Asthma reduces glioma formation by T cell decorin-mediated inhibition of microglia

Chatterjee, Jit; Sanapala, Shilpa; Cobb, Olivia; Bewley, Alice; Goldstein, Andrea K.; Cordell, Elizabeth; Ge, Xia; Garbow, Joel R.; Holtzman, Michael J.; Gutmann, David H.

doi:10.1038/s41467-021-27455-6

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Published: 08 December 2021

Asthma reduces glioma formation by T cell decorin-mediated inhibition of microglia

Jit Chatterjee¹,
Shilpa Sanapala¹,
Olivia Cobb¹,
Alice Bewley¹,
Andrea K. Goldstein¹,
Elizabeth Cordell¹,
Xia Ge²,
Joel R. Garbow²,
Michael J. Holtzman ORCID: orcid.org/0000-0001-8750-3716³ &
…
David H. Gutmann ORCID: orcid.org/0000-0002-3127-5045¹

Nature Communications volume 12, Article number: 7122 (2021) Cite this article

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Abstract

To elucidate the mechanisms underlying the reduced incidence of brain tumors in children with Neurofibromatosis type 1 (NF1) and asthma, we leverage Nf1 optic pathway glioma (Nf1^OPG) mice, human and mouse RNAseq data, and two different experimental asthma models. Following ovalbumin or house dust mite asthma induction at 4–6 weeks of age (WOA), Nf1^OPG mouse optic nerve volumes and proliferation are decreased at 12 and 24 WOA, indicating no tumor development. This inhibition is accompanied by reduced expression of the microglia-produced optic glioma mitogen, Ccl5. Human and murine T cell transcriptome analyses reveal that inhibition of microglia Ccl5 production results from increased T cell expression of decorin, which blocks Ccl4-mediated microglia Ccl5 expression through reduced microglia NFκB signaling. Decorin or NFκB inhibitor treatment of Nf1^OPG mice at 4–6 WOA inhibits tumor formation at 12 WOA, thus establishing a potential mechanistic etiology for the attenuated glioma incidence observed in children with asthma.

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Introduction

Prior case-controlled clinical studies have revealed a reduced incidence of brain tumors in children with T-cell-mediated disorders, including asthma^1,2,3,4. Similarly, in the Neurofibromatosis type 1 (NF1) brain cancer predisposition, we previously reported an inverse association between asthma and optic gliomas, the most common brain tumor in this population of at-risk children⁵. To study this inverse association between asthma and brain tumor incidence in a cancer predisposition syndrome in which atopic conditions reduce glioma incidence, we leveraged a genetically engineered mouse model of NF1-low-grade glioma of the optic pathway. This authenticated preclinical murine model exhibits high tumor penetrance (>95%) and a well-characterized temporal course of glioma progression^6,7. As such, Nf1^flox/mut; GFAP-Cre (Nf1^OPG) mice develop low-grade gliomas of the optic nerves and chiasm by 12 weeks of age, with accompanying increases in optic nerve volume and proliferation, as well as microglia and T-cell infiltration, beginning after 6 weeks of age^8,9. Moreover, the tumor-associated microglia express high levels of Ccl5, a growth factor both necessary and sufficient to drive Nf1-optic glioma formation and continued growth^10,11. Germane to the pathobiology of inflammatory disease, infiltrating T cells in the optic nerve produce Ccl4, which in turn stimulates microglia to produce Ccl5 through activation of the NFκB signaling pathway¹². Moreover, T cell entry and activation are required for Nf1-optic glioma growth in mice, and murine optic glioma stem cells do not form tumors in T cell-deficient mice¹³. As such, Nf1^OPG mice provide a tractable genetic platform to elucidate the molecular and cellular mechanisms responsible for the reduced incidence of brain tumors in children with a T cell-mediated disease like asthma. Herein, we establish a mechanistic link between asthma and gliomagenesis by demonstrating that asthma induces decorin expression in T cells to reduce microglia support of Nf1 optic glioma growth.

Results

Asthma induction inhibits Nf1 ^OPG formation

To determine whether experimental asthma induction reduces murine glioma formation and growth in vivo, Nf1^OPG mice were initially treated with ovalbumin (OVA) or house dust mite (HDM) between 4 and 6 weeks of age and euthanized at 12 weeks of age when optic gliomas are evident in >95% of mice (Fig. 1a). Experimental asthma induction was confirmed by H&E staining of lung tissue, demonstrating infiltration of immune cells in peribronchiolar locations, consistent with submucosal inflammation after OVA or HDM challenge conditions compared to PBS controls (Supplementary Fig. 1a). In addition, there were PAS⁺ airway epithelial cells with morphology consistent with goblet cells, as well as increased serum IgE in OVA-and HDM-treated mice (Supplementary Fig. 1b, c). At 12 weeks of age, the optic nerves of OVA- and HDM-treated Nf1^OPG mice exhibited reduced volumes (Fig. 1b) and proliferation (%Ki67⁺ cells; Fig. 1c), without changes in microglia (%Iba1⁺ cells, Fig. 1c) or T cell (CD3⁺ cells/nerve) (Fig. 1c) content. Importantly, this decrease in optic nerve volume and proliferation was also observed at 24 weeks (18 weeks after asthma induction) (Fig. 1d–f), demonstrating a durable effect on gliomagenesis.

