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Meningitic Escherichia coli α-hemolysin aggravates blood–brain barrier disruption via targeting TGFβ1-triggered hedgehog signaling

Abstract

Bacterial meningitis is a life-threatening infectious disease with severe neurological sequelae and a high mortality rate, in which Escherichia coli is one of the primary Gram-negative etiological bacteria. Meningitic E. coli infection is often accompanied by an elevated blood–brain barrier (BBB) permeability. BBB is the structural and functional barrier composed of brain microvascular endothelial cells (BMECs), astrocytes, and pericytes, and we have previously shown that astrocytes-derived TGFβ1 physiologically maintained the BBB permeability by triggering a non-canonical hedgehog signaling in brain microvascular endothelial cells (BMECs). Here, we subsequently demonstrated that meningitic E. coli infection could subvert this intercellular communication within BBB by attenuating TGFBRII/Gli2-mediated such signaling. By high-throughput screening, we identified E. coli α-hemolysin as the critical determinant responsible for this attenuation through Sp1-dependent TGFBRII reduction and triggering Ca2+ influx and protein kinase A activation, thus leading to Gli2 suppression. Additionally, the exogenous hedgehog agonist SAG exhibited promising protection against the infection-caused BBB dysfunction. Our work revealed a hedgehog-targeted pathogenic mechanism during meningitic E. coli-caused BBB disruption and suggested that activating hedgehog signaling within BBB could be a potential protective strategy for future therapy of bacterial meningitis.

Introduction

Bacterial meningitis is an important life-threatening infection in the central nervous system (CNS), especially in newborn infants, young teenagers, and the elder with low immunity [1,2,3]. Escherichia coli is the most common Gram-negative bacillary organism that causes meningitis [4]. Most cases of E. coli meningitis initiate from the hematogenous spread and develop as circulating pathogenic bacteria penetrate and breakdown the blood–brain barrier (BBB), destroy the brain parenchyma and thus cause CNS disorders [5].

BBB is a specialized structure composed of brain microvascular endothelial cells (BMECs), astrocytes, and pericytes. This barrier separates the brain from the bloodstream and maintains the CNS homeostasis [6,7,8]. Among these component cells, BMECs act as the first and direct barrier unit to determine the BBB function [9, 10]. In decades, multiple effectors have been reported to participate in barrier function regulation. For instance, GDNF activated the GFRα1 and led to higher trans-endothelial electrical resistance (TEER) and lower permeability of BMECs [11]. Also, Ang1/Tie2 and Flk1 were reported to promote the capillary tube-like formation of BMECs [12]. We previously demonstrated that astrocytes-derived transforming growth factor-β1 (TGFβ1) enhanced the endothelial ZO-1 expression and maintained the BBB integrity by triggering a non-canonical hedgehog signaling in BMECs, indicating that the TGFβ1-mediated intercellular communication between astrocytes and BMECs is beneficial for BBB integrity maintaining [13], and exogenous TGFβ1 addition would exhibit a protective effect on BBB. However, whether such TGFβ1-mediated intercellular cross-talking within BBB could be hijacked during meningitic E. coli infection is entirely unknown.

E. coli α-hemolysin (HlyA), a kind of Repeats-in-toxin (RTX) exoprotein, of which synthesis, activation and secretion are regulated by the hlyCABD operon [14]. The HlyB and HlyD act as the transporters which belong to ATP binding cassette (ABC) superfamily and the membrane fusion protein (MFP) family, respectively. The precursor pro-HlyA is acylated by HlyC, a fatty acid acyltransferase, and transferred outside the cells by HlyB and HlyD. The posttranslational acylation of HlyA by HlyC is determinative for the cytotoxic activity [15, 16]. HlyA is largely identified in 40-50 % uropathogenic E. coli (UPEC) strains, such as the CFT073, J96, and UTI89 [17]. It has been demonstrated that the HlyA in UPEC was involved in inflammation activation and cell death in macrophages [18], and the HlyA was shown to induce bladder epithelial cell exfoliation and urinary tract infection [17]. Meanwhile, a variety of hemolysin toxins also played essential roles in other bacterial pathogens. In Staphylococcus aureus, the hemolysin induced the disseminated intravascular coagulation and liver injury [19]. In Listeria monocytogenes, the hemolysin LLO containing PEST-sequence co-opted the host endocytosis machinery, protecting the integrity of the host plasma membrane and enabling the growth of bacteria in host cell cytosol [20]. Unfortunately, except for UPEC, the HlyA function in meningitic E. coli infection was poorly investigated so far.

In this study, we demonstrated the meningitic E. coli interference of TGFβ1-mediated intercellular communication between astrocytes and BMECs. The α-hemolysin HlyA in meningitic E. coli was shown to decrease the TGFβ1 receptor TGFBRII and the key transcription factor Gli2 of hedgehog signaling, which finally led to BBB disruption. Together with our recent conclusion that astrocytes-derived TGFβ1 facilitates BBB function via activating non-canonical hedgehog signaling in BMECs [13], we here revealed a novel strategy for meningitic E. coli induction of BBB dysfunction by disturbing the regular astrocytes-endothelium cross-talking. This finding could largely extend the current knowledge of bacterial-caused CNS dysfunction from perspective of intercellular communication within BBB, and shall be beneficial for future prevention and control of bacterial meningitis.

Methods

Bacterial strain and cell culture

E. coli strain RS218 (O18:K1:H7) was originally obtained from the cerebrospinal fluid of a neonate with meningitis and gifted from Prof. Kwang Sik Kim in Johns Hopkins University School of Medicine. E. coli strain was grown aerobically at 37 °C in Luria-Bertani medium overnight.

The hBMECs were kindly gifted from Prof. Kwang Sik Kim in Johns Hopkins University School of Medicine, and routinely cultured in RPMI 1640 supplemented with 10 % fetal bovine serum (FBS), 2 mM L-glutamine, 1 mM sodium pyruvate, essential amino acids, nonessential amino acids, vitamins, and penicillin and streptomycin (100 U/mL). The HEK-293 T cells (ATCC® CRL-3216™) were cultured in Dulbecco’s Modified Eagle’s Medium (DMEM) with 10 % FBS and penicillin and streptomycin (100 U/mL). All cells were cultured in a 37 °C incubator under 5 % CO2 until reaching monolayer confluence. In some experiments, confluent hBMECs were starved in serum-free medium (1:1 mixture of Ham’s F-12 and 199 medium) for 12–16 h before further treatment.

