Advertisement
Browse Subject Areas
?

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

Myeloid Takl Acts as a Negative Regulator of the LPS Response and Mediates Resistance to Endotoxemia

  • Christina Eftychi,

    Affiliation Institute of Immunology, Biomedical Sciences Research Center “Alexander Fleming”, Vari, Greece

  • Niki Karagianni,

    Current address: Biomedcode Hellas SA, Vari, Greece

    Affiliation Institute of Immunology, Biomedical Sciences Research Center “Alexander Fleming”, Vari, Greece

  • Maria Alexiou,

    Current address: Center for Dental Medicine, Institute of Oral Biology, University of Zurich, Zurich, Switzerland

    Affiliation Institute of Immunology, Biomedical Sciences Research Center “Alexander Fleming”, Vari, Greece

  • Maria Apostolaki †,

    † Deceased.

    Affiliation Institute of Immunology, Biomedical Sciences Research Center “Alexander Fleming”, Vari, Greece

  • George Kollias

    g.kollias@fleming.gr

    Affiliation Institute of Immunology, Biomedical Sciences Research Center “Alexander Fleming”, Vari, Greece

Myeloid Takl Acts as a Negative Regulator of the LPS Response and Mediates Resistance to Endotoxemia

  • Christina Eftychi, 
  • Niki Karagianni, 
  • Maria Alexiou, 
  • Maria Apostolaki, 
  • George Kollias
PLOS
x

Corrections

7 Sep 2012: Eftychi C, Karagianni N, Alexiou M, Apostolaki M, Kollias G (2012) Correction: Myeloid Takl Acts as a Negative Regulator of the LPS Response and Mediates Resistance to Endotoxemia. PLOS ONE 7(9): 10.1371/annotation/74add513-eb1d-4fa1-ae2e-c3d2e7e735a0. https://doi.org/10.1371/annotation/74add513-eb1d-4fa1-ae2e-c3d2e7e735a0 View correction

29 Mar 2012: Eftychi C, Karagianni N, Alexiou M, Apostolaki M, Kollias G (2012) Correction: Myeloid Takl Acts as a Negative Regulator of the LPS Response and Mediates Resistance to Endotoxemia. PLOS ONE 7(3): 10.1371/annotation/ea1a4c80-8dfd-496a-a273-d74c1fd6e069. https://doi.org/10.1371/annotation/ea1a4c80-8dfd-496a-a273-d74c1fd6e069 View correction

Abstract

TGFβ-activated kinase 1 (TAK1), a member of the mitogen-activated protein kinase kinase kinase (MAP3K) family, is considered a key intermediate in a multitude of innate immune signaling pathways. Yet, the specific role of TAK1 in the myeloid compartment during inflammatory challenges has not been revealed. To address this question, we generated myeloid-specific kinase-dead TAK1 mutant mice. TAK1 deficiency in macrophages results in impaired NF-κB and JNK activation upon stimulation with lipopolysaccharide (LPS). Moreover, TAK1-deficient macrophages and neutrophils show an enhanced inflammatory cytokine profile in response to LPS stimulation. Myeloid-specific TAK1 deficiency in mice leads to increased levels of circulating IL-1β, TNF and reduced IL-10 after LPS challenge and sensitizes them to LPS-induced endotoxemia. These results highlight an antiinflammatory role for myeloid TAK1, which is essential for balanced innate immune responses and host survival during endotoxemia.

Introduction

TGFβ-activated kinase 1 (TAK1) was originally identified as a key regulator of TGFβ/bone morphogenetic protein signaling [1]. Since then a wealth of information has been generated placing TAK1 as part of a more complex signaling network that governs basic cellular activities. Studies using complete and conditional TAK1 knockout mice revealed that TAK1 integrates signals emanating from TGFβ, TNF, IL-1β, Toll-like receptors (TLRs), B-cell receptors and T-cell receptors, to coordinate homeostasis and immunity, and that its absence can lead to carcinogenesis, inflammation or death [2][13]. In Drosophila, TAK1 is critical for antibacterial innate immunity as TAK1 mutants are highly susceptible to Gram-negative bacterial infection and do not produce antibacterial peptides [14]. In mammals, there are several lines of evidence supporting a critical role for TAK1 in innate immunity [8], [11], [15]. Genetic evidence demonstrating a role for TAK1 during innate immunoreceptor signaling has been obtained in mature immune cells by using B cell-specific TAK1-deficient mice [8]. TAK1-deficient B cells fail to activate transcription factor NF-κB and mitogen-activated protein kinases (MAPKs) in response to TLR ligands and have impaired production of IL-6, supporting an evolutionary conserved role for TAK1 in innate immunity. However, the role of TAK1 during TLR innate immune responses has not been addressed in the main cellular mediators of innate immunity, the myeloid cells.

