The role of interferon regulatory factor 8 for retinal tissue homeostasis and development of choroidal neovascularisation

Abstract

Background

Microglia cells represent the resident innate immune cells of the retina and are important for retinal development and tissue homeostasis. However, dysfunctional microglia can have a negative impact on the structural and functional integrity of the retina under native and pathological conditions.

Methods

In this study, we examined interferon-regulatory factor 8 (Irf8)–deficient mice to determine the transcriptional profile, morphology, and temporospatial distribution of microglia lacking Irf8 and to explore the effects on retinal development, tissue homeostasis, and formation of choroidal neovascularisation (CNV).

Results

Our study shows that Irf8-deficient MG exhibit a considerable loss of microglial signature genes accompanied by a severely altered MG morphology. An in-depth characterisation by fundus photography, fluorescein angiography, optical coherence tomography and electroretinography revealed no major retinal abnormalities during steady state. However, in the laser-induced CNV model, Irf8-deficient microglia showed an increased activity of biological processes critical for inflammation and cell adhesion and a reduced MG cell density near the lesions, which was associated with significantly increased CNV lesion size.

Conclusions

Our results suggest that loss of Irf8 in microglia has negligible effects on retinal homeostasis in the steady state. However, under pathological conditions, Irf8 is crucial for the transformation of resident microglia into a reactive phenotype and thus for the suppression of retinal inflammation and CNV formation.

Background

Retinal microglia cells (rMG) constitute the resident myeloid cell population in the neuroretina and are critical for retinal development, tissue homeostasis and response to cell damage. During development, rMG are in intimate contact to endothelial tip cells and contribute to postnatal vascular development [16] as well as neuronal survival by modulating programmed cell death and trophic influences [56]. During adulthood, rMG interact closely with synapses to maintain synaptic structure and electroretinal function and continuously scan the local environment for danger signals associated with injury or pathogens [56]. In response to tissue damage or infection, rMG rapidly attain an activated phenotype, migrate towards the site of injury and contribute to phagocytosis, inflammation and pathological events [4, 52, 59]. As such, activated microglia cells have been found in the subretinal space of patients with age-related macular degeneration (AMD) and in particular at sites of choroidal neovascularisation (CNV) in neovascular AMD [11, 20] which is a common cause of irreversible blindness in the elderly [10, 60]. Studies on the role of rMG in the development of CNV, however, revealed conflicting results, and both detrimental and protective roles of MG for the progression of CNV have been discussed in the past [2, 14, 36, 49, 51].

The interferon regulatory factor (IRF) family of transcription factors consists of nine members that are involved in hematopoietic differentiation, oncogenesis, Toll-like and purinergic receptor signalling and expression of interferons and interferon-inducible genes [39, 57]. In particular, Irf8 plays a pivotal role in the regulation of lineage commitment and MG cell maturation during brain development [27, 47]. Besides its essential role during development, Irf8 is crucial for the function of resident myeloid cells in the adult steady state. As such, the deletion of Irf8 in mice leads to a disturbed homeostasis of resident tissue macrophages in the liver, the kidney and brain including microglia and other CNS-associated macrophages [19, 25, 48, 58]. The role of Irf8 in regulating rMG gene expression and its influence on retinal development and neuroretinal function, however, are currently unknown.

The aim of this study was to determine the function of IRF8 in retinal microglia in the healthy as well as perturbed retina. Specifically, we aimed to investigate whether IRF8 is involved in microglial cell homeostasis, neuroretinal function and pathological CNV formation. The latter is of particular interest, as PU.1 and CSF1R signalling acting upstream and downstream of IRF8, respectively, are critical for postnatal angiogenesis and formation of pathological neovascularisation in the eye [16, 54]. For this purpose, we analysed Irf8 reporter and knockout mice by in vivo imaging, functional studies, flow cytometry, immunohistochemistry and RNA sequencing (RNA-seq). We found that Irf8-deficient MG exhibited functionally relevant alterations in gene expression patterns that were associated with a significant disruption of microglial development, normal postnatal retinal vascular and functional development, and increased CNV lesion size in the adult situation.

Methods

Mice

All animal experiments were authorized by the local animal care and use committee under the respective EU, national, federal and institutional regulations for animal experiments (ethical protocol numbers G14/89, G20/13). Mice were bred on a C57BL/6J background and devoid of the Crb1 mutation. Cx3cr1^GFP/GFP mice were crossed with C57BL/6J mice to generate Cx3cr1^GFP/+ (Irf8 WT) mice. Irf8^-/- mice were crossed with Irf8^-/-Cx3cr1^GFP/GFP mice to obtain Cx3cr1^GFP/+:Irf8^-/- (Irf8 KO) mice [24, 26]. Phage artificial chromosome-transgenic Irf8-VENUS reporter mice were used to trace the expression of IRF8 [53]. CAG::mRFP1 mice were purchased from the Jackson Laboratory (Bar Harbor, ME).

Genotyping

Transgenic mice were genotyped according to the primers and programs shown in supplemental table 1.

Laser-induced choroidal neovascularisation (CNV)

The laser-induced CNV model was used as previously described [15, 31, 50]. In brief, mice were anaesthetized by intraperitoneal administration of ketamine hydrochloride (100 mg/kg, Pharmacia & Upjohn, Erlangen, Germany) and xylazine (6 mg/kg, Bayer Vital GmbH, Leverkusen, Germany). Pupillary dilatation was achieved by applying 0.5% tropicamide (Bausch + Lomb, Berlin, Germany) and 5% phenylephrine hydrochloride (URSAPHARM Arzneimittel GmbH, Saarbrücken, Germany). After covering the cornea with a coverslip coated with dexpanthenol eye gel (50 mg/g, Bausch + Lomb, Berlin, Germany), three to six laser spots (488 nm, 150 mW, 100 μm and 100 ms) were applied to each eye using the VISULAS 532s Laser System (Carl Zeiss, Jena, Germany) in combination with ZEISS Laser Slit Lamp 532s (Carl Zeiss, Jena, Germany). Only laser spots with visible formation of vaporisation bubbles were included in this study.

Bone marrow transplantation

Bone marrow transplantation experiments were carried out as previously described [22]. In brief, a total of 12 recipient control and 14 Irf8 knockout mice were head-shielded and lethally irradiated (RS2000 irradiator, Rad Source, Kanas, USA) in two independent experiments. Meanwhile, bone marrow cells (BMCs) were collected from the tibias and femurs of CAG-mRFP1 mice and resuspended in phosphate-buffered saline (PBS). The recipient mice were intravenously injected with 3 × 10⁶ BMCs via the tail vein. Nine weeks after bone marrow transplantation, the efficiency of reconstitution was assessed by flow cytometry which will be explained below.