Interestingly, optic nerve volumes and proliferation did not return to wild-type (WT) levels following asthma induction. Since Nf1^OPG mice, like patients with NF1-OPG, are heterozygous for a germline Nf1 gene mutation in every non-neoplastic cell in their bodies, we analyzed the optic nerves of mice with a germline Nf1 mutation (Nf1^+/− mice). These Nf1^+/− mice have increased optic nerve volumes by direct measurements (Supplementary Fig. 2a, b) and increased optic nerve areas by magnetic resonance imaging (Supplementary Fig. 2c), similar to some patients with NF1 (Supplementary Fig. 2d)¹⁴. In addition, Nf1^+/− mouse optic nerves had increased microglia content (%Iba1⁺ cells; Supplementary Fig. 2e), but no change in proliferation (%Ki67⁺ cells; Supplementary Fig. 2f) or T cell content (CD3⁺ cells; Supplementary Fig. 2g) relative to WT mice, thus providing a clear separation of mice with optic gliomas (Supplementary Fig. 2h, i). In this regard, OVA- and HDM-mediated asthma induction reduces optic nerve volumes and proliferation to levels comparable to Nf1^+/− mice (Supplementary Fig. 2j, k), thus establishing that asthma blocks optic glioma formation.

Asthma reduces Nf1 ^OPG Ccl5, but not Ccl4, levels

Prior studies using Nf1^OPG mice revealed that optic glioma progression and maintenance requires T cells and microglia. In this manner, T cells are activated by Nf1-mutant neurons through the production of Ccl4 that stimulates microglia to produce Ccl5 (Supplementary Fig. 3a), the critical growth factor required for Nf1-optic glioma formation and continued growth^10,11,12. To establish where T cells are activated to express Ccl4, we analyzed Ccl4 RNA expression in the blood, optic nerves, and draining cervical lymph nodes of Nf1^OPG mice (Fig. 2a, b). Consistent with our previous findings that Nf1^+/− neurons (retinal ganglion cells) stimulate T cells to produce Ccl4, the highest levels of Ccl4 were observed in the optic nerves (Fig. 2b).

Next, to determine whether experimental asthma attenuates the increase in Ccl4 and Ccl5 expression observed in the optic nerves of Nf1^OPG mice at 12 (Fig. 2c and Supplementary Fig. 3b, c) and 24 (Supplementary Fig. 3d, e) weeks of age, quantitative real-time PCR was performed. No change in Ccl4 expression at either 12 (Fig. 2d) or 24 (Supplementary Fig. 3f) weeks of age were observed, indicating that OVA and HDM treatment does not affect T cell Ccl4 production. In striking contrast, Ccl5 expression was reduced in the optic nerves of Nf1^OPG mice following OVA and HDM treatment at 12 (Fig. 2e) and 24 (Supplementary Fig. 3g) weeks of age. As expected, Ccl4 levels were increased in the draining cervical lymph nodes of Nf1^OPG mice relative to WT controls (Fig. 2f); however, Ccl4 expression was unchanged following OVA and HDM exposure (Fig. 2g). Importantly, OVA or HDM treatment does not induce a switch between conventional microglia phenotypes (M1 and M2) (Supplementary Fig. 3h–l). The findings reveal that experimental asthma induction impairs microglia Ccl5 support of optic glioma formation and growth without altering T-cell Ccl4 expression.

Asthma reduces T cell induction of Ccl5 in microglia

T cell Ccl4 production in Nf1^OPG mice results from either T cell activation (Supplementary Fig. 4a, b) or Nf1-mutant neuron production of the pleiotrophin family member, midkine (Mdk), in the setting of Nf1-OPG (Fig. 3a)¹². Consistent with unchanged T cell Ccl4 levels following experimental asthma induction, Mdk levels were similar in OVA- and HDM-treated Nf1^OPG mice relative to controls (Fig. 3b), and Mdk does not induce Ccl5 production in microglia (Supplementary Fig. 4c). In addition, naive T cells from PBS-treated (controls) and OVA-treated Nf1^OPG mice responded similarly to Mdk stimulation, producing equivalent levels of Ccl4 (Fig. 3c).