Myeloid cells (macrophages and neutrophils) are the chief cellular agents of the inflammatory cascade during microbial infection. They initiate coordinated innate immune defenses through activation of pathogen recognition receptors that recognize specific pathogen-associated molecular patterns [16]. As a result of these interactions, immune cellular activation occurs with the release of cytokine and non-cytokine mediators. A key event in the immune response to Gram-negative bacteria is the recognition of lipopolysaccharide (LPS) by TLR4 [17]. LPS plays a key role in Gram-negative sepsis by inducing production of proinflammatory and antiinflammatory mediators, the most critical being IL-1β, TNF, IL-6 and IL-10 [18]. Cytokine production significantly influences the quality, duration, and magnitude of most inflammatory reactions.

During LPS-induced endotoxemia, serine/threonine kinase cascades are activated with pleiotropic downstream effects that include activation of protein kinases such as the MAPKs and the I-κB kinases. Although key molecules in these signaling pathways have been identified, there are still substantial gaps in our knowledge, including the role of members of the MAPK kinase kinase (MAP3K) family. Here we investigated the myeloid-specific role of the MAP3K TAK1 during LPS inflammatory responses. TAK1 deficiency in macrophages led to impaired activation of NF-κB and JNK following LPS stimulation, identifying TAK1 as an important upstream signaling molecule that regulates LPS-induced NF-κB and JNK activation in macrophages. Cytokine profile analysis of TAK1-deficient macrophages upon stimulation with LPS, revealed a hyperinflammatory phenotype characterized by increased proinflammatory (IL-1β, TNF, and IL-6) and reduced antiinflammatory (IL-10) cytokine production. A similar inflammatory cytokine profile was observed in LPS-stimulated neutrophils, although no reduction in IL-10 production was observed. Consistent with the above, mice with defective myeloid TAK1 mount an enhanced innate immune response to LPS by exhibiting increased circulating levels of IL-1β and TNF, reduced IL-10, and subsequently significantly increased mortality to LPS-induced shock. We conclude that myeloid TAK1 acts by regulating the balance between proinflammatory and antiinflammatory cytokine production thereby preventing unrestrained inflammatory responses.

Results and Discussion

Generation of ubiquitous and myeloid-specific TAK1 mutant mice

We generated mice with conditional expression of a Map3k7 allele encoding a kinase-dead truncated form of TAK1, following a similar targeting strategy to previous studies [8]. The targeting vector was constructed by placing two loxP sites flanking exon 2 of Map3k7 (Fig. 1A). Exon 2 encodes part of the kinase domain including the ATP binding pocket and can be deleted without disrupting the remainder of the reading frame. To generate mice that ubiquitously express the truncated TAK1 (Map3k7−/− mice), we crossed Map3k7flox/flox mice with transgenic mice expressing Cre in germ cells [19]. Of 101 newborn pups (19 litters) obtained by intercrossing Map3k7+/− mice, we had 71 Map3k7+/−, 30 Map3k7+/+ and no Map3k7−/− mice, confirming previous studies that TAK1 deficiency leads to embryonic lethality [4], [8], [11].

thumbnail
Figure 1. Generation of conditional TAK1-deficient mice.

(A) Schematic representation of the wild type, targeted, floxed and deleted Map3k7 genomic locus, indicating BamHI, SacI and XbaI restriction sites used for Southern blot. The Map3k7 locus comprises 17 exons; in the scheme the first 6 exons are represented. The probes used to verify homologous recombination at the 5′ and 3′ end are shown. Black arrows indicate loxP sites; red arrows indicate FRT sites. B, BamHI; S, SacI; X, XbaI. (B) Southern blot of genomic DNA isolated from BMDMs after digestion with XbaI and using the 3′ probe. (C) PCR analysis of genomic DNA isolated from FACS-sorted CD11b+F4/80+ resident peritoneal macrophages and CD11b+Gr1+ splenic neutrophils. (D) Colony formation by BM cells from Map3k7Δmyel and Map3k7flox/flox mice in response to M-CSF, G-CSF and GM-CSF. Data are shown as mean ± SEM of 4 mice per group and are representative of two independent experiments.