In vivo characterisation and analysis

Fundus morphology, retinal structure and physiological function were investigated using fundus photography, fundus fluorescein angiography (FFA), optical coherence tomography (OCT) and electroretinography (ERG) as previously described [32]. Fundus photography, FFA and OCT were performed using a Micron III retinal microscope (Phoenix Technology Group, Pleasanton, CA, USA) and the StreamPix software (Norpix Inc., Montreal, Canada). For FFA, 10% sodium fluorescein (Alcon, Freiburg, Germany) was diluted to a concentration of 50 μL/mL in 0.9% sodium chloride for injection (VWR, Leuven, Belgium) and administered intraperitoneally (2 μL/g). Ninety seconds after dye injection, the angiograms were recorded. For quantification of CNV size, hyperfluorescent areas in early-phase angiograms were measured in pixels using ImageJ. Image-guided OCT was performed using the OCT2 scan head. In OCT images, the thickness of the inner nuclear layer (INL) (200 pixels from the optic nerve head) was measured using ImageJ (https://imagej.nih.gov/ij/). For ERG, mice were dark-adapted overnight and anaesthetized by intraperitoneal injection of ketamine hydrochloride (66.8 mg/kg) and xylazine (12.76 mg/kg). ERG signals were amplified, recorded and analysed automatically using Ganzfeld Q450 (Roland-Consult, Brandenburg, Germany) with the integrated software developed by Prof. Dr. rer. nat. Michael Bach (Eye Center, University of Freiburg, Germany).

Immunohistochemistry and imaging

After intracardiac perfusion with PBS and 4% paraformaldehyde (PFA), eyes were fixated in 4% PFA for 45 min at room temperature and processed to RPE-choroidal-scleral and retinal flat mounts. After incubation in PBST/BSA blocking buffer overnight, the flat mounts were incubated with primary antibodies against collagen type IV (1:500, AB769, Merck Millipore, Darmstadt, Germany), Iba1 (1:500, #019-19741, Wako, Neuss, Germany) or alpha smooth muscle actin (SMA, 1:500, ab5694, Abcam, Cambridge, UK) for two nights at 4 °C, followed by incubation with Alexa Fluor® 568 or 647-conjugated secondary antibodies overnight at 4 °C (1:500, Life technologies, Eugene, OR, USA). Eyes of Irf8-VENUS mice were fixated in 4% PFA for 1 h and incubated in 10%, 20% and 30% sucrose for 24 h each prior to embedding in Tissue-Tek O.C.T. compound (Sakura, Aplphen aan den Rijn, The Netherlands). Seven micrometre-thick cryosections were cut using a cryostat (Leica CM1950, Leica, Nussloch, Germany). Following blocking in Ultra V block for 10 min at room temperature, the sections were incubated with primary antibodies against ßIII tubulin (1:500, ab18207, Abcam, Cambridge, UK), collagen type IV (1:1000, ab6586, Abcam, Cambridge, UK), Ceh-10 homeo domain containing homolog (CHX10, 1:200, ab16141, Abcam, Cambridge, UK), GFP (1:500, 600-101-215, ROCKLAND, Limerick, PA, USA), glial fibrillary acidic protein (GFAP, 1:500, 087A1005RE, Fremont, CA, USA) or Iba1 (1:500) for 60 min with corresponding Alexa Fluor® 568-conjugated secondary antibodies (1:500, Life technologies, Eugene, OR, USA). Nuclei were counterstained with 4,6-diamidino-2-phenylindole (DAPI). Stainings were imaged using the Nano Zoomer S60 digital slide scanner (Hamamatsu, Herrsching am Ammersee, Germany) and analysed with NDP viewer software (Hamamatsu, Herrsching am Ammersee, Germany) or with a confocal laser scanning microscope (Zeiss LSM 510 or Leica TCS SP8 or Olympus FV1000), Zen software (Carl Zeiss, Jena, Germany), LAS X software (Leica, Nussloch, Germany) or Fluoview FV1000 (Olympus, Tokyo, Japan). For a detailed list of antibodies used, see supplementary table 2.

Three-dimensional reconstruction of retinal microglia

Imaging for 3D reconstruction was performed using a Zeiss LSM 510 confocal laser scanning microscope with a 20× objective, 3× zoom and 1024 × 1024 pixel resolution. The interval thickness of the z-stacks was set to 1.0 μm. The morphology of retinal microglia in the inner plexiform layer (IPL) and outer plexiform layer (OPL) was determined by a three-dimensional reconstruction using the filament mode of IMARIS software (Bitplane, Zurich, Switzerland). Three cells per layer and mouse were reconstructed and analysed.

Fluorescence-activated cell sorting

Following transcardial perfusion with 1× PBS and enucleation, eyes were dissected in ice-cold 1× PBS to isolate the retinae of Irf8^+/+Cx3cr1^GFP/+ or Irf8^-/-Cx3cr1^GFP/+. For the lasered mice, the central parts (70%) of the retinae were used for FACS while the peripheral parts were omitted. After tissue homogenisation and filtration through a 50-μm cell strainer (Sysmex, Goerlitz, Germany), dead cell exclusion was performed by incubation with fixable viability dye 780 (1:1000, 65-0865-14, eBioscience, Waltham, MA, USA). Anti-CD16/CD32 (Fc) receptor (1:200, 553142, BD Biosciences, Heidelberg, Germany) was used to avoid unspecific binding. Following staining with anti-CD45 (1:200, 103133, BioLegend, San Diego, CA, USA), anti-CD11b (1:200, 17-0112-83, eBioscience, Waltham, MA, USA), anti-Ly6C (1:200, 560593, BD Bioscience, Heidelberg, Germany) and anti-Ly6G (1:200, 560601, BD Biosciences, Heidelberg, Germany) for 20 min at 4 °C, retinal microglia characterised as CD45^lowCD11b⁺Cx3cr1^GFP/+Ly6C^-Ly6G^- were analysed and sorted into RNA stabilisation reagent (QIAGEN, Hilden, Germany) using a MoFlo Astrios EQ High Speed Cell Sorter (Beckman Coulter, Munich, Germany). For RNA sequencing, an average number of 10,000 retinal microglia per sample was obtained from pooling 3 to 4 mice. Flow cytometric purification of wild-type retinal and brain microglia together with bone marrow–derived monocytes was described before [59]. Data are available under the GSE accession number GSE160845. For a detailed list of antibodies used, see supplementary table 2.

RNA extraction

RNA extraction, RNA library preparation and RNA sequencing were performed in collaboration with the Genomics Core Facility "KFB-Center of Excellence for Fluorescent Bioanalytics" (University of Regensburg, Germany). RNA extraction was performed according to manufacturer’s instructions using the RNeasy Plus Mini Kit (QIAGEN, Hilden, Germany). After pelleting the sample by centrifugation, the RNA stabilisation reagent was removed and replaced by RLT Plus buffer for lysing retinal microglia. Genomic DNA was removed selectively and efficiently by using gDNA Eliminator spin columns for RNA purification. After adding Ethanol to the flow-through, the sample was applied to an RNeasy MinElute spin column to collect RNA. Finally, after washing the column, total purified RNA was eluted in RNase-free water. The quality and integrity of total RNA was assessed with a Agilent 2100 Bioanalyser in combination with the RNA 6000 Pico LabChip Kit (Agilent, Palo Alto, CA, USA).

