- Open Access
CSF-1-induced DC-SIGN+ macrophages are present in the ovarian endometriosis
Reproductive Biology and Endocrinology volume 20, Article number: 48 (2022)
Researchers have found that macrophages are the predominant cells in the peritoneal fluid (PF) of endometriosis patients. CSF-1 has been found to accumulate in the lesions and PF of endometriosis patients, and CSF-1 induces THP-1-derived macrophages to polarize toward a CD169+ DC-SIGN+ phenotype. Does the cytokine CSF-1 induce monocytes to differentiate into macrophages with a DC-SIGN+ phenotype in endometriosis?
The level of CSF-1 in the endometrium of control subjects, and the eutopic, and ectopic endometrium of endometriosis patients was evaluated by real-time polymerase chain reaction (qRT–PCR) and was determined by enzyme-linked immunosorbent assay (ELISA) in the PF of control and endometriosis patients. CSF-1 expression was examined with a MILLIPLEX MAP Mouse Cytokine/Chemokine Magnetic Bead Panel. DC-SIGN+ macrophages were detected by immunohistochemical staining of tissues and flow cytometric analysis of the PF of control subjects (N = 25) and endometriosis (N = 35) patients. The phenotypes and biological activities of CSF-1 -induced macrophages were compared in an in vitro coculture system with peripheral blood lymphocytes from control subjects.
In this study, we found that the proportion of DC-SIGN+ CD169+ macrophages was higher in the abdominal immune microenvironment of endometriosis patients. CSF-1 was primarily secreted from ectopic lesions and peritoneum in mice with endometriosis. In addition, CSF-1 induced the polarization of macrophages toward a DC-SIGN+ CD169+ phenotype; this effect was abolished by the addition of an anti-CSF-1R antibody. CSF-1 induced the generation of DC-SIGN+ macrophages, leading to a depressed status of peripheral blood lymphocytes, including a high percentage of Treg cells and a low percentage of CD8+ T cells. Similarly, blockade with the anti-CSF-1R antibody abrogated this biological effect.
This is the first study on the role of DC-SIGN+ macrophages in the immune microenvironment of endometriosis. Further study of the mechanism and biological activities of CSF-1-induced DC-SIGN+ macrophages will enhance our understanding of the physiology of endometriosis.
Endometriosis (EMS) is a common but complicated disease that causes chronic pelvic pain, dyspareunia and infertility in 6–10% of women of reproductive age . Although the retrograde menstruation hypothesis has been widely accepted , in recent years, some studies have suggested that retrograde menstruation is a precondition of EMS development and that the abnormal metabolism of hormones is a secondary condition; however, immune dysfunction is a cause of EMS .
A number of studies have been conducted on peritoneal immunity in EMS, but many have been limited to a description of immune cell dysfunction [4,5,6]. Some experiments suggested the depressed state of peritoneal immunity in EMS patients [7,8,9]. With the widespread study of the immune system in the abdominal microenvironment, the profound role of macrophages in the pathological physiology of EMS is becoming clear . Crucial functions of macrophages, such as stabilizing tissue structure, driving injury, and regulating the immune microenvironment, have been observed . Our previous studies suggested that macrophages are involved in the progression of EMS . In addition, along with the high number of macrophages, the proportions of Treg and Th1 cells in the peritoneal fluid of mice with EMS were found to be increased in a previous in vivo study .
Peritoneal immunity is complex and powerful, and it is surprising that the ectopic endometrium survives during the menstrual cycle. Colony stimulating factor-1 (CSF-1), also called macrophage colony-stimulating factor (M-CSF), is a key cytokine that induces monocytes to differentiate into CD169+ macrophages . CSF-1 and its receptor CSF-1R (M-CSFR or CD115) are diffusely expressed and have frequently been reported in the context of EMS [15, 16]. A study showed that the expression of CSF-1 was increased in the PF of EMS patients . According to the literature, CD169+ macrophages are found in various diseases and indirectly affect Treg cells and CD8+ T cells [18, 19]. In a study of transplantation tolerance, CD169+ DC-SIGN+ macrophages were found to interact with lymphocytes to maintain transplant survival . Many studies have proven that FOXP3+ Treg cells play an important role in immunoregulation and immunosuppression [21, 22]. FOXP3+ Treg cells secrete cytokines, such as CCL22, CCL17, transforming growth factor-1 (TGF-1), interleukin (IL)-1, tumor necrosis factor (TNF), IL-8 and vascular endothelial growth factor (VEGF), while cooperating with other immune cells to promote the progression of EMS .
Szyllo K, et al. determined that a small percentage of CD8+ T cells are related to EMS . A study showed that CD169+ macrophages had a profound effect on the cellular immunologic response . Moreover, CD169 + macrophages were found to induce the polarization of Treg cells and regulate the immune response . Therefore, the critical aim was to identify the common targets through which macrophages communicate with Treg cells and CD8+ T cells.
