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Differential Requirement for irf8 in Formation of Embryonic and Adult Macrophages in Zebrafish

  • Celia E. Shiau ,

    wtalbot@stanford.edu (WST); shiauc@ornl.gov (CES)

    Current address: Biosciences Division, Oak Ridge National Laboratory, Oak Ridge, Tennessee, United States of America

    Affiliation Department of Developmental Biology, Stanford University School of Medicine, Stanford, California, United States of America

  • Zoe Kaufman,

    Affiliation Department of Developmental Biology, Stanford University School of Medicine, Stanford, California, United States of America

  • Ana M. Meireles,

    Affiliation Department of Developmental Biology, Stanford University School of Medicine, Stanford, California, United States of America

  • William S. Talbot

    wtalbot@stanford.edu (WST); shiauc@ornl.gov (CES)

    Affiliation Department of Developmental Biology, Stanford University School of Medicine, Stanford, California, United States of America

Differential Requirement for irf8 in Formation of Embryonic and Adult Macrophages in Zebrafish

  • Celia E. Shiau, 
  • Zoe Kaufman, 
  • Ana M. Meireles, 
  • William S. Talbot
PLOS
x

Abstract

Interferon regulatory factor 8 (Irf8) is critical for mammalian macrophage development and innate immunity, but its role in teleost myelopoiesis remains incompletely understood. In particular, genetic tools to analyze the role of Irf8 in zebrafish macrophage development at larval and adult stages are lacking. We generated irf8 null mutants in zebrafish using TALEN-mediated targeting. Our analysis defines different requirements for irf8 at different stages. irf8 is required for formation of all macrophages during primitive and transient definitive hematopoiesis, but not during adult-phase definitive hematopoiesis starting at 5-6 days postfertilization. At early stages, irf8 mutants have excess neutrophils and excess cell death in pu.1-expressing myeloid cells. Macrophage fates were recovered in irf8 mutants after wildtype irf8 expression in neutrophil and macrophage lineages, suggesting that irf8 regulates macrophage specification and survival. In juvenile irf8 mutant fish, mature macrophages are present, but at numbers significantly reduced compared to wildtype, indicating an ongoing requirement for irf8 after embryogenesis. As development progresses, tissue macrophages become apparent in zebrafish irf8 mutants, with the possible exception of microglia. Our study defines distinct requirement for irf8 in myelopoiesis before and after transition to the adult hematopoietic system.

Introduction

Myeloid cells form the innate immune system that provides the immediate response to protect the host after infection and injury. Macrophages, monocytes, and granulocytes (including neutrophils) are major myeloid cell types [14]. The proper formation of these myeloid cells during development and their continuous replenishment throughout life are essential to sustain the function of the immune system. As in mammals, hematopoiesis in zebrafish occurs in several waves [1, 5, 6]. This process begins with the primitive wave in the anterior lateral plate mesoderm of the zebrafish embryo, then transitions to the transient definitive wave in the posterior blood island (PBI), which later becomes the caudal hematopoietic tissue (CHT). Subsequently, definitive blood development takes place in the CHT and the zebrafish aorta-gonad-mesonephros (AGM) analog. At later stages, definitive hematopoiesis moves to the pronephric kidney, which is the site of adult hematopoiesis [5, 6]. More is known about the development of hematopoietic stem cells (HSCs) into different myeloid fates in the definitive wave than in the earlier waves of blood formation [2, 3, 6, 7], although the mechanisms are not fully understood in either the early or late waves.

A major determinant of macrophage/monocyte fate during hematopoiesis is the transcription factor IRF8, a member of the interferon regulatory factor (IRF) family. IRF proteins contain a conserved N-terminal DNA binding domain that recognizes the interferon consensus sequence, and they regulate transcription of interferon genes during immune response [8]. In mammals, IRF8 is critical for myeloid development. IRF8 deficiency in human and mouse leads to a significant reduction of macrophage/monocyte development but an expansion of neutrophils and undifferentiated hematopoietic progenitor cells, reminiscent of myeloid leukemia [912]. In mouse, IRF8 is strongly expressed in mononuclear phagocytes (macrophages, monocytes, and dendritic cells)[3, 13], and regulates differentiation of these phagocytes and granulocyte-macrophage progenitors [9, 10, 14]. In human, missense mutations disrupting transcriptional activity of IRF8 are linked with immunodeficiencies that severely reduce the numbers of dendritic cells and monocytes [11], indicating its role in human myeloid development. Furthermore, IRF8 is transcriptionally repressed in many acute and chronic myeloid leukemia (AML and CML, respectively) patients [15, 16], suggesting a link between IRF8 activity and these diseases. In zebrafish, transient knockdown of irf8 by translation- and splice- blocking morpholinos eliminated the embryonic macrophage population and expanded the neutrophil population [17], but mutations in zebrafish irf8 have not been available to enable long-term studies. Thus, IRF8 plays key roles in maintaining normal production of myeloid cell types, but the nature of its function in specification and maintenance of myeloid cells at different times in development are not understood, and the extent of its functional conservation across species remains to be fully explored.

To investigate the function of irf8 at different stages of development to early adulthood in zebrafish, we created irf8 null mutations. irf8 mutants are devoid of macrophages during embryogenesis, but have an increase of neutrophils and immature or apoptotic myeloid cells. As larval development progresses, some macrophages are present in the mutants, indicating that macrophages at different stages have distinct requirements for Irf8 function. The late-emerging macrophages in irf8 mutants are likely derived from different progenitors from the embryonic macrophages (HSCs versus early myeloid), which coincides with the differential dependence on irf8. Our study provides new insights into the role of irf8 in myeloid cell fate regulation in zebrafish before and after transition to the adult hematopoietic system.

