1. Immunology and Inflammation

A novel role for lipoxin A4 in driving a lymph node–eye axis that controls autoimmunity to the neuroretina

  1. Jessica Wei
  2. Mary J Mattapallil
  3. Reiko Horai
  4. Yingyos Jittayasothorn
  5. Arnav P Modi
  6. H Nida Sen
  7. Karsten Gronert  Is a corresponding author
  8. Rachel R Caspi  Is a corresponding author
  1. Vision Science Program, University of California, Berkeley, United States
  2. Laboratory of Immunology, National Eye Institute, National Institutes of Health, United States
  3. School of Optometry, University of California, Berkeley, United States
  4. Infectious Disease and Immunity Program, University of California, Berkeley, United States
https://doi.org/10.7554/eLife.51102
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Cite this article
  1. Jessica Wei
  2. Mary J Mattapallil
  3. Reiko Horai
  4. Yingyos Jittayasothorn
  5. Arnav P Modi
  6. H Nida Sen
  7. Karsten Gronert
  8. Rachel R Caspi
(2020)
A novel role for lipoxin A4 in driving a lymph node–eye axis that controls autoimmunity to the neuroretina
eLife 9:e51102.
https://doi.org/10.7554/eLife.51102
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Abstract

The eicosanoid lipoxin A4 (LXA4) has emerging roles in lymphocyte-driven diseases. We identified reduced LXA4 levels in posterior segment uveitis patients and investigated the role of LXA4 in the pathogenesis of experimental autoimmune uveitis (EAU). Immunization for EAU with a retinal self-antigen caused selective downregulation of LXA4 in lymph nodes draining the site of immunization, while at the same time amplifying LXA4 in the inflamed target tissue. T cell effector function, migration and glycolytic responses were amplified in LXA4-deficient mice, which correlated with more severe pathology, whereas LXA4 treatment attenuated disease. In vivo deletion or supplementation of LXA4 identified modulation of CC-chemokine receptor 7 (CCR7) and sphingosine 1- phosphate receptor-1 (S1PR1) expression and glucose metabolism in CD4+ T cells as potential mechanisms for LXA4 regulation of T cell effector function and trafficking. Our results demonstrate the intrinsic lymph node LXA4 pathway as a significant checkpoint in the development and severity of adaptive immunity.

Introduction

Understanding the development of adaptive immune responses to self-antigens is imperative, as prevalence of autoimmunity has increased steadfastly in recent decades (Lerner and Matthias, 2015; Bach, 2002). Posterior autoimmune uveitis accounts for 10–15% of blindness in the Western world and primarily affects working age adults (Durrani et al., 2004; Gritz and Wong, 2004). Autoimmune uveitis is mediated by pathogenic Th1 and Th17 responses to retina-specific antigens, such as interphotoreceptor retinoid-binding protein (IRBP) and retinal arrestin. EAU in mice closely recapitulates human disease. Upon peripheral immunization with retinal antigens in complete Freund’s adjuvant (CFA), T cells are primed in the inguinal lymph nodes that drain the immunization sites. Activated retina-specific T cells then traffic to the eye and elicit inflammation that starts 9–11 days and peaks 14–16 days after immunization (Caspi, 2010).

LXA4 is an endogenous arachidonic acid-derived signaling molecule that exerts anti-inflammatory and pro-resolving activities via formyl peptide receptor 2 (ALX/FPR2) in mice and humans. To control the severity and duration of acute inflammation, cells expressing 5-lipoxygenase (5-LOX) and 12/15-lipoxygenase (12/15-LOX) oxygenate arachidonic acid in tandem to synthesize LXA4 locally. 5-LOX is the only enzyme in mammals that can generate the 5,6 epoxide intermediate leukotriene A4 required for the formation of LXA4 and other epoxide intermediates of several specialized pro-resolving mediators (SPMs) (Wei and Gronert, 2017; Serhan, 2014). Even though 5-LOX also initiates the generation of pro-inflammatory leukotrienes by leukocytes, 5-LOX in the retina has protective roles (Sapieha et al., 2011; Livne-Bar et al., 2017). Emerging evidence indicates that LXA4 is an important tissue-resident pathway in eyes and draining lymph nodes that controls ocular surface inflammation and immune responses, and it is neuroprotective in the retina (Wei and Gronert, 2017; Livne-Bar et al., 2017; Kenchegowda and Bazan, 2010).

The defining functions of LXA4 include inhibition of neutrophil infiltration to the site of inflammation, promotion of macrophage efferocytosis, and reduction of inflammatory cytokine and chemokine production (Serhan, 2014; Serhan et al., 2008). In vitro studies demonstrated that LXA4 and SPMs have a role in T follicular and helper cell differentiation (Nagaya et al., 2017; Chiurchiù et al., 2016), and neutrophil-derived LXA4 was previously shown to inhibit T effector cell responses in lymph nodes in immune-driven dry eye disease (Gao et al., 2015). ALX/FPR2 is expressed on T cells (Ariel et al., 2003), providing a modality for LXA4 regulation of adaptive immunity. However, role of LXA4 and its direct action on T lymphocytes in autoimmune responses has been minimally explored.

Specific aim of this study was to uncover whether and how LXA4 regulates T effector cell function in the pathogenesis of autoimmune uveitis. Here, we report that expression of the homeostatic LXA4 pathway and endogenous LXA4 formation are dynamic and temporally defined in the target tissue, that is the eye, and the inciting lymph nodes that drain the site of immunization. T cells from LXA4-deficient (Alox5-/-) mice exhibited enhanced effector function with augmented cytokine production and altered metabolism that resulted in exacerbated disease, while LXA4 treatment in wild type (WT) mice attenuated development of autoimmune uveitis. The resident LXA4 pathway in draining lymph nodes was identified as a significant regulator of CCR7 and S1PR1, which control egress of T effector cells from lymph nodes. Lastly, LXA4 deficiency as well as LXA4 treatment regulated T cell glycolysis, an essential metabolic pathway required for T effector cell function. Our findings identify novel mechanisms and a homeostatic role for LXA4 in lymph nodes to control the development of adaptive autoimmune responses.

Results

LXA4 is generated during autoimmune uveitis in a time- and site- dependent manner

Changes of SPMs in human blood have been proposed as diagnostic markers of health and disease outcomes (Colas et al., 2014; Norris et al., 2018). Postmortem uveitic retinas are not readily available considering uveitis is not a fatal condition, therefore, we analyzed serum samples from 41 healthy subjects and 78 uveitis patients using ELISA to assess whether LXA4 levels are affected in patients diagnosed with posterior uveitis (Figure 1A). The 78 uveitis patients had posterior uveitis that was either standalone or associated with various primary conditions such as Vogt-Koyanagi-Harada disease (VKH), birdshot chorioretinopathy, panuveitis, intermediate uveitis, choroidopathy and retinopathy. Average serum level of LXA4 in patients were significantly lower than in healthy subjects (p=0.0135). Most uveitis diagnoses (n = 2 to 23 per diagnosis) had mean serum LXA4 levels that were lower than healthy controls, with the exception of VKH. However, differences between individual diagnoses and healthy subjects did not reach significance, except for the group of intermediate uveitis (n = 5, p=0.019). The overall decrease in serum LXA4 level in patients suggests that the LXA4 pathway is physiologically relevant during pathogenesis of posterior segment uveitis.

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LXA4 is generated during autoimmune uveitis in a disease- and tissue- dependent manner.