Since there were no changes in MDK expression, we then sought to determine whether the impaired microglia Ccl5 production resulted from other potential changes in the immune microenvironment of Nf1-optic gliomas. First, it is conceivable that experimental asthma induction alters T cell population infiltration into the optic nerves. Previously, we demonstrated that CD8⁺ T cells predominate in Nf1-optic gliomas (Supplementary Fig. 4d)¹², which was unaffected in Nf1^OPG mice following either OVA or HDM treatment (Fig. 3d, e). In addition, no Foxp3⁺ cells (Tregs) were observed in optic gliomas from Nf1-OPG mice treated with PBS, HDM, or OVA (Supplementary Fig. 4e). Second, it is possible that known suppressors of microglia function, like TGFβ¹⁵, or other inflammatory mediators^16,17,18 induced by asthma could be responsible. Treatment of microglia with either TGFβ alone or in combination with Ccl4 had no effect on Ccl5 expression (Supplementary Fig. 4f). While IL-3, but not IL-4 or IL-5, was induced in T cells following OVA treatment (Supplementary Fig. 4g–i), IL-3 treatment had no effect on either T cell Ccl4 or microglia Ccl5 expression (Supplementary Fig. 4j, k). Third, asthma induction could increase peripheral macrophage infiltration; however, no change in Tmem119⁺ cell (microglia) content was observed following OVA or HDM treatment (Supplementary Fig. 4l). Moreover, splenic macrophages fail to induce Ccl5 expression following Ccl4 treatment (Supplementary Fig. 4m). Similarly, OVA and HDM treatments had no effect on other functions of microglia, such as phagocytosis and viability (Supplementary Fig. 4n, o).

To test whether T cells from Nf1^OPG mice exposed to OVA or HDM could induce Ccl5 expression in microglia, we incubated naive microglia with antibody-mediated activated T cell-conditioned medium (TCM) from OVA- or HDM-treated Nf1^OPG mice. Consistent with the whole tissue results demonstrating reduced Ccl5 expression in the optic nerves of Nf1^OPG mice following OVA or HDM treatment, CD3⁺ TCM from both OVA (Fig. 3f) and HDM (Fig. 3g) mice reduced microglia Ccl5 expression. Moreover, this TCM attenuation of Ccl5 was observed in both CD4⁺ and CD8⁺ T cell populations following experimental asthma induction in Nf1^OPG mice (Fig. 3h, i).

Asthma induces T cell decorin expression to inhibit microglia Ccl5 production

Since T cell Ccl4 levels were not reduced by experimental asthma induction, we hypothesized that OVA- and HDM-treated Nf1^OPG mouse T cells might produce an inhibitor of microglia Ccl5 production. To identify this inhibitor, we performed bulk RNA sequencing on isolated spleen CD3⁺ T cells from Nf1^OPG mice treated with PBS (control) or OVA (asthma induction) (Fig. 4a and Supplementary Fig. 5a, b). Following filtering of differentially expressed transcripts (P values ≤ 0.01, false discovery rate ≤ 0.05, and log fold change ≥ 5), only one of the top 20 differentially expressed genes was predicted to be secreted (Fig. 4b). This gene, decorin (Dcn), is a member of the small leucine-rich proteoglycans (SLRPs)¹⁹, originally identified as a collagen-binding protein²⁰. Importantly, loss of decorin attenuates asthma in mice²¹, and OVA treatment of Dcn-deficient mice results in diminished lung pathology relative to WT mice²².

**Fig. 4: Asthma-induced T cell decorin inhibits microglia Ccl5 level.**

As predicted by the RNA sequencing results, Dcn RNA expression was increased in CD3⁺ T cells from the spleen (Supplementary Fig. 5c–e), cervical lymph nodes (Supplementary Fig. 5f–h), and optic nerve (Supplementary Fig. 5i–k) of OVA- and HDM-treated Nf1^OPG mice. Consistent with the ability of both CD4⁺ and CD8⁺ TCM to suppress microglia Ccl5 expression, both CD4⁺ and CD8⁺ splenic T cells from OVA-treated Nf1^OPG mice exhibited elevated Dcn levels relative to control PBS-treated mice (Fig. 4c). Relevant to the human condition, DCN expression was also increased in CD4⁺ and CD8⁺ T cells from patients with non-steroid-dependent asthma relative to healthy controls (GSE31773; Fig. 4d).

With similar levels of decorin (Dcn) RNA expression in the blood, optic nerves, and draining cervical lymph nodes of Nf1^OPG mice (Fig. 4e), we next wanted to determine whether decorin could directly suppress microglia Ccl5 production. Decorin protein levels were measured in the T cell-conditioned medium (TCM) from OVA-treated Nf1^OPG mouse CD3⁺ T cells relative to their PBS-treated counterparts (Fig. 4f).