Results

irf8 null mutants lack microglia during development and are viable

Morpholino knockdown studies have indicated that irf8 plays a role in macrophage development in zebrafish [17], but mutations in the zebrafish irf8 gene have not been available to allow analysis of a complete loss of irf8 function, or analysis at later stages. Furthermore, excess immature myeloid cells were observed in Irf8 mouse mutants but not reported in the zebrafish morpholino studies [17], so the degree of conservation of Irf8 function between zebrafish and mammals is not fully understood. To construct loss-of-function mutations in irf8, we used TALEN-mediated targeting to generate two new mutant alleles, irf8st95 and irf8st96 (Fig. 1A). Both alleles have frameshift mutations just 3’ to the translational initiation codon, and both are predicted null mutations (Fig. 1A). The zebrafish genome contains only one ortholog of mammalian Irf8, and therefore these mutations are predicted to eliminate all functions of Irf8 in zebrafish.

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Fig 1. TALEN-induced irf8 mutations st95 and st96 eliminate embryonic microglia but allow survival to adulthood.

(A) TALE nucleases target region near irf8 translational start site, creating frameshift mutations st95 and st96, which introduced premature stop codons as shown (bottom). Top panels show representative neutral red staining for microglia in irf8st95/st95 mutant that lacks all microglia, compared with a heterozygous sibling that has a wildtype microglial population (arrow). (B) Analysis of apoe RNA expression by in situ hybridization shows presence of microglia in irf8 sibling but no microglia in irf8 mutants at 3 and 6 dpf. (C) Images of heterozygous and homozygous mutant larvae at 5 dpf, showing that the mutants have normal overall morphology. Images of the whole adult zebrafish were compiled from two tiled images of the same fish. At 3 months of age, the irf8 mutant zebrafish grew to a similar size as its sibling. All images represent the st95 allele. Scale bars are shown below each set of panels or for each individual panel.

https://doi.org/10.1371/journal.pone.0117513.g001

To characterize the phenotypes of irf8st95 and irf8st96 mutants, we examined microglia, the brain-resident macrophages previously shown to be disrupted by splice- and translation- blocking morpholinos against irf8 [17]. Homozygous irf8st95/st95 and irf8st96/st96 mutants, and transheterozygous irf8st95/st96 mutants all lacked microglia at 3–6 dpf, as determined by neutral red staining [19] and expression of apoe [2022](Fig. 1A and B, and data not shown). We have focused our analysis on irf8st95, and the irf8-/- mutants pictured in the figures are irf8st95/st95 homozygotes, unless noted otherwise.

Despite the loss of microglial cells during the embryonic and larval stages, irf8-/- mutants appeared morphologically normal as early larvae (Fig. 1C). Furthermore most irf8 -/- mutants were viable as adults at approximately 3 months postfertilization (Fig. 1C), although their survival rate was reduced compared to heterozygous and wildtype siblings (S1 Fig.).

irf8 mutants have no macrophages but have excess neutrophils during embryogenesis

To further characterize the irf8 mutants, we examined the early development of myeloid cells at embryonic stages. In zebrafish, adaptive immunity begins after 3–4 weeks postfertilization [23], and macrophages and neutrophils are the main functional leukocytes in the embryo [18]. We assessed the distribution of macrophages and neutrophils by examining the cell-type specific markers mfap4 and mpx, respectively. In comparison to wildtype and heterozygous siblings, irf8-/- mutants developed no mfap4-expressing macrophages (Fig. 2A), and had a large expansion of mpx-expressing neutrophils (Fig. 2B and C). The increase in neutrophils was evident throughout the embryo, and at stages as early as 1 dpf (Fig. 2B–D). Our genetic analysis validates the embryonic phenotypes observed previously in irf8 morphants [17]. In addition, the finding that irf8 null mutants are viable as adults allows the analysis of irf8 function into adulthood.

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Fig 2. irf8 mutant embryos have no macrophages but produce excessive neutrophils.

(A) mfap4 RNA expression at 2 dpf shows a complete loss of macrophages in irf8 mutant but abundant macrophages in heterozygous sibling (arrows). (B) mpx RNA expression at 2 dpf shows an overproduction of neutrophils in irf8 mutants (arrows, bottom panels) compared with the sibling (arrow, top panels). Right column in A and B shows a higher magnification image of the trunk region from the same embryos depicted in the left column. (C) Neutrophils can first be detected on the yolk sac by 1 dpf. irf8 mutants have many yolk sac neutrophils (arrows) compared with sibling. (D) At 2 dpf, irf8 mutants continue to have more neutrophils on the yolk sac (arrows). Overall, irf8 mutants appear to have more neutrophils throughout the body. All scale bars are 100 um.

https://doi.org/10.1371/journal.pone.0117513.g002

Partial recovery of macrophages in irf8 mutants coincides with presumptive onset of hematopoiesis in the kidney

To address the possible roles of irf8 in macrophage development at later stages, we used Tg (mpeg1: EGFP) to examine GFP-labeled macrophages at stages up to 31 dpf in irf8-/- mutants and their siblings. These macrophages were examined in live fish up to 1 week old (7 dpf) and after fixation at later stages (Figs. 3 and 4). We analyzed two regions where macrophages are normally widespread: first, the caudal hematopoietic tissue (CHT) in the ventral mesenchyme of the tail, which is the major location of new blood formation at larval stages; and second, the otic or ventral area of the head that is proximal to the pronephric kidney, the location of adult hematopoiesis (Figs. 3 and 4).

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Fig 3. irf8 mutants have immature myeloid cells and excess myeloid cell death during development in the CHT.