(A) Bar graph of LXA4 concentration in pg/ml measured in human serum by ELISA. Healthy subjects, n = 41; all uveitis patients, n = 78; and breakdown of uveitis diagnoses within all patient samples, n = 2 to 23 per diagnosis. C57BL/6J mice were immunized with 300 μg IRBP651-670 and tissues collected for analyses on days 10 and 16 post-immunization for panels B-I. (B) Lipidomic analysis of inguinal lymph nodes from naïve and EAU-challenged mice on day 16. Peaks are representative multiple reaction monitoring LC-MS/MS chromatograms for specific ion transitions: LXA4 (m/z 351 > 115), 5-HETE (m/z 319 > 115), 15-HETE (m/z 319 > 175). (C) LXA4 and its pathway markers in pg per mg of tissue in whole eye globes, submandibular lymph nodes, distal (axillary + brachial) lymph nodes, and inguinal lymph nodes quantified by LC-MS/MS from unimmunized naïve and EAU-challenged mice (days 10 and 16). n = 5 per group. (D–E) Temporal expression of Alox5, Alox15 and Fpr2 in (D) retinas, and (E) inguinal lymph nodes during EAU (days 3, 7, 14) in comparison to the respective tissue from naïve mice quantified by RT-PCR. n = 6 per group. (F) Fpr2 expression on CD4+ T cells isolated from inguinal lymph nodes of naive and immunized mice, n = 6 per group. *p<0.05, **p<0.01, One-way ANOVA and Mann-Whitney test.

To investigate the role of LXA4 in posterior autoimmune uveitis, we induced EAU in C57BL/6J WT mice (Caspi, 2010; Caspi, 2003) and quantified LXA4 and pathway-specific metabolite levels in the eye, submandibular lymph nodes, distal lymph nodes and inguinal lymph nodes that drain the immunization sites. Samples were collected from naive and immunized mice at disease onset (day 10) and peak disease (day 16) (Figure 1B and C). LXA4 and its 5-LOX and 12/15-LOX pathway markers (5-HETE and 15-HETE) were significantly elevated in eyes at peak disease compared to naive unimmunized mice (Figure 1C). By contrast, LXA4, 5-HETE and 15-HETE levels were significantly downregulated at peak disease in the inguinal lymph nodes (Figure 1B and C). LXA4 levels did not change in the distal lymph nodes or eye-draining submandibular lymph nodes. Serum was analyzed at onset and peak of EAU (Figure 1—figure supplement 1A) to determine if the induced autoimmune response in mice would replicate changes in serum LXA4 observed in uveitis patients (Figure 1A). While serum LXA4 levels in EAU-challenged mice did not change compared to naïve mice, pathway markers 5-LOX and 15-LOX showed significant and progressive decreases during EAU (naïve vs. EAU day 16, p=0.0078 and p=0.0048 for 5-HETE and 15-HETE respectively). Analytes in lipidomic analysis also included DHA- and EPA-derived SPMs and leukotrienes. Pathway markers for DHA-derived SPMs (4-HDHA, 7-HDHA, 14-HDHA and 17-HDHA) were detected in all tissues, but DHA- or EPA- derived SPMs were not robustly detected or were below the signal-to-noise threshold (5:1) in our method. Leukotriene B4 (LTB4), a 5-LOX product, was detected in lymph nodes of healthy mice and during the time course of EAU (Figure 1—figure supplement 1B). However, unlike LXA4, LTB4 levels did not change significantly in inguinal lymph nodes during EAU pathogenesis. The finding is consistent with our previous lipidomic analysis that identified changes in LXA4, but not LTB4, in eye draining lymph nodes of an immune-driven dry eye disease model (Gao et al., 2015; Gao et al., 2018). Altogether, the current findings indicate selective and differential regulation of LXA4 formation at inductive and effector sites of autoimmunity in EAU.

We next assessed gene expression of the LXA4 pathway during EAU. Retinas and inguinal lymph nodes were harvested from naïve and immunized mice on day 3, day 7, and day 14 post-immunization. Expression of 5-LOX (Alox5), 12/15-LOX (Alox15), and LXA4 receptor (Fpr2) was measured by RT-PCR. In the retina, Alox5 expression was upregulated by approximately five-fold on day 14 post-immunization in comparison to earlier time points and to naive mice (Figure 1D), which directly correlated with upregulation of LXA4 formation in the eye. Alox15 expression remained comparable to naïve mice during the entire time course of EAU, whereas Fpr2 expression changed throughout the time course of EAU, likely reflecting changes in circulating leukocytes populations that express varying levels of Fpr2 in the lymph node, and in temporal regulation of the homeostatic LXA4 pathway by resident cells in the retina.

In the inguinal lymph nodes, Alox5 expression was significantly upregulated on day 3 and day 14 post-immunization, whereas Fpr2 expression was highly upregulated on day 3, but not on day 14 post-immunization (Figure 1E). Increased RNA levels of Alox5 in inguinal lymph nodes did not correlate with 5-LOX activity and LXA4 production as both 5-HETE and LXA4 levels were decreased on day 10 and day 16 (Figure 1C). Since EAU pathogenesis is mediated by retina-specific CD4+ T cells, we evaluated Fpr2 expression on CD4+ T cells isolated from inguinal lymph nodes and found that the receptor expression was significantly upregulated at peak disease in comparison to CD4+ T cells isolated from inguinal lymph nodes of naïve mice (Figure 1F). RNA expression of lipoxygenases (5-LOX and 12/15-LOX) demonstrates selective and temporal modulation of tissue-resident LXA4 pathway during EAU, while increased Fpr2 expression in CD4+ T cells in the inguinal lymph nodes potentiates their ability to interact with LXA4 during the effector phase of the immune response.

Endogenous LXA4 limits development and progression of EAU

In light of LXA4 pathway modulation observed during EAU, we investigated whether endogenous LXA4 deficiency would affect the course of autoimmune uveitis. Alox5-/- mice are LXA4 deficient (Aliberti et al., 2002), since 5-LOX is a necessary enzyme required for LXA4 biosynthesis (Figure 2A). The Alox5-/- mouse line is an established Jackson Laboratory strain that has been used to study the role of leukotrienes and LXA4 in vivo. There are no reports of compensatory upregulation of other eicosanoid pathways (cyclooxygenases, 12-LOX or 15-LOX) in this mouse line. Lipidomic analysis did not detect significant differences in basal levels of 12-HETE, 15-HETE, prostaglandin D2 (PGD2), prostaglandin E2 (PGE2), or thromboxane B2 (TXB2) in inguinal lymph nodes of Alox5-/- mice (Figure 2—figure supplement 1). Low amounts of 5-HETE and LXA4 were detected in Alox5-/- mice (Figure 2A). It is possible that one of the other mouse lipoxygenase enzymes, which do not exist in humans (e.g. 8-LOX), is able to catalyze LXA4 formation in mice with low efficiency. Age-matched Alox5-/- and WT mice were immunized with IRBP651-670 peptide (Mattapallil et al., 2015) and EAU pathogenesis was assessed by fundoscopy. Disease scores of Alox5-/- mice were significantly higher than WT mice starting on day 16 post-immunization, and retinal inflammation in Alox5-/- persisted while inflammation gradually resolved in WT by day 20 post-immunization (Figure 2B). Representative Micron III fundus images of WT and Alox5-/- mice revealed more inflammation in the Alox5-/- eye, with retinal haze resulting from severe cellular infiltration in the retina and vitreous, as opposed to clear vitreous in the WT eye allowing visualization of the underlying retinal folds (Figure 2C). Electroretinography showed that visual function of immunized Alox5-/- mice was significantly impaired compared to WT mice (Figure 2D), in line with the more severe disease phenotype in Alox5-/- mice. Flow cytometric analyses of ocular infiltrating cells revealed that there were significantly more cell infiltrates including CD4+ T cells and CD4+ IFN-γ producing T cells in eyes of Alox5-/- mice than in WT mice on day 18 post-immunization (Figure 2E,F). Lymphocytes from Alox5-/- mice exhibited higher antigen-specific proliferative responses to IRBP651-670 peptide than WT mice, as assessed by 3H thymidine-incorporation assay (Figure 2G). These results demonstrate more severe EAU development in the target tissue and at the site of T cell priming in the absence of LXA4.