Using the concentration (800 pg/ml) of decorin detected in OVA-treated Nf1^OPG mouse CD3⁺ TCM, we found that microglia Ccl5 production was reduced to 400 pg/ml (40% decrease; Fig. 5a)—levels previously shown not to increase Nf1 mouse optic glioma stem cell growth in vitro¹². To further explore the direct effect of decorin on microglia Ccl5 production, we quantified Ccl5 expression in primary microglia in response to Ccl4 exposure over a range of decorin concentrations in vitro (Fig. 5b). In contrast, other members of the SLRP family, specifically biglycan (Bgn), were not induced in OVA-treated Nf1^OPG mice relative to PBS controls (Supplementary Fig. 6a), and biglycan did not reduce microglia Ccl5 production (Supplementary Fig. 6b). Taken together, these results demonstrate that T cells from Nf1^OPG mice treated with HDM or OVA produce decorin, which impairs the ability of T cells to stimulate microglia, thus interfering with a tumor supportive microenvironment for murine Nf1-optic glioma formation.

**Fig. 5: Decorin inhibits *Nf1*-OPG formation.**

Since the receptors for Ccl4 (Ccr5 and Ccr8) are both expressed in microglia, we sought to determine which receptor might be responsible for decorin-mediated suppression of Ccl4 induction of microglia Ccl5. While decorin (DCN) treatment reduced microglia Ccl5 production, the addition of a Ccr8 inhibitor (MCV) had no further effect in suppressing microglia Ccl5 production. In contrast, the addition of a Ccr5 inhibitor (AZ058) further reduced activated T cell media-induced microglia Ccl5 levels (Fig. 5c). Based on these results, we conclude that decorin binds to the Ccr8 receptor to reduce microglia Ccl5 production (Fig. 5d).

To demonstrate that decorin is sufficient to block optic glioma formation, Nf1^OPG mice were treated with decorin (1 mg/ml) from 4 to 6 weeks of age, and then analyzed at 12 weeks of age (Fig. 5e). As observed in the experimental models of asthma (OVA and HDM induction) where decorin expression was induced in T cells, decorin treatment of Nf1^OPG mice reduced tumor proliferation (%Ki67⁺ cells), with no change in optic nerve volumes, microglia (Iba1⁺ cells), or T cells (CD3⁺ cells) in vivo (Fig. 5f, g).

Decorin inhibits microglia Ccl5 production through NFκB inhibition

Since T cell Ccl4 induction of microglia Ccl5 production is controlled by NFkB activation in microglia¹², we measured NFκB activation (IκBα^Serine32 phosphorylation) in the optic nerves of Nf1^OPG mice relative to their WT counterparts. While NFκB activation was higher in Nf1^OPG mouse optic nerves compared to WT controls (Fig. 6a), optic nerves from OVA-treated Nf1^OPG mice had reduced NFκB activation in vivo (Fig. 6b). Consistent with decorin suppression of Nf1^OPG microglia NFκB activation, the addition of decorin (800 pg/ml) reduced microglia NFκB activation (Fig. 6c), p65-NFκB activation (Ser⁵³⁶ phosphorylation; Fig. 6d), and p65-NFκB nuclear location (Fig. 6e, f) following activated T cell-conditioned medium (TCM) exposure in vitro. Similarly, both decorin (Supplementary Fig. 6c) and NFkB inhibition (CAPE; Supplementary Fig. 6d) blocked Ccl4 induction of microglia Ccl5 expression in vitro. In addition, NFkB inhibition has no effect on microglia viability (Supplementary Fig. 6e).

**Fig. 6: Decorin suppresses *Nf1*-OPG formation through microglia NFkB inhibition.**

Lastly, to directly demonstrate that NFκB activation is necessary for Nf1-optic glioma formation, Nf1^OPG mice were treated with a commercial NFκB inhibitor (10 mg/kg CAPE) from 4 to 6 weeks of age, and analyzed at 12 weeks of age (Fig. 6g). Similar to both decorin-treated and OVA/HDM-induced Nf1^OPG mice, NFκB inhibitor (CAPE) treatment blocked tumor formation (optic nerve volumes, Fig. 6h; tumor proliferation, %Ki67⁺ cells, Fig. 6i). To demonstrate that decorin suppresses T-cell-mediated microglia production of CCL5 by inhibiting NFκB activation, we show that NFκB inhibition reduces Nf1^OPG Ccl5 expression (Fig. 6j). However, in contrast to the decorin results, NFκB inhibitor treatment also reduced microglia (%Iba1⁺ cells) and T-cell (CD3⁺) content within the optic nerves of Nf1^OPG mice relative to the vehicle-treated groups (Fig. 6i), likely reflecting the effect of NFκB inhibition on microglia and T cell migration^23,24.

