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Angiostrongylus cantonensis Galectin-1 interacts with Annexin A2 to impair the viability of macrophages via activating JNK pathway



Angiostrongylus cantonensis can cause severe symptoms of central nervous system infections. In the host, this parasite localizes in the blood and cerebrospinal fluid, and its secreted components can impact immune responses. Our previous study demonstrated that immune responses were inhibited in A. cantonensis-infected mice immunized with Ac-Galectin-1 (AcGal-1). However, the mechanisms by which AcGal-1 regulates the immune responses remain unclear. Macrophages are innate immune cells that rapidly respond to infection. The direct impact of AcGal-1 on macrophages may affect the immune responses.


AcGal-1 protein was purified by nickel ion affinity chromatography. The effect of AcGal-1 on the apoptosis of macrophages was detected using CCK-8 assay, flow cytometry and western blot. Macrophage membrane proteins bound to AcGal-1 were obtained using the His-tag-based pull-down assay and identified via mass spectrometry. Co-localization of AcGal-1 and the macrophage membrane protein Annexin A2 was observed by immunofluorescence microscopy, and their interaction was validated by co-immunoprecipitation experiments. SiRNA-mediated knockdown of Annexin A2 was used to determine if AcGal-1-induced macrophage apoptosis required interaction with Annexin A2. The phosphorylation level of apoptotic signal pathway protein was detected by phospho-antibody microarray and western blot.


Our study showed that AcGal-1 caused apoptosis of the macrophages. AcGal-1 increased the expression of apoptosis proteins caspase-3, caspase-9, Bax, but reduced the expression of anti-apoptosis protein Bcl-2. AcGal-1 interacted with the membrane protein Annexin A2, and knockdown of Annexin A2 expression increased Bcl-2 but decreased Bax levels in AcGal-1-treated cells. Moreover, AcGal-1 increased JNK phosphorylation and the inhibition of JNK phosphorylation in AcGal-1-treated cells decreased the expression of caspase-3, -9, Bax and almost restored Bcl-2 to the level observed in control cells.


AcGal-1 can induce the apoptosis of macrophages by binding to Annexin A2 and activating JNK downstream the apoptotic signaling pathway.


Angiostrongylus cantonensis is a zoonotic pathogen that causes human eosinophilic meningitis [1]. Humans can be infected by accidental ingestion of undercooked intermediate hosts (e.g. Pomacea canaliculata and Achatina fulica) or third-stage larvae (L3) in drinking water [2]. After penetrating the intestinal wall, A. cantonensis transits via the circulation to the blood-brain barrier, traverses it and then affects the central nervous system [3]. Larvae in the brain tissue of infected individuals can cause brain and spinal cord symptoms such as headache, fever, vomiting, lethargy, stiff neck, and increased cerebrospinal fluid pressure [4, 5]. Once in the body, A. cantonensis can survive in the blood and cerebrospinal fluid for an indefinite period of time by evading the host immune response [6], although the underlying mechanisms remain unclear.

Angiostrongylus cantonensis was previously shown to cause apoptosis and necroptosis in the brains of infected mice; this was associated with elevated cleaved caspase-3, -4, and -6, and receptor-interacting serine/threonine-protein kinase (RIP)3 mRNA levels, RIP3, and phosphorylated (p)RIP3 protein levels relative to the levels observed in control mice. Furthermore, apoptotic and necrotic microglia, astrocytes, and neurons were observed in the parenchymal and hippocampal regions of infected mice [2].

In our previous study, using differential proteomics analysis of A. cantonensis at different stages of development, we showed that the expression level of A. cantonensis galectin (AcGal)-1 was higher in fifth-stage larvae (L5) than in third-stage larvae (L3) [7]. Galectins (Gals) constitute a family of lectins conserved across many species and are characterized by an affinity for β-galactoside and the presence of a conserved sequence motif known as the carbohydrate recognition domain (CRD) [8]. Gals are secreted by cells via an unconventional mechanism [9] and play a critical role in apoptosis, cell proliferation, inflammation, immune response, and cell adhesion and migration [10,11,12,13,14,15,16,17,18]. Parasite Gals have a sequence and structure similar to those of mammalian homologs and are presumed to participate in host-parasite interactions. Gals enable immune evasion by inhibiting the proliferation and activation of immune cells or by causing their death [19]. For example, the binding of Gal to transmembrane protein 147 receptor of peripheral blood mononuclear cells (PBMCs) increases the transcription of Toll-like receptor (TLR)-1, TLR-3 and TLR-4, and the downstream effectors myeloid differentiation primary response 88 (MyD88) and Fas-associated with death domain protein (FADD); the simultaneous activation of both the TLR and caspase pathways induces PBMC apoptosis [19]. The interaction of Gal with PBMCs also promotes the expression of voltage-dependent anion-selective channel protein 2 and induces mitochondrial apoptosis [20]. These findings suggest that AcGal-1 can induce apoptosis.

Our previous study demonstrated that immune responses were inhibited in A. cantonensis-infected mice immunized with Gal-1[21]. We speculated that A. cantonensis evades the host immune response by secreting AcGal-1 to induce the apoptosis of immune cells including macrophages, which are the first line of defense against infection [22]. To test this hypothesis, we evaluated the proliferation and apoptosis of macrophages derived from a human acute monocytic leukemia line (THP-1) cells treated with AcGal-1. Our results provide a basis for investigating host immune regulation by A. cantonensis.


Expression and purification of AcGal-1 fusion protein

Following the protein purification method of Li et al. [23], we used the pCold-III-Gal-1 vector (the empty pCold-III vector or the recombinant construct of AcGal-1) constructed by these authors, which was transformed into Escherichia coli BL21 cells. When constructing the plasmid, we added a His-tag to the primer sequence. His-tagged Gal-1 protein expression was induced with 0.1 mM isopropyl-β-d-thiogalactoside and 100 µg/ml ampicillin at 15 °C for 22 h in Luria-Bertani medium. Recombinant protein was purified by Ni-NTA His-Bind-Resin (Merck, Darmstadt, Germany) and verified by sodium dodecyl sulfate-polyacrylamide gel electrophoresis (PAGE). The BCA assay (Beyotime Institute of Biotechnology, Shanghai, China) was used to measure the protein concentration, following standard protocol.

Cell culture

THP-1 monocytes were cultured in Roswell Park Memorial Institute-1640 medium supplemented with 10% fetal bovine serum and 1 mM sodium pyruvate. Cells were maintained at a density of 5–8 × 107 cells/ml and sub-cultured every 3–4 days to ensure that they remained in the logarithmic growth phase. Cells were seeded into 6-well plates (9.5 cm2) at 106–107 cells/well. To induce differentiation, the cells were treated with 50 nM phorbol 12-myristate 13-acetate (PMA) for 48 h, and the medium was replaced with PMA-free culture medium. Cells were cultured in a fully humidified atmosphere at 37 °C and 5% CO2. To verify the differentiation of THP-1 cells into macrophages by PMA, the cells were stained with a fluorescent CD11b antibody [24, 25] (Cat# MAB1124-100; R&D Systems, Minneapolis, MN, USA) and analyzed by immunofluorescence microscopy.