https://doi.org/10.1371/journal.pone.0031550.g001

To investigate the role of myeloid-specific TAK1 in innate immunity, we crossed Map3k7flox/flox mice with LysM-Cre knockin mice, which express the Cre recombinase in macrophages and neutrophilic granulocytes [20]. This resulted in a 50% deletion in macrophages as it was assessed by Southern blot analysis of DNA extracted from bone marrow-derived macrophages (BMDMs) (Fig. 1B). Additionally, PCR analysis was performed on FACS-sorted CD11b+F4/80+ resident peritoneal macrophages and CD11b+Gr1+ splenic neutrophils for an approximate indication of deletion, suggesting a similar percentage of deletion in the macrophage population, while a higher deletion percentage was observable in neutrophils (Fig. 1C). Mice with myeloid-restricted TAK1 deficiency (Map3k7Δmyel) were born at the expected Mendelian ratio, developed normally, and did not show any gross morphological changes in the overall histology of lymphoid organs and other organs rich in myeloid cells, such as the gastrointestinal tract (data not shown). In the control groups, we observed no phenotypic difference among Map3k7flox/flox and LysM-Cre mice and thus Map3k7flox/flox mice were used as controls.

To determine if TAK1 deficiency affected the production of immature and mature myeloid cell subsets, we performed flow cytometric immunophenotypical analysis of bone marrow (BM) [21], [22], peripheral blood, spleen and peritoneal cavity cell preparations obtained from Map3k7Δmyel and Map3k7flox/flox mice. We observed no differences in the immature myeloid cell subsets in the BM of Map3k7Δmyel and Map3k7flox/flox mice as there were similar frequencies of common myeloid progenitors, granulocyte/macrophage progenitors and the myelomonocytic cell fraction (fraction of Gr-1+/Mac-1+ cells) (Table 1). In peripheral blood there were similar numbers of monocytes and neutrophils between Map3k7Δmyel and Map3k7flox/flox cell preparations (Table 1). Also, no statistically significant differences were observed in the number of peripheral splenic macrophages and neutrophils, nor in the number of resident peritoneal macrophages (Table 1).

thumbnail
Table 1. Immunophenotypical flow cytometric analysis of BM, peripheral blood, spleen and peritoneal cavity myeloid cells in Map3k7Δmyel and Map3k7flox/flox mice.

https://doi.org/10.1371/journal.pone.0031550.t001

We next investigated the ability of myeloid precursor cells to differentiate into macrophages and granulocytes in colony-forming assays upon stimulation with G-CSF, M-CSF, and GM-CSF. As shown in Fig. 1D, the numbers of colonies grown from Map3k7Δmyel and Map3k7flox/flox BM cells were comparable, suggesting that myeloid TAK1 deficiency did not affect the developmental potential of early myeloid precursor cells. It has been reported that TAK1 promotes survival signals in hematopoietic cells [12]. Nevertheless, we and others [15] did not observe any reduction in the numbers of macrophages and granulocytes in the periphery when TAK1 is inactivated in myeloid cells.

TAK1 deficiency promotes a hyperinflammatory phenotype in LPS-stimulated macrophages and neutrophils

We focused our subsequent analyses on identifying the role of TAK1 in LPS-induced inflammatory responses. For these studies we prepared BMDMs from Map3k7Δmyel and Map3k7flox/flox littermate mice and treated them with 100 ng/ml LPS. Map3k7Δmyel BMDMs exhibited reduced NF-κB (Fig. 2A) and JNK activation (Fig. 2B), consistent with similar studies in mouse monocytic cell lines for JNK activation [15], but also in other cell types such as B cells [8] and MEFs [11]. Next, we performed a detailed kinetic analysis of cytokine production upon LPS stimulation. TAK1 deficiency resulted in increased ΙL-1β, TNF, and IL-6, and decreased IL-10 production following LPS stimulation at different time points (Fig. 3A, B, C, D). A substantial increase in IL-1β production was evident at all time points up to 12 h post stimulation in Map3k7Δmyel BMDMs compared to control cells, whereas at 24 h, IL-1β declined to almost undetectable levels in both Map3k7Δmyel and Map3k7flox/flox cells (Fig. 3A). Increased production of TNF and IL-6 was also observed at early time points after LPS stimulation in Map3k7Δmyel BMDMs (Fig. 3B, C). In contrast, IL-10 production was almost 4-fold lower 3 h post LPS stimulation in Map3k7Δmyel BMDMs compared to control cells, and a significant reduction was still evident until 24 h (Fig. 3D). Thus upon LPS stimulation, Map3k7Δmyel BMDMs exhibit a hyperinflammatory phenotype.

thumbnail
Figure 2. Impaired activation of NF-κB and JNK in response to LPS stimulation in TAK1-deficient macrophages.

