Modulation of monocytes in septic patients: preserved phagocytic activity, increased ROS and NO generation, and decreased production of inflammatory cytokines
© Santos et al. 2016
Received: 5 November 2015
Accepted: 9 February 2016
Published: 16 February 2016
The nature of the inflammatory response underscoring the pathophysiology of sepsis has been extensively studied. We hypothesized that different cell functions would be differentially regulated in a patient with sepsis. We evaluated the modulation of monocyte functions during sepsis by simultaneously assessing their phagocytic activity, the generation of reactive oxygen species (ROS) and nitric oxide (NO), and the production of inflammatory cytokines (IL-6 and TNF-α).
Whole blood was obtained from patients with severe sepsis and septic shock both at admission (D0, n = 34) and after seven days of therapy (D7, n = 15); 19 healthy volunteers were included as a control group. The cells were stimulated with LPS, Pseudomonas aeruginosa, and Staphylococcus aureus. The ROS and NO levels were quantified in monocytes in whole blood by measuring the oxidation of 2,7-dichlorofluorescein diacetate and 4-amino-5-methylamino-2,7-difluorofluorescein diacetate, respectively. Intracellular IL-6 and TNF-α were detected using fluorochrome-conjugated specific antibodies. Monocyte functions were also evaluated in CD163+ and CD163− monocyte subsets.
The monocytes from septic patients presented with preserved phagocytosis, enhanced ROS and NO generation, and decreased production of inflammatory cytokines compared with the monocytes from healthy volunteers. TNF-α and IL-6 increased and ROS generation decreased in D7 compared with D0 samples. In general, CD163+ monocytes produced higher amounts of IL-6 and TNF-α and lower amounts of ROS and NO than did CD163− monocytes.
We demonstrated that monocytes from septic patients, which are impaired to produce inflammatory cytokines, display potent phagocytic activity and increased ROS and NO generation.
Sepsis has been defined as a systemic inflammatory response (SIRS) triggered by an ongoing infection  and more recently considered as the host’s deleterious, non-resolving inflammatory response to infection that leads to organ dysfunction . Understanding the nature of how the inflammatory response underscores the pathophysiology of sepsis would not only help clarify the mechanisms of the syndrome but would also lead to the identification of new therapeutic targets.
Currently, it is generally accepted that infection triggers both inflammatory and anti-inflammatory responses. Accordingly, two major mechanisms have been proposed for the injuries caused by sepsis: sustained activation of innate immunity leading to inflammation and injury  and a predominant initial hyperinflammatory phase followed by impaired immunity and an anti-inflammatory state .
One issue with this model is that the innate immune cells would be regulated in their global functions, and monocytes and neutrophils, for example, are thought to be suppressed in all of their activities in protracted septic patients . In fact, most studies that evaluated blood cells from septic patients have demonstrated an impaired production of inflammatory cytokines after in vitro stimulation [4, 5], whereas neutrophils have been shown to have both up- and down-regulated functions . Interestingly, we observed that peripheral mononuclear cells (PBMC) [7, 8] and monocytes  from septic patients, which were unable to produce inflammatory cytokines, showed an up-regulation of reactive oxygen species (ROS) generation , which was confirmed in another cohort of patients in whom the up-regulation of nitric oxide (NO) generation was also observed . These findings indicate that both a hyperresponse and a hyporesponse can occur, depending on the functions and cells evaluated and, importantly, on the ongoing sepsis process [12, 13].
Reprogramming of monocyte functions was first proposed in an LPS-tolerance model where, depending on the preconditioning treatment, LPS induced selective priming effects on the production of TNF-α and NO in mouse peritoneal macrophages . Subsequent studies demonstrated that LPS-tolerant cells do not produce inflammatory cytokines but present potent phagocytic activity and retain the ability to generate ROS [9, 15, 16]. The alternatively activated macrophages (AAM) also produce reduced levels of inflammatory cytokines and exhibited regulatory or repair activity . These cells exhibited an increased expression of CD206 (mannose receptor) and CD163 (hemoglobin-haptoglobin receptor)  receptors, considered to be typical markers of AAMs.
There is a great interest to study CD163 in sepsis. As a receptor expressed on AAM, it might be a surrogate marker of monocytes and macrophages modulation during sepsis. CD163 also functions as an innate sensor for bacteria , and activation of cell surface Toll-like receptors induces shedding of the receptor, as an acute response to extracellular pathogens . Finally, as a scavenger of Hb, CD163 contributes to the anti-inflammatory response. In clinical settings, increased detection of membrane-bound and soluble CD163 has been reported in septic patients [21, 22].