Cell proliferation assay

Cell proliferation was evaluated with a Cell Counting Kit (CCK)-8 (Beyotime Institute of Biotechnology) according to the manufacturer’s instructions. Briefly, cells were seeded in 96-well plates at 37 °C and 5% CO2. CCK-8 reagent was added to the wells and the absorbance was measured at 450 nm on a microplate reader.

Annexin V/propidium iodide (PI) double-staining and flow cytometry

Apoptotic cells were quantified with an Annexin V/fluorescein isothiocyanate (FITC) Apoptosis Detection Kit (Solarbio, Beijing, China) and analyzed by flow cytometry. Macrophages differentiated from THP-1 cells were seeded in 6-well plates at a density of 106–107 cells/well and treated with different concentrations of AcGal-1 (0.5 µg/ml, 1 µg/ml, 1.5 µg/ml, or 2 µg/ml) for 12 h at 37 °C and 5% CO2. The cells were washed with phosphate-buffered saline (PBS) and resuspended in 500 µl binding buffer. Annexin V/FITC (5 µl) and PI (5 µl) were added, and the mixture was incubated for 10 min at 37 °C in the dark. After incubation the cells were immediately analyzed by flow cytometry (BD FACSCanto II; BD Biosciences, Franklin Lakes, NJ, USA), with bovine serum albumin (BSA) and dexamethasone used as negative and positive controls, respectively.

Determination of caspase-3 activity

Adherent cells were enzymatically dissociated with trypsin and resuspended in fresh cell culture medium. The cells were collected by centrifugation at 600×g and 4 °C, washed, and lysed on ice for 15 min at a ratio of 100 µl lytic solution to 2 × 106 cells. After adding 2 mM N-acetyl-Asp-Glu-Val-Asp-p-nitroanilide (Ac-DEVD-pNA) (Beyotime Institute of Biotechnology, Shanghai, China), cells were incubated at 37 °C for 1–2 h. The absorbance was measured at 405 nm and subtracted from that of the blank control; this corresponded to the absorbance of pNA produced by caspase-3 catalysis in the sample. The amount of pNA produced in the sample was calculated from a standard curve.

Plasma membrane protein extraction

Plasma membrane protein concentrations were quantified with a Plasma Membrane Protein Extraction Kit (BioVision, San Francisco, CA, USA). Cells (0.2–10 × 108) were collected in PBS and then centrifuged at 700×g for 5 min at 4 °C. The pellet was washed with 3 ml ice-cold PBS and resuspended in 2 ml of homogenization buffer mix (provided in the Plasma Membrane Protein Extraction Kit), and the cells were homogenized 30–50 times on ice with a Dounce homogenizer. The homogenate was centrifuged at 700 ×g for 10 min at 4 °C, and the supernatant was transferred to a new tube and centrifuged at 10,000×g for 30 min at 4 °C. The pellet contained total cell membrane proteins (including those of the plasma membrane and organelle membranes).

Pull-down assay

The pull-down assay was performed with the MagpoinsTM His-Tag Immunoprecipitation Kit (Sino Biological, Beijing, China). Cells were lysed in Nonidet (N)P40 buffer, the lysate and His-AcGal-1 were mixed in pull-down buffer along with the bead/protein complex (reagents provided in the MagpoinsTM His-Tag Immunoprecipitation Kit). The mixture was incubated on a rotary mixer for 10 min at room temperature and the tube was then placed on a magnetic separator for 1 min. The supernatant was discarded, and the beads were washed four times with 300 µl binding/wash buffer before adding 100 µl His-elution buffer. The suspension was incubated on a roller for 5 min at room temperature. The metal beads on the tube wall were collected using a magnetic separator and the supernatant, which contained the eluted His-tag protein and its interaction partners, was transferred to a clean tube. Protein products were analyzed by liquid chromatography-mass spectrometry (LC-MS) and western blotting.


Each protein fraction (30 μg) was mixed with 200 µl of 8 M urea in 150 mM Tris-HCl (pH 8.5) (UA buffer) in the 30 kDa molecular weight cut-off filter unit (Millipore, MA, USA); any remaining SDS was exchanged by urea in a second washing step with 200 µl of UA buffer. The samples were then diluted with 100 µl IAA (50 mM IAA in UA) and incubated at room temperature for 30 min. These samples were mixed with 100 µl of 25 mM NH4HCO3 and centrifuged; this step was repeated twice. Each sample was diluted with 40 µl NH4HCO3 (25 mM) and digested with trypsin at 37 °C for 18 h. After digestion, the peptides were recovered by centrifugation in a new collection tube. The acidified tryptic peptides were sampled on a SC001 traps reverse phase C18 trap column and separated on a SC200 reverse phase C18 nanocolumn (Easy-nLC1000 system; Thermo/Finnigan, San Francisco, CA, USA) via a gradient. The mobile phases A and B were 0.1% formic acid in 2% acetonitrile and 0.1% formic acid in 84% acetonitrile, respectively. The LC system was coupled to an orbitrap Q Exactive mass spectrometer (Thermo/Finnigan). The MS scan range of the precursor ion was from 300 to 1800 m/z. The resolution was set to 70,000 for MS scans and 17,500 for the data-dependent MS/MS scans.

Bioinformatics analysis

For protein identification, we used the Mascot 2.2 program (MatrixScience, RRID: SCR_000307, URL: to search fragmentation spectra against a human database. For full MS or MS/MS spectra searches, an error of six parts per million (ppm) or 20 ppm was set, respectively, and two missed cleavages were allowed. The peptide mass tolerance was set to 0.5 Da and the fragment mass tolerance was set to 10 ppm. Protein identification was considered valid if at least one peptide was identified with a significance of P < 0.05; the proteins that did not satisfy these criteria were rejected. The threshold for accepting MS/MS spectra was a false discovery rate (FDR) of 0.05. A network model of protein interactions according to known protein-protein interactions was made using Retrieval of Interacting Genes (STRING, RRID:SCR_005223, URL:

Co-immunoprecipitation (co-IP)

Affinity-purified antibody was bound to AminoLink Plus Coupling Resin (Pierce, Rockford, IL, USA) in a spin column. After preparing the resin column, ice-cold IP lysis/wash buffer was added to the cells. The bait (Annexin A2), prey (AcGal-1), and controls were prepared and added to the resin along with the cell lysate. The mixture was incubated with gentle rocking at 4 °C for 18 h or overnight. The spin columns were centrifuged, and the sample was washed two more times with 200 µl IP lysis/wash buffer, with a centrifugation step after each wash. A 50 µl volume of elution buffer was added to the column in the tube, followed by incubation for 5 min at room temperature. The tube was centrifuged and the flow-through was collected and analyzed by western blotting.