DC-specific ICAM-3-grabbing nonintegrin (DC-SIGN or CD209) on CD169+ macrophages is a key target in the regulation of depressed immunity. This molecule was first described by Geijtenbeek TBH, et al., in a study about a dendritic cell-specific HIV-1-binding protein that enhances trans-infection of T cells . Mechanistically, these authors explained that DC-SIGN is an important molecule that participates in the process by which DCs interact with CD4+ T cells . Soilleux E. J. et al. proved that some specific macrophages, such as those in the placenta and decidua, expressed DC-SIGN . Marie Larsson et al. observed that DC-SIGN+ DCs regulated CD8+ T cells . Recently, some studies have suggested that DC-SIGN is a type of regulatory receptor on DCs and macrophages that alters the function of macrophages . Overall, the aim of our study was to prove that CSF-1 induces monocytes to differentiate into macrophages with a CD169+ DC-SIGN+ phenotype in endometriosis and that this macrophage phenotype can influence the differentiation of T cells.
CSF-1 was evaluated by qRT–PCR in the tissues of control subjects and endometriosis patients, and was determined by ELISA in the PF of control and endometriosis patients. Then, CSF-1 expression was examined with a MILLIPLEX MAP Mouse Cytokine/Chemokine Magnetic Bead Panel in the EMS model. DC-SIGN+ macrophages were detected by immunohistochemical staining of tissues and flow cytometric analysis of the PF of control subjects and endometriosis patients. The phenotypes and biological activities of CSF-1 -induced DC-SIGN+ macrophages were compared using flow cytometric analysis in an in vitro coculture system with peripheral blood lymphocytes.
Tissue and sample collection
For immunohistochemical staining, 39 women with EMS (American Fertility Society classification as endometriosis Stage III ( n = 30) or Stage IV (n = 9)) who were diagnosed by clinical pathologists at Shanghai First Maternity and Infant Hospital Affiliated with Tongji University School of Medicine, between June 2019 and May 2020 were recruited. Eutopic endometrial samples were obtained from women with EMS (n = 17). For the control samples, endometrial tissue samples were collected by curettage from 11 women who exhibited fallopian tube blockage and previously needed contraception by fallopian tube ligation but now needed tubal reversal, and did not have any clinical indication or history of adenomyosis or endometriosis. PF was collected, avoiding contamination with blood, from women with advanced-stage EMS (n = 35) and from control subjects (n = 25) during laparoscopic surgery. All the enrolled patients in the control group were confirmed by laparoscopy to have no endometriotic lesions, and all had a histological diagnosis of mature ovarian teratoma composed of epidermis only (n = 20) or benign cyst of the mesosalpinx (n = 5). The clinical characteristics of the patients and controls are summarized in Table 1.
Cell lines, cytokines and animals
The acute monocytic leukaemia (THP-1) cell line was a gift from the Cryomedicine Lab at Qilu Hospital of Shandong University. Recombinant human M-CSF was purchased from R&D Systems (Minnesota, USA). C57BL/6 mice were purchased from Shanghai SLAC Laboratory Animal Co., Ltd., at 4 weeks of age.
Real-time polymerase chain reaction
To test the gene expression level of CSF-1 in the endometrium of control subjects (N = 11) and the eutopic endometrium (N = 17) and ectopic (N = 39) endometrium of endometriosis patients, we conducted PCR. Total RNA was extracted from 0.2 × 0.2 × 0.1 cm tissue fragments using TRIzol Reagent (10,296,010, Invitrogen, USA) according to the product manual. RNA (0.5 μg) was reverse transcribed into cDNA with ReverTra Ace Quantitative PCR (qPCR) RT Master Mix with gDNA Remover (Code No. FSQ-301, TOYOBO, Osaka Japan). Each 20 μl PCR mixture contained 1 × SYBR Green PCR Master Mix (TOYOBO, Osaka Japan), 30 ng of cDNA and 300 nM each specific primer from Sangon Biotech (Shanghai) Co., Ltd. Quantitatie PCR was performed on an Applied Biosystems StepOnePlus RT–PCR System (Applied Biosystems, USA). Three separate experiments were performed on different cultures, and each sample was assayed in triplicate. The mean was calculated to determine the mRNA levels by quantitative real-time polymerase chain reaction (RT–PCR) analysis using the ABI StepOnePlus RT–PCR System (Applied Biosystems). The primers used to amplify CSF-1 were 5'-GCTGCTTCACCAAGGATTATG-3' (sense) and 5'-GGGTCACTGCTAGGGATG-3' (antisense), and the gene expression levels in each group was normalized to that of glyceraldehyde 3-phosphate dehydrogenase (GAPDH), which was assessed with the following primers: 5'-AGCCACATCGCTCAGACA-3' (sense) and 5'-GCCCAATACGACCAAATCC-3' (antisense). The mean relative gene expression levels were determined, and differences in expression were calculated using the 2−△△Ct method.