RNA sequencing

First-strand cDNA was generated using SMARTer Ultra Low Input RNA Kit for Sequencing v4 (Clontech Laboratories, Inc., Mountain View, CA, USA). Double-standed cDNA was amplified with LD PCR and purified with AMPure XP beads. Library preparation was constructed conforming to the Illumina Nextera XT Sample Preparation Guide (Illumina, San Diego, CA, USA). In brief, 150 pg of input cDNA was tagmented via Nextera XT transposome. The products were purified and amplified with a limited-cycle PCR program to construct sequencing libraries. The libraries were quantified with the KAPA SYBR FAST ABI Prism Library Quantification Kit (Kapa Biosystems, Wobum, MA, USA). Equimolar amounts of each library were pooled for cluster generation on the cBot using the Illumina TruSeq SR Cluster Kit v3. The sequencing run was performed on a HiSeq1000 instrument with TruSeq SBS Kit v3 according to the Illumina HiSeq 1000 System User Guide. Illumina image analysis and base calling were recorded in library base call format (.bcl) and further converted to Fastq files via the CASAVA1.8.2 software.

RNA sequencing data analysis

Quality control and transcriptome profiling including reads mapping, annotation, quantification and normalisation were performed by GenXPro (GenXPro, Frankfurt, Germany). Briefly, FastQC was performed to assess sequencing quality. After removing reads containing adapter sequences and duplicate reads via cutadapt software (GitHub, San Francisco, CA, USA) and FastUniq, the filtered reads were mapped to the mouse genome from ENSEMBL (https://www.ensembl.org/Mus_musculus/Info/Index) using bowtie2. The transcripts were functionally annotated with gene transfer format file version 90, quantified using HTSeq and normalised as transcripts per kilobase million (TPM) via DESeq2. Differential gene expression analysis with threshold (log2 fold change greater than 1.5 or less than − 1.5, p < 0.05, TPM ≥ 100 in at least one of the two compared groups) was performed using DESeq2. Data was visualised using RStudio (v1.2.1335) and R (v3.5.3). Volcano plots were created using the ggplot2 package, and Gene Ontology (GO) analysis was performed using R with the clusterProfiler 3.10.1 package [62].

Protein analysis

Protein was extracted from the choroid and the retinae using RIPA buffer (#R2078, Sigma Aldrich) containing protease inhibitor (cOmplete, Mini; edta-FREE Protease inhibitor Cocktail, Roche Diagnostics, Manheim, Germany) and phosphatase inhibitors (PhosSTOP, Roche Diagnostics, Manheim, Germany), respectively, for preservation. Total protein concentration for each sample was measured with the Pierce^TM Bicinchoninic Acid Protein Assay Kit (Thermo Fisher Scienticis, Inc., Rockland, IL, USA).

Statistical analysis

Statistical analysis was performed using GraphPad Prism v6 (La Jolla, USA) as follows: an unpaired t test was applied if the normality was given by the Kolmogorov-Smirnov test. Otherwise, the Mann–Whitney U test was used. Difference with significance was defined as p < 0.05.

Results

IRF8 is the most abundantly expressed member of the IRF family in retinal microglia

The interferon regulatory factor (IRF) family is critical for the development, maturation and function of myeloid cells [40]. Using flow cytometry and RNA sequencing, we first determined the expression levels of different IRF family members in adult retinal microglia (rMG), brain microglia (bMG) and bone marrow (BM) monocytes (Fig. 1A, B). In general, genes belonging to the IRF family were expressed at different levels in rMG, bMG and BM monocytes (Fig. 1B). Compared with other IRF family members, Irf5 and Irf8 exhibited the highest expression levels in rMG, bMG and BM monocytes. In the retina, Irf8 emerged as the most prominent IRF member in rMG. Interestingly, the expression of Irf8 in rMG exceeded the expression in bMG and BM monocytes indicating a distinct function of Irf8 for rMG. To validate Irf8 expression in adult rMG, we next analysed Irf8-VENUS reporter mice by flow cytometry and immunohistochemistry. Flow cytometry analysis revealed a strong VENUS expression (98.7% ± 0.5%) in CD45^loCD11b⁺ rMG in the steady state (Fig. 1C). In line with this finding, immunofluorescence analysis of retinal flat mounts and cryosections confirmed that IRF8 is mostly expressed in IBA1-positive microglial cells in the steady state (Fig. 1D and Supplementary Figure 1C). Since expression of Irf family members may change in response to stress and inflammation, we next assessed the expression levels of all IRF family members (1–9) and of common MG signature genes, such as Tmem119 and P2ry12, in retinal MG in 2–3 months old Cx3cr1^GFP/+ mice in the steady state and upon MG activation in the laser-induced CNV model. While the expression of the signature genes P2ry12 and Tmem119 decreased in retinal MG after laser injury, activation markers such as Cd74 were increased, as reported before [59]. However, most members of the IRF family were expressed at the same level in the rMG in the context of laser-induced inflammation compared with controls. Only Irf2 and Irf5 were slightly downregulated in retinal MG, whereas Irf7 was modestly upregulated. Notably, the expression of Irf8 in retinal MG remained stable in the laser-induced CNV model compared with controls (data not shown).

Fig. 1

Irf8 is predominantly expressed in retinal microglia (MG) and blood monocytes. A Flow chart of retinal MG RNA sequencing. B Differential expression of IRF family members in retinal MG (rMG), brain MG (bMG) and bone marrow (BM) monocytes. The gene expression profile was generated from four CD45^loCD11b⁺Ly6C^-Ly6G^- rMG samples, four CD45^loCD11b⁺Ly6C^-Ly6G^- bMG samples and four CD45⁺CD11b⁺Ssc^loCD115⁺Ly6C⁺ bone marrow (BM) monocytes. C Flow cytometry analysis of Irf8-VENUS expression in CD45^loCD11b⁺ retinal MG (98.7% ± 0.5, green solid line) in comparison with a negative control (grey dotted line). D Immunohistochemistry of the retinal flat mounts (upper panel) and cryosections (lower panel) from Irf8-VENUS mice reveal that all IBA1+ (red) rMG express Irf8-VENUS (green)

Deficiency of Irf8 has a substantial impact on morphology, distribution and transcriptional activity of retinal MG in the steady state