Discussion

Collectively, the findings presented in this report suggest a model in which brain cancer risk is modified by alterations in circulating T cell function (Fig. 6k), specifically by interfering with immune cell (T lymphocyte-microglia) communication critical for the establishment of a microenvironment supportive of glioma growth. In this manner, we provide a mechanistic explanation for the reported epidemiological risk association between asthma and a reduced incidence of brain tumors in children with and without NF1^25,26,27. Second, while allergen-induced asthma is typically linked to CD4⁺ T cell responses²⁸, the majority of the T cells in the murine Nf1^OPG tumors are CD8⁺ T cells^9,12. Since CD8⁺ T cells also have complementary roles in asthma and autoimmune conditions^29,30,31 and both murine and human CD4⁺ and CD8⁺ T cells both exhibit increased decorin expression in the setting of asthma, future studies will be required to define the individual contributions of each T cell population to the suppression of microglia-mediated optic gliomagenesis. Third, the discovery that decorin, an SLRP critical for experimental asthma induction in mice and elevated in patients with asthma, has an opposing role in glioma biology, raises the intriguing possibility that specific molecules important for causing systemic inflammatory and autoimmune diseases have different effects in the setting of brain cell axis function. In asthma, decorin potentiates IFNγ activity^32,33, such that decorin-deficient mice have reduced lung tissue inflammation²¹, while in cancer, it has anti-oncogenic properties, including the prevention of metastatic spread and angiogenesis^34,35,36. While the mechanism underlying decorin suppression of NFκB activity in response to CCL4 engagement of its cognate G protein-coupled receptor, CCR5¹² remains to be elucidated, decorin functions in other cell types to block receptor tyrosine kinase (insulin-like growth factor receptor-1, c-MET, and epidermal growth factor receptor) signaling^37,38,39. Lastly, the findings described in this report add to a growing literature implicating T lymphocyte in brain function, including learning^40,41 social behavior^42,43 and neurodegeneration in the setting of neuronal injury^44,45. In this manner, it is conceivable that other systemic conditions involving T lymphocytes, such as eczema^26,46,47, rheumatoid arthritis^48,49, and diabetes^50,51, may similarly impact gliomagenesis through overlapping or related mechanisms. Defining the molecular etiologies underlying how these T cell-mediated systemic conditions influence brain function and nervous system disease pathogenesis may also reveal unique immunomodulatory treatment strategies for neurological disorders.

Methods

Mice

Nf1^flox/mut; GFAP-Cre (Nf1^OPG) mice (Nf1^+/− mice with somatic Nf1 gene inactivation in neuroglial progenitors at E15.5), Nf1^+/− mice (neomycin sequence insertion within exon 31 of the murine Nf1 gene), and Nf1^flox/flox mice (controls)^6,12 were used in accordance with an approved Animal Studies Committee protocol at Washington University in St. Louis. All mice used in these experiments were maintained on a strict C57BL/6 background and were housed in a specific pathogen-free barrier facility with controlled light-dark cycles (12:12 h) and ad libitum access to food and water.

Experimental mouse asthma models

Two different allergen challenges were used to induce experimental asthma in Nf1^OPG mice. For the ovalbumin (OVA)-induced asthma model, mice were intraperitoneally injected with 0.5 mL of chicken egg ovalbumin (16 μg/mL) in aluminum hydroxide (2 mg/mL) weekly for two weeks (days −14 and −7), as previously reported⁵². On day 0, mice were anesthetized with an intraperitoneal injection of ketamine (100 mg/kg) and xylazine (10 mg/kg). After a desired level of anesthesia was achieved and verified by loss of the toe pinch reflex, 30 μl of ovalbumin in PBS was administered intranasally. Mice received a total of four intranasal doses of ovalbumin (2 doses, 12 h apart on day 0; 1 dose on day 1; and 1 dose on day 2). For the house dust mite (HDM)-induced asthma model^53,54, mice were anesthetized as described above and one dose of 1 µg HDM in PBS was given intratracheally (day 0). From days 6 to 10, mice were anesthetized and 40 μl of HDM solution (10 μg/ml) in PBS was administered intranasally. Optic nerve and lungs were harvested at 12, 24 weeks of age. Lungs were analyzed for asthma induction, while optic nerves were used for Iba1, Ki67, CD3, CD4, and CD8 analysis by counting the number of immunoreactive cells by immunohistochemistry.