BMDMs were stimulated with LPS (100 ng/ml) and nuclear/cytoplasmic extracts were collected at the indicated times. (A) NF-κB DNA-binding activity in nuclear extracts was determined by EMSA. The lysates used for EMSA were subjected to immunoblot analysis using a TFIIB-specific antibody as a loading control. (B) Phosphorylation of JNK (p-JNK) in cytoplasmic extracts was assessed by immunoblot with antibody specific for its phosphorylated form. The membrane was reprobed for total JNK. Results are representative of three independent experiments.

https://doi.org/10.1371/journal.pone.0031550.g002

thumbnail
Figure 3. Enhanced inflammatory cytokine profile in TAK1-deficient macrophages and neutrophils in response to LPS.

(A–D) BMDMs and (E–H) thioglycollate-elicited peritoneal neutrophils from Map3k7Δmyel and Map3k7flox/flox mice were stimulated with 100 ng/ml LPS. (A, E) IL-1β, (B, F) TNF, (C, G) IL-6, and (D, H) IL-10 production were measured in cell culture supernatants by ELISA. (A–H) Data are representative of three independent experiments with 4 mice per group and are shown as mean ± SEM. *, p≤0.05; **, p≤0.01; ***, p≤0.005.

https://doi.org/10.1371/journal.pone.0031550.g003

It was previously shown that upon LPS stimulation, reduced NF-κB activation in IKKβ-deficient macrophages leads to increased IL-1β production due to enhanced IL-1β processing [23]. Therefore, reduced NF-κB activation in TAK1-deficient macrophages could at least partly account for the increased IL-1β production observed. Interestingly, a recent study revealed a regulatory loop for the induction of IL-10 during the LPS response which involves TAK1 and AUF1 [24]. Following LPS stimulation, the RNA-binding protein AUF1 maintains proper levels of TAK1 by post-transcriptional control on Tak1 mRNA and in this way accomplishes proper NF-κB activation required for the induction of IL-10. Thus, in the absence of TAK1 several layers of transcriptional and/or post-transcriptional controls may contribute to the observed deregulated cytokine profile.

As TAK1 is deleted in both macrophages and neutrophils in Map3k7Δmyel mice, we next sought to determine whether TAK1 deficiency caused a similar cytokine profile change in neutrophils as in macrophages. For this we used thioglycollate-elicited peritoneal neutrophils from Map3k7Δmyel and Map3k7flox/flox mice and measured cytokine production 6 h and 12 h upon LPS stimulation. Paralleling the results of macrophages, LPS induced enhanced production of the proinflammatory cytokines IL-1β, TNF and IL-6 in Map3k7Δmyel peritoneal neutrophils (Fig. 3E, F, G). Notably however no reduction in the levels of IL-10 was observed in peritoneal neutrophils. In contrast, IL-10 production was significantly increased by 6 h in Map3k7Δmyel compared to Map3k7flox/flox neutrophils (Fig. 3H), suggesting that different mechanisms govern cytokine production in LPS-stimulated macrophages and neutrophils as it has been already reported for IL-1β production [23]. Interestingly, Map3k7Δmyel peritoneal neutrophils exhibited higher basal levels of TNF and IL-6 compared to almost undetectable levels in Map3k7flox/flox neutrophils. Bearing in mind that thioglycollate-elicited neutrophils are not in a steady state, this could imply a general mechanism of deregulated cytokine production upon activation of myeloid cells, in the absence of TAK1.

These results demonstrate that upon LPS stimulation, TAK1 deficiency alters the cytokine profile in macrophages and neutrophils in favor of a proinflammatory profile. This is a quite unexpected finding, as TAK1 is traditionally considered a proinflammatory molecule [8], [11]. In B cells, TAK1 deficiency was reported to result in diminished IL-6 production upon LPS stimulation [8]. Additional studies are required to delineate the molecular pathways underlying the deregulated cytokine production upon LPS stimulation in the absence of myeloid TAK1.