Establishment of the EMS model
All mice were maintained under specific pathogen-free (SPF) conditions. All procedures were approved by the Animal Care and Use Committee of Tongji University (Shanghai, China). The estrous stage was monitored daily by obtaining a vaginal smear every morning for 2 weeks, and mice with a normal estrous cycle were used in the following experiments. Endometriosis was established by intraperitoneal injection of endometrial segments. Briefly, donor mice were sacrificed, and the uteri were isolated and collected in a Petri dish containing phosphate-buffered saline (PBS). The isolated uterine horns were treated identically, including longitudinal splitting with a pair of scissors, isolation of endometrial tissue and gentle disruption to generate small, uniform fragments of approximately 1 mm. Then, these fragments were intraperitoneally injected into recipient mice through a 1 ml syringe with a 25 G needle. Equal amounts of endometrial fragments from one donor mouse were injected into two recipient mice. Specifically, 15 endometrial segments in 200 μl of sterile PBS were injected into each recipient mouse. However, mice in the control groups only received injections of 200 µL of sterile PBS. Finally, ten mice from the endometriosis and control groups were sacrificed 42 days after the model was established.
Analysis of CSF-1 with a MILLIPLEX MAP Mouse Cytokine/Chemokine Magnetic Bead Panel
A MILLIPLEX® MAP kit for analysis was used to evaluate tissue (uterus, peritoneum, and ectopic lesions) cytokine production (CSF-1) and release in the PF of EMS mice, in accordance with the manufacturer’s instructions. In addition, the plate was analyzed on a Luminex 200 system. The sample data were analyzed using xPONENTLX200 software (Madison, WI, USA).
To detect DC-SIGN+, CD169+, and CSF-1R+ macrophages and FOXP3+ T cells in the tissues of control subjects (N = 25) and endometriosis patients (N = 35), we conducted immunohistochemical staining. For each sample, 4 μm thick sections were dewaxed and rehydrated in ethanol and water. Antigen retrieval was performed in citrate buffer (pH 6.0, 15 min), and endogenous peroxidase activity was quenched by incubation in 3% hydrogen peroxide. The tissue sections were incubated overnight at 4 °C with rabbit primary antibodies against human CD169 (ab183356, Abcam, Cambridge, UK; 1:100), CSF-1R (ab183316, Abcam, Cambridge, UK; 1:100), and DC-SIGN (ab5715, Abcam, Cambridge, UK; 1:50) and mouse monoclonal antibodies against human CD68 (ab955, Abcam, Cambridge, UK; 1:200) and FOXP3 (ab20034, Abcam, Cambridge, UK; 1:50). A secondary antibody kit (CWBIO, Beijing, China) was utilized to label the primary antibodies. The sections were counterstained with hematoxylin, dehydrated in ethanol and xylene, and mounted in PermountTM mounting medium. Images were acquired using a microscope (BX53, Olympus, Tokyo, Japan), which was fitted with a digital camera (cellSens Standard, Olympus). A series of five images was randomly selected from six sections per tissue sample. Positive cells in images acquired at 400 × magnification were counted manually by two independent investigators blinded to the treatment groups. Cells were counted in at least five different areas in ectopic lesions, and data were plotted as the percentage of positive cells relative to the total number of cells, as previously described . The percentage of positive cells was calculated by counting positive cells among a total of 200 cells in three separate fields.
Macrophage induction and culture
THP-1 cells were induced to differentiate into macrophages in accordance with a previously reported method . Cells cultured in 24-well plates were stimulated by adding 100 ng/ml phorbol 12-myristate 13-acetate (PMA; Sigma, USA) for 48 h and were than washed three times with PBS to eliminate the effect of PMA.
Cellular Immunofluorescence Analysis
To detect the DC-SIGN+ and CD169+ macrophages derived from THP-1 cells induced by CSF-1 and blocked with CSF-1R, we conducted a cellular immunofluorescence analysis. We treated the differentiated macrophages with CSF-1 (50 ng/ml) and cultured them for 48 h. For confirmation, we cultured the differentiated macrophages with RPMI 1640 medium (Gibco, China) containing anti-CSF-1R (Abcam, UK, 1:20) for 2 h and then added CSF-1 (R&D Systems, USA, 50 ng/ml) to the medium for 48 h. Cellular immunofluorescence staining was performed as previously described . The target macrophages were washed twice with PBS, fixed with 4% paraformaldehyde (pH 7.0) for 30 min, permeabilized with 0.1% Triton X-100 (Sigma) for 10 min, blocked with 10% normal goat serum for 1 h, and incubated overnight with rabbit anti-human CD169 (ab183356, Abcam, UK; 1:100) or anti-DC-SIGN (ab5715, Abcam, UK; 1:50) antibodies and a mouse monoclonal antibody against human CD68 (ab955, Abcam, UK; 1:200) at 4 °C. The cells were then washed with PBS three times and incubated at room temperature with a DyLight 488-conjugated donkey anti-rabbit secondary antibody (1:400; Abcam, UK) or a DyLight 594-conjugated donkey anti-goat secondary antibody (1:400; Abcam, UK) for 1 h. After the plates were washed, cell nuclei were counterstained with fluorescent mounting medium with 4’,6-diamidino-2-phenylindole (Abcam, UK).