Mouse treatments

Four-week-old Nf1^OPG mice were treated with 10 mg/kg NFκB inhibitor (NFκB-IN; Caffeic acid phenethyl ester, Fisher Scientific, 274310) or 1 mg/ml Decorin (R&D System 1060-DE-100) intraperitoneally every other day for 2 weeks between 4 and 6 weeks of age. Brains and optic nerves were harvested when mice reached 12 weeks of age, and Iba1, Ki67, and CD3-positive cells were analyzed by counting the number of cells showing a positive signal after immunohistochemistry.

Optic nerve volume analysis

Micro-dissected optic nerves were photographed using Leica DFC 3000 G camera. Measurements were performed using Image-J software beginning at the chiasm (D0) and at 150 (D150), 300 (D300) and 450 µm (D450) anterior to the chiasm to generate optic nerve volume estimates, as previously reported⁷. The volumes for regions 1, 2, and 3 calculated at the three 150 µm high truncated cones were combined using the diameter (D0, D150, D300, and D450) values from each optic nerve measurement. The following equation was used to calculate the total optic nerve volume:

$$V1=\frac{1}{12}\,\pi h({D}_{0}^{2}+{D}_{0}{D}_{150}+{D}_{150}^{2})$$

Human magnetic resonance imaging

T2-weighted axial magnetic resonance images from patients managed at the St. Louis Children’s Hospital Neurofibromatosis Clinical Program (D.H.G.) were de-identified. The MRI scans were de-identified images from children cared for at the St. Louis Children’s Hospital NF Clinical Program. No IRB consent is required, as the use of anonymized human samples is not considered human subjects research by the Washington University IRB.

Mouse magnetic resonance imaging

Mice were intraperitoneally injected with 70 mM MnCl₂ in 100 mM Bicine, pH 7.4 at 140 mg/Kg body weight (10x μL) 16–24 h before imaging. Mice were then subcutaneously injected with 0.5 mL 0.9% saline to minimize magnesium toxicity, and half of the mouse cage was placed on a medium heating pad setting. T1-weighted images (T1W) were collected as previously reported⁵⁵. T1W were collected with 2D spin-echo (SEMS, at 4.7 T): TR/TE, 300 ms/11 ms; matrix size, 128 × 128; FOV, 16 × 16 mm²; slice thickness, 0.5 mm; averages, 16 × 2 (10 × 2 min.). In addition, the 3D T1W were collected using a gradient-echo sequence (GE3D): Matrix size, 128 × 128 × 128; FOV, 24 × 24 × 24 mm³; TR/TE, 4 ms/2 ms; Flip angle, 12°; averages, 8 (9 min). All image data were zero-padded and applied with a Gaussian filter (Sigma 0.75) before conversion to a NIfTI format for analysis.

Immunohistochemistry, H&E, and PAS staining

Nf1^OPG mice were euthanized and transcardially perfused with Ringer’s solution, followed by 4% paraformaldehyde (PFA). Optic nerves and lungs were harvested and processed for paraffin embedding and sectioning in either the Ophthalmology (optic nerves) or Pulmonary Morphology (lungs) core facilities. H&E and PAS staining were performed as previously reported^8,12,52,53. Serial 4-μm paraffin sections of the optic nerve were immunostained with the antibodies listed in Supplementary Table 1. Development was performed using the Vectastain ABC kit (Vector Laboratories, PK4000), and imaged for quantitation in Zeiss AxioScan-Z1 and Leica ICC50W microscope using LAS EZ software.

T cell isolation

Mouse spleens were homogenized into single-cell suspensions by digesting in PBS containing 0.1% BSA and 0.6% Na-citrate, washed, and incubated with 120 Kunitz units of DNase I for 15 min following red blood cell lysis (eBioscience, 00433357)¹². Cells were then filtered through a 30-µm cell strainer to generate a single-cell suspension. CD4⁺ and CD8⁺ T cells were isolated using CD8a (Miltenyi Biotec, 130-104-075) and CD4 (Miltenyi Biotec, 130-117-043) T cell isolation kits, respectively. T cells were maintained at 2.5 × 10⁶ cells/ml in RPMI-1640 medium supplemented with 10% FBS and 1% P/S. T cells were activated using 1.25 µg/ml anti-mouse CD3 (Fisher Scientific, 16-0031-85) and 2 µg/ml anti-mouse CD28 (Fisher Scientific, 16-0281-82) antibody treatment for 2d. Recombinant mouse midkine (R&D Systems, 9760-MD-050) was added, and Ccl4 levels were quantitated by ELISA (R&D Systems, MMB00). Conditioned medium was collected from activated T cells for chemokine assays and microglia co-culture experiments. Cell viability was measured using a commercial WST-1 cell viability assay (Millipore).