Increased mortality to endotoxemia and deregulated cytokine production in mice defective in myeloid TAK1

We next sought to investigate the pathophysiological significance of the inflammatory phenotype exhibited by LPS-induced macrophages and neutrophils. For this, mice were intraperitoneally (i.p.) challenged with 100 ìg of LPS and serum samples were obtained at various intervals (0, 1.5, 3, and 6 h) after injection, for the assessment of the concentrations of circulating cytokines (Fig. 4A, B, C, D). The induction of proinflammatory cytokines was greatly enhanced in Map3k7Δmyel mice compared to the Map3k7flox/flox control mice, consistent with the in vitro data. A marked increase in IL-1β was observed already within the first 1.5 h, and continued to increase in the serum of Map3k7Δmyel mice, until it reached a peak concentration at 3 h that was 2-fold higher than the amount detected in Map3k7flox/flox mice (Fig. 4A). The levels of serum TNF were also significantly higher in Map3k7Δmyel mice compared to Map3k7flox/flox mice. TNF peaked at 1.5 h both in Map3k7Δmyel and Map3k7flox/flox mice, but a 1.5-fold increase was observed in the Map3k7Δmyel mice after which, TNF levels declined and by 6 h became identical in Map3k7Δmyel and Map3k7flox/flox mice (Fig. 4B). Additionally, a trend towards an increase in serum IL-6 was observed, although this result did not reach statistical significance (Fig. 4C). In contrast to the augmented production of proinflammatory cytokines, circulating levels of the antiinflammatory IL-10 were significantly reduced in the serum of Map3k7Δmyel mice compared to the Map3k7flox/flox controls. At 1.5 h post LPS challenge, IL-10 levels were identical but a more acute decline was observed in the serum of the Map3k7Δmyel mice at 3–6 h (Fig. 4D).

thumbnail
Figure 4. Increased LPS-induced mortality and altered circulating cytokine levels in mice deficient in myeloid TAK1.

(A) IL-1β, (B) TNF, (C) IL-6, and (D) IL-10 serum levels after LPS administration (100 ìg/mouse) in Map3k7Δmyel and Map3k7flox/flox mice. Data are represented as mean ± SEM of 8–15 mice, pooled from three independent experiments. *, p≤0.05; **, p≤0.01; ***, p≤0.005. (E) Survival of Map3k7Δmyel (n = 16), Map3k7flox/flox (n = 15) and LysM-Cre (n = 5) mice after LPS injection (20 mg/kg).

https://doi.org/10.1371/journal.pone.0031550.g004

High circulating cytokine levels are associated with endotoxemia and contribute to the increased mortality associated with this condition. Map3k7Δmyel mice and Map3k7flox/flox littermates, as well as LysM-Cre control mice, were i.p. challenged with a high dose of LPS (20 mg/kg of body weight) and survival was monitored for 72 h. In this acute inflammation model, death occurs within a few days depending on the dose response to LPS. Map3k7Δmyel mice were indeed highly sensitive to LPS challenge, as only 19% (3 out of 16) survived within 24 h, compared to a survival rate of 93% (14 out of 15) for the Map3k7flox/flox mice and 100% (5 out of 5) for the LysM-Cre control mice (Fig. 4E). Over a period of 72 h, the survival of Map3k7Δmyel mice was 12%, significantly lower than the 50% survival of Map3k7flox/flox mice and 60% for LysM-Cre mice (Fig. 4E).

In conclusion, these data demonstrate that myeloid TAK1 is an essential regulator of LPS-induced inflammatory responses. Notably, an increased sensitivity to LPS-induced endotoxemia is also observed in myeloid-specific IKKβ-deficient mice [23]. Similarly, reduced NF-κB activation in the absence of TAK1 could account for the deregulated IL-1β production and the resulting increase in sensitivity to LPS challenge. Yet, myeloid-specific TAK1-deficiency also affects the production of other cytokines (TNF, IL-6) reflecting additional regulatory pathways that are simultaneously affected by TAK1.

Recently, Courties et al. reported that RNA interference-mediated knockdown of myeloid cell derived-TAK1 ameliorates inflammation and bone damage in collagen-induced arthritis [15], a finding that could raise interest in targeting TAK1 in chronic inflammatory diseases, such as rheumatoid arthritis. Further analysis revealed that knockdown of myeloid TAK1 directly attenuated Th1 responses, which play a significant role in mediating inflammation and development of collagen-induced arthritis, highlighting a modulatory role for myeloid-specific TAK1 in the adaptive immune response. Similar to our present results, in the study by Courties et al. [15] , LPS-induced JNK activation was also found to be reduced in a mouse monocytic cell line that was transiently transfected with siRNAs against TAK1. However, in the same study, despite a downregulated systemic proinflammatory response, the myeloid-specific contribution in proinflammatory cytokines was not addressed. It would be interesting to compare myeloid-specific cytokine responses in a chronic setting, such as in the collagen-induced arthritis model, with the enhanced acute myeloid response that we have observed with LPS. Our study combined with previous findings highlights a context and tissue dependence of the proinflammatory and antiinflammatory functions of TAK1 that could have implications for the future development of therapeutic concepts targeting TAK1 function in human inflammatory disease.