Diagram of a zebrafish larva showing the regions of analysis in the CHT: red box, region in A and B; blue box, region in C and D; and dotted lines in blue box indicate area of TUNEL quantification in E. (A-B) Lateral view. Right panels, higher magnification of the dotted box shown on the left. Analysis at 2.5 dpf (A) and 5 dpf (B) shows that siblings have many macrophages strongly expressing mpeg1:EGFP; these cells have elaborate processes and complex morphologies, and some have migrated into other tissues (white arrows). By contrast, irf8 mutants have cells weakly expressing mpeg1:EGFP that appear immature and different from macrophages in siblings. A few strongly expressing cells are first detected in mutants at 5 dpf (B, blue arrows), indicating recovery of a few macrophages. (C-D) Early myeloid reporter pu.1:gal4-UAS-GFP at 5 dpf shows abnormally small cellular specks restricted to the CHT in all mutants (D, arrows, n = 9/9 at 3 and 5 dpf) but not in the siblings (C, n = 5/5 at 3 and 5 dpf). Bottom, TUNEL labeling of apoptotic cells at 5 dpf. The small pu.1 reporter expressing cellular specks in the CHT are similar in size and appearance to small-sized dying cells labeled by TUNEL, which are shown in another 5 dpf stage-matched irf8 mutant larva (compare arrows in top panel with arrowheads in bottom panel from different larvae). TUNEL labeling (middle) and area traces of the TUNEL+ nuclei (bottom) are shown for each genotype. (E) Quantification of TUNEL assay as represented in C-D shows a significant increase in total dying cells in the CHT of irf8 mutants (n = 3) compared with siblings (n = 6; p = 0.0039). This is largely accounted for by a significant increase in very small-sized TUNEL+ cells measuring less than 26 pixels in area (p = 0.0017). No significant difference was found in larger TUNEL+ cells (≥ 26 pixels in area, p = 0.16). Error bars represent S.E.M. Statistical significance was determined by two-tailed Student’s t-test. **, p < 0.01; *, p < 0.05; n.s., not significant; CHT, caudal hematopoietic tissue. All scale bars are 50 um and are the same for each set of panels.

https://doi.org/10.1371/journal.pone.0117513.g003

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Fig 4. Partial recovery of macrophages in irf8 mutants begins by ~7 dpf in the head region.

Diagrams of zebrafish showing region of quantification (pink box), which was taken using the same magnification and field size of view at all stages. The field of view in older stages covers a relatively smaller region of the head because the fish are larger (comparing B with A). Red dotted box shows the region of the fluorescent images. (A) Expression of macrophage reporter mpeg1:EGFP at 6 and 7 dpf. Arrows show macrophages. At 6 dpf, most irf8 mutants have no macrophages in the CHT (n = 7/12), while most have a few macrophages in the head (n = 10/13); image shows the head region of a mutant at 6 dpf with no macrophages. Panels show the tail CHT region of the irf8 mutants at 6 and 7 dpf with no macrophages; a few autofluorescent pigment cells are present after PTU treatment. (B) Distribution of macrophages expressing mpeg1:EGFP at 14 dpf and 31 dpf. Arrows point to macrophages. (C) Quantification of the number of macrophages per field in the head region over time (pink box in left diagram). (D) Quantification of the number of macrophages per field in the tail region over time (pink box in right diagram). At 6 dpf, n = 20 for siblings and n = 13 for mutants; at 14 dpf, n = 8 for siblings and n = 7 for mutants; at 31 dpf, n = 7 for siblings and n = 5 for mutants. Statistical significance was determined by two-tailed Student’s t-test. Error bars represent S.E.M. ***, p < 0.001; **, p < 0.01; *, p < 0.05; CHT, caudal hematopoietic tissue; E, eye. All scale bars are 50 um. irf8-/- in this figure represents trans-heterozygous irf8st95/st96 mutants.

https://doi.org/10.1371/journal.pone.0117513.g004

Although there was a lack of mature mfap4-expressing macrophages at embryonic stages (Fig. 2), we observed small cells that weakly expressed mpeg1:EGFP at 2.5 dpf in the mutants. These cells were restricted to blood-forming regions in the tail—they did not disperse to other tissues, in contrast to wildtype macrophages (Fig. 3A). These cells may be immature myeloid cells, based on their location and weak mpeg1 reporter expression, lack of detectable mfap4 expression (Fig. 2), and the previous finding that Irf8 knockout mice have unchecked proliferation of immature myeloid cells [9, 12, 24]. Alternatively, these small cells in the mutants may be dying myeloid cells or cell debris.

By 5 dpf, a few strongly labeled mpeg1-expressing macrophages were present in some homozygous irf8 mutants, but other mutants appeared to have no macrophages (Figs. 3B and 4). At this time, the mutants also showed significantly increased cell death in the CHT region (Fig. 3C and D), evidenced by an increase of very small TUNEL-positive cells (Fig. 3E). In addition, we detected aberrant, small-sized or rounded cells and fragments expressing the pu.1 reporter transgene in all mutants analyzed but not in the siblings (Fig. 3C–E), which is consistent with myeloid precursor cell death in irf8 mutants. In summary, irf8 mutants have abnormally small cells that weakly express mpeg1:EGFP, and they have significantly increased cell death in the pu.1+ myeloid precursors.

By 7dpf, irf8 mutants contained macrophages strongly expressing mpeg1:EGFP in the head and thymic region near the otic vesicle (Fig. 4A). These first-appearing macrophages in the irf8 mutants appear less mature than wildtype, being rounded with few or no processes (Fig. 4A). In the ventral head at 14 dpf and 31 dpf (Fig. 4B), the number of macrophages increased in irf8 mutants, but it remained less than half of that in wildtype and heterozygous siblings in the head and tail regions (Fig. 4C and D).