We hypothesized that different cell functions would be differentially regulated in a patient with sepsis. Thus, we evaluated monocyte modulation during sepsis by simultaneously assessing their phagocytic activity, the generation of ROS and NO, and the production of inflammatory cytokines (IL-6 and TNF-α). Furthermore, we determined if the modulation of monocytes’ function during sepsis is associated with the phenotype of cells expressing CD163.
Patients and healthy volunteers
Patients admitted to the intensive care units of the Sao Paulo, Albert Einstein, and Sirio-Libanes Hospitals with a clinical diagnosis of sepsis according to the ACCP/SCCM consensus conference , from April 2014 to June 2015, were enrolled in the study. The protocol was approved by the ethics committees of the participating hospitals.
Blood samples were obtained from 34 septic patients at admission (D0), and 15 of the patients had a second sample collected after 7 days (D7) of therapy. Samples were also collected from 19 healthy volunteers who were matched according to age and gender.
LPS, gram-negative, and gram-positive bacteria
LPS from Salmonella abortus equi was a generous gift from C. Galanos (Max-Planck Institute of Immunobiology, Germany). Pseudomonas aeruginosa (ATCC27853) and S. aureus (ATCC 25923) were purchased from Oxoid Limited, Basingstoke, Hampshire, UK.
Induction and detection of the production of ROS and NO in monocytes in whole blood
ROS and NO were measured constitutively and after stimulation with LPS and heat-killed S. aureus, and P. aeruginosa for 30 min. Based on the dose-response curves, 100 ng/mL LPS and 2.4 × 108 colonies/mL S. aureus were used for induction of ROS and NO. The concentration of P. aeruginosa was 2.4 × 107 colonies/mL for ROS and 2.4 × 108 colonies/mL for NO. The ROS and NO levels were quantified in monocytes in whole blood by measuring the oxidation of 2,7-dichlorofluorescein diacetate (DCFH-DA; Sigma, St. Louis, MO) and 4-amino-5-methylamino-2,7-difluorofluorescein diacetate (DAF-FMDA; Invitrogen, Carlsbad, CA), respectively, as previously described [11, 23]. Briefly, the tubes from each sample were incubated in the presence of 0.06 mM DCFH-DA or 0.01 mM DAF-FMDA in a 37 °C shaking water bath for 30 min. After incubation, 2 mL of 3 mM EDTA (Sigma) or phosphate-buffered saline (PBS) was added to each tube for ROS and NO determination, respectively, and the mixture was then centrifuged (800g for 5 min at 4 °C). Erythrocytes were lysed in hypotonic saline, and the pellets were incubated with 6 μL of CD14-PerCP clone MΦP9 (BD Bioscience, San Jose, CA, USA) and anti-CD163-PE clone GHI/61 (BD Bioscience) at room temperature for 15 min in the dark. Then, 2 ml of PBS was added to each tube, and the mixture was centrifuged (800g for 5 min at 4 °C). The supernatants were discarded, and the pellets were resuspended in 300 μL of PBS for flow cytometric analysis.
Intracellular detection of cytokines in monocytes in whole blood
Whole blood was diluted 1:2 in RPMI and incubated with LPS and heat-killed bacteria (LPS: 100 ng/mL, P. aeruginosa and S. aureus: 2.4 × 108/mL), or without stimulus in 5-mL propylene tubes at 37 °C in the presence of 5 % CO2. After 30 min, 5 μL (1 mg/mL) of Brefeldin A (Sigma, Saint Louis, MO, USA) was added to the samples, and they were incubated for an additional 4 h. After washing, the red blood cells were ruptured with 2 mL lysis solution (FACS lysing solution, BD Bioscience). After washing with 2 mL PBS, the samples were incubated with the fluorochrome-conjugated monoclonal antibodies CD14-PerCP clone MΦP9 (BD Bioscience) and anti-CD163-PE clone GHI/61 (BD Bioscience) for surface staining for 15 min in the dark at room temperature. The samples were washed in 2 mL PBS, centrifuged, and fixed with 500 μL fixation buffer (PBS 4 % paraformaldehyde) for 30 min in the dark at 4 °C. After centrifugation, 50 μL permeabilization buffer (PBS 1 % FCS; 0.1 % saponin), anti-IL-6-APC clone MQ2-13A5 (BD Bioscience), and anti-TNF-PE-Cy7 clone Mab11 (BD Bioscience) were added to the tubes. The tubes were incubated for 30 min in the dark on ice. Then, the samples were washed with 2 mL permeabilization buffer, and the cells were suspended in Macs buffer for flow cytometric analysis .