Materials and Methods

Ethics Statement

All animal experiments conformed to all current national and European legislation and were approved by the Prefecture of Attica (approval ID 1463A) and by the Institutional Animal Care and Use Committee of the Biomedical Sciences Research Center “Alexander Fleming” (approval ID 2350B).

Generation of conditional TAK1-deficient mice

For the generation of conditional TAK1-deficient mice, a targeting vector was constructed in which a 0.6 kb fragment of Map3k7 containing exon 2 was flanked by loxP sites. The targeting vector also contained an FRT-neo-FRT selection cassette next to the first loxP site and before exon 2 (Fig. 1A). An upstream 3.3 kb and a downstream 4.0 kb fragment were used as ‘arms’ for homology. Bruce-4 ES cells derived from C57BL/6 mice [25] were cultured, transfected and selected using standard protocols. Targeted ES cell clones were selected by Southern blotting with 5′ and 3′ probes, after digestion with SacI and BamHI respectively. The FRT-neo-FRT selection cassette was excised using flipper mice [26]. Generation of heterozygous floxed Map3k7 mice (Map3k7flox/+) was carried out by following standard procedures. The mice used in this study were 6–12 wks old and were maintained on a C57BL/6 genetic background. All mice were housed under specific pathogen-free conditions.

Progenitor cell assays

Colony-forming assays were performed by plating single cell suspensions of BM (3–5×104 cells/ml) in triplicate in 1 ml methylcellulose medium in 35 mm Petri dishes. Cells were incubated for 8 days in methylcellulose medium containing GM-CSF (MethoCult M3001) or incomplete methylcellulose medium (MethoCult M3231, Stem Cell Technology) supplemented with 10 ng/ml G-CSF or M-CSF (PeproTech). Colonies were scored on day 8.

Flow cytometric analysis

Single cell suspensions were prepared from BM, blood, spleen and peritoneal cavity. Where required, red blood cells were excluded by Gey's lysis solution and debris was removed by cell strainer (70 µm, BD Falcon). After blockade of Fc-receptors with CD16/32 blocking antibody, cells were stained with antibodies conjugated with fluorochromes for 30 min on ice and washed twice before FACS analysis. For antibodies not directly conjugated to fluorochromes, staining with a secondary antibody was required for 20–30 min on ice, followed by a wash step. Data were collected by FACS Canto II and analyzed by using FACS Diva software (Becton Dickinson). For cell sorting a FACS Vantage SE II was used (Becton Dickinson). Cells were labelled using monoclonal antibodies against: CD11b (M1/70, BD Biosciences), Gr1 (RB6-8C5, e-Bioscience), F4/80 (BM8, e-Bioscience), Ly-6C (AL-21, BD Biosciences), c-Kit (2B8, e-Bioscience), Sca-1 (D7, e-Bioscience), TER-119 (TER119, e-Bioscience), B220 (RA3-6B2, e-Bioscience), CD3e (145-2C11, e-Bioscience), CD34 (RAM34, e-Bioscience), CD16/32 (93, e-Bioscience); these antibodies are conjugated with different markers, such as fluorescein isothiocyanate (FITC), phycoerythrin (PE), allophycocyanin (APC), APC-Alexa750, Alexa700, PE-Cy5.5 or biotin. Streptavidin coupled to FITC or APC (BD Biosciences) was used as a secondary antibody.

Cell cultures

For BMDMs preparation, BM cells were cultured in complete RPMI in the presence of 20% medium conditioned by L929 mouse fibroblasts (as a source of M-CSF). On day 8, BMDMs were collected and used as indicated. To isolate neutrophils, mice were i.p. injected with 1 ml of 4% thioglycollate (DIFCO) and peritoneal neutrophils were flushed out 3–5 h later. The percentages of neutrophils in the peritoneal cell populations were similar between Map3k7Δmyel (83,4±4,2, n = 3) and Map3k7flox/flox (82,0±5,7, n = 3) littermates as analyzed by flow cytometry.

