Google Scholar
Magupalli, V. G. et al. HDAC6 mediates an aggresome-like mechanism for NLRP3 and pyrin inflammasome activation. Science https://doi.org/10.1126/science.aas8995 (2020).
Article PubMed PubMed Central Google Scholar
Balázs, A. A.-O. & Mall, M. A.-O. Mucus obstruction and inflammation in early cystic fibrosis lung disease: Emerging role of the IL-1 signaling pathway. Pediatr Pulmonol. 54 (Suppl 3), S5–S12 (2019).
Rymut, S. M. et al. Reduced microtubule acetylation in cystic fibrosis epithelial cells. Am. J. Physiol. Lung Cell. Mol. Physiol. 305, L419-431. https://doi.org/10.1152/ajplung.00411.2012 (2013).
Article CAS PubMed PubMed Central Google Scholar
Rymut, S. M. et al. Ibuprofen regulation of microtubule dynamics in cystic fibrosis epithelial cells. Am. J. Physiol. Lung Cell. Mol. Physiol. 311, L317-327. https://doi.org/10.1152/ajplung.00126.2016 (2016).
Article PubMed PubMed Central Google Scholar
Wang, B. et al. Microtubule acetylation amplifies p38 kinase signalling and anti-inflammatory IL-10 production. Nat Commun. 5, 3479 (2014).
White, N. M. et al. Altered cholesterol homeostasis in cultured and in vivo models of cystic fibrosis. Am. J. Physiol. Lung Cell. Mol. Physiol. 292, L476-486. https://doi.org/10.1152/ajplung.00262.2006 (2007).
Article CAS PubMed Google Scholar
Rymut, S. M. et al. Role of exchange protein activated by cAMP 1 in regulating rates of microtubule formation in cystic fibrosis epithelial cells. Am. J. Respir. Cell Mol. Biol. 53, 853–862. https://doi.org/10.1165/rcmb.2014-0462OC (2015).
Article CAS PubMed PubMed Central Google Scholar
Lu, B., Corey, D. A. & Kelley, T. J. Resveratrol restores intracellular transport in cystic fibrosis epithelial cells. Am. J. Physiol. Lung Cell. Mol. Physiol. 318, L1145–L1157. https://doi.org/10.1152/ajplung.00006.2020 (2020).
Article CAS PubMed PubMed Central Google Scholar
Wiech, N. L., Fisher, J. F., Helquist, P. & Wiest, O. Inhibition of histone deacetylases: A pharmacological approach to the treatment of non-cancer disorders. Curr. Top. Med. Chem. 9, 257–271. https://doi.org/10.2174/156802609788085241 (2009).
Article CAS PubMed Google Scholar
Brindisi, M. et al. Efficacy of selective histone deacetylase 6 inhibition in mouse models of Pseudomonas aeruginosa infection: A new glimpse for reducing inflammation and infection in cystic fibrosis. Eur. J. Pharmacol. 936, 175349. https://doi.org/10.1016/j.ejphar.2022.175349 (2022).
Article CAS PubMed Google Scholar
Bodas, M., Mazur, S., Min, T. & Vij, N. Inhibition of histone-deacetylase activity rescues inflammatory cystic fibrosis lung disease by modulating innate and adaptive immune responses. Respir. Res. 19, 2. https://doi.org/10.1186/s12931-017-0705-8 (2018).
Article CAS PubMed PubMed Central Google Scholar
Hsu, F. C. et al. Histone deacetylase 3 is required for T cell maturation. J. Immunol. 195, 1578–1590. https://doi.org/10.4049/jimmunol.1500435 (2015).
Article CAS PubMed Google Scholar
Hamm, C. A. & Costa, F. F. Epigenomes as therapeutic targets. Pharmacol. Ther. 151, 72–86. https://doi.org/10.1016/j.pharmthera.2015.03.003 (2015).
Article CAS PubMed Google Scholar
Husain, M. & Cheung, C. Y. Histone deacetylase 6 inhibits influenza A virus release by downregulating the trafficking of viral components to the plasma membrane via its substrate, acetylated microtubules. J. Virol. 88, 11229–11239. https://doi.org/10.1128/jvi.00727-14 (2014).
Article PubMed PubMed Central Google Scholar
Tokesi, N. et al. TPPP/p25 promotes tubulin acetylation by inhibiting histone deacetylase 6. J. Biol. Chem. 285, 17896–17906. https://doi.org/10.1074/jbc.M109.096578 (2010).
Article CAS PubMed PubMed Central Google Scholar
Barbato, E., Darrah, R. & Kelley, T. J. The circadian system in cystic fibrosis mice is regulated by histone deacetylase 6. Am. J. Physiol. Cell Physiol. 323, C1112-c1120. https://doi.org/10.1152/ajpcell.00248.2022 (2022).
Article CAS PubMed PubMed Central Google Scholar
Hubbert, C. et al. HDAC6 is a microtubule-associated deacetylase. Nature 417, 455–458. https://doi.org/10.1038/417455a (2002).
Article ADS CAS PubMed Google Scholar
Matsuyama, A. et al. In vivo destabilization of dynamic microtubules by HDAC6-mediated deacetylation. EMBO J. 21, 6820–6831. https://doi.org/10.1093/emboj/cdf682 (2002).
Article CAS PubMed PubMed Central Google Scholar
Langlois, R. A. et al. Oseltamivir treatment prevents the increased influenza virus disease severity and lethality occurring in chronic ethanol consuming mice. Alcohol. Clin. Exp. Res. 34, 1425–1431. https://doi.org/10.1111/j.1530-0277.2010.01226.x (2010).
Article PubMed PubMed Central Google Scholar
Roesch, E. A., Nichols, D. P. & Chmiel, J. F. Inflammation in cystic fibrosis: An update. Pediatr. Pulmonol. 53, S30-s50. https://doi.org/10.1002/ppul.24129 (2018).
Article PubMed Google Scholar
Rymut, S. M. et al. Improved growth patterns in cystic fibrosis mice after loss of histone deacetylase 6. Sci. Rep. 7, 3676. https://doi.org/10.1038/s41598-017-03931-2 (2017).
Article ADS CAS PubMed PubMed Central Google Scholar
Dang, H. et al. Mining GWAS and eQTL data for CF lung disease modifiers by gene expression imputation. PloS One 15, e0239189. https://doi.org/10.1371/journal.pone.0239189 (2020).
Article CAS PubMed PubMed Central Google Scholar
Barbato, E., Darrah, R. & Kelley, T. J. Tubulin polymerization promoting protein affects the circadian timing system in C57Bl/6 mice. J. Circadian Rhythms 19, 5. https://doi.org/10.5334/jcr.207 (2021).
Article PubMed PubMed Central Google Scholar
Shirato, K. & Sato, S. Macrophage meets the circadian clock: Implication of the circadian clock in the role of macrophages in acute lower respiratory tract infection. Front. Cell Infect. Microbiol. 12, 826738. https://doi.org/10.3389/fcimb.2022.826738 (2022).
Article CAS PubMed PubMed Central Google Scholar
Geyer, R. R., Musa-Aziz, R., Qin, X. & Boron, W. F. Relative CO(2)/NH(3) selectivities of mammalian aquaporins 0–9. Am. J. Physiol. Cell Physiol. 304, C985-994. https://doi.org/10.1152/ajpcell.00033.2013 (2013).
Article PubMed Google Scholar