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LXA4 deficiency exacerbates disease progression.

(A) Chromatograms from LC-MS/MS analyses showing LXA4 and 5-HETE formation in naïve WT and Alox5-/- mice. (B) Fundoscopy scores of WT and Alox5-/- mice immunized with 150 µg of IRBP651-670. n = 15 per group through day 18, n = 6–9 per group on day 20. Combined from two experiments. (C) Representative Micron III fundus images of immunized WT and Alox5-/- mice taken on day 14 post-immunization. (D) Electroretinography of EAU-challenged WT and Alox5-/- mice measured on day 13 post-immunization following dark adaptation, n = 10 eyes per group. (E) Representative flow plots of CD4+ vs. CD8+ and IFN-γ vs. IL-17A producing CD4+ cells in the eyes of WT and Alox5-/- mice. (F) Flow cytometry analyses of total numbers of ocular infiltrates in EAU-challenged WT and Alox5-/- gated on live cells, CD4+, CD4+ CD44+, CD4+ IFN-γ+, CD4+ IL-17A+ populations, n = 9–10 mice per group. (G) Representative bar graphs of antigen-specific cell proliferation performed on inguinal lymph nodes harvested on day 18 post-immunization from WT and Alox5-/- mice, pooled n = 6–9 mice per group. Showing one representative from three experiments with the same trend. *p<0.05, **p<0.01, Wilcoxon matched-pairs signed rank test and unpaired t test.

LXA4 treatment attenuates development of uveitis

We next assessed if amplifying the LXA4 pathway could limit EAU progression. To this end, WT mice were immunized with IRBP651-670 peptide and were treated with either 1 µg of LXA4 or vehicle control daily, starting on the day of immunization. LXA4-treated immunized mice developed significantly less disease compared to the vehicle-treated group (Figure 3A). Retinal histology assessed by H and E stained sections confirmed that LXA4 treatment conferred protection in comparison to vehicle-treated group (Figure 3B and C). The retinas of vehicle-treated group exhibited more severe cellular infiltration that contributed to retinal folds. In contrast, the posterior segment of eyes from LXA4-treated mice maintained largely normal retinal morphology with no inflammatory exudate resembling that of naïve unimmunized mice, despite presence of intravitreal cell infiltrates consistent with a mild form of uveitis (Figure 3C). Inducible cyclooxygenases-2 (COX-2), a hallmark of many inflammatory diseases, was used as an inflammation marker for the retina. Immunohistochemistry revealed COX-2 localization in the outer plexiform, choroid, retinal pigmented epithelium (RPE) and photoreceptor layers of the eye, while CD4+ T cell infiltration was observed in the choroid, RPE and into the photoreceptor layers (Figure 3D). In LXA4-treated mice, the number of CD4+ T cells and the level of COX-2 expression were significantly reduced in comparison to vehicle-treated mice (Figure 3E).

Figure 3
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LXA4 treatment attenuates the development of uveitis.

Mice were immunized with 300 μg of IRBP651-670 to induce EAU and treated with LXA4 or vehicle control starting on the day of immunization. (A) Clinical scores of retinal inflammation assessed by fundoscopy, n = 10 per group. (B) Histology scores of eyes at peak inflammation, n = 24 per group combined from three experiments. (C) Representative H and E staining of the posterior segment of the eye. 20X, scale bar = 50 µm. (D) Representative immunohistochemistry images of eyes harvested at peak inflammation. Top row: central retina, bottom row: peripheral retina. 10X, scale bar = 100 µm. (E) Fiji quantification of CD4 and COX-2 fluorescence particle intensity of immunohistochemistry images, n = 3–7 per group. (F) Representative flow plots of eyes harvested at peak inflammation. Numbers in green are the total cell counts in the gated population. (G) Total number of ocular infiltrates at peak inflammation, n = 6 experiments (pooled 4–6 mice per group). (H) Bar graphs of proliferation assay performed on lymph nodes harvested at peak inflammation, pooled n = 6 mice per group. Representative assay of 3 separate experiments. (I) Fundoscopy scores of a representative adoptive transfer experiment out of 3. 5 × 106 R161H CD90.1 lymphocytes were activated with antigen IRBP161-180 in vitro for 3 days and transferred into WT CD90.2 recipients. Recipients were treated with indicated doses of LXA4 starting on the day of cell transfer. *p<0.05, **p<0.01, Mann-Whitney test and One-way ANOVA.

Th1 and Th17 are T cell subsets that drive EAU pathogenesis (Damsker et al., 2010). Flow cytometry analyses of eyes harvested during peak inflammation confirmed that LXA4 treatment significantly reduced ocular infiltration of pathogenic IFN-γ and IL-17A producing CD4+ T cells (Figure 3F and G). Immune cells from inguinal lymph nodes of vehicle-treated mice proliferated dose-dependently after IRBP651-670 peptide challenge. In contrast, antigen-specific recall responses of lymphocytes from inguinal lymph nodes of LXA4-treated mice were markedly decreased (Figure 3H).

Since LXA4 treatment reduced antigen-specific recall responses, we investigated whether LXA4 could regulate disease during the effector phase. We used in vitro-activated T cells from T cell receptor transgenic mice that express a receptor specific for IRBP161-180 (R161H) on the B10. RIII background and develop spontaneous uveitis (Horai et al., 2015). Lymph node T cells from CD90.1 congenic R161H mice were cultured with IRBP161-180 peptide for three days in vitro, which resulted in ~70% of IFN-γ producing T cells (data not shown). IRBP-primed cells were injected into B10.RIII WT CD90.2 recipient mice and received either LXA4 or vehicle control treatment starting on the day of cell transfer. LXA4-treated mice developed significantly lower disease in a dose-dependent manner than vehicle-treated mice (Figure 3I). These findings provide direct evidence that LXA4 inhibits the actions of antigen-primed lymphocytes in vivo and also regulates the effector phase of the adaptive immune response.

LXA4 modulates T cell trafficking in inguinal lymph nodes that drain the immunization site

To identify the genes that are regulated by LXA4 treatment, we compared RNA expression in eyes and peripheral lymph nodes from immunized mice treated with LXA4 or vehicle. Tissues were harvested on day 16 post-immunization and gene expression analyzed by nanoString. Eyes of vehicle-treated mice exhibited increased expression of inflammatory markers Icam1, Il1b, Mapk1, Mapk3, Nfkb1, Ptgs2 (Cox-2), Tgfb, Tnfaip3, and Vcam1 in eyes, whereas LXA4 treatment downregulated the expression of these markers during EAU. By contrast, expression of these genes was comparable in the inguinal lymph nodes of vehicle vs. LXA4-treated animals (Figure 4A). These data suggest that systemic LXA4 treatment reduced expression of inflammatory genes in the effector site, that is eyes, but not in the inductive site, that is lymph nodes draining the site of immunization.