Phagocytosis of monocytes in whole blood
Phagocytosis of monocytes was measured using Escherichia coli conjugated to FITC (Phagotest™, Glycotope Biotechnology, Heidelberg, Germany), accordingly to the manufacturer instructions.
Detection of phagocytosis and the production of ROS, NO, IL-6, and TNF-α by monocytes in whole blood was performed by multiparameter flow cytometry (LSRFORTESSA (BD Bioscience)). Events acquisition was performed using FACSDiva software (BD Bioscience). For detection of the production of ROS, NO, IL-6, and TNF-α by monocytes, 5000 events were acquired using forward- and side-scatter parameters combined with CD14-positive cells. For the detection of phagocytosis, 15,000 events were acquired using forward- and side-scatter parameters to determine the monocyte population. All events were acquired and stored, and the analysis was performed using FlowJo (Tree Star INC. Ashland, OR, USA).
Detection of the production of ROS, NO, IL-6, and TNF-α
Monocyte analysis was performed by assessing individual cells (singlets) combined with side-scatter parameters versus CD14 positiveness. Monocytes were further characterized as CD163+ or CD163− cells. The quadrant for CD163+ cells was established based on isotype control.
Co-location of gp91phox and p47phox by immunofluorescence
PBMCs were obtained using the Ficoll density gradient method (Ficoll-Paque PLUS; GE Healthcare Bio-Sciences AB, Uppsala, Sweden) and stored in liquid nitrogen until use. After defrosting, the cells were spun on glass slides. The cells were incubated overnight with the primary antibodies goat anti-Nox2 (1:200) and rabbit anti-p47 (1:100) and then incubated with red fluorescent Alexa Fluor 594 (donkey anti-goat; 1:400), and/or green fluorescent Alexa Fluor 488 (donkey anti-rabbit; 1:200). Nuclear material was stained with 4, 6-diamidino-2-phenylindole (DAPI; Sigma-Aldrich, USA). Images of stained cells were captured using a confocal microscope SP5 (Leica, USA). The images were analyzed in the program ImageJ (National Institutes of Health, Bethesda, Maryland, USA) using the plugincolocalizationanalysis/colocalizationhighlighter (co-localized points—8 bit). That tool generated a new image that presented the points of co-localization of p47phox and gp91phox. Those points of co-localization were quantified from the average fluorescence intensity corresponding to two to four cells/randomly selected field.
The results were analyzed using SPSS (Statistical Package for Social Sciences v 19.0) (IBM, Armonk, NY, USA). The Shapiro-Wilk test was applied to determine the normality of the results. Comparisons between healthy volunteers and patients were performed using the Mann-Whitney U test, and comparisons between patient samples (D7 vs. D0) were performed using the Wilcoxon signed-rank test. Group comparisons were performed by using the Kruskal-Wallis test. The variables that showed differences among the three groups were compared group to group by the Mann-Whitney test.
The interactions of CD163 with ROS, NO, IL-6, and TNF levels were analyzed by two-way repeated measures analysis of variance (ANOVA) with the Bonferroni posttest. P values ≤0.05 were considered significant.
Patient demographic and clinical data
Demographic data and outcomes from septic patients included in the study
Cohort of septic patients (n = 34)
Age [mean (SD)]
Gender [N (%)]
Stages of sepsis [N (%)]
SOFA score (D0)
In hospital mortality [N (%)]
Outcome accordingly to stage at enrollment [N (%)]
Sources of infection [N (%)]
Phagocytosis, ROS and NO production, and intracellular detection of cytokines in monocytes in whole blood
No differences were found in monocyte phagocytosis of opsonized E. coli between healthy volunteers (median, GMFI, 15.499; range 8.722–24.879) and septic patients at D0 (median, GMFI, 19.707; range 5.207–35.075) (P = 0.178). Similarly, no differences were found when patients were classified as having severe sepsis or septic shock: severe sepsis (median, GMFI, 23.733; range 6.118–35.075) and septic shock (median, GMFI, 17.116; range 5.207–32.877) (P = 0.112).