Immunoblot analysis

Proteins were resolved by SDS PAGE and were transferred to nitrocellulose membranes by electroblot. Non-specific binding sites were blocked by incubation in 10 mM Tris-HCl pH 7.5, 150 mM NaCl, containing 0.5% Tween-20 and 5% dry milk. Membranes were blotted with antibodies against p-JNK (#46685, Cell Signaling), JNK (sc-7345, Santa Cruz) and TFIIB (sc-225, Santa Cruz) according to the manufacturer's instructions for each antibody.

EMSA

Nuclear extracts were prepared and EMSA was performed as previously described [27]. The sequences of the oligonucleotides used for NF-κB with two tandemly positioned NF-κB binding sites (underlined) were as follows: NF-κBF (5′-ATCAGGGACTTTCCGCTGGGGACTTT-3′) and NF-κBR (5′-CGGAAAGTCCCCAGCGGAAAGTCCCT-3′).

Endotoxemia

Mice (8–12 wks) were i.p. injected with a sublethal dose (20 mg/kg) of LPS (Escherichia coli 0111:B4, Sigma) and were monitored for survival. For serum cytokine measurements, mice were i.p. injected with 100 µg of LPS and at indicated time points were euthanized and blood serum was collected.

Cytokine ELISA measurements

Serum cytokine levels and cytokines secreted from primary cells were determined by ELISA. Macrophages were plated in duplicate per mouse at 5×105 cells/well in 24-well plates and were allowed to adhere for 3 h before stimulation. Neutrophils isolated from 4 mice were pooled and plated in quadruplicate at 1×106 cells/well in 24-well plates. Cells were stimulated with 100 ng/ml LPS for the times indicated, followed by incubation with 1 mM ATP for 30 min for IL-1β measurements, and supernatants were taken for cytokine measurements. ELISA kits for TNF, IL-6, IL-10 (e-Bioscience) and IL-1β (BD Biosciences) were used according to manufacturer's instructions.

Statistical analysis

Statistical comparisons were performed using unpaired Student's two tailed t test, with p values ≤0.05 considered statistically significant.

Acknowledgments

We would like to thank Dr Colin Stewart for providing us with Bruce-4 ES cells, Dr Sofia Grammenoudi, operator of the Flow Cytometry facility of BSRC “Alexander Fleming”, for her help with cell sorting, and Nikos Giannakas, Panos Athanasakis and Spiros Lalos for technical support.

Author Contributions

Conceived and designed the experiments: CE NK M. Apostolaki GK. Performed the experiments: CE M. Alexiou. Analyzed the data: CE NK M. Apostolaki GK. Wrote the paper: CE M. Apostolaki GK.