Immunofluorescence microscopy

Macrophages were seeded on coverslips in a 6-well plate and treated with His-AcGal-1. Lactose (100 mM) served as a negative control. A total of 106 cells were fixed with 4% paraformaldehyde for 15 min at 37 °C. To reduce non-specific interactions, the cells were blocked with 10% BSA for 3 h. The cells were then incubated for 3 h at 37 °C with rabbit anti-human Annexin A2 antibody (Cat# 8235, RRID:AB_11129437; Cell Signaling Technology, Boston, USA) (1:100), followed by fluorescein (FITC)-conjugated anti-rabbit antibody (Cat# 711-095-152, RRID:AB_2315776); Jackson ImmunoResearch Labs, Lancaster, CA, USA (1:200)) and Rhodamine (TRITC)-conjugated mouse anti-His (to detect His-tagged Gal-1) antibody (Cat# 715-025-151, RRID:AB_2340767; Jackson ImmunoResearch Labs, Lancaster, CA, USA) (1:200). The cells were washed, and a drop of cell suspension was placed on a glass microscope slide along with ProLong anti-fade mounting medium (Thermo Fisher Scientific, Waltham, MA, USA). Images of FITC and TRITC fluorescence were acquired on a microscope. To confirm antibody specificity, primary antibodies were omitted in control samples.

RNA interference

All of the small interfering RNAs (siRNA) used in this study were designed and synthesized by Shanghai GenePharma (Shanghai, China). THP-1 cells, grown to 80% confluence in 6-well plates in 2 ml medium, were treated with PMA 48 h prior to liposome-mediated transfection. Macrophages were transfected with 30 µl siRNA (the final concentration was 300 nM) specific for human ANXA2 gene (Annexin A2-siRNA, sense 5’-GCA AGU CCC UGU ACU AUU ATT-3’). The negative control siRNA was a scrambled siRNA for ANXA2 (siNC, sense 5’-UUC UCC GAA CGU GUC ACG UTT-3’). All siRNAs were transfected into cells using GP-Transfect-Mate/Lipofectamine transfection reagent (Invitrogen, Carlsbad, CA, USA). ANXA2 expression in the transfected cells was tested by quantitative real-time RT-PCR assays, as well as western blotting.


Total RNA from macrophages was extracted using Trizol reagent (Invitrogen). We next used an Agilent Mx3000P qPCR System (Agilent, Santa Clara, CA, USA) in conjunction with One Step SYBR® PrimeScript™ RT-PCR Kit II (Takara Bio, Beijing, China) to analyze viral gene expression. The housekeeping gene β-actin was chosen as an internal control, and the data was analyzed by the real-time quantitative PCR software. The sequences of primers used for ANXA2 and β-actin are listed in Table 1. The amplification conditions of real-time quantitative PCR were as follows: 95 °C denaturation for 3 min, followed by 40 cycles of 95 °C annealing for 12 s, 62 °C extension for 40 s.

Table 1 Sequences of primers used for real-time PCR

Human phospho-mitogen-activated protein kinase (pMAPK) array

The Human Phospho-MAPK Array Kit (Cat# ARY002B; R&D System, Minneapolis, MN, USA) was used according to the manufacturer’s instructions to identify proteins phosphorylated upon AcGal-1 treatment. Briefly, 2 ml of Array Buffer 5 was pipetted into each well of a 4-well plate, which was then incubated for 1 h on a rocking platform shaker. Samples were prepared by adding up to 400 µl of sample to separate tubes. The final volume was adjusted to 1.5 ml with Array Buffer 1. A 20 µl volume of reconstituted detection antibody cocktail was added to each sample, followed by mixing and incubation at room temperature for 1 h. Array Buffer 5 was removed by aspiration and the prepared sample/antibody mixture was incubated overnight at 2 °C on a rocking platform shaker. After washing the membrane with 1× wash buffer for 10 min on the shaker, 2 ml of diluted streptavidin-horseradish peroxidase was pipetted into each well followed by incubation for 30 min at room temperature. Finally, 1 ml of Chemi Reagent Mix was pipetted onto the membrane, which was exposed to X-ray film for 1–10 min.

Western blot analysis

Cells were treated with 50 μg/ml recombinant AcGal-1 for 30 min and activation of intracellular signaling pathways was evaluated by western blotting; samples treated with 100 µg/ml BSA or left untreated served as negative controls. Cells were lysed in radioimmunoprecipitation assay (RIPA) buffer and centrifuged, 10,000×g for 5 min, and proteins in the supernatant were quantified with the bicinchoninic acid assay (BCA) (Beyotime Institute of Biotechnology, Shanghai, China).

Total protein was lysed by RIPA and quantitated by BCA assay. Proteins were separated on a 10% Bis-Tris PAGE gel in Tris-HCl buffer and transferred to a PVDF membrane that was incubated with antibodies against B cell lymphoma (Bcl-2) (Cat. # 4223, RRID:AB_1903909; Cell Signaling Technology, Boston, MA, USA), Bcl-2-associated X protein (Bax) (Cat# 5023, RRID:AB_10557411; Cell Signaling Technology, Boston, MA, USA), cleaved-caspase-3 (Cat# 9661, RRID:AB_2341188; Cell Signaling Technology, Boston, MA, USA), cleaved-caspase-9 (Cat# 9501, RRID:AB_331424; Cell Signaling Technology, Boston, MA, USA), and glyceraldehyde 3-phosphate dehydrogenase (GAPDH; loading control) (Cat# AT0002; CMC-TAG, San Diego, CA, USA) for 2 h at room temperature. The membrane was developed by enhanced chemiluminescence (ECL) using ECL Plus reagent (Bio-Rad, Hercules, CA, USA).

Cell were treated with SP600125 (Cat#S1460; Selleck Chemicals, Houston, TX, USA) to block JNK phosphorylation and MAPK signaling was analyzed by western blotting. Extracellular signal-regulated kinase (ERK)1/2 (pERK1/2) (Cat# 4370, RRID:AB_2315112; Cell Signaling Technology, Boston, MA, USA) phospho-c-Jun N-terminal kinase (pJNK) (Cat# 4668, RRID:AB_823588; Cell Signaling Technology, Boston, MA, USA), Bcl-2, Bax, and cleaved-caspase-3 and -9 as well as GAPDH were detected by western blotting as described above. The grayscale value of signal intensity for each protein was determined using ImageJ software (National Institutes of Health, Bethesda, MD, USA), and the ratio of target protein to GAPDH was calculated.