Reagents and antibodies

The hedgehog pathway agonist SAG and protein kinase A (PKA)inhibitor H89 were purchased from MedchemExpress (Princeton, NJ, USA). The immunofluorescence (IF) staining kits containing Cy3-labeled goat anti-rabbit IgG and FITC-labeled goat anti-rabbit IgG, 4’,6-diamidino-2-phenylindole (DAPI) reagent, EGTA, and Fluo-3-AM probe were obtained from Beyotime (Shanghai, China). Anti-Gli1, anti-Gli2, and anti-ZO-1 antibodies were from Proteintech (Chicago, IL, USA). The anti-Sp1 antibody, HRP-conjugated anti-rabbit IgG antibody, HRP-conjugated anti-mouse IgG antibody, and SimpleChIP® Plus Enzymatic Chromatin IP Kit (Magnetic Beads) were purchased from Cell Signaling Technology (Danvers, MA, USA). Anti-ZO-1 antibody for IF was from Abcam (Cambridge, MA, USA). Anti-β-actin antibody was obtained from HuaAn Biotechnology Co., Ltd. (Hangzhou, China). The lipofectamine 3000 transfection reagent was obtained from Invitrogen (Carlsbad, CA, USA). Mouse recombinant TGFβ1 was obtained from R&D system (Minneapolis, MN, USA). Evan’s blue dye was purchased from Santa Cruz Biotechnology (Santa Cruz, CA, USA).

Mice infection assays

The 21-day-old specific-pathogen-free (SPF) female Kunming mice were obtained from the experimental animal center at China Three Gorges University (Hubei Province, China). For the infection, mice were challenged with E. coli strain RS218 via tail vein at 3 × 106 CFUs. The brains from moribund and control mice were subjected to IF or Western blot assays. In some assays, the recombinant TGFβ1 protein or SAG was injected through the tail vein 12 h before or synchronously with the E. coli challenge as indicated.

Western blot

Mice brains or hBMECs cultures were homogenized or lysed in RIPA buffer containing protease inhibitor cocktail and centrifuged at 15,000 g for 30 min at 4 °C to remove the insoluble cell debris. Protein concentrations of brain lysates or cell lysates were measured with a BCA protein assay kit (NCM Biotech, China), and equivalent protein samples were subjected to Western blot assay as previously described [21].

RT-PCR and qPCR

Total RNA was extracted by the TRIzol reagent (Thermo Fisher Scientific, Waltham, MA, USA), and the RNA purity and concentration were assessed by NanoDrop 2000 Ultramicro spectrophotometer (Thermo Fisher Scientific). RT-PCR was performed to generate cDNA using HiScript II Q RT SuperMix for qPCR (+ gDNA wiper) (Vazyme, Nanjing, China). The qPCR was performed with qTOWER3/G quantitative real-time PCR thermal cycler (Analytikjena, Jena, Germany) using MonAmp SYBR Green qPCR Mix (Monad Biotech Co., Ltd, Wuhan, China) following the manufacturer’s instructions. The primers used for qPCR were listed in Additional file 1: Table S2. Expression of the target genes was normalized against GAPDH. Each assay was performed in triplicate.

Immunofluorescence (IF)

For IF, paraffin sections of the challenged mice brains were deparaffinized and rehydrated in xylene and ethanol. IF experiments were performed according to the instructions provided by the relevant kits. Briefly, sections were washed with PBS three times and then fixed with 4 % paraformaldehyde for 30 min. The fixed cells or sections were then treated with 1 % Triton X-100 in PBS prior to non-specific site blocking and antibody incubation. Here, TGFBRII, Gli2, and ZO-1 were labeled with Cy3, and CD31 was labeled with FITC. The sections were observed with the ECHO REVOLVE microscope (Echo Laboratories, San Diego, USA).

Electric cell-substrate impedance sensing

Electric cell-substrate impedance sensing (ECIS) Zθ system (Applied BioPhysics, NY, USA) was employed to monitor the barrier function of hBMECs with specific treatments as previously reported [22]. Briefly, cells were seeded on the collagen-coated and gold-plated electrodes in 96-well chamber slides (96W1E+) at 7 × 104 cells per well and cultured until reaching confluence. The TEER was continuously monitored to reflect the formation of the barrier. After stable maximal resistance was reached, the specific reagents or treatments were added into the wells at indicated concentration, and the TEER changes were automatically monitored by the ECIS system. All data recorded in the ECIS system were analyzed and normalized as the Rb values (Norm. Parameter Values), representing the barrier function alteration along with time. Each treatment was performed with 5 parallel duplications.

CRISPR/Cas9 genomic editing

For CRISPR/Cas9 deletion in prokaryotic cells, the α-hemolysin operon genes hlyC, hlyA, hlyB, and hlyD in RS218 were knocked out via CRISPR/Cas9 following the previous description [23]. In brief, the left homologous arm (HA-L) and right homologous arm (HA-R) of the hly genes were cloned respectively from RS218 genomic DNA and combined as the donor DNA (HA) through fusion PCR amplification. The corresponding sgRNA was synthesized and inserted into plasmid pTargetF (Addgene: #62,226) via inverse-PCR. RS218 strain containing pCas plasmid (Addgene: #62,225) was then transformed with donor DNA and the pTargetF plasmid containing sgRNA sequence. The transformant was grown and screened by kanamycin (200 µg/mL) and spectinomycin (100 µg/mL), and the possible mutations were PCR identified with sequencing. Except for the deletion, the CDS region of hlyCA was cloned in pMD19-T Vector and transformed in the corresponding deletion mutant to complement the hlyA knock-out. The primers used for these genes editing were listed in Additional file 1: Table S6.