In our time course analysis of mpeg1:EGFP expression at different stages, it was clear that the number of mpeg1:EGFP expressing macrophages was more strongly reduced in the tail than in the head (Fig. 4C and D). The increased number of macrophages in the ventral head region may reflect proximity to the pronephric kidney, which becomes the predominant site of blood formation starting at about the same time that the first macrophages became evident in irf8 mutants. The absence of macrophages in irf8 mutants before 5–6 dpf indicates that irf8 is a key regulator of all macrophage populations in the embryo and early larva. The recovery that begins in mid-larval stages at ~7 dpf suggests that later precursor cells, such as the hematopoietic stem cells (HSCs) from the kidney marrow, may depend on a combination of irf8 and other factors. Despite this transition, irf8 is essential to achieve normal macrophage numbers over the long-term, as the recovery of macrophages in irf8 mutants is incomplete.

irf8 mutants recover macrophages but apparently lack microglia at 31 dpf

The presence of macrophages in the head of irf8 mutants at 14 dpf and later stages prompted us to determine whether microglia are also present at these stages. We examined microglia in sections of the midbrain at 31 dpf using antibodies against leukocyte marker L-plastin, which labels microglia in the uninjured adult zebrafish brain [25]. At 31 dpf, wildtype fish contained many cells expressing L-plastin with the elaborate morphologies characteristic of microglial cells (S2 Fig.). In irf8 mutants, we were unable to identify similar cells in the brain parenchyma, but instead observed only a few putative macrophages that were located in the ventricular zone, adjacent to vasculature or in the interstitial space between the brain and the head epithelium (S2 Fig.). These results suggest that microglia are absent in irf8 mutants at stages up to 31 dpf, several weeks after other macrophages were evident in irf8 mutants. Our analysis is consistent with previous studies showing that microglia originate from primitive macrophages at early stages but not from later-forming definitive macrophages or monocytes [26, 27].

irf8 mutants have myeloid cells and neutrophils competent to become macrophages after expression of wildtype irf8

A previous irf8 morpholino study suggested that knockdown of irf8 caused macrophage progenitors to switch to a neutrophil fate [17], while our data suggested that irf8 mutants have undifferentiated and dying myeloid cells (Fig. 3) in addition to increased neutrophils. To investigate the possibilities that irf8 can regulate the specification and survival of macrophage precursors and the fate decisions of neutrophil-macrophage precursors, we sought to restore macrophages in irf8 mutants by expression of wildtype irf8 in the macrophage and neutrophil lineages, respectively. Regulatory sequences for mpeg1, lyz, huc, and krt4, as previously described [21], were used to express irf8 in macrophages, neutrophils, neurons, and skin cells, respectively (Fig. 5). These constructs also contain the cmlc2-GFP cassette to allow the analysis of animals with successful integration, as detected by strong GFP expression in the heart. We assessed microglial cells by neutral red staining at 4 dpf and the total macrophage population with the marker mfap4 at 2.5 dpf (Fig. 5). We analyzed the action of the transgenes in embryos from irf8 heterozygous intercrosses in order to evaluate the effect of irf8 expression in mutant and wildtype siblings.

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Fig 5. Specific expression of irf8 in macrophage or neutrophil lineage is sufficient to restore macrophage fates in irf8 mutants.

(A) Neutral red staining for microglia at 4 dpf in irf8 siblings and mutants in control uninjected conditions or after tol2-mediated expression of irf8 driven by tissue specific regulatory sequences. Expression of mpeg1:irf8 or lyz:irf8 was sufficient to restore some microglia in irf8 mutants (arrows), but not expression in the neurons (huc) or skin (krt4). (B) Analysis of total macrophage population by mfap4 RNA expression at 2.5 dpf after expression of irf8 in different tissues. Specific expression of mpeg1:irf8 or lyz:irf8 was also sufficient to restore macrophages on yolk sac and embryo proper (arrows) in irf8 mutants. (C) Plot showing frequency of microglia rescue. (D) Plot showing frequency of macrophage recovery. Purple denotes >25 macrophages and green shows partial recovery of less than 25 but more than 1. Numbers below bar graphs represent n, total number of embryos analyzed. sib, irf8+/+ and irf8+/-; mut, irf8-/-.

https://doi.org/10.1371/journal.pone.0117513.g005

When wildtype irf8 expression was introduced transiently under the control of macrophage-specific regulatory sequences for mpeg1, we detected some recovery of macrophages by 2.5 dpf and microglia by 4 dpf in irf8 mutants, which normally lack all macrophages and microglia at these stages (Fig. 5). The ability to rescue macrophages in irf8 mutants using the mpeg1:irf8 transgene provides further evidence that the cells weakly expressing the mpeg1 reporter in irf8 mutants are immature cells competent to become mature macrophages when wildtype irf8 is expressed.

To test the other possibility that irf8 can restore macrophage fate in the expanded neutrophils in irf8 mutants, we transiently expressed the wildtype irf8 coding sequence in neutrophils. Strikingly, ectopic expression of irf8 in neutrophils using lyz regulatory sequences led to a partial recovery of microglia and macrophages in the irf8-/- mutants (Fig. 5). The rescue of macrophages with the mpeg1:irf8 and lyz:irf8 constructs appeared specific to the macrophage and neutrophil lineages, because the transgenes driving expression in skin and neurons did not rescue macrophages or microglia in irf8 mutants (Fig. 5). Interestingly, none of the irf8 expression constructs appeared to affect the overall number and distribution of macrophages and microglia in wildtype and irf8 heterozygotes (Fig. 5 and data not shown). These experiments suggest that both immature myeloid and neutrophil populations in irf8 mutants are capable of developing into mature macrophages after expressing wildtype irf8.

Discussion

Our study reveals that specification of all macrophages requires irf8 during a discrete early period of zebrafish hematopoiesis that includes the primitive and transient definitive waves in zebrafish (Fig. 6). The macrophage deficiency and overproduction of neutrophils and progenitor cells in zebrafish irf8 mutants are similar to the phenotypes of humans and mice carrying loss-of-function mutations in Irf8 [1012, 30]. Also similar to Irf8 knockout mice and human patients homozygous for inactivating mutations of Irf8 [11, 12], zebrafish irf8 null mutants were viable. Zebrafish irf8 mutants thereby provide a new model to understand the diverse roles of irf8 in development and innate immunity that will likely be relevant to mammalian Irf8.