Statistical analysis

Data are presented as the mean ± standard deviation. Statistical analyses were performed using Prism v.5.0 (GraphPad, La Jolla, CA, USA) and SPSS v.20.0 (SPSS Inc., Chicago, IL, USA) software. Differences between groups were evaluated by a one-way analysis of variance (ANOVA) followed by the LSD, and P < 0.05 was considered statistically significant (Additional file 1: Table S1).


AcGal-1 inhibits macrophage viability

We expressed the His-AcGal-1 fusion protein in E. coli, then purified and quantitated this protein [23]. To investigate the effects of AcGal-1 on macrophage viability, we used the THP-1 monocyte cell line and induced its differentiation in vitro. A microscopic examination of THP-1 cells in suspension revealed that these cells were round, translucent, uniform in size, and occasionally formed clusters. PMA induction altered cell morphology, with an increase in volume and protrusion of pseudopodia, and these cells were able to adhere to the walls of the culture dishes (Fig. 1a). The myeloid differentiation marker, CD11b, was highly expressed in THP-1 upon treatment with PMA [24, 25], suggesting that PMA induced the differentiation of THP-1 cells into macrophage-like cells.

Fig. 1

AcGal-1 decreases the viability of THP-1-derived macrophages. a PMA treatment of THP-1 cells (left) induced the differentiation into macrophage-like cells (middle). Immunofluorescence staining of CD11b (as a marker for monocyte-derived macrophages) expression on macrophage-like cells (right). b The effects of AcGal-1 concentration and treatment time on macrophage viability were evaluated with the CCK-8 assay. Data represent the mean ± standard deviation (SD; vertical bars) of triplicate experiments. Scale-bars: 50 µm

Using the CCK-8 assay, we observed that AcGal-1 decreased the viability of differentiated THP-1 cells. Treatment with 100 μg/ml AcGal-1 for 6 h decreased survival to approximately 70% of that in the control group (Fig. 1b). About 50% of the cells survived (IC50 = 49.8) after treatment with 49.8 µg/ml AcGal-1. We therefore used an AcGal-1 concentration of 50 µg/ml in subsequent experiments. The results of the CCK-8 assay also showed that the cell viability was stable at 12 and 18 h, and the latter was therefore selected as the treatment duration.

AcGal-1 induces macrophage apoptosis/necrosis

The reduced viability of macrophage upon treatment with AcGal-1 led us to ask if AcGal-1 might induce macrophage apoptosis. Flow cytometry analysis revealed that the percentages of both early stage apoptotic cells (Annexin V+/PI-) and late apoptotic cells (Annexin V+/PI+) in the AcGal-1-treated group were higher than in cells treated with BSA (Fig. 2a, b). The other cells were living cells (Annexin V-/PI-) or necrotic cells (Annexin V-/PI+) and the latter was also slightly increased to some degree in cells treated with AcGal-1. Western blot analysis revealed that the expression of several apoptosis- or anti-apoptosis-related markers was altered by AcGal-1 treatment (Fig. 2c, d). Compared to levels in the control and BSA groups, the relative expression levels of cleaved-caspase-3 and -9 and Bax were upregulated (2.28 ± 0.13%, 2.15 ± 0.28%, and 2.26 ± 0.21%, respectively), whereas the expression of the anti-apoptotic factor Bcl-2 was downregulated. We further evaluated the enzymatic activity of caspase-3 in macrophages treated with AcGal-1 (or BSA as a control) using Ac-DEVD-pNA. We found that AcGal-1 increased the activity of caspase-3 (28.85 ± 1.72%) relative to untreated cells (11.44% ± 1.06%) and those treated with BSA (12.74 ± 0.98%) (Fig. 2e). Taken together, these results indicated that AcGal-1 induced the apoptosis of macrophages.

Fig. 2

AcGal-1 induces macrophage apoptosis. a Flow cytometry analysis showing that apoptosis (revealed by the levels of Annexin V and PI) in AcGal-1-treated macrophages was higher than that in BSA-treated cells (control). b Quantitation of the percentage of Annexin V+ cells. c Expression levels of proteins associated with apoptosis/anti-apoptosis as determined by western blot in different cell groups (control, BSA and AcGal-1). AcGal-1 induced macrophage apoptosis by increasing the levels of cleaved caspase-3, -9, Bax, and decreasing the expression level of Bcl-2. d Quantitation of expression intensity of each protein. e AcGal-1 increased the enzymatic activity of caspase-3 in macrophages, treated as in b. Data represent the mean ± standard deviation (SD; vertical bars) of triplicate experiments. *P < 0.05, **P < 0.01, ***P < 0.001

AcGal-1 interacts with Annexin A2 expressed on the macrophage plasma membrane

As an exogenous glycoprotein, AcGal-1 is likely to bind to the receptors on the cell membrane. To investigate the molecular basis for the impact of AcGal-1 on macrophages apoptosis, lysates from macrophages from the THP-1 cell line were incubated with His-tag fused to AcGal-1 antibody-conjugated beads and bound proteins were eluted. We carried out co-IP under stringent conditions to pull down only the proteins that strongly interacted with AcGal-1. Several proteins were found in the AcGal-1 precipitate of macrophages (Fig. 3a). The precipitated proteins were then analyzed by LC-MS (Table 2); 26 cell membrane proteins contained more than two unique peptide counts. Among these, three peptides of human Gal-1 were identified as being A. cantonensis Gal-1 by BLAST alignment (Table 3). Bioinformatics analysis of these cell membrane proteins with STRING predicted that AcGal-1 may interact with Annexin A2 (Additional file 2: Figure S1). In addition, previous studies have reported that membrane Annexin A2 contains galactoside oligosaccharide residues [26, 27]. Thus, we hypothesized that AcGal-1 with a carbohydrate recognition domain could bind to Annexin A2.

Fig. 3

Annexin A2 on the macrophage cell surface interacts with AcGal-1. a The different types of proteins were analyzed by sodium dodecyl sulfate-polyacrylamide gel electrophoresis and visualized by Coomassie brilliant blue staining. The “pull-down protein” (red box) that may interact with AcGal-1 was obtained using His-Tag-based immunoprecipitation assay. b Immunofluorescence detection of cell surface Annexin A2 and colocalization with AcGal-1, which was abolished by treatment with the glycosylation inhibitor lactose. Macrophages were immunolabeled for Annexin A2 (revealed by FITC, green) and stained for AcGal-1 with (TRITC, red), and then examined using confocal microscopy. c, d Interaction of Annexin A2 and AcGal-1 were verified by IP, followed by western blot detection of Annexin A2 and AcGal-1. c Resin with affinity-purified His-antibody was incubated with AcGal-1-treated or untreated macrophage cell lysates. The Annexin A2 that interacted with His-AcGal-1 was pulled down along with His-mediated immunoprecipitation (IP) and revealed by immunoblot (IB) with the Annexin A2 antibody. AcGal-1 was blotted using the anti-His antibody. d Reverse co-IP confirmed the interaction between AcGal-1 and Annexin A2. AcGal-1-treated macrophage cell lysates were incubated with or without the resin bound by affinity-purified Annexin A2-antibody. AcGal-1 that interacted with Annexin A2 was pulled down along with Annexin A2-mediated IP and revealed by IB with the anti-His antibody. Annexin A2 was blotted using the Annexin A2 antibody. Scale-bars: b, 10 µm