Transfection

HEK-293 T or hBMECs cells grown to 70 % confluence were subjected to transfection experiments with Lipofectamine 3000 reagent according to the manufacturer’s instructions (Invitrogen, MA, USA). Briefly, 5 µg of plasmids, 10 µL of P3000, 7.5 µL of Lipo3000, and 500 µL of Opti-MEM were mixed gently and incubated at room temperature for 15 min. The mixture was then added dropwise to the cells in the 6-well plates and incubated at 37 ℃ with 5 % CO2 for 24 h. For Sp1 overexpression in hBMECs, fresh medium with G418 (1 mg/ml) was applied for another 21 days to screen and maintain the positively transfected cells.

Dual-luciferase reporter assay

Prior to luciferase reporter assay, the coding sequence (CDS) of human Sp1 were amplified and cloned into pcDNA3.1(+) vector to generate the overexpression plasmid pcDNA3.1-Sp1. The promotor region of tgfbr2 was amplified and cloned into the firefly luciferase reporter vector pGL3-basic to generate the wild-type reporter plasmids pGL3-tgfbr2-promo-WT. Meanwhile, a serial of truncated promoter, as well as site-directed mutation of promotor, were similarly constructed into pGL3-basic (Fig. 3). The potential binding sites were identified with the JASPAR database online (http://jaspar.genereg.net/). All primers used in the dual-luciferase assays were listed in Additional file 1: Table S3.

For dual-luciferase reporter assay, the pcDNA3.1 overexpression plasmid, the corresponding pGL3 reporter plasmid, and pRL-TK plasmid were co-transfected into HEK-293 T cells in 24-wells plates. Both firefly luciferase activity and renilla luciferase activity were tested after 36 h of transfection by Dual-Luciferase Reporter assay system (Promega, WI, USA) with Spark 10 M multimode microplate reader (Tecan, Männedorf, Switzerland). Relative luciferase activity was calculated by the ratio of reporter activity (firefly fluorescence) to that of control activity (renilla fluorescence), and the results were shown as the representative of three independent assays.

Chromatin immunoprecipitation

Chromatin immunoprecipitation (ChIP) was performed to test the interaction between transcription factors and its potential target genes using SimpleChIP® Plus Enzymatic Chromatin IP Kit (CST) following the manufacturer’s instructions. Briefly, cells in the dishes were fixed in formaldehyde to cross-link proteins with DNAs. Cells were next digested by micrococcal nuclease and subjected to the immunoprecipitation procedure. The products were treated with protease K and then subjected to DNA isolation. Purified DNA was used in the following qPCR amplification. The primers used for ChIP-qPCR were listed in Additional file 1: Table S4.

Bacterial infection of hBMECs

Escherichia coli strain RS218 infection of hBMECs was performed following our previously described methods [24]. Briefly, the confluent hBMECs were starved in serum-free medium for 12–16 h. Overnight E. coli cultures were resuspended and diluted in the same serum-free medium and added to the cells at a multiplicity of infection of 100 for the indicated time points. Cells were then washed three times with pre-chilled PBS and collected for RNA isolation using TRIzol reagent or protein extraction with RIPA lysis buffer.

Construction and screening of RS218 Tn5-transposon mutant library

The Tn5-transposon mutant library of RS218 strain was constructed with pUTmini-Tn5 Cm Kit following the protocol (Biomedal, Spain). The pUTmini-Tn5 Cm plasmid was transformed into RS218 through conjugation transfer with the donor strain E. coli X7213. The transformants were screened on plates containing chloramphenicol at 50 µg/mL to select the positive insertions, as we previously reported [25]. Next, the mutants in this library were subjected to the firefly luciferase activity screening, specifically targeting gli2 promotor activity. Briefly, each RS218 mutant was inoculated into HEK-293 T cells containing pGL3-gli2-promo-WT in 96-wells plates and incubated for 2 h to establish the infection, with the wild-type RS218 (RS218-WT) as the positive control. The luciferase activities in all wells were high-throughput measured with the Spark 10 M multimode microplate reader by using Luc-Pair™ Firefly Luciferase HS Assay Kit (iGene Biotechnology Co., Ltd., China) following the instruction. The mutants that could not significantly attenuate the luciferase activity were picked and double-checked, and the genomic DNA was extracted to amplify and analyze the flanking sequence of Tn insertion sites through the thermal asymmetric interlaced PCR (TAIL-PCR) as reported previously [26, 27]. Primers used for TAIL-PCR were listed in Additional file 1: Table S5.

Expression and purification of the recombinant HlyA

HlyA (the active α-hemolysin) and pro-HlyA (inactive α-hemolysin precursor) were cloned and expressed as previously reported [28]. Briefly, the CDS of the hlyA gene and the CDS of hlyCA were cloned into the pET-28a(+) vector to generate the pET28a-hlyA and pET28a-hlyCA expression plasmids. An additional T7 promotor-lacO element was introduced between hlyC and hlyA in pET28a-hlyCA, so that hlyC and hlyA genes were under the same control of transcription and translation initiation signals. The HlyA and pro-HlyA proteins were expressed in E. coli BL21(DE3) strain under the induction of 1 mM isopropyl β-D-1-thiogalactopyranoside (IPTG) for 4 h at 37 ℃. The products were finally solubilized and purified with the Ni-NTA agarose column. Primers used for the cloning were listed in Additional file 1: Table S7.

Intracellular Ca2+ determination

The confluent hBMECs were starved in serum-free medium for 16 h and then in medium containing Fluo-3-AM (5 µM) for another 1 h. The medium was replaced by the complete medium and incubated at 37 ℃ for 20 min. Subsequently, the cells were challenged with RS218 or the recombinant HlyA/pro-HlyA protein at the indicated dose for 2 h. The cells were observed with the ECHO REVOLVE microscope, and the fluorescence intensity of intracellular Ca2+ level was measured with Spark 10 M multimode microplate reader or analyzed through BD FACSVerse™ flowcytometry (BD, CA, USA).

PKA activity test

PKA activity was measured using the PepTag Non-Radioactive Protein Kinase Assay specific for PKA (Promega, WI, USA) following the manufacturer’s instructions. Briefly, cells were challenged with RS218 or treated with recombinant HlyA/pro-HlyA protein, and then collected and homogenized in PKA extraction buffer. The lysates were centrifuged, and the supernatant was incubated with the reaction mix for another 30 min. Samples were finally separated on the 0.8 % agarose gel for 20 min to analyze the activity reflected by the P-peptide.