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Fig 6. Summary model for role of irf8 in macrophage ontogeny in zebrafish.

irf8 is required for development of all macrophages in the early developmental period until 5–6 dpf (solid orange bar). Coinciding with the onset of the adult phase hematopoiesis in the kidney starting at ~7 dpf, hematopoiesis relies on irf8 and other factors for macrophage specification and differentiation (dotted orange bar). RBI, rostral blood island; PBI, posterior blood island; CHT, caudal hematopoietic tissue; AGM, aorta-gonad-mesonephros analog; hpf, hours postfertilization; dpf, days postfertilization.

https://doi.org/10.1371/journal.pone.0117513.g006

Our analysis underscores different genetic controls of hematopoiesis at early and late stages. Despite the complete absence of macrophages in irf8 mutants at early stages, some mature macrophages were present in irf8 mutants by mid-larval stages. The recovery of macrophages in irf8 mutants is more prominent in the head than in the tail through one month of age. This suggests that the late-emerging macrophages in irf8 mutants may be derived from hematopoietic stem cells (HSCs) in the developing kidney, which is located near the ventral head. The different origins of the macrophages at different stages (primitive myeloid cells early and HSCs later) may explain their differential dependence on irf8 (Fig. 6). Kidney-derived HSCs may utilize a combination of irf8 and other factors to specify macrophages, whereas the early myeloid progenitors in the embryo all require irf8 to develop as macrophages, possibly reflecting a more homogenous population that requires the same genetic program for macrophage differentiation at early stages.

Our data in combination with the analysis of irf8 morphants [17] provide evidence that irf8 is essential to regulate granulocyte-macrophage fate decisions in myeloid progenitors and maturation of macrophage precursors. This is consistent with recent characterization of IRF8-EGFP reporter mice that shows strong upregulation of IRF8 reporter expression in granulocyte-myeloid progenitors and monocytic/macrophage progenitors, but low expression in granulocytes [13]. We show that driving expression of irf8 in the macrophage and neutrophil lineages in irf8 mutants is sufficient to restore macrophage fate. Similarly, in mouse, induced Irf8 expression in Irf8-/- myeloid progenitors in vitro allowed their differentiation into mature macrophages [10]. Although irf8 expression in neutrophils does restore some macrophages in irf8 mutants, many excess neutrophils were not converted to macrophages. This likely reflects, in part, the mosaic expression of irf8 in these assays, but it is also possible that some of the excess neutrophils arise as a secondary consequence of the loss of macrophages, increased myeloid cell death, or both, and not from alterations of progenitor cell fates. Thus, some excess neutrophils may not be competent to convert to macrophages. In mammals, macrophage depletion can cause neutrophilia, possibly due to defective clearance of apoptotic cells after macrophage loss [31], and wounds depleted of macrophages are populated by large numbers of neutrophils [32].

The conservation of Irf8 in macrophage/monocyte specification seems clear, although the extent of the Irf8 requirement appears more far-reaching in zebrafish than in mammals. All macrophages and microglia are eliminated in the irf8 mutant zebrafish embryo, whereas Irf8 deficient mice lose a subset of macrophages/monocytes and dendritic cells at embryonic and adult stages [14, 3336]. This includes a severe but incomplete reduction of the yolksac c-kit+ erthryomyeloid precursors that give rise to microglia [27]. Mouse Irf8 mutants also retain varied levels of other tissue macrophages including Langerhans cells [36]. At the time of macrophage recovery, zebrafish irf8 mutants do not appear to lack specific subpopulations of macrophages based on anatomical distribution, with the apparent exception of microglia. However, we cannot exclude the possibility that microglia arise at later stages, or that other subsets of macrophage/monocyte are lacking in zebrafish irf8 mutants.

In summary, we show that Irf8 is essential for the development of all macrophage fates through the early waves of zebrafish hematopoiesis (primitive and transient definitive), but not adult-phase hematopoiesis (Fig. 6). Although the nature of its function changes over time, Irf8 is continuously required to allow normal production of macrophages in zebrafish. Besides its role in myeloid development, Irf8 has essential roles in host defense [3739]. The generation of zebrafish irf8 mutants thus provides a new in vivo model to dissect the different functions of Irf8 in hematopoiesis and host defense.

Materials and Methods

Zebrafish lines and embryos

Embryos from wildtype (TL, AB/TU, and WIK), transgenic (Tg(lyz:EGFP)[28], Tg(mpeg1:EGFP)[29], and Tg(pu.1:Gal4-UAS-EGFP)[22]), and irf8st95 and irf8st96 heterozygous intercross backgrounds were raised at 28.5°C, and staged by established standards [40]. Embryos were treated with 0.003% 1-phenyl-2-thiourea (PTU) in methylene blue embryo water to inhibit pigmentation. For in situ hybridization and TUNEL staining, zebrafish embryos and larvae were fixed immediately at the indicated time points of analysis using 4% paraformaldehyde/PBS for overnight fixation at 4°C. For fluorescent imaging, zebrafish embryos and larvae up to 7 dpf were imaged in the living animals at the time of analysis, and older larvae up to 31 dpf were imaged after fixation; they were briefly anesthetized using 0.02% MS-222 (tricaine) prior to overnight fixation in 4% paraformaldehyde/PBS. All euthanasia and procedures followed the protocols approved by the Stanford Institutional Animal Care and Use Committee.