Figure 4
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LXA4 modulates T cell trafficking in inguinal lymph nodes that drain the immunization site.

All tissues were collected from mice immunized with 150 μg of IRBP651-670. (A–B) Heat maps showing gene expression of inflammation and cell trafficking markers in the eyes and inguinal lymph nodes harvested from EAU-challenged mice treated with vehicle or LXA4. (A) Inflammation markers and (B) migration markers analyzed by nanoString. Each sample was pooled from 3 to 4 mice on day 16 post-immunization. (C) S1pr1 expression relative to β-actin from eyes and various lymph nodes of mice treated with vehicle or LXA4 harvested on day 16 post-immunization, same samples as panels A and B. (D) Fold change in S1pr1 expression of CD4+ T cells isolated from WT and Alox5-/- on day 14 post-immunization, n = 11 from three experiments combined. (E) Transwell migration assay of CD4+ T cells isolated from immunized WT and Alox5-/- on day 13 post-immunization. CD4+ T cells were pre-stimulated with anti-CD3 and anti-CD28 antibodies for 18 hr and transferred to transwell culture plates and incubated for 4 hr in the absence or presence of CCL19 and CCL21, n = 12 per group. One representative experiment of 4 showing the same trend. **p<0.01, unpaired Welch’s t test. (F–G) Representative flow plots of CCR7 and S1PR1 expression on in vitro anti-CD3 and anti-CD28 stimulated CD4+ T cells treated with vehicle control or 10 nM, 100 nM, 1 μM, and 2 μM of LXA4. Cells were gated on live single cells then CD4+ cells. Gray overlays indicate fluorescence minus one controls. Showing one representative experiment out of three.

Because LXA4 treatment reduced T cell migration into the eye (Figure 3G), we examined gene expression of the T cell trafficking marker Ccr7 and its cognate ligands Ccl19 and Ccl21a, as well as the Th1-associated chemokine receptor Cxcr3, and Th17-associated chemokine receptor Ccr6. Compared to vehicle- treated mice, eyes of LXA4 treated mice had downregulated expression of Ccr7, Cxcr3 and Ccl19 (Figure 4B), which paralleled the reduced numbers of total CD4+ T cells and CD4+ IFN-γ+ T cells in the ocular infiltrate (Figure 3G). In contrast, Ccr7 and Ccl21a were highly upregulated in the inguinal lymph nodes of LXA4-treated mice compared to controls (Figure 4B). We next assessed whether LXA4 treatment also impacts expression of S1pr1, which regulates lymphocyte egress from lymphoid tissues (Garris et al., 2014). LXA4 treatment downregulated expression of S1pr1 in the inguinal lymph nodes that drain the site of immunization, but not in the eye, submandibular lymph nodes that drain the eye, or distal lymph nodes (Figure 4C). To examine whether downregulation of S1pr1 under conditions of LXA4 deficiency can be detected in uveitis-relevant T cells, we assessed S1pr1 expression in CD4+ T cells from inguinal lymph nodes of EAU-challenged Alox5-/- and WT mice by RT-PCR. S1pr1 expression showed a trend of higher expression in CD4+ T cells from Alox5-/- mice (Figure 4D). The opposing expression of lymphocyte migration-associated receptors and ligands between the eyes and the inguinal lymph nodes identifies a potential mechanism for LXA4 to control the magnitude of an adaptive immune response, specifically by regulating of Ccr7 and S1pr1 expression that mediate T cell egress from lymph nodes.

Next, we assessed whether LXA4 deficiency impacts migration of CD4+ T cells from secondary lymphoid tissues in vitro. CD4+ T cells were isolated from inguinal lymph nodes and spleens of EAU-challenged WT and Alox5-/- mice on day 13 post-immunization and stimulated in vitro with anti-CD3 and anti-CD28 for 18 hr prior to being subjected to a transwell migration assay. Significantly higher numbers of CD4+ T cells from LXA4-deficient mice migrated toward CCL19 and CCL21 chemokine gradients than CD4+ T cells from WT mice (Figure 4E). These results suggest that the absence of tissue-resident LXA4 increases migration of activated lymph node T cells and may explain exacerbated EAU in LXA4-deficient mice (Figure 2). To confirm the direct regulation of chemokine receptors on T cells by LXA4, S1PR1 and CCR7 expression was assessed by flow cytometry on in vitro stimulated T cells treated with LXA4. CCR7 expression was modestly upregulated (Figure 4F) while S1PR1 expression was downregulated (Figure 4G) in a dose-dependent manner. Together, these data are compatible with the interpretation that LXA4 acts directly on T cells and modulates trafficking through regulation of S1PR1 and CCR7 expression.

Disease-limiting effect of LXA4 is T cell-mediated

Next, we examined whether enhanced EAU in the absence of LXA4 is a T cell-mediated effect. We immunized WT and Alox5-/- donor mice to expand IRBP-specific T cells, and on day 11 purified CD3+ T cells from inguinal lymph nodes and spleens. The donor T cells were transferred into TCRb-/- mice, which lack their own T cells, and three weeks after transfer the recipients were challenged for EAU with IRBP651-670 peptide (Figure 5A). Consistent with the phenotype of exacerbated EAU in Alox5-/- mice (Figure 2), recipients of Alox5-/- T cells developed more severe EAU, with more granulomatous lesions and damage in the photoreceptor cell layer, than recipients of WT T cells (Figure 5B and C). Similar results, more severe EAU, were also observed in TCRb-/- recipients of Fpr2-/- T cells (Figure 5—figure supplement 1).

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Disease limiting effect of LXA4 is T cell-mediated.

(A) Scheme of T cell transfer. Following EAU induction, 1 × 107 CD3+ T cells were enriched from inguinal lymph nodes and spleens of WT or Alox5-/- mice and injected i.p. into TCRb-/- mice. (B) Fundoscopy scores of WT or Alox5-/- T cell-transferred TCRb-/- recipients immunized with EAU, n = 6 mice per group. (C) Representative H and E histology of the posterior segment of the eye from TCRb-/- recipients of WT or Alox5-/- T cells, scale bar = 50 µm. (D, F) Flow cytometry analysis of total numbers of live cells and frequencies of CD4+ T cell populations producing IFN-γ or IL-17A in (D) eyes and (F) inguinal lymph nodes of WT and Alox5-/- T cell recipients, n = 6 per group. (E, G) Flow cytometry analysis of chemokine receptor expression on activated CD4+ T cells in (E) eyes and (G) inguinal lymph nodes of TCRb-/- recipients of WT and Alox5-/- T cells, n = 6 per group. *p<0.05, **p<0.01, Wilcoxon matched-pairs signed rank test and unpaired Welch’s t test.

To elucidate effector T cell phenotype and expression of trafficking molecules on uveitogenic CD4+ donor T cells, transferred T cells were harvested from eyes and inguinal lymph nodes of TCRb-/- recipient mice on day 20 post-immunization and analyzed by flow cytometry. Eyes of Alox5-/- T cell recipients had significantly more total ocular infiltrates, specifically total CD4+ T cells and IFN-γ producing CD4+ T cells than WT donor T cell recipients (Figure 5D). However, there was no apparent difference in expression of the trafficking markers CXCR3, CCR6 and CCR7 by T cells that had infiltrated the eye (Figure 5E). In the inguinal lymph nodes, the frequency of IFN-γ+ donor CD4+ T cells from Alox5-/- mice, but not total or IL-17A+ donor CD4+ T cells, was higher than that from WT (Figure 5F). Migration marker analysis showed higher frequency of CXCR3+ in Alox5-/- donor CD4+ T cells in the inguinal lymph nodes, whereas frequency of activated CD4+ CCR7+ donor T cells from Alox5-/- mice was significantly lower (Figure 5G). The downregulation of CCR7 expression and increased ocular infiltration of CD4+ T cells support the hypothesis that egress of effector T cells from inguinal draining lymph nodes is augmented in LXA4-deficient mice.