Microglia isolation

Microglia were isolated from mouse brains as previously described¹². Briefly, mouse brains were perfused with D-PBS (Fisher Scientific, 14287072), and single-cell suspensions were generated using the multi-tissue dissociation kit (Miltenyi-130-110-201), as per the manufacturer’s protocol. The resulting cells were maintained in minimal essential medium supplemented with 1 mM l-glutamine, 1 mM sodium pyruvate, 0.6% d-(+)-glucose, 1 ng/ml GM-CSF, 100 μg/ml P/S, and 10% FBS for 2 weeks. Microglia were separated from astrocytes by shaking (200 g, 5 h, 37 °C) after 2 weeks. In total, 5 × 10⁵ microglia were grown in T cell-conditioned media (TCM) for 48 h^8,9, followed Ccl5 (R&D Systems, MMR00) and decorin (Abcam, ab155454) determinations by ELISA. Mouse recombinant Decorin protein (R&D Systems, 1060-DE-100), AZ084(CCR8IN; MedChemExpress, CAS No-929300-19-6), Maraviroc (CCR5IN; MedChemExpress, CAS no-376348-65-1) was added to the TCM microglia co-culture, and Ccl5 levels were quantified by ELISA. Mouse recombinant CCL4 (R&D Systems, 451-MB-010/CF), Mouse recombinant Biglycan (R&D Systems, 8128-CM-050), Mouse recombinant TGFβ1 (R&D Systems, 7666-MB-005), Caffeic acid phenethyl ester (NFκB-IN; Fisher Scientific, 274310) was added to the Viability were added to the microglia and Ccl5 levels quantified by ELISA. Viability was determined using WST-1 assay reagent (Abcam, ab155902).

Phagocytosis assay

Phagocytosis was determined using green fluorescent latex beads (Sigma, L1030-1ML) pre-opsonized in fetal bovine serum (FBS) (1:5 ratio) for 1 h at 37 °C at a ratio of 1:5 before dilution to a final concentration of 0.01% (v/v) and 0.05% (v/v) in DMEM. Purified microglia were plated at a density of 50,000 cells/cm², as previously reported¹¹. After 24 h, the cells were incubated with fluorescent latex beads in FBS for 1 h at 37 °C, washed, and then fixed in 4% PFA for 15 min. Microglia were blocked prior to incubation with primary antibody (Iba1,1:200 Wako Chemicals 019-1794, Japan) overnight at 4 °C, washed, and then incubated with secondary antibody for 1 h. Images were acquired on a Leica DFC3000G fluorescent microscope using a ×10 objective with associated Leica Application Suite X software. The number of phagocytic cells with beads relative to the total number of cells was calculated and expressed as a percentage: N_{cell with beads}/N_total.

RNA extraction and real-time qRT-PCR

RNA was isolated from cells and transcardially perfused optic nerves using the NucleoSpin® RNA Plus kit (Takara- 740984.205), as per the manufacturer’s instructions. Total RNA was then reverse transcribed into cDNA using the Applied Biosystems High-Capacity cDNA Reverse Transcription Kit (#4374967), as per the manufacturer’s instructions. Real-time quantitative PCR (qPCR) was performed by TaqMan gene expression (Supplementary Table 2). ΔΔCT values were calculated using Gapdh as an internal control.

RNA sequencing and analysis

RNA from PBS- and OVA-treated spleen CD3⁺ T cells was isolated and sequenced on an Illumina HiSeq platform. Base calls and demultiplexing were performed with Illumina’s bcl2fastq software, and a custom python demultiplexing program with a maximum of one mismatch in the indexing read. The analysis was generated using Partek Flow software, v9.0. RNA-seq reads were aligned to the Ensembl release 99 top-level assembly with STAR v2.6.1d. Gene counts and isoform expression were derived from Ensembl output. Sequencing performance was assessed for the total number of aligned reads, the total number of uniquely aligned reads, and features detected⁵⁶. Normalization size factors were calculated for all gene counts by median ratio. Differential genetic analysis was then performed using DESeq2 to analyze for differences between conditions⁵⁷. Results for OVA samples compared separately with controls were filtered for only those genes with P values ≤ 0.01, false discovery rates ≤ 0.05, and log fold changes ≥ 5.

Human microarray analysis

Raw Affymetrix U133 Plus 2.0 microarray data were obtained from the Gene Expression Omnibus (GSE31773) derived from samples of circulating CD4⁺ and CD8⁺ T cells from non-severe asthma patients (perfect control of their asthma with 0–1000 μg/d inhaled beclomethasone or an equivalent dosage; n = 4; donors 1–4) and healthy control (n = 5; donors 1, 3, 4, 6, 8) subjects⁵⁸. The analysis was performed using Partek Flow software, v9.0. mRNA was aligned to the Ensembl release 100 top-level assembly with STAR v2.7.3a. Gene counts and isoform expression were derived from Ensembl output. Non-coding RNA data were excluded from further analysis. Normalization size factors were calculated for all gene counts by CPM to adjust for differences in library size. Gene-specific analysis was performed using the lognormal with shrinkage model (limma-trend method) to analyze for differences between disease and cell-type conditions. The GSA (gene-specific analysis) results were filtered for the DCN gene. The cut-off used for significance was P value ≤ 0.05.