In vivo BBB permeability assay

BBB permeability was evaluated using Evan’s blue dye (961 Da) as we previously described [29]. Briefly, mice were intravenously challenged by bacterial strains for 6 h or the indicated SAG for 12 h. After that, 500 µL Evan’s blue (5 mg/mL) was injected via the tail vein to allow circulation for 10 min before mice being sacrificed and perfused. Brains were collected and photographed for extravascular staining of the dye.

Statistical analysis

Data were expressed as the mean ± standard error of the mean (mean ± SEM) from at least three replicates. Statistical significance of each group’s differences was analyzed by a one-way analysis of variance (ANOVA) or two-way ANOVA embedded in GraphPad Prism, version 6.0 (GraphPad Software Inc., La Jolla, CA, USA). P < 0.05 (*) was considered significant, and p < 0.01 (**) was considered extremely significant.

Results

Meningitic E. coli disturbed the astrocytes-endothelium communication by attenuating TGFβ1-mediated non-canonical hedgehog signaling

We have previously demonstrated that meningitic E. coli infection could break the tight junctions and caused BBB integrity disruption [21, 29]. Here, we further validated this phenotype by challenging the mice with meningitic E. coli strain RS218. The IF assay showed that the ZO-1 in BMECs of the infected mice was largely decreased compared to the control mice (Fig. 1A), and the BBB permeability was obviously increased in the challenged mice brain, evaluated by Evan’s blue dye infiltration (Fig. 1B). Noticeably, we have recently evidenced that astrocytes-derived TGFβ1 could facilitate the BBB barrier function by increasing ZO-1 expression in BMECs via a non-canonical hedgehog signaling [13]. We therefore presumed that such TGFβ1-mediated intercellular communication between astrocytes and endothelium was largely disturbed during meningitic E. coli infection. To verify this hypothesis, we treated mice with rTGFβ1 (i.v.) prior to or along with meningitic E. coli RS218 injection. As presented in Fig. 1C, the mice pretreated with rTGFβ1 prior to infection were largely protected from death (8 of 10 were survived), while most mice receiving rTGFβ1 synchronously at the infection failed to survive (3 of 10 were survived), exhibiting a similar survival rate as the challenged mice without any treatment (2 of 10 were survived). These outcomes reflected that strengthen the BBB integrity by rTGFβ1 prior to bacterial challenge could well protect mice from death, while in contrast rTGFβ1 co-treating with the infection could not provide mice the effective protection. Meningitic E. coli could subvert this TGFβ1-regulated barrier homeostasis during the infection.

Fig. 1
figure1

Meningitic E. coli infection broke the BBB integrity and caused death in challenged mice. A The expression of ZO-1 on BMECs of the mice in response to RS218 infection via IF. The BMECs were marked with CD31 in green. Scale bars indicated 50 μm. B Evan’s blue assay assessing the BBB permeability upon RS218 infection (n = 3). C Effects of the rTGFβ1 pre-treatment (for 12 h) or co-treatment (synchronously) (at 1 µg/kg) on the survival of mice challenged with RS218 (n = 10). Survival data were collected and shown as Kaplan–Meier survival curves, and the statistical analysis was carried out by Log-rank (Mantel–Cox) test. *p < 0.05

To address this concern, we firstly analyzed the expression of the TGFβ1 receptor on BMECs of the mice challenged with meningitic E. coli RS218 via IF. As shown, meningitic E. coli infection significantly decreased the expression of TGFBRII on the BMECs (labeled with CD31) of the RS218-challenged mice (Fig. 2A). In vitro, RS218 infection also caused a significant decrease of TGFBRII in hBMECs (Fig. 2B). We next predicted the Sp1 that would act as the potential transcription factor targeting TGFBRII promotor, and both Western blot and qPCR data showed that Sp1 was also decreased in hBMECs along with RS218 infection (Fig. 2C). By overexpression of Sp1 in hBMECs (Fig. 2D, left panel), we further observed that the infection-caused TGFBRII reduction was completely restored detected by Western blot and qPCR (Fig. 2D). These observations indicated that transcription factor Sp1 was involved in meningitic E. coli-induced TGFBRII decrease.

Fig. 2
figure2

Meningitic E. coli infection specifically suppressed TGFBRII expression in BMECs via attenuated Sp1. A The expression of TGFBRII on BMECs of the mice in response to RS218 infection via IF. The BMECs were marked with CD31 in green. Scale bars indicated 50 μm. B, C Expression alteration of TGFBRII (B) or Sp1 (C) in hBMECs along with RS218 infection at indicated time points. **p < 0.01. D The effect of Sp1 overexpression on the RS218 infection-caused TGFBRII reduction in hBMECs by qPCR and Western blot. The Sp1 was cloned in pcDNA3.1(+) and transfected into hBMECs for the overexpression (left panel). **p < 0.01. The qPCR assays were performed in triplicates, and results were presented as mean ± SEM

According to Sp1 binding motif (Fig. 3A), there were 3 potential Sp1 binding sites on the tgfbr2 promotor region (Fig. 3B). Since functioning as the transcription factor, we next validated these potential Sp1 binding sites on the tgfbr2 promotor by the dual-luciferase reporter assays. The 3 predicted Sp1 binding sites on tgfbr2 promotor region (site 1–3) were shown in Fig. 3B. The tgfbr2 promotor regions, including the full-length promotor region and a series of truncations and site-mutations, were cloned and constructed. Dual-luciferase reporter assays from both truncations and site-mutations clearly indicated that the site 3, 5’-CGGGCGGAGA-3’ (from + 19 to + 28), was the Sp1 binding region on tgfbr2 promotor (Fig. 3C and D). Besides, through ChIP-qPCR with anti-Sp1 antibody, the flanking sequences of the site 3 were positively detected, and Sp1 binding with this promotor region in hBMECs was also significantly decreased upon RS218 infection (Fig. 3E). These results together suggested that meningitic E. coli infection decreased the TGFBRII expression in hBMECs through Sp1-regulated tgfbr2 promotor, thus disturbing the TGFβ1-mediated astrocytes-endothelium communication.