To assess the role of IRF8 in distribution and cell morphology of rMG in the adult situation, we next examined retinal flat mounts from 8-week-old Irf8 knockout (KO) mice by immunofluorescence microscopy (Fig. 2A,B). Irf8 KO mice revealed a strikingly altered rMG distribution and morphology compared with wild-type (WT) animals, characterised by slightly reduced MG numbers in the inner plexiform layer (IPL, Irf8 WT: 104 ± 7 cells/mm², Irf8 KO: 88 ± 5 cells/mm², p = 0.09) and highly significant decrease of cell numbers in the outer plexiform layer (OPL, Irf8 WT: 116 ± 6 cells/mm²; Irf8 KO: 43 ± 1 cells/mm², p < 0.0001, Fig. 2B,C). Quantitative morphometric analysis using IMARIS revealed a severely altered morphology of retinal microglia in Irf8 KO mice, including significantly shorter length of dendrites (IPL: Irf8 KO: 356.5 ± 14.3 μm, Irf8 WT 1043.0 ± 59.4 μm, p = 0.009; OPL: Irf8 KO: 297.7 ± 35.6 μm, Irf8 WT: 788.8 ± 26.1 μm, p = 0.01), and reduced number of dendrite segments (IPL: Irf8 KO: 62 ± 4, Irf8 WT: 167 ± 14, p = 0.009; OPL: Irf8 KO: 44 ± 6, Irf8 WT: 139 ± 6, p = 0.01), branch points (IPL: Irf8 KO: 30 ± 2, Irf8 WT: 82 ± 7, , p = 0.009; OPL: Irf8 KO: 21 ± 3, Irf8 WT: 68 ± 3, p = 0.01) and terminal points (IPL: Irf8 KO: 33 ± 2, Irf8 WT: 86 ± 7, p = 0.009; OPL: Irf8 KO: 23 ± 3, Irf8 WT: 71 ± 3, p = 0.01, Fig. 2D,E) compared with controls. Having established a profoundly altered rMG distribution and phenotype in the adult situation, we next explored rMG cell numbers at earlier stages of postnatal development. Interestingly, reduced microglia cell numbers were already present in the neuroblast layer at postnatal day 1 (P1) and later in the OPL at P7 but only transiently in the IPL at P7 that could be compensated until adulthood (Suppl. Figure 2A, B). These findings suggest an impaired MG distribution specifically in the deeper layers of the retina which is already present shortly after birth and persists into adulthood.

Fig. 2

Irf8 deficiency alters retinal MG distribution, morphology and transcriptional profile. A Breeding scheme. B Irf8 KO mice demonstrate reduced density of Cx3cr1-GFP⁺ (green) retinal MG. Quantitative analysis are shown in (C). Pictures are representative for n = 5 mice in each group. C Quantification in microglial numbers in the inner plexiform (IPL) and outer plexiform layer (OPL). n = 5 mice were analysed per group. Data are shown as mean ± SEM. D 3D reconstruction of retinal MG by IMARIS reveals that Irf8 deficiency alters morphology of retinal MG, resulting in shorter total length of dendrites, less dendrite segments and attenuated branching. E Quantitative analysis of retinal morphology. Four to six cells were reconstructed per mouse per IPL and OPL separately. Statistics were performed with the mean values per mouse (n = 6–7 in the Irf8 WT and n = 3–4 in the Irf8 KO group). Data are shown as mean ± SEM

To explore the associated transcriptional changes in Irf8-deficient rMG, we next performed RNA sequencing (RNA-seq) of FACS-sorted rMG from adult Irf8 KO mice and controls. We determined 277 differentially expressed genes (DEGs) of which 142 were significantly upregulated, and 135 genes were downregulated in Irf8 KO microglia compared with microglia of control mice (Fig. 3A). Gene ontology (GO) cluster analysis revealed that most of these downregulated genes contribute to processes such as “cell migration” (GO:0016477, p.adj. < 1.3 × 10^-5), “cell motility” (GO:0048870, p.adj. < 4.8 × 10^-5), “localization of cells” (GO:0051674, p.adj. < 4.8 × 10^-5), “regulation of cell proliferation” (GO:0032944, p.adj. < 3.5 × 10^-3) and “cell adhesion” (GO:0007155, p.adj. < 7.7 × 10^-4) suggesting a reduced migratory potential of retinal microglia in the Irf8 KO mice compared with controls (Fig. 3B). Among the downregulated DEGs, we found numerous microglia signature genes essential for microglia homeostasis, including the spalt like transcription factor 1 (Sall1, log2FC = − 10.69, − log10p = 24.57), allograft inflammatory factor 1 (Aif1 or Iba1, log2FC = − 2.73, − log10p = 35.04), purinergic receptor P2Y, G-Protein couple 12 (P2ry12, log2FC = − 2.50, − log10p = 45.06) and transmembrane 119 (Tmem119, log2FC = − 2.13, − log10p = 24.57) (Fig. 3A,C). In accordance with the RNA-seq data, we found a strong immunoreactivity for TMEM119 and P2RY12 in Irf8-competent rMG cells, which was almost absent in Irf8-deficient rMG. Conversely, we found an increased immunoreactivity for the mannose receptor (CD206, Mrc1) in Irf8-deficient rMG, consistent with and further supporting the RNA-seq results (Fig. 3D). In addition, flow cytometry analysis of homeostatic CD45⁺CD11b⁺ rMG confirmed our RNA-seq results showing a reduced but still detectable protein expression of CX₃CR1 and CD64 in Irf8-deficient rMG compared with controls with a trend towards lower MERTK and higher F4/80 expression as reported before in bMG [44] (Fig. 3E).

Fig. 3

Irf8 deficiency leads to expression loss of homeostatic signature genes. A Volcano plot of differentially expressed genes in Irf8 KO retinal MG (n = 3) compared with control (n = 5). Significantly up- and downregulated genes are shown in red and blue, respectively. The top significantly up- and downregulated genes are labelled. B The top 5 downregulated GO clusters in Irf8 KO retinal MG. Significance is represented as p.adjust, the size of each data circle indicates the number of genes involved in each enriched GO term. C Representative signature genes found to be highly expressed in competent retinal MG are significantly downregulated in the Irf8 KO mice. D Immunohistochemistry of retinal flat mounts demonstrate a strong immunoreactivity for P2RY12 and TMEM119 shown as colour-coded signal intensity in Irf8-competent retinal MG that is reduced or absent in Irf8 KO mice. The mannose receptor CD206 (encoded by Mrc1) is absent under homeostatic conditions but detectable under Irf8-deficient conditions. E Myeloid expression levels shown as transcripts per million (TPM) and analogue surface marker expression, as determined by flow cytometry, of Irf8 WT (blue) and Irf8 KO (red) mice, expressed as mean fluorescence intensity (MFI) (left). Representative histograms are shown (right) including fluorescence minus one controls (grey line). Six mice per group were analysed for CX₃CR1, CD64 and MERTK, three mice per group for F4/80. Data are shown as mean ± SEM

Taken together these results strongly suggest that IRF8 plays a critical role in maintaining the distribution, morphology and homeostasis of retinal microglia and has a substantial impact on the transcriptional activity of rMG in the steady state.