Table 2 Mass spectrometry-based identification of membrane proteins obtained by IP
Table 3 The peptide data, BLAST of AcGal-1 and Annexin A2

Using immunofluorescence microscopy, we observed co-localization of His-Ac-Gal-1 and Annexin A2 at the plasma membrane (Fig. 3b). Binding of AcGal-1 to the macrophage surface was revealed by a TRITC-labelled antibody, and binding of Annexin A2 to the membrane was demonstrated using a FITC-labelled antibody. The significant co-localization of red fluorochrome and FITC (merge-yellow) illustrated specific interaction of AcGal-1 to Annexin A2 at the macrophage membrane, which was abolished by treatment with lactose. A further co-immunoprecipitation assay was performed to validate the specific binding of AcGal-1 to Annexin A2 (Fig. 3c, d). Macrophage lysates (membrane proteins) were incubated with AcGal-1 that was connected to the His-AcGal-1-antibody-conjugated nickel beads and bound proteins were pulled down using the anti-His antibody. Annexin A2 was observed in these immunoprecipitates (Fig. 3c). Reverse IP was performed by incubating AcGal-1 with macrophage lysates that were first incubated with the Annexin A2 antibody-conjugated resin and bound proteins were pulled down using the anti-Annexin A2 antibody. His-AcGal-1 was detected in these immunoprecipitates (Fig. 3d). These results confirmed the interaction between AcGal-1 and Annexin A2.

Reduced Annexin A2 expression in macrophages affects AcGa-1-induced apoptosis

Next, we investigated whether AcGal-1-induced apoptosis was mediated via interaction with Annexin A2 on the macrophage membrane by knocking down Annexin A2 using siRNAs. The qRT-PCR and western blot analysis showed that upon transfection, Annexin A2-siRNA efficiently reduced the level of Annexin A2 compared to control siRNA (siNC) at both RNA and protein levels (Fig. 4a, b). Further western blot analysis showed that AcGal-1 treatment increased the expression of apoptotic proteins caspase-3, -9, and Bax, and reduced the level of Bcl-2, consistent with our above findings (Fig. 4b, c). Compared to control cells, Annexin A2-siRNA-transfected cells did not show significant changes in the expression of caspase-3 and -9, but had significantly reduced Bax and increased Bcl-2 expression after AcGal-1 treatment (Fig. 4b, c), suggesting that reduced Annexin A2 expression in macrophages may prevent macrophages from apoptosis. These results indicated that AcGal-1-induced macrophages apoptosis was at least in part mediated by Annexin A2.

Fig. 4

Reduced Annexin A2 expression in macrophages affects AcGa-1-induced apoptosis. a Relative expression of ANXA2 by qRT-PCR in macrophage cells treated with or without indicated siRNAs. b The expression of apoptosis-associated proteins Bax, caspase-3, caspase-9 and the expression of anti-apoptotic protein Bcl-2 in indicated groups of cells treated with or without AcGal-1. c Quantitation of expression intensity of each protein in b. Data represent the mean ± standard deviation (SD; vertical bars) of triplicate experiments. *P < 0.05, **P < 0.01, ***P < 0.001

JNK signaling mediates AcGal-1-induced macrophage apoptosis

The Annexin A2-chickpea lectin interaction at the membrane lattice is essential for ligand-induced MAPK pathway-mediated induction of cancer cell apoptosis [28]. To determine whether the interaction between Annexin A2 and AcGal-1 affects MAPK signaling in macrophages, we used a human pMAPK array to screen for phosphorylated proteins in this pathway (Fig. 5a, Table 4). AcGal-1 suppressed the phosphorylation of ERK1/2 while increasing pJNK expression. Western blot analysis using specific phosphorylated antibodies confirmed that compared to control, AcGal-1 reduced the level of pERK1/2 (0.76 ± 0.17 vs 1.55 ± 0.41) but increased the expression of pJNK (2.64 ± 0.75 vs 0.76 ± 0.53) (Fig. 5b, c).

Fig. 5

Phosphorylation of MAPK signaling pathway proteins following AcGal-1 treatment. a Results of MAPK phospho-antibody microarray. The proteins outlined in a red box showed a significant increase in phosphorylation levels, including JNK and HSP27, and a decrease in pERK1/2, following AcGal-1 treatment. b The levels of pJNK and pERK1/2 were confirmed by western blotting. SP600125 was used to inhibit JNK phosphorylation, and cells treated with EGF were used as a positive control to reflect the EGFR/MAPK pathway activation. c Quantitation of expression intensity of each protein in b. d Western blot analysis of apoptosis/anti-apoptosis -related proteins in AcGal-1-treated or non-treated macrophages in the presence or absence of the JNK inhibitor SP600125 on macrophage apoptosis. e Quantitation of expression intensity of each protein in d. Data represent the mean ± standard deviation (SD; vertical bars) of triplicate experiments. *P < 0.05, **P < 0.01, ***P < 0.001

Table 4 Statistical results of MAPK phospho-antibody microarray

To identify the downstream effectors, macrophages were treated with AcGal-1 and the expression of apoptosis-related proteins was evaluated. Consistently, Bcl-2 was downregulated whereas cleaved-caspase-9 and -3 and Bax were upregulated in the presence of AcGal-1 (Fig. 5d, e). Suppressing JNK phosphorylation with the inhibitor SP600125 decreased the expression of the latter three proteins and restored Bcl-2 to a level similar to that in control cells. These results suggested that JNK phosphorylation might play a critical role in AcGal-1-induced apoptosis of macrophages.


Previous studies have reported the apoptosis and necroptosis of parenchymal and hippocampal astrocytes, neurons, and microglia in mice infected with A. cantonensis [2]. However, we do not know the factors playing a role in apoptosis. In our previous proteomic analysis, we discovered expression of galectin-1 protein from A. cantonensis (AcGal-1) by two-dimensional electrophoresis (2-DE) combined with immunoblotting assay [29]. AcGal-1 was cloned into a prokaryotic expression vector, expressed, and purified. Western blot analysis showed that the recombinant protein was recognized by sera from mice infected with A. cantonensis and the agglutination reaction test indicated that AcGal-1 had good biological activity [23, 30]. The results of the present study provide evidence that AcGal-1 is identified as a new factor for macrophage apoptosis, which may provide explanations for neuro-angiostrongyliasis. Apoptosis is induced via activation of caspases including caspase-3, caspase-9, and other apoptosis-associated proteins, while the anti-apoptotic protein Bcl-2 expression inhibits apoptosis [31, 32]. To the best of our knowledge, this is the first report demonstrating that AcGal-1 can induce apoptosis in macrophages derived from THP-1 cells, which are a widely used human monocytic leukemia cell line for monocyte/macrophage differentiation and function [33] owing to various advantages over primary monocytes such as a homogenous genetic background that ensures reproducibility [34].