Fig. 3
figure3

Dual-luciferase reporter assays detected Sp1 binding sites on tgfbr2 promotor. A The sequence logo of the Sp1 binding motif. B Schematic of the 3 predicted Sp1 binding sites on tgfbr2 promotor and their binding sequences accordingly. The binding sites were located at -1135 to -1125 (site 1), -105 to -95 (site 2) and + 19 to + 28 (site 3) of the tgfbr2 promotor. The tgfbr2 luciferase activities tested by applying a series of truncations (C) as well as site-targeted mutations (D) on the tgfbr2 promoter, along with pcDNA3.1-Sp1 and pRL-TK plasmids. The specific constructs used in the truncation assays (C) included pGL3-basic vector, pGL3-tgfbr2-promo-WT (containing promotor region from − 1405 to + 98), pGL3-tgfbr2-promo-truncation1 (from − 1085 to + 98), pGL3-tgfbr2-promo-truncation2 (from − 746 to + 98), pGL3-tgfbr2-promo-truncation3 (from − 402 to + 98), pGL3-tgfbr2-promo-truncation4 (from − 41 to + 98) and pGL3-tgfbr2-promo-truncation4&mut3 (from − 41 to + 98 which lacking site 3). The specific constructs used in the site-mutation assays (D) included pGL3-basic vector, pGL3-tgfbr2-promo-WT (containing all 3 sites), pGL3-tgfbr2-promo-mut1 (lack of site 1), pGL3-tgfbr2-promo-mut2 (lack of site 2), or pGL3-tgfbr2-promo-mut3 (lack of site 3). The luciferase activities were determined and presented as the ratio of firefly luciferase activity and renilla luciferase activity. The assays were performed with 3 replicates, and data were presented as mean ± SEM. **p < 0.01. ns, no significance. E Schematic of the evidenced Sp1 binding site on tgfbr2 promotor and ChIP-qPCR verification of Sp1 binding with the tgfbr2 promotor at the site around + 19 in hBMECs upon infection. The ChIP procedure was performed with an anti-Sp1 antibody, and rabbit IgG was employed as the negative control. The qPCR was assayed with 3 replicates, and data were presented as mean ± SEM. **p < 0.01

Previously we have evidenced that astrocytes-derived TGFβ1 facilitated the BBB barrier function in BMECs via a non-canonical hedgehog signaling [13]. Here, our in vivo assay also demonstrated that the hedgehog signaling transcription factor Gli2 in mice BMECs was largely reduced in response to RS218 infection (Fig. 4 A). And the in vitro qPCR and Western blot assay also showed a time-dependent reduction of Gli2 in hBMECs upon the infection (Fig. 4B). Although we here did not observe the significant decrease of Gli1 expression upon the infection, the nucleus/cytoplasm extraction clearly showed that the nucleus-located Gli1 significantly decreased in response to RS218 infection (Fig. 4B). These findings indicated that the hedgehog signaling transcription factor Gli1/2 was hijacked by meningitic E. coli for disturbing this astrocytes-endothelium communication. However, how meningitic E. coli targets Gli1/2 is yet to be investigated.

Fig. 4
figure4

Meningitic E. coli infection attenuated the hedgehog signaling in BMECs. A The expression of Gli2 on BMECs of the challenged mice via IF. The BMECs were marked with CD31 in green. White triangles indicated Gli2 in BMECs. Scale bars indicated 50 μm. B Expression alterations of Gli1 and Gli2 in hBMECs along with RS218 infection via qPCR and Western blot, and the subcellular localization of Gli1 in hBMECs 2 h post infection. **p < 0.01. The qPCR assays were performed in triplicates, and results were presented as mean ± SEM

α-Hemolysin was the primary virulence determinant responsible for RS218-caused Gli2 and ZO-1 decrease in hBMECs

Subsequently, we attempted to explore the mechanism of meningitic E. coli targeting Gli1/2. Since Gli2 as well as the gene promotor activity in hBMECs was observed to be significantly decreased by meningitis E. coli RS218 (Fig. 4B and Additional file 1: Fig S1A), we therefore transfected the pGL3-gli2-promo-WT reporter plasmid into HEK-293 T cells, and preliminarily tested the regulative effect of RS218 on Gli2 transcription. As shown, the gli2 luciferase activity exhibited a significantly time-dependent decrease in response to meningitic E. coli RS218 infection. In contrast, the non-meningitic E. coli K12 strain MG1655 did not show any decreased effect on the gli2 luciferase activity (Fig. 5 A). This data indicated the availability of this screening approach and suggested that there should be some specific virulence determinants responsible for the decrease of Gli2. Next, our previously generated Tn5 transposon mutation library in RS218 was applied for high-throughput screening of the bacterial determinants associated with Gli2 activity. The mutations inducing higher luciferase activity compared with the RS218-WT were picked. The sequences flanking the transposon insertion site were amplified with TAIL-PCR, and the products were subjected to sequencing and genome alignment (Fig. 5B). A total of 40 Tn5-mutations were found unable to decrease but induced much higher gli2 promotor luciferase activity than the RS218-WT (Additional file 1: Fig. S1B). After sequencing and duplicates removal, 29 distinct mutations were finally identified (Table S1), and 23 of them were identified as α-hemolysin operon hlyCABD insertions (Additional file 1: Fig. S1C). Among these 23 mutations, the CDS regions of hlyA, hlyB, and hlyD were inserted by Tn5 transposon for 21 times, and the reported regulative region upstream of hlyC was inserted by Tn5 transposon twice. These results implied that α-hemolysin was likely to be an important determinant which was responsible for the downregulation of Gli2.