TALEN-targeting to create irf8 mutations

A pair of transcription activator-like effector nucleases (TALENs) was designed to target a 5′ region of irf8 near the translational start site that encompasses a unique AvaI restriction site (see Fig. 1A). The web tool TAL Effector-Nucleotide Targeter 2.0 (TALE-NT 2.0; https://tale-nt.cac.cornell.edu) was used to design the TALENs. Recognition sequences for the left and right TALENs are, respectively: 5′-TGAAGTAAAGGTCTACAAGA-3′ and 5′-TATAAGCCACTGTTTCAGTC-3′. The PCR/Golden Gate cloning protocol for creating the TALENs was used [41]. 400–800 pg of TALE nuclease mRNA (transcribed by Sp6 mMessage mMachine Kit, Ambion) was injected into 1–2 cell stage embryos and raised at 28.5°C. To identify founders, injected fish were crossed and a subset of the F1 progeny was assayed for the presence of a mutation in the irf8 locus based on disruption of the AvaI site; when a mutation was identified the remaining progeny were raised to adulthood. Individual F1 adults carrying an irf8 mutation disrupting the AvaI site were further analyzed by sequencing, which enabled identification of two specific alleles, st95 and st96, that contain frameshift mutations. To genotype st95 and st96, a PCR fragment of irf8 exon1 was amplified using the following primers: 5′-ACATAAGGCGTAGAGATTGGACG-3′ and 5′-GAAACATAGTGCGGTCCTCATCC-3′, followed by a digest with AvaI on the PCR product.

Neutral red assay

For phenotypic analyses of microglia in live fish, neutral red assay was used. 3–6 dpf larvae were incubated in embryo water containing 2.5 μg/ml neutral red at 28.5°C for 2–3 hours, followed by 1–2 water changes, and then analyzed 0.5–24 hours later using a dissecting microscope.

Whole mount RNA in situ hybridization, TUNEL assay and immunostaining

In situ hybridization on whole zebrafish embryos and larvae from 20 hpf to 3 dpf was performed using standard methods. Antisense riboprobes used were: lyz, mfap4, and apoeb (or apoe), as described [21]. TUNEL assay (In situ Cell Death Detection Kit, TMR Red, Roche) was performed as previously described [21]. Subsequent immunostaining was performed using the anti-L-plastin (LCP) antibody [42] at 1:250–500 dilution, followed by DAPI staining. For the cell death analysis, 5 dpf larvae from irf8 heterozygous intercrosses were processed for TUNEL and L-plastin immunostaining, and genotyped. Images of the sibling and mutant larvae were taken from the same anatomical region caudal to the end of yolk extension on an upright Zeiss Axio Imager.M2 microscope using the 20x (NA 0.8) objective. Most TUNEL signals were concentrated in the CHT of the larval tail; the images were cropped to analyze TUNEL signals only in the CHT using ImageJ. The anatomical region is illustrated in Fig. 3 diagram. Similar threshold levels were set for all images and adjusted to accurately reflect the TUNEL signals to measure area of the nuclei labeled by TUNEL (Fig. 3C,D). Representative tracing of the TUNEL signals to determine area of each labeled nucleus is shown in Fig. 3C,D below the actual fluorescent image of the TUNEL staining. Total number and number of small and other sized TUNEL-positive cells were quantified.

Time-lapse and fluorescent imaging

For live imaging, embryos were embedded in 1.5% low melting point agarose on glass slides. Fluorescent images were taken on a spinning-disk confocal microscope (Perkin Elmer UltraVIEW VoX imaging system using the Zeiss Axio Observer Z.1 microscope base with the Yokogawa CSU-X1 scanner unit and Hamamatsu EM-CCD C9100–13 camera), unless noted otherwise. The Volocity Acquisition suite was used for 3-dimensional multichannel recording. The following objectives were used: EC Plan-NeoFluar 10x/0.3 Ph1 DIC, Plan-Apochromat 25x/0.8W, and C-Aprochromat 63x/1.2W Korr. Images were analyzed using the Volocity software and ImageJ, and processed using Adobe Photoshop CS5. Static images of live and fixed larvae for analysis of macrophage numbers in Fig. 4 were taken on a Zeiss LSM 5 Pascal confocal microscope using the 20x (NA 0.75) objective. ImageJ Cell Counter tool was used to count the number of cells.

Cryosectioning for brain microglia analysis

Larvae were fixed overnight in 4% paraformaldehyde/PBS and washed three times in PBS with 0.1% tween. Post-fixed larvae were equilibrated to 30% sucrose, embedded in O.C.T. medium, and snap frozen in dry ice-ethanol bath. Samples were sectioned at 12–14 μm in the head region, and subsequently imaged on an upright Zeiss Axio Imager.M2 microscope using the 10x/0.45 and 40x/0.95 objectives.

Expression constructs and embryo injection

Full-length irf8 coding sequence (NM_001002622) was cloned from 5 dpf wildtype cDNA into pCR8/GW/TOPO and verified by sequencing. Tissue-specific expression vectors (mpeg1:irf8; lyz:irf8; huc:irf8; krt4:irf8) were assembled using multisite Gateway methods [43] in a destination vector containing Tol2-transposon sequences for genomic integration, and cmlc2-EGFP for selection. Each plasmid expressing a transgene was co-injected at 12–25 pg along with 50–100 pg of Tol2 transposase mRNA (transcribed by Sp6 mMessage mMachine Kit, Ambion) at 1–4 cell stage. Injected embryos were selected for further analysis based on strong expression of GFP in the heart by the cardiac reporter cmlc2:EGFP.

Supporting Information

S1 Fig. Kaplan-Meier plot showing survival of homozygous irf8 mutant zebrafish into adulthood past 3 months of age.

A survival study of the progeny from heterozygous irf8 intercross showed survival of all wildtype irf8+/+ progenies (n = 10/10), nearly all heterozygous irf8+/- fish (n = 16/17), and some homozygous irf8-/- mutants (n = 3/5) at 100 dpf. The genotypes of the fish were determined by fin clip assay at 30 dpf, and survival was monitored thereafter, until 100 dpf. Between these stages, 60% of the homozygous mutants survived in this analysis.

https://doi.org/10.1371/journal.pone.0117513.s001

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S2 Fig. Thin brain sections reveal many microglial cells in wildtype but not in irf8 mutants, which appear to have only macrophages at 31 dpf.