Nematode galectins have a specific affinity for β-galactosides through an evolutionarily conserved sequence motif [35]. Proteins can be modified into multiple glycoforms with variable binding avidity for Gals; N-glycans are the major Gal ligand at the cell surface [36, 37]. The binding avidity for individual glycoproteins increases with the number of N-glycans per protein [38].

We identified Annexin A2 as a putative binding partner of AcGal-1 by LC-MS and demonstrated that this interaction mediates macrophage apoptosis. Moreover, the interaction of these two proteins was confirmed by immunofluorescence analysis and the impact on macrophage apoptosis by this interaction was evaluated using the siRNA-mediated knockdown of Annexin A2. An earlier study reported that the membrane protein Annexin A2 has a galactosyl side chain [39] with at least one asparagine (N)-linked biantennary mannosyl residue [40]. We propose that the CRD AcGal-1 binds to the N-glycan of Annexin A2, leading to glycosylation and phosphorylation of Annexin A2; the binding of AcGal-1 to Annexin A2 on the cytomembrane of macrophages observed in this study may trigger an intracellular signaling cascade that activates cell apoptosis. Interestingly, we observed that the level of Annexin A2 expression markedly influences AcGal-1-induced apoptosis. In particular, silencing ANXA2 with siRNA led to a significant decrease in the expression of apoptosis proteins, especially Bax, but increased Bcl-2 expression. This suggests that a decrease in the level of Annexin A2 affected the molecular apoptotic pathway induced by AcGal-1. Although there were no apparent changes in the levels of caspases in this particular experiment, our finding suggests that Annexin A2 is at least partially required for the AcGal-1-induced apoptosis of macrophages.

Annexins are phospholipid-binding proteins conserved in animals and plants that play an important role in membrane/cytoskeleton linkage for exo-/endocytosis [41]; they also participate in the formation of membrane domains via their phospholipid-binding function [42]. Annexin A2 functions as a scaffold that organizes signaling proteins to regulate cellular processes such as proliferation, differentiation and apoptosis. Annexin A2 has previously been identified as an EGFR-interacting molecule and the interaction between EGFR and Annexin A2 at the membrane surface is critical for downstream EGFR/MAPK signaling in cells [43]. Annexin A2 is also a substrate of Src; the membrane-bound Annexin A2/EGFR/Src signaling complex activates downstream signaling pathways [44,45,46,47]. Additionally, Annexin A2 interacts with Gal-3 at membrane lattices, which is important for EGFR/MAPK signaling in the survival, growth and progression of triple-negative breast cancer [48].

Activated EGFR/MAPK signaling regulates cell proliferation, infiltration, metastasis and angiogenesis and promotes apoptosis [49, 50]. In this study, we found that AcGal-1-induced activation of JNK, a member of the MAPK superfamily that also comprises p38 and ERK [51], could be increased. AcGal-1 activated JNK and induced apoptosis signaling via activation of caspase-3 and -9, as determined by western blotting. The pro-apoptotic effect of AcGal-1 in macrophages was diminished by blocking JNK phosphorylation using SP600125, as evidenced by the restoration of cleaved-caspase-9 and -3, Bax, and Bcl-2 levels, supporting that AcGal-1 induces macrophage apoptosis via JNK signaling.

In conclusion, we found that AcGal-1 induces macrophage apoptosis via interaction with Annexin A2 expressed on the macrophage cell surface and activation of JNK signaling. These findings provide a basis for investigating the pathogenesis and mechanisms of host immune evasion by A. cantonensis, which can lead to the development of effective anti-parasite strategies or treatments in cases of infection by this parasite.


This study investigated the effect of A. cantonensis galectin 1 (AcGal-1) on the viability of macrophages and the signaling pathways involved, as well as the interaction between AcGal-1 and Annexin A2 expressed on the cell membrane of macrophages. We found that AcGal-1 interacted with Annexin A2 and induced apoptosis in macrophages, which resulted in reduced viability. AcGal-1 increased the phosphorylation of c-Jun N-terminal kinase (JNK), whereas treatment with the JNK phosphorylation inhibitor SP600125 diminished the apoptosis-inducing effects of AcGal-1. We believe that our study may reveal the mechanisms for A. cantonensis-mediated immune evasion and may suggest strategies to prevent or treat cases of A. cantonensis infection.

Availability of data and materials

Data supporting the conclusions of this article are included within the article and its additional files. The datasets used in the present study are available from the corresponding author upon reasonable request.





A. cantonensis Galectin-1


B cell lymphoma 2-associated X protein


B cell lymphoma 2


bovine serum albumin




cell counting kit 8




carbohydrate recognition domain


enhanced chemiluminescence


epidermal growth factor receptor


extracellular signal-regulated kinase


fluorescein isothiocyanate






glyceraldehyde 3-phosphate dehydrogenase


c-Jun N-terminal kinase


third-stage larvae


microtubule-associated protein 1A/1B-light chain 3-II


liquid chromatography-mass spectrometry


mitogen-activated protein kinase


mechanistic target of rapamycin


Nonidet P40


peripheral blood mononuclear cell


propidium iodide


phorbol 12-myristate 13-acetate


receptor-interacting serine/threonine-protein kinase


human acute monocytic leukemia line


Toll-like receptor


  1. 1.

    Lv S, Zhang Y, Steinmann P, Utzinger J, Zhou XN. The genetic variation of Angiostrongylus cantonensis in the People’s Republic of China. Infect Dis Poverty. 2017;6:125–36.

    PubMed  PubMed Central  Article  Google Scholar 

  2. 2.

    Mengying Z, Yiyue X, Tong P, Yue H, Limpanont Y, Ping H, et al. Apoptosis and necroptosis of mouse hippocampal and parenchymal astrocytes, microglia and neurons caused by Angiostrongylus cantonensis infection. Parasit Vectors. 2017;10:611.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  3. 3.

    Chen KY, Chiu CH, Wang LC. Anti-apoptotic effects of Sonic hedgehog signalling through oxidative stress reduction in astrocytes co-cultured with excretory-secretory products of larval Angiostrongylus cantonensis. Sci Rep. 2017;7:41574.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  4. 4.

    Yii CY. Clinical observations on eosinophilic meningitis and meningoencephalitis caused by Angiostrongylus cantonensis on Taiwan. Am J Trop Med Hyg. 1976;25:233–49.