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Acknowledgements

We acknowledge the use of the Leica microscopes in the Genetics Department Imaging Facility at Case Western Reserve University³⁰, made available through a National Center for Research Resources (NIH-NCRR) Shared Instrumentation Grant (S10 RR021228). The authors thank Elisha Barbato, MD in the CF RDP Histology Core for image analysis and tissue processing. The authors thank P. Bead for technical assistance.

Funding

This work is supported by CFF grant KELLEY21I0 and CFF RDP R447-CR11 (DRUMM15R0/CFF). Mouse studies supported by the CF Mouse Resource Center at Case Western Reserve University (CFF HODGES19R1).

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Authors and Affiliations

Department of Pediatrics, Case Western Reserve University, Cleveland, USA
Tori Endres
Department of Genetics and Genome Sciences, Case Western Reserve University, 825 BRB, 10900 Euclid Avenue, Cleveland, OH, 44106-4955, USA
Lori Duesler, Deborah A. Corey & Thomas J. Kelley
Rainbow Babies and Children’s Hospital, Cleveland, OH, USA
Tori Endres

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Lori Duesler
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Deborah A. Corey
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Thomas J. Kelley
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Contributions

T.E. assisted with study design, performed infection and inflammation studies, performed data analysis and participated with manuscript preparation. L.D. also performed infection studies and acquiring data and assisted with manuscript review. D.C. oversaw imaging and assisted with manuscript review. T.K. was responsible for study design, data analysis, and manuscript preparation.

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Correspondence to Thomas J. Kelley.

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Endres, T., Duesler, L., Corey, D.A. et al. In vivo impact of tubulin polymerization promoting protein (Tppp) knockout to the airway inflammatory response. Sci Rep 13, 12272 (2023). https://doi.org/10.1038/s41598-023-39443-5

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Received: 18 May 2023
Accepted: 25 July 2023
Published: 28 July 2023
DOI: https://doi.org/10.1038/s41598-023-39443-5

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