(A) The midbrain optic tectum, where many microglia normally reside, was the region of analysis. (B) Higher magnification of the brain region indicated in dotted box in A. 12–14 um cryosections were taken from wildtype irf8+/+ and heterozygous irf8st95/+ fish (n = 4) to compare with irf8st95/st9 mutants (n = 3) at 31 dpf. Immunostaining for L-plasin (with DAPI as a counterstain) was used to identify macrophages in relation to all cell bodies in the sections. Microglia were identified by their L-plastin expression, elaborate morphology with fine processes, and location in the parenchyma (white arrows). Cells in or adjacent to the interstitial space, vasculature, and ventricular zone were likely macrophages. Autofluorescence in the green channel helped to define the vasculature and distinguish actual L-plastin signal from vasculature autofluorescence in the red channel. irf8 mutants had a few L-plastin positive cells in the interstitial region and near the ventricular zone that lack fine processes (blue arrows), suggesting that these cells were not microglia. OT, midbrain optic tectum; DC, diencephalon. All scale bars are 50 um.

https://doi.org/10.1371/journal.pone.0117513.s002

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Acknowledgments

We are grateful to M. Barna and S. Kim for sharing microscopes. We thank D. Lyons and H. Sidik for critical reading of the manuscript, members of our laboratory for insightful discussions, and T. Reyes and C. Hill for fish care.

Author Contributions

Conceived and designed the experiments: CES WST. Performed the experiments: CES ZK AM. Analyzed the data: CES AM WST. Wrote the paper: CES AM WST.