    CAS  PubMed  Article  Google Scholar 

  5. 5.

    Martins YC, Tanowitz HB, Kazacos KR. Central nervous system manifestations of Angiostrongylus cantonensis infection. Acta Trop. 2015;141:46–53.

    PubMed  Article  Google Scholar 

  6. 6.

    Stijlemans B, De Baetselier P, Magez S, Van Ginderachter JA, De Trez C. African trypanosomiasis-associated anemia: the contribution of the interplay between parasites and the mononuclear phagocyte system. Front Immunol. 2018;9:218–33.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  7. 7.

    Song Z, Huang H, Tan F, Zhang E, Hu J, Pan C. Differential proteomics analysis of female and male adults of Angiostrongylus cantonensis. Exp Parasitol. 2012;131:169–74.

    CAS  PubMed  Article  Google Scholar 

  8. 8.

    Vasta GR. Galectins as pattern recognition receptors: structure, function, and evolution. Adv Exp Med Biol. 2012;946:21–36.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  9. 9.

    Seelenmeyer C, Stegmayer C, Nickel W. Unconventional secretion of fibroblast growth factor 2 and galectin-1 does not require shedding of plasma membrane-derived vesicles. FEBS Lett. 2008;582:1362–8.

    CAS  PubMed  Article  Google Scholar 

  10. 10.

    Ahmed H, AlSadek DMM. Galectin-3 as a potential target to prevent cancer metastasis. Clin Med Insights Oncol. 2015;9:113–21.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  11. 11.

    Gendronneau G, Sidhu SS, Delacour D, Dang T, Calonne C, Houzelstein D, et al. Galectin-7 in the control of epidermal homeostasis after injury. Mol Biol Cell. 2008;19:5541–9.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  12. 12.

    Rabinovich GA, van Kooyk Y, Cobb BA. Glycobiology of immune responses. Ann N Y Acad Sci. 2012;1253:1–15.

    CAS  PubMed  Article  Google Scholar 

  13. 13.

    De Oliveira FL, Gatto M, Bassi N, Luisetto R, Ghirardello A, Punzi L, et al. Galectin-3 in autoimmunity and autoimmune diseases. Exp Biol Med. 2015;240:1019–28.

    Article  CAS  Google Scholar 

  14. 14.

    Boscher C, Zheng YZ, Lakshminarayan R, Johannes L, Dennis JW, Foster LJ, et al. Galectin-3 protein regulates mobility of N-cadherin and GM1 ganglioside at cell-cell junctions of mammary carcinoma cells. J Biol Chem. 2012;287:32940–52.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  15. 15.

    Colin Hughes R. Galectins as modulators of cell adhesion. Biochimie. 2001;83:667–76.

    Article  Google Scholar 

  16. 16.

    Yabuta C, Yano F, Fujii A, Shearer TR, Azuma M. Galectin-3 enhances epithelial cell adhesion and wound healing in rat cornea. Ophthalmic Res. 2014;51:96–103.

    CAS  PubMed  Article  Google Scholar 

  17. 17.

    Fortin S, Le Mercier M, Camby I, Spiegl-Kreinecker S, Berger W, Lefranc F, et al. Galectin-1 is implicated in the protein kinase C ε/vimentin-controlled trafficking of integrin-β1 in glioblastoma cells. Brain Pathol. 2010;20:39–49.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  18. 18.

    Liu W, Hsu DK, Chen H-Y, Yang RY, Carraway KL, Isseroff RR, et al. Galectin-3 regulates intracellular trafficking of epidermal growth factor receptor through Alix and promotes keratinocyte migration. J Invest Dermatol. 2012;132:2828–37.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  19. 19.

    Wang W, Yuan C, Wang S, Song X, Xu L, Yan R, et al. Transcriptional and proteomic analysis reveal recombinant galectins of Haemonchus contortus down-regulated functions of goat PBMC and modulation of several signaling cascades in vitro. J Proteomics. 2014;98:123–37.

    CAS  PubMed  Article  Google Scholar 

  20. 20.

    Li Y, Yuan C, Wang L, et al. Transmembrane protein 147(TMEM147): another partner protein of Haemonchus contortus galectin on the goat peripheral blood mononuclear cells (PBMC). Parasit Vectors. 2016;9:355.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  21. 21.

    Yan LZ, Shi XM, Zu YW, Shen YY, Chen XX, Zhao MJ, et al. The opposite roles of PAS-5 and Galectin-1 in immune response during the early infection of Angiostrongylus cantonensis. Parasit Vectors. 2018;11:318.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  22. 22.

    Dunn JD, Bosmani C, Barisch C, Raykov L, Lefrançois LH, Cardenal-Muñoz E, et al. Eat prey, live: Dictyostelium discoideum as a model for cell-autonomous defenses. Front Immunol. 2017;8:1906–36.

    PubMed  Article  CAS  Google Scholar 

  23. 23.

    Li XP, Zhao MJ, Shi XM, Yan LZ, Yan BL, Huang HC. Cloning of galectin-1 gene of Angiostrongylus cantonensis and testing the agglutination property of the galectin-1 protein. Chin J Parasitol Parasitic Dis. 2017;35:48–52.

    Google Scholar 

  24. 24.

    Chen PY, Yen JH, Kao RH, Chen JH. Down-regulation of the oncogene PTTG1 via the KLF6 tumor suppressor during induction of myeloid differentiation. PLoS One. 2013;8:e71282.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  25. 25.

    Dumrese C, Slomianka L, Ziegler U, Choi SS, Kalia A, Fulurija A, et al. The secreted Helicobacter cysteine-rich protein A causes adherence of human monocytes and differentiation into a macrophage-like phenotype. FEBS Lett. 2009;583:1637–43.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  26. 26.

    Nangia-Makker P, Balan V, Raz A. Regulation of tumor progression by extracellular Galectin-3. Cancer Microenviron. 2008;1:43–51.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  27. 27.

    Gong HC, Honjo Y, Nangia-Makker P, Hogan V, Mazurak N, Bresalier RS. The NH2 terminus of galectin-3 governs cellular compartmentalization and function in cancer cells. Cancer Res. 1999;59:6239–45.

    CAS  PubMed  Google Scholar 

  28. 28.

    Shetty P, Bargale A, Patil BR, Mohan R, Dinesh US, Vishwanatha JK, et al. Cell surface interaction of annexin A2 and galectin-3 modulates epidermal growth factor receptor signaling in Her-2 negative breast cancer cells. Mol Cell Biochem. 2016;411:221–33.

    CAS  PubMed  Article  Google Scholar 

  29. 29.

    Huang HC, Yao LL, Song ZM, Li XP, Hua QQ, Li Q, et al. Developmentspecific differences in the proteomics of Angiostrongylus cantonensis. PLoS One. 2013;8:e76982.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  30. 30.