Production of ROS, NO, IL-6, and TNF-α by monocytes of septic patients and healthy volunteers
9 · 6
The percentages of monocytes producing IL-6 was lower in severe sepsis and septic shock patients than in healthy volunteers following LPS, P. aeruginosa, and S. aureus stimulation (P < 0.05, Kruskal-Wallis); no differences were found between patients with severe sepsis and septic shock (Fig. 3c).
Similarly, TNF-α production differed among healthy volunteers, severe sepsis patients and septic shock patients in all conditions tested (P < 0.05, Kruskal-Wallis). In this case, differences were found in the septic group, with lower detection in patients with septic shock than in those with severe sepsis for all stimuli tested (Fig. 3d).
ROS generation was positively correlated with SOFA score in the control condition (R = 0.371, P = 0.034) and after LPS (R = 0.414, P = 0.017) and P. aeruginosa (R = 0.409, P = 0.018) stimulation, but not with S. aureus (R = 0.109, P = 0.545). No correlations were found between the organ dysfunction score and any other cell functions evaluated in any of the conditions tested (Pearson correlation test).
Interaction between monocyte functions and cell surface expression of CD163
Dynamics of monocyte functions in patient follow-up samples
There was no difference in the phagocytic activity of monocytes from septic patients at admission (D0) (Median, GMFI, 19.473; range 5.207−35.075) and after 7 days of follow-up (Median, GMFI, 18.887; range 6.023−31.803) (P = 0.875).
Analysis of groups, including healthy volunteers and patients at D0 and D7, showed that differences between D7 and healthy volunteers were no longer significant for NO after P. aeruginosa and IL-6 and TNF-α after S. aureus stimulation.
Co-location of gp91phox and p47phox by immunofluorescence
Our results show that monocytes from septic patients are modulated during the ongoing infection process, with preserved phagocytosis, increased ROS and NO generation, and decreased production of inflammatory cytokines. These results are consistent with our previously reported findings obtained in monocytes from septic patients [7, 9–11] and further support the concept of “reprogramming,” or modulation of cell functions rather than hyporesponsiveness during sepsis [12, 24].
These results also indicate the similarities between monocyte modulation in LPS-tolerance models and monocyte modulation in sepsis [12, 15, 16]. Multiple mechanisms have been shown to be involved in tolerance to LPS. Foster et al. reported the epigenetic mechanisms driving the modulation of LPS-response in LPS-tolerant cells. They found two groups of differentially regulated genes: the “tolerizeable” (T) and the “nontolerizeable” (NT) genes. The pro-inflammatory cytokine genes were found to be down-regulated (T), whereas antimicrobial genes were found to be up-regulated (NT), thus supporting their hypothesis that TLR-induced gene expression with different biological functions is distinctly regulated . These findings were extended to human monocytes by Del Fresno and coworkers, who found down-regulation of pro-inflammatory cytokines and antigen presentation genes and up-regulation of anti-inflammatory factors, such as IRAK-M, and antimicrobial effectors . In our own study, which focused on the TLR pathway, we observed down-regulation of TNF-α, IL-12, and CCL2 and up-regulation of IL-10 and colony stimulating factors (CSF2 and CSF3) in tolerant cells .
Down-regulation of inflammatory cytokines, measured at intracellular level in our study, has been consistently reported in the literature upon the in vitro stimulation of monocytes from septic patients [8, 27, 28]. Modulation of the monocyte response during sepsis occurred despite preservation of LPS binding to monocytes and of TLR2 and TLR4 expression on the monocyte cell surface [7, 9, 13]. The regulation of IL-10 production is more controversial. In this study, we found no differences in intracellular levels of IL-10 in monocytes in a subset of patients (N = 12) and healthy volunteers (N = 12) (data not shown); this finding is consistent with our previous results in whole blood supernatants .
Monocytes in whole blood presented increases in ROS and NO generation in vitro after stimulation with LPS, and Gram-negative and Gram-positive clinically significant bacteria, P. aeruginosa, and Staphylococcus aureus, respectively. This finding is consistent with our previously reported results in two other series of septic patients [10, 11]. To further link ROS generation to phagocytosis, we evaluated the co-localization of p47phox and NOX-2 (gp91phox) in monocytes of septic patients. Co-localization was found in septic patients, mainly in the admission samples, and not in healthy volunteers, indicating that increased NADPH-oxidase activity is a source of ROS in septic patients. In addition to the role of ROS in antimicrobial defense, ROS is associated with cell and organ toxicity in sepsis. Consistent with previous findings , we found that ROS generation correlated with the SOFA score in most conditions.