Coculture of peripheral blood mononuclear cells (PBMCs) with THP-1-derived macrophages
To check the influence of DC-SIGN+ CD169+ macrophages derived from THP-1 cells on T cells, we cocultured PBMCs with THP-1-derived macrophages. PBMCs were prepared as previously described . Volunteers were recruited from among healthy women without dysmenorrhea (n = 7) and with a regular menstrual cycle. PBMCs were isolated from 15 ml of venous blood using Ficoll-Cardiografin (Tian Jin Hao Yang Biological Manufacture, China). After centrifugation, PBMCs were collected from the interphase layer and washed four times with PBS. For coculture, PBMCs were suspended in RPMI 1640 medium supplemented with FBS at a concentration of 1 × 106 cells/ml. The coculture system simulated the lesion site in the human body. Transwell membranes (Corning, USA) were used to allow the exchange of macrophage secretions with PBMCs. First, Transwell membranes were inserted into a 24-well plate, and the upper chamber was preseeded with macrophages derived from THP-1 cells. In addition, 100,000 PBMCs were counted and seeded on the membrane. Second, two groups of macrophages derived from THP-1 cells were treated with a rabbit anti-human DC-SIGN (Abcam, UK; 1:50) or CSF-1R (Abcam, UK; 1:20) antibody and with CSF-1 (50 ng/ml) for 48 h. Third, we cocultured the differentiated macrophages with PBMCs, as shown in (Fig. 5A). Then, the Transwell plates were placed in a 5% CO2 incubator at 37 °C for 2 days. After incubation, the cocultured PBMCs were collected.
The remaining peritoneal cells collected from the controls and the patients were divided into two equal parts for analysis by flow cytometry (FCM). To determine the percentages of the DC-SIGN+ CD169+ macrophage subset, cells in the PF at a density of 0.5 × 105 cells/tube were used and stained in duplicate in the dark at 4 °C for 30 min with the following antibodies: APC-anti-human CD209 (clone: 9E9A8, Biolegend, USA), FITC-anti-human CD45 (clone: 2D1, Biolegend, USA), PerCP-Cy5.5-anti-human CSF-1R (clone: 9-4D2-1E4, Biolegend, USA) and PE-anti-human CD169 (clone: 7–239, Biolegend, USA). Fluorophore-conjugated and isotype-matched antibodies served as the negative controls. The proportions of Treg cells and CD8+ T cells in the PBMCs collected from the coculture system were determined using FCM. PBMCs at a density of 0.5 × 105 cells/tube were fixed, permeabilized, and stained in duplicate with the following antibodies: APC-anti-human FoxP3 (clone: 3G3, Assay Genie, Ireland), FITC-anti-human CD45 (clone: 2D1, Biolegend, USA), PerCP-Cy5.5-anti-human CD8 (clone: SK1, Biolegend, USA), and PE-anti-human CD4 (clone: SK3, Biolegend, USA). The proportions of distinct subpopulations were eventually characterized on a BD FACSCalibur (BD, USA). The resulting data were examined using FlowJo software. A representative graph from three or more repeated experiments is shown. Positive gates were set separately for each sample type and label and were set to include less than 1% of the acquired events in the unstained sample.
Enzyme-linked immunosorbent assay (ELISA)
First, an aliquot of each preparation was kept for protein estimation using a Bradford protein concentration assay kit (P0006C) from Beyotime. The CSF-1 levels in the PF of EMS patients and controls were quantified using each ELISA kit (R&D Systems), according to the manufacturer’s instructions. The absorbance of the streptavidin–horseradish peroxidase colorimetric reaction product was measured with a microplate reader capable of measuring the absorbance at 450 nm, with the correction wavelength set at 540 nm or 570 nm. The optical density values were compared with those of serial dilutions of recombinant human CSF-1 as a standard. The relevant concentration was calculated, and standard curves were generated.
All statistical analyses were completed using Prism software, version 5 (GraphPad, San Diego, CA, USA), and the measurement data are presented as the mean ± SD values. Statistical significance was assessed using Student’s t test for univariate analyses of two sets of data by one-way or two-way analysis of variance (ANOVA) when multiple comparisons were necessary. P < 0.05 was considered to indicate significance.
The proportion of DC-SIGN+ macrophages was higher in endometriosis patients
We collected peritoneal cells from the PF of patients for flow cytometry and performed a series of analyses (Fig. 1). Macrophages express higher levels of the CD45 antigen, which is exclusively expressed on all nucleated cells of the hematopoietic system, and the different proportions of the monocyte/macrophage populations in the peritoneal cavity can be further confirmed in morphological cytograms showing the FSC (forward scatter) and SSC (side scatter) parameters obtained by flow cytometry  (Fig. 1A-B). We analyzed the coexpression of DC-SIGN and CD169 by macrophages (Fig. 1C-D) and the coexpression of CSF-1R and CD169 by macrophages (Fig. 1E-F). From the data analysis, we found that in the PF of endometriosis patients, the coexpression of DC-SIGN and CD169 at macrophages was greater than that in the control group, and the coexpression of CSF-1R and CD169 by macrophages was greater than that in the control group (Fig. 1G).