LXA4 pathway regulates the metabolism of CD4+ T cells

T cell metabolic programming closely shapes T cell development and responses. Upon TCR stimulation, activated T cells engage in aerobic glycolysis to support effector T cell function (Almeida et al., 2016; Buck et al., 2015). We investigated whether LXA4 deficiency impacts effector T cell metabolism since our findings indicate that the lymph node resident LXA4 pathway regulates effector T cell function and migration (Figure 4E and 5G). CD4+ T cells were isolated from inguinal lymph nodes and spleens of EAU-challenged WT and Alox5-/- mice and were stimulated for 18 hr with anti-CD3 and anti-CD28 antibodies. Cell metabolism was analyzed by the Seahorse Glycolytic Rate Assay. To accurately quantify glycolysis-derived extracellular acidification rate, mitochondrial CO2-contributed acidification was measured and subtracted from total proton efflux rate, yielding the glycolytic proton efflux rate (glycoPER). CD4+ T cells from Alox5-/- mice achieved significantly higher glycoPER at baseline as well as after inhibition of the mitochondrial electron transport chain with rotenone and antimycin A (Rot/AA) (Figure 6A–C). Seahorse Glycolytic Rate assay was also used to assess the direct effect of LXA4 on T cell glycolysis. CD4+ T cells from WT mice were treated in vitro with LXA4 or vehicle control. LXA4 treated CD4+ T cells had significantly lower glycoPER at base line and after mitochondrial inhibition (Figure 6D), as well as lower basal (Figure 6E) and compensatory (Figure 6F) glycolysis. Thus, both ex vivo evidence from CD4+ T cells of EAU-challenged LXA4-deficient mice and in vitro experiments of LXA4-treated CD4+ WT T cells indicate that lymph node resident LXA4 has a direct role in regulating metabolic functions of CD4+ T cells.

Figure 6
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The LXA4 pathway regulates effector function and metabolism of CD4+ T cells.

Inguinal lymph nodes and spleens were harvested from EAU-challenged WT and Alox5-/- mice on day 13 post-immunization. (A) CD4+ T cells isolated from immunized WT and Alox5-/- mice were stimulated with anti-CD3 and anti-CD28 antibodies for 18 hr then subjected to glycolytic rate assay by Seahorse analyzer, n = 12 mice per group. (B–C) Bar graphs of (B) basal glycolysis and (C) compensatory glycolysis from the glycolytic rate assay in (A). (D) WT CD4+ T cells isolated from immunized WT and Alox5-/- mice were pretreated with vehicle or LXA4 in vitro and stimulated with anti-CD3 and anti-CD28 antibodies for 18 hr then subjected to glycolytic rate assay by Seahorse analyzer, n = 11 mice per group. (E–F) Bar graphs of (E) basal glycolysis and (F) compensatory glycolysis from the glycolytic rate assay in (D). *p<0.05, ***p<0.001, Wilcoxon matched-pairs signed rank test and Mann-Whitney test.

Discussion

In this study, we demonstrate that the resident LXA4 pathway in lymph nodes is important in regulating T cell effector functions during development and progression of ocular autoimmunity. A key finding is the downregulation of basal LXA4 levels in lymph nodes that accompany the adaptive immune response in a mouse model of autoimmune uveitis. Reduced levels of serum LXA4 were also identified in serum of human patients with posterior uveitis diagnoses, suggesting that the LXA4 pathway is dynamically regulated in human uveitis. In contrast, LXA4 levels were elevated in the uveitic eyes of mice, which is consistent with the established role of LXA4 as an induced counter-regulatory mediator that is generated at sites of inflammation. Despite the established role of LXA4 in innate immune cell regulation, direct regulation of adaptive immune responses by endogenous LXA4 is not well defined in vivo, as most research efforts have focused on LXA4’s ability to dampen and resolve acute inflammation elicited by innate immune cells. Beneficial anti-inflammatory effects of LXA4 have been previously reported in the LPS-induced anterior uveitis model, however, pathogenesis of LPS-induced uveitis is driven exclusively by innate immune responses (Karim et al., 2009). In a murine asthma model induced by allergen immunization, LXA4 treatment reduced airway inflammation by increasing natural killer cell-mediated eosinophil apoptosis (Barnig et al., 2013), demonstrating LXA4 regulation of innate responses in vivo. Our data indicate that downregulated endogenous LXA4, specifically in inguinal lymph nodes that drain the immunization site, is a key feature of developing adaptive immunity, that is EAU. This is consistent with a previous report, which linked lower LXA4 levels in draining lymph nodes to exacerbated dry eye disease in female mice (Gao et al., 2015). LXA4-deficient Alox5-/- mice and adoptive transfer in T cell-deficient mice also demonstrated that in vivo disruption of the LXA4 pathway amplifies effector T cell responses in autoimmune uveitis. These experiments provide strong evidence for LXA4 regulation of adaptive immune responses initiated in lymph nodes by demonstrating that (a) LXA4 deficiency causes dysregulated T effector cell function that leads to exacerbated autoimmune pathogenesis and (b) supplementation with exogenous LXA4 reverses this effect. Thus, we identified a new role for LXA4 in T cell-driven adaptive autoimmunity and uncovered a lymph node – eye axis that regulates this process.

It is not possible to capture changes in LXA4 tissue levels after a low dose (1 μg) injection of LXA4 at the time of tissue harvest since increases of LXA4 in eye or lymph nodes are likely rapid and of short duration. LXA4, like all eicosanoids, is enzymatically inactivated in minutes when not bound to an endogenous carrier protein such as albumin. However, several research groups have established that tail vein, intraperitoneal, subcutaneous or subconjunctival injections of LXA4 or other SPMs (10 ng-1 μg) in mouse disease models induce long-lasting protective actions through changes in lymphocyte and neutrophil function and macrophage phenotype at distant tissue sites (Livne-Bar et al., 2017; Serhan et al., 2008; Gao et al., 2015; Fosshaug et al., 2019; Wei and Gronert, 2019), which indicate direct actions at the target tissue.

Our findings provide evidence for LXA4 regulation of T cell trafficking as a potential mechanism for controlling EAU progression. The S1PR1-sphingosine-1 phosphate axis is a primary mechanism for regulating lymph node T cell egress and lymphocyte recirculation. LXA4 treatment selectively downregulated S1pr1 expression only in inguinal lymph nodes of WT EAU-challenged mice. Pharmacological downregulation of S1PR1 prevents trafficking of autoreactive T cells and is an FDA-approved treatment for multiple sclerosis (Garris et al., 2014). Hence, a role of the lymph node LXA4 pathway in regulating S1pr1 expression in lymphocytes warrants further investigation into the crosstalk between these two classes of lipid mediators. The CCR7-CCL19/CCL21 axis facilitates naïve T cell homing to secondary lymphoid organs, activated T cell egress, and the interaction between T cells and dendritic cells (DC) to induce peripheral tolerance or to elicit an adaptive immune response (Comerford et al., 2013). LXA4 treatment differentially regulated this axis at the effector and initiation sites of the adaptive immune response by reducing Ccr7 and Ccl19 expression in the eye and increasing Ccr7 and Ccl21 expression in inguinal lymph nodes.