IRF8 is not required for the development of the retinal structure, vasculature and function

Having established the quantitative and qualitative changes in Irf8-deficient rMG, we next investigated whether Irf8-deficiency influences retinal structure and electroretinal function during steady state. To this end, we examined the retina of adult Irf8-deficient and control mice using color fundus photography (CF), fluorescein angiography (FA), optical coherence tomography (OCT), electroretinography (ERG) and immunohistochemical staining of retinal flat mounts for retinal vessels (Suppl. Figure 3).

In general, Irf8 KO mice showed regular retinal structure, vasculature and function compared with controls. Qualitative assessment of retinal structure and vessels on CF and FA images of Irf8-deficient and control mice revealed no gross abnormalities, particularly no vascular dye leakage as an indicator of disturbed vascular architecture or spontaneous neovascularisation (Suppl. Figure 3A,B). In OCT images, the thickness of the inner nuclear layer (INL) and the outer nuclear layer (ONL) containing the photoreceptors (PR) was similar in Irf8-deficient mice (INL: 15.2 ± 0.5 μm, ONL: 69.8 ± 1.0 μm) compared with control animals (INL: 15.8 ± 0.4 μm, ONL: 72.3 ± 1.0 μm, Suppl. Figure 3C). ERG measurements demonstrated similar dark-adapted scotopic and light-adapted photopic responses in Irf8 KO mice and controls (Suppl. Figure 3D). Specifically, no significant difference was detected between Irf8 KO mice and controls with respect to scotopic a-waves emanating from rods, scotopic b-waves corresponding to depolarisation of bipolar cells, and photopic b-waves arising from cones. Immunohistochemical staining of retinal flat mounts revealed a regular retinal vasculature in Irf8 KO mice, including equal numbers of arteries labelled by smooth muscle actin (SMA, Irf8 WT 6.2 ± 0.4, Irf8 KO: 5.9 ± 0.3 per animal) and major vessels stained with Isolectin-B₄ (IB4, Irf8 WT: 11.3 ± 0.5, Irf8 KO: 11.0 ± 0,5 per retinal per animal, Suppl. Figure 3E). Additionally, branch points in the central superficial vascular plexus (Irf8 WT: 17.0 ± 2.7, Irf8 KO 22.1 ± 2.4 per animal), central deep plexus (Irf8 WT: 8.7 ± 4.7, Irf8 KO: 74.0 ± 3.4 per animal), peripheral superficial plexus (Irf8 WT: 29.0 ± 3.5, Irf8 KO: 28.1 ± 2.0 per animal) and peripheral deep plexus (Irf8 WT: 59.0 ± 5.1, Irf8 KO: 63.9 ± 5.7 per animal) were similar between both groups (Suppl. Figure 3F).

Overall, these data show that Irf8 is not essential for the development and maintenance of homeostatic retinal structure, vascular network and function. This is particularly surprising given the significant changes in rMG cell numbers in the Irf8 KO mice during development and in the adult. Thus, the impaired retinal MG cell morphology and expression profile in otherwise unremarkable retinal homeostasis in Irf8-deficient mice provide a unique opportunity to investigate the role of retinal MG in the development of CNV.

Irf8 deficiency aggravates CNV formation

Retinal MG change their phenotype and transcriptional profile after tissue injury and modulate the development of pathological CNV, which represents a hallmark of neovascular AMD [59]. To investigate the role of IRF8 in microglial cell activation after tissue injury and formation of CNV, we next studied Irf8-deficient and control mice in the laser-induced CNV model. Both Irf8 KO and Irf8 WT mice developed typical laser-induced CNV 7 days after laser photocoagulation visible, as hyperfluorescent lesions with clear demarcation in FA images (Fig. 4A). Quantification of hyperfluorescent CNV areas in angiograms revealed more than 2-fold larger CNV lesions in Irf8 KO mice (8603 ± 1309 pixels per animal) compared with controls (3697 ± 425 pixels per animal, p < 0.005). Measurement of collagen type IV-labelled CNV area on RPE/choroidal flat mounts confirmed significantly enlarged CNV lesions in Irf8 KO mice (52143 ± 7670 μm²) compared with Irf8 WT (25203 ± 4156 μm², p < 0.005, Fig. 4B). As expected, microscopic evaluation of RPE/choroidal flat mounts revealed that activated amoeboid Cx3cr1-GFP⁺ cells accumulate at CNV lesions in Irf8 KO mice as well as in controls. The number of Cx3cr1-GFP⁺ cells around CNV lesions, however, was significantly decreased in Irf8 KO mice (34 ± 7 cells per lesion per animal) compared with control animals (84.6 ± 8.8 cells per lesion per animal, p < 0.001, Fig. 4C). In addition, the number of rMG significantly increased in the IPL above CNV areas in controls, whereas no such increase was observed in Irf8 KO mice, further pointing to a defect in rMG migration (Suppl. Figure 4).

Fig. 4

Irf8-deficiency aggravates CNV formation. A Fundus fluorescein angiography at day 7 following laser treatment demonstrates enlarged CNV lesions in Irf8 KO mice (n = 11) compared with Irf8 WT (n = 13). Data are presented as mean ± SEM. B 3D reconstruction of collagen type IV-labelled CNV lesions using IMARIS. IHC of RPE-choroid-scleral flat mounts confirms that Irf8 deficiency (n = 11) increases CNV severity in comparison with control mice (n = 12). Data are presented as mean ± SEM. C Less Cx3cr1^GFP/+ (green) cells around CNV lesions (red) at day 7 after laser treatment were observed in the Irf8 KO mice (n = 6) compared with control mice (n = 7). Data are presented as mean ± SEM

Taken together, Irf8-deficient mice revealed reduced MG cell numbers suggesting an impaired MG migratory behaviour under physiological and pathological conditions which was associated with increased CNV lesion size in the laser-CNV model.