We also conducted immunohistochemical staining and performed a series of analyses of the immune cells detected in all the tissues (Fig. 2A). In ovarian endometriotic lesions, we observed significantly more CD68+ macrophages and DC-SIGN+ macrophages than in the normal endometrium and in the eutopic endometrium of endometriosis patients. Additionally, in ovarian endometriotic lesions, we observed significantly higher numbers of FOXP3+ T cells than in the normal endometrium or in the eutopic endometrium of the endometriosis patients. In contrast, concerning CD169+ macrophages and CSF-1R+ macrophages, there were no significant differences between the ovarian endometriotic lesions, the normal endometrium and the eutopic endometrium of the endometriosis patients (Fig. 2B).
CSF-1 levels are elevated in peritoneal fluid and ectopic endometrium from women with endometriosis
We observed a relative increase in CSF-1 gene expression in ectopic endometrial tissue compared with the paired eutopic endometrial tissue and normal endometrial tissue (Fig. 3A). Our data demonstrated that peritoneal fluid from women with endometriosis contained a significantly higher percentage of CSF-1 than that from control subjects (Fig. 3B). In the EMS model, we found that cytokine production and CSF-1 levels were elevated in the ectopic lesions and peritoneum of mice with endometriosis, although there was no difference between the peritoneal fluid, peritoneal cells, and endometrium of normal mice and mice with endometriosis (Fig. 3C-D). Although there were high levels of CSF-1 in the peritoneum of normal mice and mice with endometriosis, the level of CSF-1 in the peritoneum of mice with endometriosis was higher than that in normal mice; however, there was no statistically significant difference (Fig. 3D).
CSF-1 induced macrophages to acquire a DC-SIGN+ phenotype, which could be abolished by the addition of anti-CSF-1R
The successful induction of macrophages from THP-1 cells was monitored by evaluating the characteristic CD68-positive cells (Fig. 4). A significant increase in CD169+ macrophages was observed in the CSF-1-treated group, while in this model, immunofluorescence staining showed that, after the CSF-1 antagonist anti-CSF-1R was added, the expression of CD169 was low (Fig. 4A). Similarly, CSF-1-treated macrophages demonstrated significant upregulation of DC-SIGN, but after the anti-CSF-1R antibody was added, the expression of DC-SIGN was decreased (Fig. 4B).
CSF-1 induced the generation of DC-SIGN+ macrophages, leading to a suppressive phenotype of peripheral blood lymphocytes, while blockade with anti-CSF-1R abrogated this biological effect
On the basis of the successful induction of macrophage differentiation from THP-1 cells, we established a coculture system with macrophages and peripheral blood lymphocytes (Fig. 5A). Lymphocytes express higher levels of the CD45 antigen, which is exclusively expressed on all nucleated cells of the hematopoietic system, and the different proportions of the monocyte/macrophage populations in the PBMC coculture system can be further confirmed in morphological cytograms showing the FSC (forward scatter) and SSC (side scatter) parameters obtained by flow cytometry (Fig. 5B). The number of CD8-positive T cells among the PBMCs in the CO2 group (treated with only CSF-1) was significantly lower than that in the NC group (not cocultured) and CO3 group (treated with both CSF-1 and the anti-CSF-1R antibody), while the number of Treg cells among the PBMCs in the CO2 group (treated with only CSF-1) was significantly higher than that in the NC group (not cocultured) and CO3 group (treated with both CSF-1 and the anti-CSF-1R antibody) (Fig. 5B). Interestingly, there were no differences in the numbers of CD8-positive T cells and Treg cells among the PBMCs in the CO4 group (treated with both CSF-1 and the anti-DC-SIGN antibody), CO2 group (treated with only CSF-1), NC group (not cocultured) and CO3 group (treated with both CSF-1 and the anti-CSF-1R antibody) (Fig. 5B). Similarly, there were no differences in the numbers of CD8-positive T cells and Treg cells among the PBMCs in the CO1 group (cocultured only), CO2 group (treated with only CSF-1), NC group (not cocultured) and CO3 group (treated with both CSF-1 and the anti-CSF-1R antibody) (Fig. 5B). Through data analysis, we clearly found that the DC-SIGN+ macrophages induced by CSF-1 led to a depressed phenotype of peripheral blood lymphocytes, while the CSF-1 antagonist anti-CSF-1R abrogated this biological effect (Fig. 5C).
CSF-1 is a cytokine that induces monocytes to differentiate into CD169+ macrophages . Our study was consistent with this observation, and we found that the CSF-1 antagonist anti-CSF-1R abolished this effect. Additionally, we found that CSF-1 induced monocytes to differentiate into DC-SIGN+ macrophages; similarly, anti-CSF-1R abolished this effect. Moreover, we found that DC-SIGN+ macrophages led to a suppressive phenotype of peripheral blood lymphocytes, including a high percentage of Treg cells and a low percentage of CD8+ T cells, which was agreement with previous study ; and this biological effect can be abrogated by anti-CSF-1R.