The endogenous role of LXA4 in regulating effector T cell function through Ccr7 was confirmed with Alox5-/- mice using T cell adoptive transfer and in vitro migration experiments. LXA4 deficiency was coincident with dysregulated (i.e. lower) expression of CCR7 in T cells from inguinal lymph nodes, increased IFN-γ production and an almost two-fold increase of CD4+ T cell migration towards CCL19/21 gradient. Ccr7 is expressed predominantly in DC and T cells, and its ligands CCL19 and CCL21 can be secreted by several cell types. In this study, we did not investigate the cellular source of CCL19 and CCL21 in tissues, the effect of LXA4 on Ccr7 expression in DC or assess direct LXA4 regulation of Ccr7 expression on T cells. LXA4 has established actions with DC and other cell types, therefore, we cannot rule out that LXA4 also controls T cell responses in inguinal lymph nodes through priming by DC and/or regulation of CCL19 and CCL21 production by other cell types.

T cell glycolysis is vital in regulating T cell effector function. Metabolic switch from oxidative phosphorylation to glycolysis is required to sustain T effector function and cytokine production (Coe et al., 2014; Salmond, 2018). Inhibition of glycolysis abrogates IFN-γ production in activated CD4+ T cells, implicating glycolysis as regulator of sustained T effector responses (Chang et al., 2013). LXA4 treatment decreased CD4+ T cells glycolytic responses and reduced IFN-γ production from CD4+ T cells, providing evidence of direct regulation of T cell function by LXA4. Increased glycolytic responses of CD4+ T cells from Alox5-/- mice underscores the relevance of lymph node resident LXA4 in controlling T cell effector function. T cell glycolysis and mitochondrial metabolism as potential therapeutic targets are supported by elevated glycolytic metabolism in T cells of systemic lupus erythematosus (SLE) patients and reduced IFN-γ production and disease biomarkers upon inhibition of CD4+ T cell glycolysis in mouse models of SLE (Yin et al., 2015). The ability of LXA4 to downregulate glycolysis in activated CD4+ T cell is of interest and suggests that the lymph node resident LXA4 pathway is a potential checkpoint to limit inflammatory cytokine production and the magnitude of adaptive immune responses.

In mice and humans, LXA4 cognate receptor ALX/FPR2 is expressed in T cells, B cells and innate lymphoid cells (Wei and Gronert, 2019), and has been shown to regulate CD4+ T cell cytokine production in vitro (Chiurchiù et al., 2016). During peak EAU, Fpr2 expression in CD4+ T cells was highly upregulated in the inguinal lymph nodes that drain the site of immunization, suggesting that increased capacity of LXA4 signaling in T cells is a counter-regulatory mechanism in response to the development of adaptive immunity. Consistent with our hypotheses that dysregulated LXA4 signaling allows for development of EAU and facilitates augmented effector T cell functional responses, adoptive transfer of either Alox5-/- or Fpr2-/- T cells to TCRb-/- recipients caused exacerbated EAU (Figure 5—figure supplement 1A). Transferred T cells from Fpr2-/- and Alox5-/- mice induced different signatures of inflammatory ocular infiltrates (Figure 5—figure supplement 1B and C), likely due to differential regulation of donor T cells and innate effector cells by the host LXA4 pathway in TCRb-/- recipient mice. However, unlike Alox5-/- mice, global Fpr2-/- mice (which generate LXA4) did not develop more severe EAU than WT controls after immunization (Figure 5—figure supplement 1D). A second LXA4 receptor GPR32 has been identified in humans (Dalli and Serhan, 2019), which currently has no mouse homolog. Our data suggest that additional receptors for LXA4 may exist in mice. Incomplete abrogation of LXA4 signaling due to a putative second receptor may explain why immunized global Fpr2-/- mice did not develop more severe autoimmune disease.

EAU is an induced and well characterized model of autoimmune uveitis that recapitulates features of human posterior autoimmune uveitis. Although the immune-regulatory roles of LXA4 in human draining lymph nodes remain to be defined, LXA4 has been identified as an abundant SPM in human axillary lymph nodes (Colas et al., 2014). While it is important to note that there are significant differences in mouse and human immune responses (Seok et al., 2013), LXA4 pathway and receptors are conserved in humans and mice and are targeted as novel therapies based on promising results from animal studies.

In summary, our data established that the basal tone of LXA4 in lymph nodes is selectively downregulated in the draining lymph node during development of an adaptive immune response. We identified regulation of CCR7 and S1PR1 expression and glycolytic responses in CD4+ T cells as new mechanisms for LXA4 to control effector T cell functions and egress from lymph nodes, which establishes LXA4 as an important homeostatic regulator for fine tuning adaptive immune responses. Thus, amplification of the resident lymph node LXA4 pathway may be a potential target to prevent the development of pathogenic adaptive immune responses and autoimmunity.

Materials and methods

Patients and healthy controls

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Male and female patients ages 30–76 with clinical diagnosis of non-infectious posterior segment uveitis were enrolled in the National Eye Institute protocol number 16-EI-0046. Healthy controls were NIH blood bank donors of both sexes with a similar age range. Serum samples were obtained from male and female patients ages 30–76 with clinical diagnosis of non-infectious posterior uveitis, healthy controls were NIH blood bank donors of both sexes with a similar age range whose samples were de-identified and sent to the lab. Patients were enrolled from May 2017 to July 2018 under a clinical research protocol (NCT02656381), approved by the institutional review board of the National Institutes of Health. Informed consent (including publishing language as required by NIH IRB) were obtained from all subjects. The study adhered to the tenets of the Declaration of Helsinki.

Serum ELISA assay

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Serum LXA4 levels were measured by ELISA (Neogen, KY) per manufacturer instruction and read on SpectraMax iD3 microplate reader (Molecular Devices, CA).

Mice, EAU induction and LXA4 treatment

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C57BL/6J mice between 8 and 12 weeks of age were purchased from the Jackson Laboratory and were used as the WT strain. All experimental procedures were approved by the Animal Care and Use Committee at University of California, Berkeley (protocol AUP-2016-04-8691-1), and the National Eye Institute at the National Institutes of Health (animal protocol NEI-581) and are in accordance with the National Institutes of Health Guide for the Care and Use of Laboratory Animals. All animals were maintained on the NIH-31 Open Formula diet: 4.7% Fat, 1.2% monounsaturated fatty acids, 2.1% polyunsaturated fatty acids, with 1.9% C18:2 ω6 linoleic acid and 0.2% C18:3 ω3 linolenic acid (Envigo, WI), starting at 3 weeks of age through the duration of the experiments. For induction of EAU, each mouse was immunized with 150 or 300 µg IRBP651-670 peptide (Genscript, NJ or BioBasic, NY) as indicated, emulsified in CFA supplemented with 2.5 mg/ml Mycobacterium tuberculosis (Sigma, MO), and injected with 1 µg pertussis toxin (Sigma, MO) as reported earlier (Mattapallil et al., 2015). Alox5-/- mice (B6.129S2-Alox5tm1Fun/J, stock number 004155) and TCRb-/- mice (B6.129P2-Tcrbtm1Mom/J, stock number 002118) were purchased from the Jackson Laboratory. Fpr2-/- mice (Dufton et al., 2010) were gifted by Dr. Asma Nusrat from the University of Michigan. For assessing therapeutic effects of LXA4, either 1 µg/100 µl of LXA4 (Cayman Chemical, MI), which was resolved in 100% EtOH and diluted to 10% in PBS, or 100 µl of 10% EtOH in PBS (vehicle control) was injected subcutaneously and intraperitoneally starting at day 0 of disease induction. IRBP-specific TCR transgenic R161H mice (Horai et al., 2013) generated on the congenic CD90.1 B10.RIII background and WT CD90.2 B10.RIII mice (Jackson Laboratory, ME) were maintained in house at the NIH animal facility.