Western blotting

Total protein was extracted using RIPA buffer and quantified using the Pierce BCA protein assay kit (Fisher scientific, PI23225). Subcellular fractions were isolated following the manufacturer’s protocol (Thermo scientific 78840). In all, 40 µg of total protein lysate was separated in precast SDS-polyacrylamide gels by electrophoresis and transferred onto PVDF membranes, followed by blocking and incubation with the indicated antibody (Supplementary Table 1) overnight. Proteins were detected with IRDye-conjugated secondary antibodies in LI-COR Odyssey Imaging system using Image Studio v5.2.

Statistical analysis

Data were analyzed using GraphPad Prism software. To determine differences between two groups, two-tailed Student’s t test was used whereas multiple comparisons were analyzed by one-way analysis of variance (ANOVA) with Dunnett’s multiple comparisons test. Statistical significance was set at P ≤ 0.05. All experiments were independently repeated at least three times.

Reporting summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

Data availability

The RNA-seq data were deposited in GEO (Accession number 166551). The Raw Affymetrix U133 Plus 2.0 microarray data used in this study are available in the GEO database under accession code GSE31773. The remaining data are available within the Article, Supplementary Information or Source Data file. Source data are provided with this paper.

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Acknowledgements

This work is funded by a grant from the National Institute of Neurological Disorders and Stroke (1-R35-NS07211-01 to D.H.G.) and National Heart, Lung, and Blood Institute (R35-HL145242 to M.J.H.). E.C. was supported by NIH T35 NHLBI Training Grant (5-T35-HL007815) and a POST grant from Alex’s Lemonade Stand Foundation. We thank the Genome Technology Access Center in the Department of Genetics at Washington University School of Medicine for help with genomic analysis. The authors thank the Ophthalmology and Pulmonary Morphology Cores at the Washington University School of Medicine for tissue processing. The Washington University Ophthalmology Core facility support is supported by funding from the National Eye Institute (P30EY002687), while the Washington University Genome Engineering and iPSC Core Center is subsidized by funding from an NCI Cancer Center Support Grant (P30-CA091842) and by ICTS/CTSA Grant# UL1TR002345 from the National Center for Research Resources (NCRR), a component of the National Institutes of Health (NIH), and NIH Roadmap for Medical Research. This publication is solely the responsibility of the authors and does not necessarily represent the official view of NCRR or NIH. We thank Washington University Center for Cellular Imaging (WUCCI) supported by Washington University School of Medicine, The Children’s Discovery Institute of Washington University and St. Louis Children’s Hospital (CDI-CORE-2015-505 and CDI-CORE-2019-813), and the Foundation for Barnes-Jewish Hospital (3770 and 4642). Figure illustrations were created with BioRender.com.

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Department of Neurology, Washington University School of Medicine, St. Louis, MO, USA
Jit Chatterjee, Shilpa Sanapala, Olivia Cobb, Alice Bewley, Andrea K. Goldstein, Elizabeth Cordell & David H. Gutmann
Mallinckrodt Institute of Radiology, Washington University School of Medicine, St. Louis, MO, USA
Xia Ge & Joel R. Garbow
Department of Pulmonary and Critical Care Medicine, Washington University School of Medicine, St. Louis, MO, USA
Michael J. Holtzman

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Contributions

Conceptualization: J.C. and D.H.G.; methodology: J.C. and M.J.H.; writing: J.C. and D.H.G.; investigation: J.C. performed most of the experiments; S.S., A.K.G., and E.C. performed some of the mouse and immunohistochemistry experiments; O.C. performed the mouse RNA sequencing analysis; A.B. performed the human RNA sequencing analysis; X.G. and J.R.G. performed the mouse MRI analysis. Resources: D.H.G.; supervision: D.H.G.; funding: D.H.G.

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Correspondence to David H. Gutmann.

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D.H.G. has a licensing agreement with the Tuberous Sclerosis Alliance (GFAP-Cre mice). J.C., S.S., A.K.G., E.C., X.G., J.R.G., and M.J.H. declare no competing interests.

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Chatterjee, J., Sanapala, S., Cobb, O. et al. Asthma reduces glioma formation by T cell decorin-mediated inhibition of microglia. Nat Commun 12, 7122 (2021). https://doi.org/10.1038/s41467-021-27455-6

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Received: 10 March 2021
Accepted: 23 November 2021
Published: 08 December 2021
DOI: https://doi.org/10.1038/s41467-021-27455-6

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