Retinal microglia rather than infiltrating monocytes account for the larger CNV lesions in the Irf8 KO mice

Since Cx3cr1 is expressed in retinal microglia and infiltrating monocyte-derived macrophages from the blood [26], the observed Cx3cr1^GFP/+ positive cells around CNV lesions could belong to both cell populations. However, Irf8-deficient mice are characterized by a low number of peripheral monocytes, which suggests that very few monocytes from the blood infiltrated the CNV lesion (Terry et al, 2015 PMID: 25277331). To investigate the influence of peripheral monocytes in our model, we next performed bone marrow transplantation experiments with bone marrow from CAG-RFP reporter animals to restore the peripheral monocyte pool in Irf8-deficient mice with Irf8 potent monocytes (Fig. 5A). Following head-shielded bone marrow transplantation, we observed a successful reconstitution of RFP⁺ Irf8-potent peripheral monocytes in Irf8-deficient animals compared with controls by using flow cytometry (Irf8 KO: 95.78 ± 0.59% (RFP⁺Ly6C^hi), 97.42 ± 0.14% (RFP⁺Ly6C^lo), Irf8 WT: 31.19 ± 4.85% (RFP⁺Ly6C^hi), 40.24 ± 5.5% (RFP⁺Ly6C^lo), Fig. 5B). The observed higher recombination efficiency of Ly6C^hi and Ly6C^lo monocytes in Irf8 KO is likely due to the initially low abundance of these cells and their respective progenitors in Irf8 KO mice. Of note, due to the head shielding, the recipients’ bone marrow in the skull is still active and not substituted by the donor cells that could explain the comparably lower recombination efficiency in Irf8 WT mice (Mildner et al, 2007 PMID: 18026096). Interestingly, the reconstituted Irf8-deficient animals still demonstrated increased CNV lesion size that was approximately twice as large compared with reconstituted Irf8 WT animals (Irf8 KO 82,009 ± 16,242 μm²; Irf8 WT 53,386 ± 4793 μm², p = 0.06) which was associated with slightly reduced numbers of RFP^-GFP⁺ microglia at sites of CNV (Irf8 KO 74 ± 16.5; Irf8 WT 197.3 ± 12.1, p = 0.14) (Fig. 5C,D). The numbers of reconstituted RFP⁺GFP^- monocyte-derived macrophages, in contrast, were around twofold increased in Irf8-deficient mice compared with controls (Irf8 KO 96.6 ± 20.1; Irf8 WT 49.25 ± 5.3, p = 0.07) (Fig. 5D).

Fig. 5

Bone marrow chimera experiments: reconstituted Irf8-deficient mice contain similar monocyte numbers as controls and reveal increased CNV lesion size. A Experimental setup. After head-shielded irradiation, bone marrow of CAG-RFP mice was transplanted intravenously to irradiated control (Irf8^+/+:Cx3cr1^GFP/+) and Irf8-deficient mice (Irf8^-/-:Cx3cr1^GFP/+) at the age of 8 weeks, respectively. Nine weeks after transplantation, flow cytometry was performed to check the reconstitution of blood cells. Ten weeks after transplantation, all mice underwent laser treatment to induce CNV. Analysis was performed at day 7 after laser induction. B After bone marrow transplantation, reconstitution of the blood cells was analyzed. Following head-shielded bone marrow transplantation, we observed a successful reconstitution of RFP⁺ peripheral CD45⁺CD11b⁺CD115⁺SSc^loLy6C^hi/lo monocytes in Irf8-deficient animals compared with controls by using flow cytometry. Irf8 KO (n = 6) and Irf8 WT (n = 8) mice were used per group. Data are presented as mean ± SEM. C,D Following bone marrow transplantation, Irf8-deficient mice exhibit a 2-fold increase of laser-induced CNV compared with control mice, while the number of Cx3cr1^GFP/+ GFP-positive and RFP-negative microglia at sites of CNV was similar in both groups. The number of reconstituted RFP-positive and GFP-negative blood-derived monocytes were increased in Irf8-deficient mice compared with controls. Irf8 KO (N = 12) and Irf8 WT (n = 14) mice were used per group. Data are presented as mean ± SEM

Transcriptional profile of Irf8 KO retinal microglia during CNV formation

In order to decipher the molecular mediators of enhanced CNV formation in Irf8 KO mice, we next isolated CNV-associated rMG from Irf8 KO and control mice by flow cytometry and analysed the cells using RNA-seq. In total, we found 84 genes that were differentially upregulated and 78 genes that were downregulated in Irf8-deficient microglia 7 days following laser injury. In line with the RNA-seq analysis under homeostatic conditions, we identified similar DEG that were down- or upregulated in Irf8-deficient microglia after tissue injury, such as Sall1, P2yr12 and Mrc1 (Fig. 6A). The downregulation of P2ry12 in laser-treated Irf8 KO mice prompted us to explore the expression of other purinergic receptors which are critical for MG cell activation and migration. Here, we found several other genes encoding purinergic receptors to be strongly downregulated in Irf8-deficient MG, such as Adora1, P2ry12 and P2ry13, underlining the proposed migration defect upon laser injury (Fig. 6B). Furthermore, we analysed the expression of key M1 (Cd86, H2-Ab1, Tlr2) and M2 signature genes (CD163, Mrc1) in isolated CNV-associated MG in Irf8-deficient mice and control animals (Suppl. Figure 5). We found that common M1 markers such as Cd86, H2-Ab1 and Tlr2 were significantly downregulated in Irf8-deficient MG compared with Irf8-potent MG in the laser CNV model. On the other hand, some of the common M2 markers, such as Cd163 and Mrc1, were significantly upregulated in Irf8-deficient retinal MG compared with Irf8-potent MG at sites of CNV suggesting a M1 to M2 polarization in Irf8-deficient MG compared with wild-type MG in the laser CNV model.

Fig. 6

Transcriptional profiling of Irf8 KO mice during CNV formation. A Volcano plot of differentially expressed genes in Irf8 KO retinal MG (n = 4) compared with control (n = 5) after laser photocoagulation. Significantly up- and downregulated genes are shown in red and blue, respectively. The top significantly up- and downregulated genes are labelled. B The top 5 upregulated GO clusters in retinal MG of lasered Irf8 KO mice. Significance is represented as p.adjust, the size of each data circle indicates the number of genes involved in each enriched GO term. C Differential expression of purinergic receptors in rMG from Irf8 KO compared with Irf8 WT mice. D Cnet-plot links Fibronectin (Fn1) to the GO terms inflammatory response, angiogenesis and cell adhesion. Genes written in bold belong to the top differentially upregulated genes (see A). E Expression of Fn1 is significantly increased on transcriptional level in Irf8-deficient microglia, shown as transcripts per million (Irf8 KO N = 4, Irf8 WT n = 5). Data are presented as mean ± SEM. F Expression of FN1 is significantly increased on protein level in Irf8-deficient microglia, measured by ELISA. N = 5 mice per group. Data are presented as mean ± SEM. G Expression of Fn1 can be traced back to myeloid Cx3cr1-GFP⁺ cells at the boarder of the CNV lesion at day 7 following laser. H Fibronectin and Collagen IV are strongly associated in the CNV lesions in both Irf8 WT and Irf8 KO mice