Evaluation of EAU by fundoscopy and histology

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Funduscopic scoring system was used to evaluate activity of inflammation in the retina. Mice were anesthetized with ketamine and xylazine (7:3) and the retinas were examined under a binocular microscope after pupil dilation with tropicamide and phenylephrine. Scores ranging from 0 to 4 were assigned to each eye according to the extent and severity of inflammatory lesions (Agarwal et al., 2012). For histological evaluation, eyes were enucleated, pre-fixed in 4% glutaraldehyde for 1 hr, post-fixed in 10% buffered formalin, embedded in paraffin and processed for H and E staining. Scores were determined in a blinded manner on a scale of 0–4 in half-point increments according to published EAU scoring criteria that are based on the type, size, severity and number of lesions (Caspi, 2003).

Electroretinography and fundus imaging

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Mice were dark-adapted overnight, and experiments were performed under dim red illumination. Electroretinograms were recorded using Espion E2 System (Diagnosys LLC, MA) that generated and controlled light stimuli at 10 cds/m2 for a-wave and b-wave (Chen et al., 2013). A reference electrode was inserted above the tongue, corneal electrodes were placed at the center of corneas with sterile lubricant eye gel applied to the corneal electrodes. The amplitudes of a-wave and b-wave were analyzed and measured using Espion software. Images was captured using Micron III retinal imaging microscope (Phoenix Research Labs, CA) for small rodents.

Tissue harvest and processing

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Eyes, lymph nodes and spleens were harvested from vehicle and LXA4-treated immunized mice 16 days post-immunization after extensive perfusion through the heart. Enucleated eyes were trimmed of lenses and connective tissues, minced and treated with 1 mg/ml collagenase D for 40 min at 37°C. Lymph nodes and spleens were mashed, cells filtered through 40 µm strainers and resuspended to make single cell suspensions. Red blood cells in spleens were lysed with ACK lysis buffer. Whole blood was allowed to clot for 30 min at room temperature. Samples were centrifuged and serum supernatant collected for analysis.

Real-time quantitative PCR

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RNA was isolated from mouse tissues using RNeasy isolation kit (Qiagen, Germany), and reverse transcribed with High Capacity cDNA kit (Applied Biosystems, CA). Mouse β-actin was used as the endogenous reference gene. PCR was performed using Taqman gene expression assays (Thermo Fisher Scientific, MA) with following primer/probe sets. Alox5: Mm01182747_m1, Alox15: Mm00507789_m1, Fpr2: Mm00484464_s1, S1pr1: Mm00514644_m1.

Detection of endogenous formation of eicosanoids

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Whole lymph nodes and eye globes were harvested at disease onset and peak inflammation from mice induced for EAU by immunization with IRBP651-670 peptide. Tissues from naïve mice served as healthy controls. Tissues were homogenized in 66% MeOH containing deuterated internal standards with Bead Ruptor, and lipid mediators were extracted using solid phase C-18 columns. Mouse serum was combined with 2 volumes of ice cold MeOH containing deuterated internal standards. Diluted serum samples were vortexed and incubated at −80°C for 1 hr to precipitate proteins. Supernatants were collected and extracted using solid phase C-18 columns (Gao et al., 2018). Lipid mediators were then quantified by liquid chromatography-tandem mass spectrometry (LC-MS/MS). Extraction recovery was calculated based on deuterated internal standards (PGE2-d4, LTB4-d4, 15-HETE-d8, LXA4-d5, DHA-d5, AA-d8). The LC-MS/MS system was composed of Agilent 1200 series HPLC, Kinetex C18 minibore column (Phenomenex, CA), and AB Sciex QTRAP 4500 mass spectrometer (SCIEX, MA). Analyses were performed in negative ion mode with scheduled multiple reaction monitoring using 4–5 transition ions per lipid mediator (Livne-Bar et al., 2017; von Moltke et al., 2012).

Flow cytometry analyses of T cells

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Single cell suspensions were prepared from isolated tissues. Samples of 1 × 106 cells were stained with anti-mouse antibodies conjugated with following fluorochromes: BV421, BV510/V500, FITC, PE, PerCP-Cy5.5/PerCP-eF710, PE-Cy7, APC, APC Cy7/APC-eF780, BV650/SB645, BV785. Surface staining was performed using antibodies against F4/80, Ly6G, CD3, CD4, CD11b, CD44, CCR6, CXCR3, CCR7, and S1PR1. Ghost Dye UV 450 or Red 780 (Tonbo, CA) were used to exclude dead cells. Intracellular staining was performed after stimulating cells with 50 ng/ml PMA and 1 µg/ml Ionomycin (MilliporeSigma, MA) in the presence of Brefeldin A (Golgi Plug, BD Biosciences, CA) for 4–6 hr at 37°C in cell culture media. Following the surface and viability staining, cells were fixed with 4% paraformaldehyde (PFA) and permeabilized with Triton buffer (0.5% Triton X-100% and 0.1% BSA in PBS). Fluorochrome-conjugated (see above) anti-mouse Foxp3, IL-17A, and IFN-γ were used for intracellular staining. Cells were acquired on BD LSR Fortessa (BD Biosciences, CA), MACSQuant Analyzer (Miltenyi Biotec, Germany), or Cytoflex (Beckham Coulter, CA). Fcs files were analyzed using FlowJo (FlowJo LLC, OR).

Immunohistochemistry

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Tissues were embedded in OCT and cryosectioned into 7 µm sections. Tissues sections were fixed in 4% PFA and blocked with serum prior to primary antibody staining. Primary antibodies against mouse CD4 (Biolegend, CA) and COX-2 (Abcam, UK) were used. Anti-goat AlexaFluor 488 and AlexaFluor 568 (ThermoFisher Scientific, MA) secondary antibodies were used for immunofluorescent labeling. Cells were counterstained with DAPI at 1:3000 dilution (Sigma, MO). Fluorescent images were acquired with a Zeiss AxioImager microscope at 10X and 20X.

Quantitation of immunohistochemistry images

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Images were quantified in Fiji software. Particle mean intensity was measured in each fluorescent channel of retina and choroid tissues. Statistical significance was calculated on 3–7 mice per experimental group.

T cell proliferation assays

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5 × 105 lymph node cells resuspended in HL-1 media (Lonza, GA) were plated in 96-well round bottom plates and stimulated with serial dilutions of IRBP651-670 peptide. Cells were cultured for 2 days and 1 µCi/well of [3H] thymidine was added and incubated for 16 hr. Samples were harvested and counted by liquid scintillation (Perkin Elmer, MA).

Adoptive transfer of retina-specific T cells and LXA4 treatment

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To elicit EAU by adoptive T cell transfer, 5 × 106 IRBP161-180 in vitro-activated (2 µg/ml for 3 days) lymph node cells from R161H CD90.1 mice were injected intraperitoneally into B10.RIII WT CD90.2 mice. LXA4 was administered at the doses of 1 µg or 250 ng every day throughout the disease course. Fundoscopy was assessed starting on day four after cell transfer to track disease development. Alternatively, donor C57BL/6 WT and Alox5-/- mice were immunized with IRBP651-670 peptide, and CD3+ T cells purified with T cell enrichment columns (R and D Systems, MN) from lymph nodes that drain immunization sites and spleens on day 11 post-immunization. WT or Alox5-/- T cells (1 × 107 each) were transferred intraperitoneally into TCRb-/- recipients. Three weeks after the cell transfer, TCRb-/- recipient mice were immunized with 150 µg IRBP651-670 in CFA and pertussis toxin as described above.