DC-SIGN is expressed in human DCs and macrophages [28, 37]. Importantly, DC-SIGN is involved in multiple aspects of the immunological response ; Yvette van Kooyk’s laboratory proposed that DC-SIGN can actively contribute to the maintenance of an immunosuppressive tissue environment ; as previously described, CD169+ macrophages, which are known as CD169+ suppressive macrophages , play a role in various diseases; but the role of DC-SIGN+ CD169+ macrophages in the pathogenesis of endometriosis has not been studied. We found that the proportion of CD169+ DC-SIGN+ macrophages was higher in the PF of endometriosis patients; this phenomenon was not in agreement with observations in tissues. Although DC-SIGN+ macrophages were more abundant in the ectopic endometrium group than in the eutopic endometrium and the normal endometrium groups, the number of CD169+ macrophages was not different among the three groups. These differences may be due to the diversity of phenotypic differentiation of macrophages in different tissues and regions.
We also found that macrophages coexpressing CSF-1R and CD169 were more abundant in the PF of endometriosis patients than in that of controls. A previous study proved that CSF-1R inhibition altered macrophage polarization and blocked glioma progression . CSF-1R and its ligand, CSF-1, are expressed diffusely and have been frequently reported in patients with EMS [15, 16]. However, in the tissue of ectopic lesions, CSF-1R expression did not differ from that in the normal endometrium and the eutopic endometrium of endometriosis patients. This result is not consistent with a previous study in which CSF-1R was found in nearly 70% of endometriosis patients and was found at a statistically significantly lower percentage in normal endometrium , hence this difference needs to be defined in more studies.
Although the protein expression level of CSF-1R in the ectopic lesions of endometriosis patients was not different from that in the eutopic endometrium of endometriosis patients and the normal endometrium, the gene expression level of CSF-1 was significantly higher in these lesions. The level of the CSF-1 cytokine in the PF of endometriosis patients was higher than that in the PF of controls. Our in vivo experiment showed that the peritoneum of all mice contained high levels of the cytokine CSF-1, while the level of the cytokine CSF-1 was significantly higher in the ectopic endometrial tissue of mice with endometriosis than in the eutopic endometrial tissue of mice with endometriosis and the normal endometrium of control mice. The principal source of CSF-1 may be ectopic lesions in mice with endometriosis. This result was in agreement with a previous study that proved that compared with eutopic tissue, ectopic endometrial tissue exhibited a 3.5-fold increase in CSF-1 expression . Therefore, CSF-1 may be an important cytokine that induces monocytes to differentiate into CD169+ DC-SIGN+ suppressive macrophages.
Overall, CSF-1 and its receptor, CSF-1R, are important for the induction of CD169+ DC-SIGN+ macrophages. We also demonstrate here that CSF-1-induced DC-SIGN+ macrophages inhibit the increase in CD8+ T cells and the decrease in Treg cells. We are studying the detailed mechanism by which DC-SIGN+ macrophages affect the proliferation and differentiation of T cells in EMS. This study provides a framework for developing CSF-1-based in vitro protocols to generate therapeutic macrophages for clinical use to regulate the immune environment of endometriosis.
Availability of data and materials
The datasets used and analyzed during the present study are available from the corresponding author on reasonable request.
Devogelaer JP, Nagant DDC, Donnez J. Endometriosis. Lancet. 1993;341(8840):312–3.
Stilley JA, Birt JA, Sharpe-Timms KL. Cellular and molecular basis for endometriosis-associated infertility. CELL TISSUE RES. 2012;349(3):849–62.
Burns KA, Thomas SY, Hamilton KJ, Young SL, Cook DN, Korach KS. Early Endometriosis in Females Is Directed by Immune-Mediated Estrogen Receptor alpha and IL-6 Cross-Talk. Endocrinology. 2018;159(1):103–18.
Na YJ, Lee DH, Kim SC, Joo JK, Wang JW, Jin JO, Kwak JY, Lee KS. Effects of peritoneal fluid from endometriosis patients on the release of monocyte-specific chemokines by leukocytes. ARCH GYNECOL OBSTET. 2011;283(6):1333–41.
Scheerer C, Bauer P, Chiantera V, Sehouli J, Kaufmann A, Mechsner S. Characterization of endometriosis-associated immune cell infiltrates (EMaICI). ARCH GYNECOL OBSTET. 2016;294(3):657–64.
Zhang C, Maeda N, Izumiya C, Yamamoto Y, Kusume T, Oguri H, Yamashita C, Nishimori Y, Hayashi K, Luo J, et al. Killer immunoglobulin-like receptor and human leukocyte antigen expression as immunodiagnostic parameters for pelvic endometriosis. AM J REPROD IMMUNOL. 2006;55(2):106–14.
Chang KK, Liu LB, Jin LP, Zhang B, Mei J, Li H, Wei CY, Zhou WJ, Zhu XY, Shao J, et al. IL-27 triggers IL-10 production in Th17 cells via a c-Maf/RORgammat/Blimp-1 signal to promote the progression of endometriosis. CELL DEATH DIS. 2017;8(3):e2666.
Li MQ, Wang Y, Chang KK, Meng YH, Liu LB, Mei J, Wang Y, Wang XQ, Jin LP, Li DJ. CD4+Foxp3+ regulatory T cell differentiation mediated by endometrial stromal cell-derived TECK promotes the growth and invasion of endometriotic lesions. CELL DEATH DIS. 2014;5:e1436.