References

  1. 1. Bennett CM, Kanki JP, Rhodes J, Liu TX, Paw BH, et al. (2001) Myelopoiesis in the zebrafish, Danio rerio. Blood 98: 643–651. pmid:11468162
  2. 2. Richards DM, Hettinger J, Feuerer M (2013) Monocytes and macrophages in cancer: development and functions. Cancer Microenviron 6: 179–191. pmid:23179263
  3. 3. Hettinger J, Richards DM, Hansson J, Barra MM, Joschko AC, et al. (2013) Origin of monocytes and macrophages in a committed progenitor. Nat Immunol 14: 821–830. pmid:23812096
  4. 4. Rosenbauer F, Tenen DG (2007) Transcription factors in myeloid development: balancing differentiation with transformation. Nat Rev Immunol 7: 105–117. pmid:17259967
  5. 5. Stachura DL, Traver D (2011) Cellular dissection of zebrafish hematopoiesis. Methods Cell Biol 101: 75–110. pmid:21550440
  6. 6. Chen AT, Zon LI (2009) Zebrafish blood stem cells. J Cell Biochem 108: 35–42. pmid:19565566
  7. 7. Terry RL, Miller SD (2014) Molecular control of monocyte development. Cell Immunol. pmid:25594139
  8. 8. Taniguchi T, Ogasawara K, Takaoka A, Tanaka N (2001) IRF family of transcription factors as regulators of host defense. Annu Rev Immunol 19: 623–655. pmid:11244049
  9. 9. Scheller M, Foerster J, Heyworth CM, Waring JF, Lohler J, et al. (1999) Altered development and cytokine responses of myeloid progenitors in the absence of transcription factor, interferon consensus sequence binding protein. Blood 94: 3764–3771. pmid:10572090
  10. 10. Tamura T, Ozato K (2002) ICSBP/IRF-8: its regulatory roles in the development of myeloid cells. J Interferon Cytokine Res 22: 145–152. pmid:11846985
  11. 11. Hambleton S, Salem S, Bustamante J, Bigley V, Boisson-Dupuis S, et al. (2011) IRF8 mutations and human dendritic-cell immunodeficiency. N Engl J Med 365: 127–138. pmid:21524210
  12. 12. Holtschke T, Lohler J, Kanno Y, Fehr T, Giese N, et al. (1996) Immunodeficiency and chronic myelogenous leukemia-like syndrome in mice with a targeted mutation of the ICSBP gene. Cell 87: 307–317. pmid:8861914
  13. 13. Wang H, Yan M, Sun J, Jain S, Yoshimi R, et al. (2014) A Reporter Mouse Reveals Lineage-Specific and Heterogeneous Expression of IRF8 during Lymphoid and Myeloid Cell Differentiation. J Immunol. pmid:25552543
  14. 14. Aliberti J, Schulz O, Pennington DJ, Tsujimura H, Reis e Sousa C, et al. (2003) Essential role for ICSBP in the in vivo development of murine CD8alpha + dendritic cells. Blood 101: 305–310. pmid:12393690
  15. 15. Schmidt M, Nagel S, Proba J, Thiede C, Ritter M, et al. (1998) Lack of interferon consensus sequence binding protein (ICSBP) transcripts in human myeloid leukemias. Blood 91: 22–29. pmid:9414265
  16. 16. Pogosova-Agadjanyan EL, Kopecky KJ, Ostronoff F, Appelbaum FR, Godwin J, et al. (2013) The prognostic significance of IRF8 transcripts in adult patients with acute myeloid leukemia. PLoS One 8: e70812. pmid:23967110
  17. 17. Li L, Jin H, Xu J, Shi Y, Wen Z (2011) Irf8 regulates macrophage versus neutrophil fate during zebrafish primitive myelopoiesis. Blood 117: 1359–1369. pmid:21079149
  18. 18. Rhodes J, Hagen A, Hsu K, Deng M, Liu TX, et al. (2005) Interplay of pu.1 and gata1 determines myelo-erythroid progenitor cell fate in zebrafish. Dev Cell 8: 97–108. pmid:15621533
  19. 19. Herbomel P, Thisse B, Thisse C (2001) Zebrafish early macrophages colonize cephalic mesenchyme and developing brain, retina, and epidermis through a M-CSF receptor-dependent invasive process. Dev Biol 238: 274–288. pmid:11784010
  20. 20. Svahn AJ, Graeber MB, Ellett F, Lieschke GJ, Rinkwitz S, et al. (2013) Development of ramified microglia from early macrophages in the zebrafish optic tectum. Dev Neurobiol 73: 60–71. pmid:22648905
  21. 21. Shiau CE, Monk KR, Joo W, Talbot WS (2013) An Anti-inflammatory NOD-like Receptor Is Required for Microglia Development. Cell Rep 5: 1342–1352. pmid:24316075
  22. 22. Peri F, Nusslein-Volhard C (2008) Live imaging of neuronal degradation by microglia reveals a role for v0-ATPase a1 in phagosomal fusion in vivo. Cell 133: 916–927. pmid:18510934
  23. 23. Novoa B, Figueras A (2012) Zebrafish: model for the study of inflammation and the innate immune response to infectious diseases. Adv Exp Med Biol 946: 253–275. pmid:21948373
  24. 24. Tsujimura H, Nagamura-Inoue T, Tamura T, Ozato K (2002) IFN consensus sequence binding protein/IFN regulatory factor-8 guides bone marrow progenitor cells toward the macrophage lineage. J Immunol 169: 1261–1269. pmid:12133947
  25. 25. Kyritsis N, Kizil C, Zocher S, Kroehne V, Kaslin J, et al. (2012) Acute inflammation initiates the regenerative response in the adult zebrafish brain. Science 338: 1353–1356. pmid:23138980
  26. 26. Ginhoux F, Greter M, Leboeuf M, Nandi S, See P, et al. (2010) Fate mapping analysis reveals that adult microglia derive from primitive macrophages. Science 330: 841–845. pmid:20966214
  27. 27. Kierdorf K, Erny D, Goldmann T, Sander V, Schulz C, et al. (2013) Microglia emerge from erythromyeloid precursors via Pu.1- and Irf8-dependent pathways. Nat Neurosci 16: 273–280. pmid:23334579
  28. 28. Hall C, Flores MV, Storm T, Crosier K, Crosier P (2007) The zebrafish lysozyme C promoter drives myeloid-specific expression in transgenic fish. BMC Dev Biol 7: 42. pmid:17477879
  29. 29. Ellett F, Pase L, Hayman JW, Andrianopoulos A, Lieschke GJ (2011) mpeg1 promoter transgenes direct macrophage-lineage expression in zebrafish. Blood 117: e49–56. pmid:21084707
  30. 30. Wang H, Lee CH, Qi C, Tailor P, Feng J, et al. (2008) IRF8 regulates B-cell lineage specification, commitment, and differentiation. Blood 112: 4028–4038. pmid:18799728
  31. 31. Gordy C, Pua H, Sempowski GD, He YW (2011) Regulation of steady-state neutrophil homeostasis by macrophages. Blood 117: 618–629. pmid:20980680
  32. 32. Goren I, Allmann N, Yogev N, Schurmann C, Linke A, et al. (2009) A transgenic mouse model of inducible macrophage depletion: effects of diphtheria toxin-driven lysozyme M-specific cell lineage ablation on wound inflammatory, angiogenic, and contractive processes. Am J Pathol 175: 132–147. pmid:19528348
  33. 33. Schiavoni G, Mattei F, Sestili P, Borghi P, Venditti M, et al. (2002) ICSBP is essential for the development of mouse type I interferon-producing cells and for the generation and activation of CD8alpha(+) dendritic cells. J Exp Med 196: 1415–1425. pmid:12461077
  34. 34. Tailor P, Tamura T, Morse HC, Ozato K (2008) The BXH2 mutation in IRF8 differentially impairs dendritic cell subset development in the mouse. Blood 111: 1942–1945. pmid:18055870
  35. 35. Qi CF, Li Z, Raffeld M, Wang H, Kovalchuk AL, et al. (2009) Differential expression of IRF8 in subsets of macrophages and dendritic cells and effects of IRF8 deficiency on splenic B cell and macrophage compartments. Immunol Res 45: 62–74. pmid:18663414
  36. 36. Schiavoni G, Mattei F, Borghi P, Sestili P, Venditti M, et al. (2004) ICSBP is critically involved in the normal development and trafficking of Langerhans cells and dermal dendritic cells. Blood 103: 2221–2228. pmid:14615368
  37. 37. Turcotte K, Gauthier S, Malo D, Tam M, Stevenson MM, et al. (2007) Icsbp1/IRF-8 is required for innate and adaptive immune responses against intracellular pathogens. J Immunol 179: 2467–2476. pmid:17675508
  38. 38. Marquis JF, LaCourse R, Ryan L, North RJ, Gros P (2009) Disseminated and rapidly fatal tuberculosis in mice bearing a defective allele at IFN regulatory factor 8. J Immunol 182: 3008–3015. pmid:19234196
  39. 39. Yoshida Y, Yoshimi R, Yoshii H, Kim D, Dey A, et al. (2014) The transcription factor IRF8 activates integrin-mediated TGF-beta signaling and promotes neuroinflammation. Immunity 40: 187–198. pmid:24485804
  40. 40. Kimmel CB, Ballard WW, Kimmel SR, Ullmann B, Schilling TF (1995) Stages of embryonic development of the zebrafish. Dev Dyn 203: 253–310. pmid:8589427
  41. 41. Sanjana NE, Cong L, Zhou Y, Cunniff MM, Feng G, et al. (2012) A transcription activator-like effector toolbox for genome engineering. Nat Protoc 7: 171–192. pmid:22222791
  42. 42. Redd MJ, Kelly G, Dunn G, Way M, Martin P (2006) Imaging macrophage chemotaxis in vivo: studies of microtubule function in zebrafish wound inflammation. Cell Motil Cytoskeleton 63: 415–422. pmid:16671106
  43. 43. Kwan KM, Fujimoto E, Grabher C, Mangum BD, Hardy ME, et al. (2007) The Tol2kit: a multisite gateway-based construction kit for Tol2 transposon transgenesis constructs. Dev Dyn 236: 3088–3099. pmid:17937395