NanoString assays for transcriptomic analysis

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RNA was extracted from snap frozen tissues using RNeasy (Qiagen, Germany) and analyzed by nCounter Analysis Technology using the mouse cancer immunology panel (nanoString, WA). Data were normalized to housekeeping genes and analyzed using nSolver software. Gene expression threshold was set at 30 counts to eliminate background signals.

Transwell migration assay and in vitro T cell assay

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CD4+ T cells were isolated using CD4 T cell isolation kit (STEMCELL Technologies, Canada) from inguinal lymph nodes and spleens of mice immunized with IRBP651-670 and stimulated in vitro with 2 µg of anti-CD3 and 1 µg of anti-CD28 antibodies for 18 hr. Stimulated T cells were seeded at 2 × 105 per transwell insert (Corning, MA) and allowed to migrate toward 100 ng of CCL19 and 100 ng of CCL21 chemokine ligands (R and D systems, MN) in 2% FCS for 4 hr. 10 nM – 2 μM of LXA4 was added to stimulated T cells cultured in HL-1 media supplemented with 0.5% normal mouse serum and stained for chemokine receptors. Cells were analyzed on Cytoflex.

Seahorse metabolic assays

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Seahorse XFe96 Extracellular Flux Analyzer (Agilent Technologies, CA) was used to measure glycolysis. CD4+ T cells were harvested from WT or Alox5-/- mice immunized with IRBP651-670 and stimulated with anti-CD3 and anti-CD28 antibodies for 18 hr. The glycolysis proton efflux rate (glycoPER) for each well was calculated from cells subjected to XF Glycolytic Rate assays with the following concentrations of injected compounds: 50 mM 2-DG and 0.5 µM rotenone/antimycin A. For assays with LXA4 treatment, CD4+ T cells were preincubated with 1 µM of LXA4 or vehicle control for 1 hr before anti-CD3 and anti-CD28 stimulation.

Statistical analysis

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Statistics were performed using GraphPad Prism 8 (GraphPad, CA). Statistical differences were determined by ANOVA, Welch’s t-tests, and Wilcoxon matched-pairs signed rank test for parametric variables and Mann-Whitney test for nonparametric variables. All error bars are standard error mean. p value < 0.05 was considered statistically significant and is denoted with *p≤0.05, **p≤0.01, ***p≤0.001 in the figures.

Data availability

All data needed to evaluate the conclusions of the paper are present in the main text and supplementary materials.

References

Article and author information

Author details

  1. Jessica Wei

    1. Vision Science Program, University of California, Berkeley, Berkeley, United States
    2. Laboratory of Immunology, National Eye Institute, National Institutes of Health, Bethesda, United States
    Contribution
    Conceptualization, Formal analysis, Investigation
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-7329-2812

  2. Mary J Mattapallil

    Laboratory of Immunology, National Eye Institute, National Institutes of Health, Bethesda, United States
    Contribution
    Resources, Formal analysis, Investigation
    Competing interests
    No competing interests declared

  3. Reiko Horai

    Laboratory of Immunology, National Eye Institute, National Institutes of Health, Bethesda, United States
    Contribution
    Formal analysis, Investigation, Methodology
    Competing interests
    No competing interests declared

  4. Yingyos Jittayasothorn

    Laboratory of Immunology, National Eye Institute, National Institutes of Health, Bethesda, United States
    Contribution
    Investigation, Methodology
    Competing interests
    No competing interests declared

  5. Arnav P Modi

    School of Optometry, University of California, Berkeley, Berkeley, United States
    Contribution
    Investigation, Methodology
    Competing interests
    No competing interests declared

  6. H Nida Sen

    Laboratory of Immunology, National Eye Institute, National Institutes of Health, Bethesda, United States
    Contribution
    Resources
    Competing interests
    No competing interests declared

  7. Karsten Gronert

    1. Vision Science Program, University of California, Berkeley, Berkeley, United States
    2. School of Optometry, University of California, Berkeley, Berkeley, United States
    3. Infectious Disease and Immunity Program, University of California, Berkeley, Berkeley, United States
    Contribution
    Conceptualization, Resources, Supervision, Funding acquisition, Project administration
    For correspondence
    kgronert@berkeley.edu
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-5329-7907

  8. Rachel R Caspi

    Laboratory of Immunology, National Eye Institute, National Institutes of Health, Bethesda, United States
    Contribution
    Conceptualization, Resources, Supervision, Funding acquisition, Project administration
    For correspondence
    caspir@nei.nih.gov
    Competing interests
    No competing interests declared

Funding

National Eye Institute (EY026082)

  • Karsten Gronert

National Eye Institute (EY000184)

  • Rachel R Caspi

The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.

Acknowledgements

Funding: This work was supported by grants EY026082 to KG and EY000184 NEI Intramural funding to RRC. Competing interests: The authors declare no financial interests. Data and materials availability: All data needed to evaluate the conclusions of the paper are present in the main text and Supplementary Materials. The authors thank Ryan Salvador and Jihong Tang for assistance in tissue harvest, Amy Zhang for advice on statistical analyses, Benjamin Smith for developing the fluorescence quantification program in Fiji, Julie Laux, Rafael Villasmil, Arvydas Maminishkis, Jennifer Kielczewski, Phyllis Silver, Allison Chan, Victoria Ly, Nicole Rossi, Kimberly Tang, Julia Yoo and Karthik Mouli for technical support, and members of the Caspi lab for helpful discussions.

Ethics

Human subjects: Male and female patients ages 30 - 76 with clinical diagnosis of non-infectious posterior segment uveitis were enrolled in the National Eye Institute protocol number 16-EI-0046. Healthy controls were NIH blood bank donors of both sexes with a similar age range. Serum samples were obtained from male and female patients ages 30 - 76 with clinical diagnosis of non-infectious posterior uveitis, healthy controls were NIH blood bank donors of both sexes with a similar age range whose samples were de-identified and sent to the lab. Patients were enrolled from May 2017 to July 2018 under a clinical research protocol 428 (NCT02656381), approved by the institutional review board of the National Institutes of Health. Informed consent (including publishing language as required by NIH IRB) were obtained from all subjects. The study adhered to the tenets of the Declaration of Helsinki.

Animal experimentation: All experimental procedures were approved by the Animal Care and Use program at University of California, Berkeley, and the National Eye Institute at the National Institutes of Health.(protocols AUP-2016-04-8691-1 and NEI-581).

Copyright

This is an open-access article, free of all copyright, and may be freely reproduced, distributed, transmitted, modified, built upon, or otherwise used by anyone for any lawful purpose. The work is made available under the Creative Commons CC0 public domain dedication.

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  1. Jessica Wei
  2. Mary J Mattapallil
  3. Reiko Horai
  4. Yingyos Jittayasothorn
  5. Arnav P Modi
  6. H Nida Sen
  7. Karsten Gronert
  8. Rachel R Caspi
(2020)
A novel role for lipoxin A4 in driving a lymph node–eye axis that controls autoimmunity to the neuroretina
eLife 9:e51102.
https://doi.org/10.7554/eLife.51102

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