Wei C, Mei J, Tang L, Liu Y, Li D, Li M, Zhu X. 1-Methyl-tryptophan attenuates regulatory T cells differentiation due to the inhibition of estrogen-IDO1-MRC2 axis in endometriosis. CELL DEATH DIS. 2016;7(12):e2489.
Smith KA, Pearson CB, Hachey AM, Xia DL, Wachtman LM. Alternative activation of macrophages in rhesus macaques (Macaca mulatta) with endometriosis. Comp Med. 2012;62(4):303–10.
Perdiguero EG, Geissmann F. The development and maintenance of resident macrophages. NAT IMMUNOL. 2016;17(1):2–8.
An M, Li D, Yuan M, Li Q, Zhang L, Wang G. Interaction of macrophages and endometrial cells induces epithelial-mesenchymal transition-like processes in adenomyosis. BIOL REPROD. 2017;96(1):46–57.
Yuan M, Li D, An M, Li Q, Zhang L, Wang G. Rediscovering peritoneal macrophages in a murine endometriosis model. HUM REPROD. 2017;32(1):94–102.
Fontana MF, de Melo GL, Anidi C, Hamburger R, Kim CY, Lee SY, Pham J, Kim CC. Macrophage Colony Stimulating Factor Derived from CD4+ T Cells Contributes to Control of a Blood-Borne Infection. PLOS PATHOG. 2016;12(12):e1006046.
Budrys NM, Nair HB, Liu YG, Kirma NB, Binkley PA, Kumar S, Schenken RS, Tekmal RR. Increased expression of macrophage colony-stimulating factor and its receptor in patients with endometriosis. FERTIL STERIL. 2012;97(5):1129–35.
Chan R, Lee CL, Ng E, Yeung W. Co-culture with macrophages enhances the clonogenic and invasion activity of endometriotic stromal cells. Cell Prolif. 2017;50(3):e12330.
Fukaya T, Sugawara J, Yoshida H, Yajima A. The role of macrophage colony stimulating factor in the peritoneal fluid in infertile patients with endometriosis. TOHOKU J EXP MED. 1994;172(3):221–6.
Bajwa A, Huang L, Kurmaeva E, Gigliotti JC, Ye H, Miller J, Rosin DL, Lobo PI, Okusa MD. Sphingosine 1-Phosphate Receptor 3-Deficient Dendritic Cells Modulate Splenic Responses to Ischemia-Reperfusion Injury. J AM SOC NEPHROL. 2016;27(4):1076–90.
Teijaro JR. Too much of a good thing: Sustained type 1 interferon signaling limits humoral responses to secondary viral infection. EUR J IMMUNOL. 2016;46(2):300–2.
Conde P, Rodriguez M, van der Touw W, Jimenez A, Burns M, Miller J, Brahmachary M, Chen HM, Boros P, Rausell-Palamos F, et al. DC-SIGN(+) Macrophages Control the Induction of Transplantation Tolerance. Immunity. 2015;42(6):1143–58.
He L, Zhou S, Qi Q, Chi Y, Zhu J, Xu Z, Wang X, Hoellwarth J, Liu F, Chen X, et al. The regulation of regulation: interleukin-10 increases CD4(+) CD25(+) regulatory T cells but impairs their immunosuppressive activity in murine models with schistosomiasis japonica or asthma. Immunology. 2018;153(1):84–96.
Shevach EM. Mechanisms of foxp3+ T regulatory cell-mediated suppression. Immunity. 2009;30(5):636–45.
Wang XQ, Zhou WJ, Luo XZ, Tao Y, Li DJ. Synergistic effect of regulatory T cells and proinflammatory cytokines in angiogenesis in the endometriotic milieu. HUM REPROD. 2017;32(6):1304–17.
Szyllo K, Tchorzewski H, Banasik M, Glowacka E, Lewkowicz P, Kamer-Bartosinska A. The involvement of T lymphocytes in the pathogenesis of endometriotic tissues overgrowth in women with endometriosis. Mediators Inflamm. 2003;12(3):131–8.
Habbeddine M, Verthuy C, Rastoin O, Chasson L, Bebien M, Bajenoff M, Adriouch S, den Haan J, Penninger JM, Lawrence T. Receptor Activator of NF-kappaB Orchestrates Activation of Antiviral Memory CD8 T Cells in the Spleen Marginal Zone. CELL REP. 2017;21(9):2515–27.
Xu X, Bian L, Shen M, Li X, Zhu J, Chen S, Xiao L, Zhang Q, Chen H, Xu K, et al. Multipeptide-coupled nanoparticles induce tolerance in “humanised” HLA-transgenic mice and inhibit diabetogenic CD8(+) T cell responses in type 1 diabetes. Diabetologia. 2017;60(12):2418–31.
Geijtenbeek TB, Kwon DS, Torensma R, van Vliet SJ, van Duijnhoven GC, Middel J, Cornelissen IL, Nottet HS, KewalRamani VN, Littman DR, et al. DC-SIGN, a dendritic cell-specific HIV-1-binding protein that enhances trans-infection of T cells. Cell. 2000;100(5):587–97.