Fig. 5
figure5

High-throughput screening of Tn5-transposon mutation library identified α-hemolysin that regulating Gli2 transcription in hBMECs. A Firefly-luciferase reporter assay testing the effect of RS218 infection on the gli2 promoter activity. E. coli K12 strain MG1655 was compared as the control. Results were obtained from three independent assays and presented as mean ± SEM. **p < 0.01. B Schematic diagram showing the screening process of Tn5-transposon mutation library in RS218. C Hemolysis rings of RS218-WT, RS218-ΔhlyA, and RS218-ΔhlyA-phlyCA growing on sheep blood agar plates

To confirm this hypothesis, we generated a serial of deletion mutants of hlyCABD operon via CRISPR/Cas9 system and evaluated their hemolytic abilities in vitro. As presented in Fig. 5C, the hlyA-deleted strain (RS218-ΔhlyA, shown as the representative) obviously loss the hemolytic ability on the sheep blood agar plate compared with the wild-type strain, while the complemented strain (RS218-ΔhlyA-phlyCA) completely restored this hemolysis phenotype (black triangles indicated the hemolysis ring), suggesting the successful genetic and functional deletion as well as complementation of hlyA. Moreover, we found the significantly decreased expression of ZO-1 and Gli2 in hBMECs in response to RS218-WT strain and the complement strain RS218-ΔhlyA-phlyCA, while the mutant RS218-ΔhlyA did not decrease both expression (Fig. 6A). Similarly, the other α-hemolysin deletion mutants, including RS218-ΔhlyC, RS218-ΔhlyB, RS218-ΔhlyD, and RS218-ΔhlyCABD were also tested and they were all unable to decrease the expression of Gli2 and ZO-1 in hBMECs (Fig. 6A). In vivo, the mice challenged with RS218-ΔhlyA strain showed 100 % survival, while those challenged with RS218-WT and RS218-ΔhlyA-phlyCA exhibited around 80 % death within 48 h post infection (Fig. 6B). Meanwhile, the mice BBB permeability was assessed via Evan’s blue assay and showed that both RS218-WT and RS218-ΔhlyA-phlyCA strains caused the significantly increased permeability, demonstrated by the heavy Evan’s blue dye effusion out of the brain vessels. While in contrast, the mutant strain RS218-ΔhlyA did not show too much damage to the vessel permeability (Fig. 6C). The IF results also supported that both Gli2 and ZO-1 expression (labeled with Cy3) around the BMECs (labeled with anti-CD31-FITC) were significantly reduced by the RS218-WT and RS218-ΔhlyA-phlyCA infection, while the RS218-ΔhlyA strain did not influence the expression of Gli2 and ZO-1 (Fig. 6C). Together, these findings largely evidenced that RS218 α-hemolysin was the major determinant contributing to the infection-caused Gli2 and ZO-1 decrease in BMECs.

Fig. 6
figure6

E. coli α-hemolysin was responsible for the infection-caused decrease of Gli2 and ZO-1 as well as the BBB integrity damage. A The expression of ZO-1 and Gli2 in hBMECs in response to RS218-WT, RS218-ΔhlyA, and RS218-ΔhlyA-phlyCA strains, as well as other α-hemolysin operon genes mutants. B Mice survival upon the infection of RS218-WT, RS218-ΔhlyA, and RS218-ΔhlyA-phlyCA strains (n = 10). Survival data were collected and shown as Kaplan–Meier survival curves, and the statistical analysis was carried out by Log-rank (Mantel–Cox) test. **p < 0.01. ns, no significance. C Evan’s blue and IF assays showing the BBB permeability and both Gli2 and ZO-1 expression in brains of mice challenged by RS218-WT, RS218-ΔhlyA, and RS218-ΔhlyA-phlyCA strains. The white triangles indicated Gli2 in BMECs. Scale bar indicated 50 μm

α-Hemolysin-triggered Ca2+ influx and PKA activation accounted for the decreased expression of Gli2 and ZO-1 in hBMECs

The α-hemolysin HlyA was a kind of prototype RTX toxin and contained repeating RTX domains that consist of several glycine- and aspartate- rich nonapeptide units for Ca2+ binding [30]. We therefore presumed that Ca2+ played a certain role in the α-hemolysin-induced effects. By applying Fluo-3-AM, a specific probe to indicate Ca2+, we measured the intracellular Ca2+ level in hBMECs by the infection of RS218-WT, RS218-ΔhlyA, and RS218-ΔhlyA-phlyCA. As shown, both RS218-WT and RS218-ΔhlyA-phlyCA strains induced strong Ca2+ influx in hBMECs, while the RS218-ΔhlyA mutant could not increase the intracellular Ca2+ level (Fig. 7A). The flow cytometry also supported this observation that both RS218-WT and RS218-ΔhlyA-phlyCA strains induced much higher levels of intracellular Ca2+, compared with that induced by the mutant RS218-ΔhlyA (Fig. 7B). In addition, when extracellular Ca2+ was chelated by EGTA, the RS218-induced time-dependent downregulation of ZO-1 and Gli2 was suppressed entirely (Fig. 7C). Meanwhile, we similarly tested the Ca2+ influx in hBMECs by the treatment of recombinant HlyA protein, including the active HlyA as well as its inactive form pro-HlyA, and results showed that the active HlyA caused a significantly increased and much higher level of intracellular Ca2+, compared with the treatment by pro-HlyA (Additional file 1: Fig. S2A and S2B). Consistently, the active HlyA, not the pro-HlyA, was shown to downregulate ZO-1 and Gli2 expression in hBMECs, while this HlyA-induced downregulation of ZO-1 and Gli2 were completely prevented by treating with Ca2+ chelator EGTA (Fig S2C).