References

  1. 1. Yamaguchi K, Shirakabe K, Shibuya H, Irie K, Oishi I, et al. (1995) Identification of a member of the MAPKKK family as a potential mediator of TGF-beta signal transduction. Science 270: 2008–2011.
  2. 2. Bettermann K, Vucur M, Haybaeck J, Koppe C, Janssen J, et al. (2010) TAK1 suppresses a NEMO-dependent but NF-kappaB-independent pathway to liver cancer. Cancer Cell 17: 481–496.
  3. 3. Inokuchi S, Aoyama T, Miura K, Osterreicher CH, Kodama Y, et al. (2010) Disruption of TAK1 in hepatocytes causes hepatic injury, inflammation, fibrosis, and carcinogenesis. Proc Natl Acad Sci U S A 107: 844–849.
  4. 4. Jadrich JL, O'Connor MB, Coucouvanis E (2006) The TGF beta activated kinase TAK1 regulates vascular development in vivo. Development 133: 1529–1541.
  5. 5. Kajino-Sakamoto R, Inagaki M, Lippert E, Akira S, Robine S, et al. (2008) Enterocyte-derived TAK1 signaling prevents epithelium apoptosis and the development of ileitis and colitis. J Immunol 181: 1143–1152.
  6. 6. Liu HH, Xie M, Schneider MD, Chen ZJ (2006) Essential role of TAK1 in thymocyte development and activation. Proc Natl Acad Sci U S A 103: 11677–11682.
  7. 7. Omori E, Matsumoto K, Sanjo H, Sato S, Akira S, et al. (2006) TAK1 is a master regulator of epidermal homeostasis involving skin inflammation and apoptosis. J Biol Chem 281: 19610–19617.
  8. 8. Sato S, Sanjo H, Takeda K, Ninomiya-Tsuji J, Yamamoto M, et al. (2005) Essential function for the kinase TAK1 in innate and adaptive immune responses. Nat Immunol 6: 1087–1095.
  9. 9. Sato S, Sanjo H, Tsujimura T, Ninomiya-Tsuji J, Yamamoto M, et al. (2006) TAK1 is indispensable for development of T cells and prevention of colitis by the generation of regulatory T cells. Int Immunol 18: 1405–1411.
  10. 10. Sayama K, Hanakawa Y, Nagai H, Shirakata Y, Dai X, et al. (2006) Transforming growth factor-beta-activated kinase 1 is essential for differentiation and the prevention of apoptosis in epidermis. J Biol Chem 281: 22013–22020.
  11. 11. Shim JH, Xiao C, Paschal AE, Bailey ST, Rao P, et al. (2005) TAK1, but not TAB1 or TAB2, plays an essential role in multiple signaling pathways in vivo. Genes Dev 19: 2668–2681.
  12. 12. Tang M, Wei X, Guo Y, Breslin P, Zhang S, et al. (2008) TAK1 is required for the survival of hematopoietic cells and hepatocytes in mice. J Exp Med 205: 1611–1619.
  13. 13. Wan YY, Chi H, Xie M, Schneider MD, Flavell RA (2006) The kinase TAK1 integrates antigen and cytokine receptor signaling for T cell development, survival and function. Nat Immunol 7: 851–858.
  14. 14. Vidal S, Khush RS, Leulier F, Tzou P, Nakamura M, et al. (2001) Mutations in the Drosophila dTAK1 gene reveal a conserved function for MAPKKKs in the control of rel/NF-kappaB-dependent innate immune responses. Genes Dev 15: 1900–1912.
  15. 15. Courties G, Seiffart V, Presumey J, Escriou V, Scherman D, et al. (2010) In vivo RNAi-mediated silencing of TAK1 decreases inflammatory Th1 and Th17 cells through targeting of myeloid cells. Blood.
  16. 16. Medzhitov R, Janeway C Jr (2000) Innate immune recognition: mechanisms and pathways. Immunol Rev 173: 89–97.
  17. 17. Beutler B, Rietschel ET (2003) Innate immune sensing and its roots: the story of endotoxin. Nat Rev Immunol 3: 169–176.
  18. 18. Dinarello CA (1997) Proinflammatory and anti-inflammatory cytokines as mediators in the pathogenesis of septic shock. Chest 112: 321S–329S.
  19. 19. Lakso M, Pichel JG, Gorman JR, Sauer B, Okamoto Y, et al. (1996) Efficient in vivo manipulation of mouse genomic sequences at the zygote stage. Proc Natl Acad Sci U S A 93: 5860–5865.
  20. 20. Clausen BE, Burkhardt C, Reith W, Renkawitz R, Forster I (1999) Conditional gene targeting in macrophages and granulocytes using LysMcre mice. Transgenic Res 8: 265–277.
  21. 21. Akashi K, Traver D, Miyamoto T, Weissman IL (2000) A clonogenic common myeloid progenitor that gives rise to all myeloid lineages. Nature 404: 193–197.
  22. 22. Ye M, Iwasaki H, Laiosa CV, Stadtfeld M, Xie H, et al. (2003) Hematopoietic stem cells expressing the myeloid lysozyme gene retain long-term, multilineage repopulation potential. Immunity 19: 689–699.
  23. 23. Greten FR, Arkan MC, Bollrath J, Hsu LC, Goode J, et al. (2007) NF-kappaB is a negative regulator of IL-1beta secretion as revealed by genetic and pharmacological inhibition of IKKbeta. Cell 130: 918–931.
  24. 24. Sarkar S, Han J, Sinsimer KS, Liao B, Foster RL, et al. (2011) RNA-binding protein AUF1 regulates lipopolysaccharide-induced IL10 expression by activating IkappaB kinase complex in monocytes. Mol Cell Biol 31: 602–615.
  25. 25. Kontgen F, Stewart CL (1993) Simple screening procedure to detect gene targeting events in embryonic stem cells. Methods Enzymol 225: 878–890.
  26. 26. Farley FW, Soriano P, Steffen LS, Dymecki SM (2000) Widespread recombinase expression using FLPeR (flipper) mice. Genesis 28: 106–110.
  27. 27. Tzima S, Victoratos P, Kranidioti K, Alexiou M, Kollias G (2009) Myeloid heme oxygenase-1 regulates innate immunity and autoimmunity by modulating IFN-beta production. J Exp Med 206: 1167–1179.