Next, we analysed the DEG that were upregulated in Irf8-deficient MG by GO cluster analysis and found an activation of biological processes such as “defense response” (GO:0006952, p.adj. < 8.4 × 10^-6), “biological adhesion” (GO:0022610, p.adj. < 2.9 × 10^-4), “cell adhesion” (GO:0007155, p.adj. < 6.1 × 10^-4), “inflammatory response” (GO:0006954, p.adj. < 9.5 × 10^-6) and “positive regulation of cell substrate adhesion” (GO:0010811, p.adj. < 1.9 × 10^-3) in Irf8-deficient MG (Fig. 6C). A closer look at the DEG of three key GO clusters essential for CNV development, namely "angiogenesis", "inflammatory response" and "cell adhesion", revealed Fibronectin, a profibrotic mediator encoded by Fn1, as a prominent upregulated gene in Irf8-deficient MG linking all three biological processes (Fig. 6D). In addition, we found a marked increase in the expression of other pro-fibrotic factors such as Fgf2 and Spp1 and a subtle increase in the expression of Tgfb1 in CNV-associated retinal MG in Irf8-deficient mice compared with control mice (data not shown). Consistent with the increased number of Fn1 transcripts in Irf8-deficient MG, we found significantly increased FN1 protein levels in the RPE/choroid of Irf8-deficient mice (3314 ± 587.1 pg/μg protein) compared with controls (1550 ± 268.5 pg/μg protein, p < 0.05) using ELISA on tissue lysates (Fig. 6E, F). Immunohistochemical studies showed that FN1 expression was restricted to the area of CNV lesions and expressed by microglia at sites of CNV (Fig. 6G). In addition to the enlarged collagen IV-positive CNV lesion described above, Irf8-deficient mice showed a markedly enlarged FN1-positive CNV lesion compared with WT mice, indicating increased fibrosis (Fig. 6H).

Taken together, these studies show that Irf8-deficient microglia exhibit a significantly altered expression profile in the laser CNV model with downregulated migratory genes, such as purinergic receptors, and upregulated pro-fibrotic factors, such as Fn1.

Discussion

The interferon regulatory factor 8 (IRF8) is an essential transcription factor for the development, maturation and homeostasis of microglia (MG) in the brain and other tissue macrophages [19, 21, 27]. However, the role of IRF8 for retinal MG (rMG) during homeostasis and neovascular eye disease has not been elucidated so far. In this study, we show that Irf8 is essential for a mature rMG gene expression profile and influences MG morphology, migration and the response to pathological neovascularisation.

Our results show that Irf8 is strongly expressed in rMG in the steady state compared with other IRF family members. The expression of Irf8 in rMG was even substantially higher than in brain MG (bMG), suggesting a distinct and tissue-specific function of Irf8 in microglia of the retina. Morphological analysis revealed that Irf8-deficient mice exhibited an overall reduced branching of rMG as well as a decreased MG cell number specifically in the outer plexiform layer, which was already observed during postnatal development. These findings recapitulate findings in the brain [21, 27, 39, 44] and point to a migratory defect that is already present during postnatal retinal layering and maintained into adulthood. To gain further insight into the molecular changes in Irf8-deficient rMG, we isolated rMG by flow cytometry and analysed their transcriptional profile by RNA sequencing. Our analysis revealed significant transcriptional differences between Irf8-potent and Irf8-deficient microglia, which is consistent with several in vitro studies [25, 40]. We found that Sall1 was the most downregulated MG signature gene in the retina of Irf8-deficient mice. This is of particular functional importance since SALL1 is a critical transcription factor for maintaining the homeostatic gene expression pattern of MG and thus regulates, for example, the expression of MG signature genes such as Aif1, P2ry12 and Tmem119 [6, 33, 55]. Accordingly, we found Tmem119 and P2ry12 as significantly reduced in Irf8-deficient rMG recapitulating the findings from human brain microglia which suggest a dependence of P2RY12 expression on IRF8 signalling [5]. Notably, because SALL1 is not exclusively expressed by microglia but also by astrocytes and oligodendrocytes [8, 38, 48], non-cell autonomous effects of this gene cannot be excluded. Further, single-cell RNA-seq (scRNA-Seq) of conditional Irf8 KO mice (Fcgr1-Cre:Irf8^fl/fl) revealed a strong downregulation of Sall1, Aif1, Tmem119 and P2ry12 in bMG while other genes, typically expressed in macrophages, like Mrc1, encoding the mannose receptor CD206, were upregulated [58]. In line with this study, we found a strong upregulation of Mrc1 on transcriptional level and the encoded mannose receptor CD206 on protein level in Irf8-deficient rMG which is consistent with data from Irf8-deficient bMG [44]. In addition, other myeloid genes like Fcgr1, also known as CD64, were downregulated on RNA and protein level. These findings strongly support common transcriptional changes between retinal MG and brain MG under Irf8-deficient conditions, as shown before in a direct comparison of wild-type rMG and bMG by scRNA-seq [59]. Furthermore, it underscores that retinal microglial differentiation and maturation are highly dependent on a defined transcriptional program instructed by PU.1 [16], SALL1 [29] and IRF8.

To identify functionally related gene signatures, we performed a gene ontology (GO) enrichment analysis that revealed a downregulation of the clusters “cell migration“, “cell motility”, “cell adhesion” and “regulation of cell proliferation” in adult Irf8-deficient rMG in the steady state. The downregulation of these GO terms was consistent with the reduced number of rMG in the OPL in adult Irf8 KO mice, supporting previous in vitro data describing IRF8 as an essential transcription factor for microglial motility and migration [28, 39]. The significant downregulation of genes relevant for cell migration could also explain the observed developmental phenotype and point to an impaired Irf8-dependent perception of guiding cues. During development, neurons constantly release guiding cues, such as purines and other extracellular nucleotides which guide microglia to colonise the developing outer retina [1, 37]. Irf8-dependent downregulation of sensors that detect these guiding cues, such as Adora1 or P2yr12, may be responsible for the disruption of purinergic signalling in Irf8-deficient rMG, which attenuates their migratory capacity. Indeed, in vitro cultivated brain MG lacking Irf8 had a strongly reduced phosphorylation of AKT after ATP treatment, thereby diminishing the ATP-mediated signalling pathways of P2RY12 [40]. This hypothesis is supported by in vitro studies showing a diminished entry of rMG into retinal explant cultures following an interruption of purinergic signalling [37]. Furthermore, proliferation of myeloid cells relies on IRF8 signalling [61] which could explain the insufficient compensatory expansion of MG in the OPL and contribute to the niche-dependent phenotype with reduced microglial density especially in the OPL in adult Irf8-deficient mice.

Despite the aforementioned significant changes in MG cell density and transcriptional profile, Irf8-deficient mice exhibited a normal retinal structure, vascular supply, and physiological function. This is particularly surprising as retinal MG are in close contact with retinal vessels, especially during development, and are known to shape the mature retinal vasculature [9, 13, 16, 18]. This suggests that Irf8-deficient MG are functionally sufficient to accompany physiological retinal development and that minor developmental disturbances, which we cannot completely rule out, can be compensated over time. The fact that Irf8-deficient microglia exhibit transcriptional changes that reduce their responsiveness while maintaining a normal retinal phenotype, provides an ideal setting to study the role of microglia in the development of choroidal neovascularisation, which is known to be associated with significant microglia activation and migration [35, 52, 59].