Fig. 7
figure7

The HlyA-triggered Ca2+ influx and PKA activation accounted for the infection-caused ZO-1 and Gli2 reduction. A, B Ca2+ influx of hBMECs upon infection of RS218-WT, RS218-ΔhlyA, and RS218-ΔhlyA-phlyA strains for 2 h determined by the Fluo-3-AM probed through the fluorescence microscopy (A) and flow cytometry (B). The assay was performed with 3 replicates, and data were presented as mean ± SEM. ** p < 0.01. ns, no significance. Scale bar indicated 100 μm. Cells in Blank group were not treated. Cells in Control group, RS218-WT group, RS218-ΔhlyA group, and RS218-ΔhlyA-phlyA group were loaded with Fluo-3-AM and treated as indicated. C The expression of ZO-1 and Gli2 in hBMECs upon RS218 infection, as well as upon infection with pre-treatment of Ca2+ chelator EGTA (5 mM) or PKA activity inhibitor H89 (20 µM). D PKA activity in hBMECs upon the infection of RS218-WT, RS218-ΔhlyA, and RS218-ΔhlyA-phlyA strains, and upon the infection in the presence of EGTA (5 mM)

It was known that PKA was an essential transducer of intracellular electrical activity [31] and was recognized as the suppressor of Gli2 in cells [32]. We next measured the PKA activity in hBMECs by the infection of RS218-WT, RS218-ΔhlyA, and RS218-ΔhlyA-phlyCA strains. The results suggested that RS218-WT and RS218-ΔhlyA-phlyCA infection of hBMECs largely enhanced the PKA activity, demonstrated by an increased level of P-peptide, and this increased PKA activity by both RS218-WT and RS218-ΔhlyA-phlyCA infection could be entirely suppressed by the treatment of EGTA (Fig. 7D). However, the RS218-ΔhlyA strain was shown unable to effectively activate PKA activity, demonstrated by a relatively higher level of the nonP-peptide (Fig. 7D). The recombinant active HlyA was also shown to increase PKA activity by a relatively higher P-peptide level, while the pro-HlyA did not (Additional file 1: Fig. S2D). Moreover, we observed that meningitic E. coli RS218-caused time-dependent downregulation of ZO-1 and Gli2 was totally suppressed by the pre-treatment of EGTA and the PKA inhibitor H89 (Fig. 7C), and the same results were also observed with HlyA and pro-HlyA treatment (Additional file 1: Fig. S2C). Therefore, these findings largely supported that the Ca2+ influx and PKA activation induced by α-hemolysin were the reason for the decreased expression of Gli2 and ZO-1 herein. Noticeably, we above showed that meningitic E. coli attenuating TGFBRII largely disturbed the TGFβ1-mediated astrocytes-endothelium communication, we additionally found that this TGFBRII reduction could also be mediated by α-hemolysin, by the demonstration that the RS218-WT and RS218-ΔhlyA-phlyCA significantly decreased the TGFBRII in hBMECs, while the α-hemolysin deletion mutant RS218-ΔhlyA did not (Additional file 1: Fig. S3). Meanwhile, both Ca2+ chelator EGTA and PKA inhibitor H89 could not stop this reduction, suggesting that the α-hemolysin-caused TGFBRII reduction was independent of Ca2+ influx and PKA activation (Additional file 1: Fig. S3). Anyway, these data revealed that α-hemolysin-triggered Ca2+ influx and PKA activation accounted for the decreased expression of Gli2 and ZO-1 in hBMECs.

Hedgehog signaling agonist SAG protected the BBB integrity from being disrupted by meningitic E. coli

Since we have evidenced the importance of TGFβ1-triggered hedgehog signaling in astrocytes-endothelium communication and BBB function maintaining [13], we thus hope to see whether activating hedgehog signaling by the known agonist SAG could show some protective effects against bacterial challenge. Here, we firstly tested the possible effects of SAG treatment on the hBMECs barrier function in vitro. As the ECIS results shown, SAG effectively increased the barrier resistance of monolayer hBMECs in a dose-dependent manner (Fig. 8A), implying a potential barrier protection role of SAG. In vivo, by intravenous injection of SAG, the TJ protein ZO-1 in mice brain presented a high expression around the blood vessels (labeled with CD31) (Fig. 8B). We moreover evaluated the effect of SAG administration in the challenge of RS218 and found that both pre-treatment and co-treatment of SAG with RS218 challenge exhibited promising protective effects in mice (Fig. 9A), and both SAG administration methods significantly attenuated the RS218 infection-induced decrease of ZO-1 expression in mice brains (Fig. 9B). Meanwhile, the brain permeability assays with Evan’s blue showed that both SAG treatments could significantly protect the BBB from being disrupted by the infection, and the IF showed that RS218 infection-caused downregulation of ZO-1 in mice BMECs were significantly prevented by both pre-treatment and co-treatment of SAG (Fig. 9C). These data suggested that activating the hedgehog signaling in BMECs has great potential in the protection of BBB, as well as prevention and control of meningitic E. coli infection.

Fig. 8
figure8

SAG enhanced the barrier function of BMECs. A The effect of SAG treatment at different dosages on the barrier resistance via ECIS. The left panel indicated the TEER value of hBMECs, and the right panel, representing the factored parameter from TEER values, indicated the barrier function of hBMECs. Each treatment contained 5 replicates, and data were presented as mean ± SEM. B The effect of SAG treatment (10 mg/kg) on the ZO-1 expression in mice BMECs. Scale bar indicated 50 μm

Fig. 9
figure9

SAG treatment showed good BBB protection in response to RS218 infection. A Both pre-treatment (for 12 h) and co-treatment (synchronously) of SAG (10 mg/kg) provided the promising protection in mice against RS218 infection (n = 10). **p < 0.01. B The effect of both SAG treatments (10 mg/kg) on the RS218-caused decrease of ZO-1 in mice brains. C Evan’s blue and IF assays assessing the SAG-induced protective effects on the BBB permeability as well as the preventive effects on the infection-caused ZO-1 reduction, respectively. Scale bar indicated 50 μm

Discussion

The intercellular communication between astrocytes and endothelium is essential for BBB integrity and CNS homeostasis. Previously, we observed an increased TEER of BMECs in vitro when co-cultured with astrocytes U251, and demonstrated that astrocytes-derived TGFβ1 could physiologically help to maintain BBB integrity and function through stabilizing ZO-1 expression in BMECs, in a hedgehog signaling-dependent manner [13]. Since astrocytes-derived TGFβ1 exhibited an endothelial barrier protective effect, while our early studies and data in this work (Fig. 1) supported the disruptive outcomes of the endothelial barrier caused by meningitic E. coli infection [21, 29], then there come the questions that whether and how meningitic E. coli hijacks this TGFβ1-mediated barrier-maintaining pathway (TGFβ1-TGFBRI/II-Smads-Gli1/2-ZO-1 axis) for its BBB penetration. Here, we demonstrated the TGFβ1 receptor TGFBRII, as well as the hedgehog signaling key transcription factor Gli1/2, were targeted by meningitic E. coli. Specifically, on the one hand, the expression of TGFBRII was shown to be significantly decreased in BMECs by the infection of meningitic E. coli RS218, during which the transcription factor Sp1 mediated this TGFBRII downregulation. On the other hand, the Gli1/2 in BMECs was also shown to be affected by RS218 challenge, supported by the significantly reduced Gli2 expression and Gli1 nucleus translocation. Such a dual-targeting strategy completely blocked the communication between endothelial cells and astrocytes mediated by TGFβ1, which led to the destruction of BBB caused by meningitic E. coli.