Geijtenbeek TB, Torensma R, van Vliet SJ, van Duijnhoven GC, Adema GJ, van Kooyk Y, Figdor CG. Identification of DC-SIGN, a novel dendritic cell-specific ICAM-3 receptor that supports primary immune responses. Cell. 2000;100(5):575–85.
Soilleux EJ, Morris LS, Lee B, Pohlmann S, Trowsdale J, Doms RW, Coleman N. Placental expression of DC-SIGN may mediate intrauterine vertical transmission of HIV. J PATHOL. 2001;195(5):586–92.
Larsson M, Wilkens DT, Fonteneau JF, Beadle TJ, Merritt MJ, Kost RG, Haslett PA, Cu-Uvin S, Bhardwaj N, Nixon DF, et al. Amplification of low-frequency antiviral CD8 T cell responses using autologous dendritic cells. AIDS. 2002;16(2):171–80.
Rappocciolo G, Jenkins FJ, Hensler HR, Piazza P, Jais M, Borowski L, Watkins SC, Rinaldo CJ. DC-SIGN is a receptor for human herpesvirus 8 on dendritic cells and macrophages. J IMMUNOL. 2006;176(3):1741–9.
Kommagani R, Szwarc MM, Kovanci E, Gibbons WE, Putluri N, Maity S, Creighton CJ, Sreekumar A, DeMayo FJ, Lydon JP, et al. Acceleration of the glycolytic flux by steroid receptor coactivator-2 is essential for endometrial decidualization. PLOS GENET. 2013;9(10):e1003900.
Dehai C, Bo P, Qiang T, Lihua S, Fang L, Shi J, Jingyan C, Yan Y, Guangbin W, Zhenjun Y. Enhanced invasion of lung adenocarcinoma cells after co-culture with THP-1-derived macrophages via the induction of EMT by IL-6. IMMUNOL LETT. 2014;160(1):1–10.
Akoum A, Lawson C, Herrmann-Lavoie C, Maheux R. Imbalance in the expression of the activating type I and the inhibitory type II interleukin 1 receptors in endometriosis. HUM REPROD. 2007;22(5):1464–73.
Egawa H, Fujiwara H, Hirano T, Nakayama T, Higuchi T, Tatsumi K, Mori T, Fujii S. Peripheral blood mononuclear cells in early pregnancy promote invasion of human choriocarcinoma cell line. BeWo cells HUM REPROD. 2002;17(2):473–80.
Rogler G, Hausmann M, Vogl D, Aschenbrenner E, Andus T, Falk W, Andreesen R, Scholmerich J, Gross V. Isolation and phenotypic characterization of colonic macrophages. CLIN EXP IMMUNOL. 1998;112(2):205–15.
Soilleux EJ, Morris LS, Leslie G, Chehimi J, Luo Q, Levroney E, Trowsdale J, Montaner LJ, Doms RW, Weissman D, et al. Constitutive and induced expression of DC-SIGN on dendritic cell and macrophage subpopulations in situ and in vitro. J Leukoc Biol. 2002;71(3):445–57.
van Kooyk Y, Geijtenbeek TB. DC-SIGN: escape mechanism for pathogens. NAT REV IMMUNOL. 2003;3(9):697–709.
van Gisbergen KP, Aarnoudse CA, Meijer GA, Geijtenbeek TB, van Kooyk Y. Dendritic cells recognize tumor-specific glycosylation of carcinoembryonic antigen on colorectal cancer cells through dendritic cell-specific intercellular adhesion molecule-3-grabbing nonintegrin. CANCER RES. 2005;65(13):5935–44.
Pyonteck SM, Akkari L, Schuhmacher AJ, Bowman RL, Sevenich L, Quail DF, Olson OC, Quick ML, Huse JT, Teijeiro V, et al. CSF-1R inhibition alters macrophage polarization and blocks glioma progression. NAT MED. 2013;19(10):1264–72.
Mettler L, Schmutzler AG, Koch K, Schollmeyer T, Salmassi A. Identification of the M-CSF receptor in endometriosis by immunohistochemistry and RT-PCR. AM J REPROD IMMUNOL. 2004;52(5):298–305.
We want to thank Cryomedicine Lab, Qilu Hospital of Shandong University give the cells, THP-1, as the present to us. We thank all of the patients for agreeing to participate in our study.
The project was funded by a grant 81801417 from the National Natural Science Foundation of China.
Ethics approval and consent to participate
The regional ethics committee of Shanghai First Maternity and Infant Hospital approved the study (KS1953). Written informed consent was obtained from all the enrolled participants. The animal ethics committee of School of medicine, Tongji University allow this study (TJLAC-019–125).
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Written informed consent for publication was obtained from all participants.
All the authors report no conflict of interest.
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Xiaocui, L., Wei, H., Yunlang, C. et al. CSF-1-induced DC-SIGN+ macrophages are present in the ovarian endometriosis. Reprod Biol Endocrinol 20, 48 (2022). https://doi.org/10.1186/s12958-022-00901-w
- DC-SIGN+ macrophages
- Treg cells