In the follow-up samples, decreased production of ROS and increased production of inflammatory cytokines were observed under all stimuli compared to the admission samples, which indicated a trend toward the restoration of homeostasis. Interestingly, under S.aureus, stimulation levels of IL-6 and TNF-α in patients’ follow-up samples did not differ from healthy volunteers.
In further support of modulation rather than hyporesponse in monocytes during sepsis, we found that the phagocytic activity of monocytes was preserved during the ongoing infection process, even in patients with septic shock. This finding is in agreement with previous studies of LPS-induced tolerance in vitro [15, 16].
In addition to the above described similarities with LPS-tolerant monocytes, the pattern of activities of monocytes from septic patients in this study resembles that described for macrophages under the effects of pro-resolving mediators, which present enhanced phagocytic activity without evoking pro-inflammatory responses .
We evaluated whether the differences in the modulation of inflammatory cytokines and ROS/NO generation observed between septic patients and healthy volunteers were influenced by the expression of CD163 on monocytes. In general, CD163+ monocytes produced higher amounts of TNF-α and IL-6 and lower amounts of ROS and NO than did CD163− monocytes. An interaction between the expression of CD163 with cytokine production was found upon stimulation with LPS or bacteria, with CD163+ monocytes producing higher amounts of cytokines in both patients and healthy volunteers. An interaction between the expression of CD163 and ROS generation was also found after S. aureus and P. aeruginosa stimulation. In this case, differences between CD163+ and CD163− cells were only observed in septic patients; under both bacterial stimuli, ROS generation was higher in sepsis patients than in healthy volunteers for both CD163+ and CD163− monocytes.
Detection of higher levels of inflammatory cytokines in CD163+ cells than in CD163− cells was unexpected because of the anti-inflammatory role of alternatively activated macrophages . However, this finding is consistent with the concept of a dual role of CD163+ monocytes in sepsis. CD163 may be important for controlling inflammation by removing free hemoglobin secondary to hemolysis and converting heme to its anti-inflammatory metabolites, but it also may function as a sensor of bacteria . Accordingly, Fabriek and coworkers demonstrated the binding of Gram-positive and Gram-negative bacteria to CD163 and induction of inflammatory cytokines in CD163-expressing CHO cells and suppression of bacteria-induced cytokines in human monocytes by blocking antibodies against CD163 . Supporting our results with septic patients, we observed that modulation of cytokines production in a model of LPS tolerance occurred regardless of the expression of CD163 on monocytes cell surface .
We demonstrated that monocytes from septic patients, which have impaired inflammatory cytokine production, display potent phagocytic activity and increased ROS and NO generation. This modulation represents a state in which the host attempts to control the initial systemic inflammatory response while maintaining control over infection. As we previously suggested, this modulation may represent the return to homeostasis in cases of successful antimicrobial therapy and recovery of underlying disease. In contrast, failure to mount a robust inflammatory response may represent a state of immunosuppression in protracted patients .
We are in debt to Renato Arruda Mortara for the contribution on confocal microscopy, to Ana Cristina Gales for providing the bacteria used for the monocyte stimulation, and to Gianni Santos for the statistic support. This work was supported by the Fundacao de Amparo a Pesquisa do Estado de Sao Paulo (FAPESP)—grant number 2011/20401-4 and Conselho Nacional de Desenvolvimento Cientifico e Tecnologico—CNPq—grant number 305685/2011-2. SS Santos has a fellowship from Coordenação de Aperfeiçoamento de Pessoal de Nível Superior—CAPES.
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made.