    Huang HC, Yao LL, Zhou ZB, Zheng LN, Pan CW. Analysis and identification of peptide epitope of the fifth stage larvae of Angiostrongylus cantonensis. Natl Med J China. 2014;94:1095–8.

    Google Scholar 

  31. 31.

    Peña-Blanco A, García-Sáez AJ. Bax, bak and beyond-mitochondrial performance in apoptosis. FEBS J. 2018;285:416–31.

    PubMed  Article  CAS  Google Scholar 

  32. 32.

    Fulda S. Apoptosis pathways and neuroblastoma therapy. Curr Pharm Des. 2009;15:430–5.

    CAS  PubMed  Article  Google Scholar 

  33. 33.

    Aldo PB, Craveiro V, Guller S, Mor G. Effect of culture conditions on the phenotype of THP-1 monocyte cell line. Am J Reprod Immunol. 2013;70:80–6.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  34. 34.

    Qin Z. The use of THP-1 cells as a model for mimicking the function and regulation of monocytes and macrophages in the vasculature. Atherosclerosis. 2012;221:2–11.

    CAS  PubMed  Article  Google Scholar 

  35. 35.

    Arata Y, Hirabayashi J, Kasai K. Structure of the 32-kDa galectin gene of the nematode Caenorhabditis elegans. J Biol Chem. 1997;272:26669–77.

    CAS  PubMed  Article  Google Scholar 

  36. 36.

    Patnaik SK, Potvin B, Carlsson S, Sturm D, Leffler H, Stanley P. Complex N-glycans are the major ligands for Galectin-1, -3, and -8 on Chinese hamster ovary cells. Glycobiology. 2006;16:305–17.

    CAS  PubMed  Article  Google Scholar 

  37. 37.

    Karmakar S, Stowell SR, Cummings RD, McEver RP. Galectin-1 signaling in leukocytes requires expression of complex-type N-glycans. Glycobiology. 2008;18:770–8.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  38. 38.

    Lau KS, Partridge EA, Grigorian A, Silvescu CI, Reinhold VN, Demetriou M, et al. Complex N-Glycan number and degree of branching cooperate to regulate cell proliferation and differentiation. Cell. 2007;129:123–34.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  39. 39.

    Patchell BJ, Wojcik KR, Yang TL, White SR, Dorscheid DR. Glycosylation and annexin II cell surface translocation mediate airway epithelial wound repair. Am J Physiol Lung Cell Mol Physiol. 2007;293:354–63.

    Article  CAS  Google Scholar 

  40. 40.

    Chao PZ, Hsieh MS, Cheng CW, Hsu TJ, Lin YT, Lai CH, et al. Dendritic cells respond to nasopharygeal carcinoma cells through Annexin A2-recognizing DC-SIGN. Oncotarget. 2015;6:159–70.

    PubMed  Google Scholar 

  41. 41.

    Lizarbe MA, Barrasa JI, Olmo N, Gavilanes F, Turnay J. Annexin-phospholipid interactions functional implications. Int J Mol Sci. 2013;14:2652–83.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  42. 42.

    Gerke V, Moss SE. Annexins: from structure to function. Physiol Rev. 2002;82:331–71.

    CAS  PubMed  Article  Google Scholar 

  43. 43.

    Shetty PK, Thamake SI, Biswas S, Johansson SL, Vishwanatha JK. Reciprocal regulation of Annexin A2 and EGFR with Her-2 in Her-2 negative and herceptin-resistant breast cancer. PLoS One. 2012;7:e44299.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  44. 44.

    Finn RS. Targeting Src in breast cancer. Ann Oncol. 2008;19:1379–86.

    CAS  PubMed  Article  Google Scholar 

  45. 45.

    Dua R, Zhang J, Nhonthachit P, Penuel E, Petropoulos C, Parry G. EGFR over-expression and activation in high HER2, ER negative breast cancer cell line induces trastuzumab resistance. Breast Cancer Res Treat. 2010;122:685–97.

    CAS  PubMed  Article  Google Scholar 

  46. 46.

    Hayes MJ, Moss SE. Annexin 2 has a dual role as regulator and effector of v-Src in cell transformation. J Biol Chem. 2009;284:10202–10.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  47. 47.

    Zhang S, Huang WC, Li P, Guo H, Poh SB, Brady SW, et al. Combating trastuzumab resistance by targeting SRC, a common node downstream of multiple resistance pathways. Nat Med. 2011;17:461–9.

    PubMed  Article  CAS  Google Scholar 

  48. 48.

    Jorissen RN, Walker F, Pouliot N, Garrett TPJ, Ward CW, Burgess AW. Epidermal growth factor receptor: mechanisms of activation and signalling. Exp Cell Res. 2003;284:31–53.

    CAS  PubMed  Article  Google Scholar 

  49. 49.

    Jutten B, Rouschop KMA. EGFR signaling and autophagy dependence for growth, survival, and therapy resistance. Cell Cycle. 2014;13:42–51.

    CAS  PubMed  Article  Google Scholar 

  50. 50.

    He Y, Hu Y, Jiang X, Chen T, Ma Y, Wu S, et al. Cyanidin-3-O-glucoside inhibits the UVB-induced ROS/COX-2 pathway in HaCaT cells. J Photochem Photobiol B. 2017;177:24–31.

    CAS  PubMed  Article  Google Scholar 

  51. 51.

    Davis RJ. Signal transduction by the JNK group of MAP kinases. Cell. 2000;103:239–52.

    CAS  PubMed  Article  Google Scholar 

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This study was supported by grants from the National Natural Science Foundation of China (No. 81471234), the Science and Technology Project of Zhejiang Province of China (No. 2017C33067), and the Natural Science Foundation of Zhejiang Province of China (No. LQ17H190005).

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HCH and BLY conceived and designed the experiments. XS, JWL and HCH wrote the manuscript. XMS, MRX, ZYX and QS performed the experiments. XMS and YJZ collected and analyzed the data. HCH, BLY and JWL participated in technological guidance and coordination. All authors read and approved the final manuscript.

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Correspondence to Baolong Yan or Huicong Huang.

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Supplementary information

Additional file 1: Table S1.

Statistical comparisons presented in figures.

Additional file 2: Figure S1.

Bioinformatics analysis of these cell membrane proteins with STRING predicted that AcGal-1 may interact with Annexin A2.

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Shi, X., Xiao, M., Xie, Z. et al. Angiostrongylus cantonensis Galectin-1 interacts with Annexin A2 to impair the viability of macrophages via activating JNK pathway. Parasites Vectors 13, 183 (2020).

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  • Angiostrongylus cantonensis
  • Galectin-1
  • Macrophage apoptosis
  • Annexin A2
  • JNK signaling