In the laser-induced CNV model, which mimics aspects of neovascular AMD, we found significantly increased CNV lesion size under Irf8-deficient conditions. At the same time, the overall numbers of Irf8-deficient Cx3cr1-GFP⁺ cells were significantly reduced around the lesions compared with wild type. In line with this finding, MG density in the IPL above CNV lesions was significantly decreased in Irf8 KO mice compared with wild type. These observations may be mediated either by a migration defect caused by impaired purinergic signalling [45] or by reduced microglial proliferation of Irf8-deficient MG, or both, as discussed above. Interestingly, the present study shows that impaired migration and a lower number of MG in the vicinity of CNV are associated with a more severe CNV phenotype in Irf8-deficient mice. This finding is in contrast to previous studies showing that depletion of retinal or circulating myeloid cells by clodronate is associated with reduced CNV size suggesting an anti-angiogenic effect of myeloid cells on CNV [14, 34, 51]. On the other hand, however, our results are consistent with reports showing that increased accumulation of myeloid cells in neovascular lesions is associated with decreased CNV and that myeloid cells use FasL (CD95L) to inhibit CNV formation [2]. These seemingly contradictory contributions of myeloid cells to CNV development could be reconciled by the potentially different roles of resident MG and infiltrating monocyte-derived macrophages. To investigate the distinct roles of these cellular populations, this study exploits Irf8-deficient mice which are characterized by a near absence of circulating monocytes and, at the same time, altered but present resident retinal microglia. The enlarged CNV lesions in Irf8-deficient mice associated with reduced numbers of Cx3cr1-GFP⁺ resident microglia cells may thus be interpreted as a consequence of dysfunctional pro-fibrotic Irf8-deficient MG or as a result of insufficient numbers of CNV-suppressing microglia in Irf8-deficient animals. The latter may in turn indicate a general protective role of wild-type microglia which would be in line with previous studies [2, 46]. The hypothesis that deficient microglia substantially influence CNV size in Irf8-deficient mice is further supported by the head-shielded bone marrow transplantation experiments performed in this study, which showed enlarged CNV in Irf8-deficient animals compared with controls despite successful reconstitution of Irf8-potent peripheral monocytes. However, we cannot exclude the possibility that other Irf8-expressing cell types in the retina or from the blood contribute to the increased CNV lesion size in Irf8-deficient mice. Since Irf8 expression in the retina was mainly restricted to retinal microglial cells, which represent the most numerous myeloid cell population in CNV, in contrast to a low number of infiltrating peripheral monocytes [59], we consider this possibility rather unlikely. Furthermore, heterozygous Cx3cr1^GFP/+ expression could have an impact on myeloid cells and be associated with an inflammatory phenotype. However, since both Irf8 wild-type and knockout mice in our study were consistently heterozygous for Cx3cr1, we consider this effect negligible and used the Cx3cr1^GFP/+ line to visualise Irf8 wild-type and knockout mice in a comparable manner, since other standard markers such as IBA1 are dysregulated and cannot be used [44].

To explore potential mechanisms in Irf8-deficient retinal MG contributing to CNV formation, we next performed RNA-sequencing on sorted retinal MG at sites of CNV.

Among others, we found that purinergic receptors, encoded by genes such as P2ry12, P2ry13 and Adora1, were significantly downregulated in Irf8 KO rMG after laser injury. Since these receptors are critical for the recognition of ATP released during tissue injury and thus control cell migration, their downregulation may be at least partly responsible for the reduced MG cell number at sites of CNV in Irf8-deficient mice [12, 23, 30]. This hypothesis is in line with in vitro work by Masuda et al. showing a downregulation of genes encoding purinergic receptors, including P2ry12 and P2rx4, in Irf8-deficient brain microglia which was associated with a migration defect in vitro [39]. It is interesting to note that Irf8-deficient retinal microglia accumulating at CNV showed less M1 and more M2 signature gene expression compared with wild-type MG at CNV, suggesting increased M1 to M2 polarization in Irf8-deficient MG. This is of particular clinical interest as some studies have suggested that more M2-like macrophages, which are assumed to be pro-angiogenic, accumulate at the site of wet compared with dry AMD and that the pathological shift of macrophage polarization may contribute to the pathogenesis of CNV in neovascular AMD [7]. The expression signatures or myeloid cells at the lesion site are likely to be more complex than the aforementioned polarization state; however, it confirms an altered signature of a set of well-known and characterized markers. Furthermore, GO cluster analysis showed that Irf8-deficient rMG exhibit increased activity of biological processes that are critical for inflammation and cell adhesion, which points to an interaction of microglia with extracellular matrix components driving CNV formation. We hereby identified Fibronectin, encoded by the Fn1 gene, as being significantly higher expressed in Irf8 KO rMG and linking the GO terms "cell adhesion", "inflammatory response" and "angiogenesis". The immunohistochemical and ELISA analyses confirmed that the expression of Fibronectin protein was also significantly increased at sites of CNV, suggesting that Irf8-deficient MG or other cells affected by the loss of Irf8 contribute to increased Fibronectin abundance at sites of CNV. Of note, collagen IV fibers were reported to depend on an established Fibronectin matrix directly co-localizing with Fibronectin fibers in vitro that could be functionally related to our observation of increased CNV lesion size promoted by higher Fibronectin expression in rMG [42, 43]. Furthermore, we found a marked increase in the expression of the pro-fibrotic factors Fgf2 and Spp1 and a subtle increase in the expression of Tgfb1 in CNV-associated retinal MG in Irf8-deficient mice compared with control mice. Since FGF2 and SPP1 are important mediators of scarring and have been identified in human choroidal neovascular membranes [17, 52], overexpression of these factors in retinal MG may have further contributed to increased CNV lesion size in Irf8-deficient mice. This is of particular interest as pharmaceutical inhibition of SPP1 has been shown to modulate CNV formation and inhibition of FGF2 was associated with reduced CNV and subretinal fibrosis in a laser-induced mouse CNV model [3, 41, 52].

Conclusions

In conclusion, this study identifies IRF8 as a critical mediator for the morphology, distribution and expression profile of retinal microglia, and for transformation to a reactive phenotype. The niche-dependent phenotype already present during postnatal development, the altered morphology and the disturbed rMG distribution did not lead to any impairment of retinal morphology and function in the steady state, but to enlarged lesions in the laser CNV model. This highlights the importance of IRF8 and retinal MG for the development of pathological neovascularisation in the eye and highlights the potential of immunomodulatory therapeutic interventions of rMG recruitment in retinal disease.