- Bone RC, Balk RA, Cerra FB, Dellinger RP, Fein AM, Knaus WA, Schein RM, Sibbald WJ (1992) Definitions for sepsis and organ failure and guidelines for the use of innovative therapies in sepsis. The ACCP/SCCM Consensus Conference Committee. American College of Chest Physicians/Society of Critical Care Medicine. Chest 101:1644–1655View ArticlePubMedGoogle Scholar
- Vincent JL, Opal SM, Marshall JC, Tracey KJ (2013) Sepsis definitions: time for change. Lancet 381:774–775PubMed CentralView ArticlePubMedGoogle Scholar
- Xiao W, Mindrinos MN, Seok J, Cuschieri J, Cuenca AG, Gao H, Hayden DL, Hennessy L, Moore EE, Minei JP, Bankey PE, Johnson JL, Sperry J, Nathens AB, Billiar TR, West MA, Brownstein BH, Mason PH, Baker HV, Finnerty CC, Jeschke MG, Lopez MC, Klein MB, Gamelli RL, Gibran NS, Arnoldo B, Xu W, Zhang Y, Calvano SE, McDonald-Smith GP, Schoenfeld DA, Storey JD, Cobb JP, Warren HS, Moldawer LL, Herndon DN, Lowry SF, Maier RV, Davis RW, Tompkins RG (2011) A genomic storm in critically injured humans. J Exp Med 208:2581–2590PubMed CentralView ArticlePubMedGoogle Scholar
- Hotchkiss RS, Monneret G, Payen D (2013) Immunosuppression in sepsis: a novel understanding of the disorder and a new therapeutic approach. Lancet Infect Dis 13:260–268PubMed CentralView ArticlePubMedGoogle Scholar
- Riedemann NC, Guo RF, Ward PA (2003) Novel strategies for the treatment of sepsis. Nat Med 9:517–524View ArticlePubMedGoogle Scholar
- Brown KA, Brain SD, Pearson JD, Edgeworth JD, Lewis SM, Treacher DF (2006) Neutrophils in development of multiple organ failure in sepsis. Lancet 368:157–169View ArticlePubMedGoogle Scholar
- Brunialti MK, Martins PS, Barbosa de Carvalho H, Machado FR, Barbosa LM, Salomao R (2006) TLR2, TLR4, CD14, CD11B, and CD11C expressions on monocytes surface and cytokine production in patients with sepsis, severe sepsis, and septic shock. Shock 25:351–357View ArticlePubMedGoogle Scholar
- Rigato O, Salomao R (2003) Impaired production of interferon-gamma and tumor necrosis factor-alpha but not of interleukin 10 in whole blood of patients with sepsis. Shock 19:113–116View ArticlePubMedGoogle Scholar
- Salomao R, Brunialti MK, Kallas EG, Martins PS, Rigato O, Freudenberg M (2002) Lipopolysaccharide-cell interaction and induced cellular activation in whole blood of septic patients. J Endotoxin Res 8:371–379PubMedGoogle Scholar
- Martins PS, Brunialti MK, Martos LS, Machado FR, Assuncao MS, Blecher S, Salomao R (2008) Expression of cell surface receptors and oxidative metabolism modulation in the clinical continuum of sepsis. Crit Care 12:R25PubMed CentralView ArticlePubMedGoogle Scholar
- Santos SS, Brunialti MK, Rigato O, Machado FR, Silva E, Salomao R (2012) Generation of nitric oxide and reactive oxygen species by neutrophils and monocytes from septic patients and association with outcomes. Shock 38:18–23View ArticlePubMedGoogle Scholar
- Salomao R, Brunialti MK, Rapozo MM, Baggio-Zappia GL, Galanos C, Freudenberg M (2012) Bacterial sensing, cell signaling, and modulation of the immune response during sepsis. Shock 38:227–242View ArticlePubMedGoogle Scholar
- Salomao R, Martins PS, Brunialti MK, Fernandes Mda L, Martos LS, Mendes ME, Gomes NE, Rigato O (2008) TLR signaling pathway in patients with sepsis. Shock 30(Suppl 1):73–77View ArticlePubMedGoogle Scholar
- Zhang X, Morrison DC (1993) Lipopolysaccharide-induced selective priming effects on tumor necrosis factor alpha and nitric oxide production in mouse peritoneal macrophages. J Exp Med 177:511–516View ArticlePubMedGoogle Scholar
- Fernandes ML, Mendes ME, Brunialti MK, Salomao R (2010) Human monocytes tolerant to LPS retain the ability to phagocytose bacteria and generate reactive oxygen species. Braz J Med Biol Res 43:860–868View ArticlePubMedGoogle Scholar
- del Fresno C, Garcia-Rio F, Gomez-Pina V, Soares-Schanoski A, Fernandez-Ruiz I, Jurado T, Kajiji T, Shu C, Marin E, Gutierrez del Arroyo A, Prados C, Arnalich F, Fuentes-Prior P, Biswas SK, Lopez-Collazo E (2009) Potent phagocytic activity with impaired antigen presentation identifying lipopolysaccharide-tolerant human monocytes: demonstration in isolated monocytes from cystic fibrosis patients. J Immunol 182:6494–6507View ArticlePubMedGoogle Scholar
- Mosser DM, Edwards JP (2008) Exploring the full spectrum of macrophage activation. Nat Rev Immunol 8:958–969PubMed CentralView ArticlePubMedGoogle Scholar
- Mantovani A, Sica A, Sozzani S, Allavena P, Vecchi A, Locati M (2004) The chemokine system in diverse forms of macrophage activation and polarization. Trends Immunol 25:677–686View ArticlePubMedGoogle Scholar
- Fabriek BO, van Bruggen R, Deng DM, Ligtenberg AJ, Nazmi K, Schornagel K, Vloet RP, Dijkstra CD, van den Berg TK (2009) The macrophage scavenger receptor CD163 functions as an innate immune sensor for bacteria. Blood 113:887–892View ArticlePubMedGoogle Scholar
- Weaver LK, Hintz-Goldstein KA, Pioli PA, Wardwell K, Qureshi N, Vogel SN, Guyre PM (2006) Pivotal advance: activation of cell surface Toll-like receptors causes shedding of the hemoglobin scavenger receptor CD163. J Leukoc Biol 80:26–35View ArticlePubMedGoogle Scholar
- Brunialti MK, Santos MC, Rigato O, Machado FR, Silva E, Salomao R (2012) Increased percentages of T helper cells producing IL-17 and monocytes expressing markers of alternative activation in patients with sepsis. PLoS One 7:e37393View ArticlePubMedGoogle Scholar
- Moller HJ, Moestrup SK, Weis N, Wejse C, Nielsen H, Pedersen SS, Attermann J, Nexo E, Kronborg G (2006) Macrophage serum markers in pneumococcal bacteremia: prediction of survival by soluble CD163. Crit Care Med 34:2561–2566View ArticlePubMedGoogle Scholar
- Kojima H, Nakatsubo N, Kikuchi K, Kawahara S, Kirino Y, Nagoshi H, Hirata Y, Nagano T (1998) Detection and imaging of nitric oxide with novel fluorescent indicators: diaminofluoresceins. Anal Chem 70:2446–2453View ArticlePubMedGoogle Scholar
- Cavaillon JM, Adib-Conquy M (2006) Bench-to-bedside review: endotoxin tolerance as a model of leukocyte reprogramming in sepsis. Crit Care 10:233PubMed CentralView ArticlePubMedGoogle Scholar
- Foster SL, Hargreaves DC, Medzhitov R (2007) Gene-specific control of inflammation by TLR-induced chromatin modifications. Nature 447:972–978PubMedGoogle Scholar
- Mendes ME, Baggio-Zappia GL, Brunialti MK, Fernandes Mda L, Rapozo MM, Salomao R (2011) Differential expression of Toll-like receptor signaling cascades in LPS-tolerant human peripheral blood mononuclear cells. Immunobiology 216:285–295View ArticlePubMedGoogle Scholar
- Ertel W, Kremer JP, Kenney J, Steckholzer U, Jarrar D, Trentz O, Schildberg FW (1995) Downregulation of proinflammatory cytokine release in whole blood from septic patients. Blood 85:1341–1347PubMedGoogle Scholar
- Munoz C, Carlet J, Fitting C, Misset B, Bleriot JP, Cavaillon JM (1991) Dysregulation of in vitro cytokine production by monocytes during sepsis. J Clin Invest 88:1747–1754PubMed CentralView ArticlePubMedGoogle Scholar
- Chiang N, Fredman G, Backhed F, Oh SF, Vickery T, Schmidt BA, Serhan CN (2012) Infection regulates pro-resolving mediators that lower antibiotic requirements. Nature 484:524–528PubMed CentralView ArticlePubMedGoogle Scholar
- Etzerodt A, Moestrup SK (2013) CD163 and inflammation: biological, diagnostic, and therapeutic aspects. Antioxid Redox Signal 18:2352–2363PubMed CentralView ArticlePubMedGoogle Scholar
- Alves-Januzzi AB, Brunialti MK, Salomao R (2015) CD163 and CD206 expression does not correlate with tolerance and cytokine production in LPS-tolerant human monocytes. Cytometry Part B, Clinical cytometryGoogle Scholar