We next investigated how RS218 targeted this non-canonical hedgehog activation for the BBB disruption. Since Gli1/2 act as the key transcription factor of hedgehog signaling and Gli2 was observed herein to be significantly decreased in response to RS218, we therefore constructed the Tn5-transposon mutant library in RS218 to screen the key bacterial determinant that targeting Gli2. Fortunately, our screening results specifically pointed to the α-hemolysin operon hlyCABD, one of the RTX family members, as the main virulence factor of RS218 to decrease Gli2, thus led to a decrease of ZO-1 expression as well. RTX family were a group of exoproteins secreted from Gram-negative bacteria via the type I secretion system (T1SS), with glycine-aspartate (GD)-rich nonapeptide repeats of the consensus sequence G-G-X-G-(N/D)-D-x-(L/I/F)-X near C-terminus [33], and their secretion, maturation, and function were closely related to Ca2+ binding. When the toxin was exported outside the T1SS conduit, the high concentration of extracellular Ca2+ promoted the correct folding of the C-terminal and prevented its backsliding in the conduit [34]. The binding and perforation of the toxin on the membrane were considered to be receptor-independent. Once perforated on the host cell membrane, the toxin may trigger the influx of Ca2+ [35]. As expected, we observed that α-hemolysin HlyA induced the Ca2+ influx, leading to the intracellular PKA activation and finally the Gli2 as well as ZO-1 reduction in hBMECs. Noticeably, we also observed a slight Ca2+ alteration in hBMECs by the treatment of pro-HlyA, which might due to the weak hemolytic activity of pro-HlyA without the HlyC acylation [36]. For PKA, it was considered a typical inhibitor of Gli2, along with glycogen synthase kinase 3β (GSK-3β) and casein kinase 1 (CK1) [37, 38]. Previous studies in Drosophila have shown that PKA could phosphorylate Ci (the alias of Gli in Drosophila) at multiple serine/threonine (Ser/Thr) residues of the C-terminal region, and the GSK-3β and CK1 phosphorylation of Ci might be primed by PKA phosphorylation nearby the Ser/Thr residues. The phosphorylated Ci region created the binding site of the so-called SCF (Skp1, Cdc53, and F-box) complex, one of the ubiquitin ligase complexes that normally targets phosphorylated substrates, and finally led to the degradation of Ci [39]. And in mammals, the PKA, GSK-3β, and CK1 were also observed to modulate Gli2 via phosphorylation in a similar manner [40]. Therefore, these data together with the Tn5-transposon library screening basically revealed the mechanism of meningitic E. coli disturbing the intercellular communication between astrocytes and BMECs. In brief, meningitic E. coli exported α-hemolysin HlyA to perforate and trigger the subsequent Ca2+ influx and PKA activation, finally led to Gli2 and ZO-1 degradation in hBMECs. Surprisingly, we additionally observed that α-hemolysin HlyA also participated in the RS218-targeted reduction of TGFBRII, but in a Ca2+-PKA independent manner. The underlying mechanism of this HlyA-associated TGFBRII reduction was still unclear at this time, but anyway, these findings all supported that α-hemolysin facilitated meningitic E. coli subversion of the astrocytes-endothelium communication by attenuating TGFβ1-mediated non-canonical hedgehog signaling.

Both astrocytes-derived TGFβ1 and the hedgehog agonist SAG were previously reported to maintain the vascular and BBB stabilization under stroke or HIV infection [41,42,43]. As an extension of this study, we also discussed the potential protection of rTGFβ1 and SAG in mice against meningitic E. coli infection with two routes of administration, prior to-challenge administration and simultaneous administration. For rTGFβ1 (Fig. 1C), pre-administration of rTGFβ1 better protected the challenged mice, while in contrast, treatment with rTGFβ1 while challenged did not reverse the death of challenged mice. This outcome may be attributed to the significant downregulation of the TGFβ1 receptor TGFBRII induced by meningitic E. coli, and the simultaneous TGFβ1 treatment could not exert the timely and effective barrier protection effect due to the lack of its receptor. In contrast, for hedgehog agonist SAG (Fig. 9), both pre-treatment and co-treatment of SAG in mice, all exhibited the protective effects against RS218 challenge, which supported a promising potential of SAG in control of the infection, especially when applied simultaneously. This remarkable effect was further supported by the significant recovery of the infection-caused ZO-1 decrease and the BBB disruption in mice brains with both routes of SAG treatment. Besides, the previous work has also demonstrated that activating hedgehog signaling in BBB could reduce Th1 and Th17 cells’ adherence to BMECs and suppress neuroinflammatory responses, thus helping maintain CNS immune quiescence [44]. These reports, together with our observations herein, largely suggested that activating hedgehog signaling by SAG in BMECs would be beneficial for the BBB protection, as well as for the prevention and control of bacterial-induced CNS dysfunction.

In summary, together with our previous finding, we demonstrated a TGFβ1-mediated cell-to-cell communication for maintaining the normal BBB function, as well as its disturbance by meningitic E. coli for the BBB disruption. As presented in Fig. 10, the astrocytes-derived TGFβ1 triggered the TGFβ1-TGFBRII-Smad2/3-Gli1/2-ZO-1 axis in BMECs which accounted for the physiological BBB function maintaining [13], while meningitic E. coli craftily disturbed this intercellular cross-talking by attenuating both TGFβ1 receptor TGFBRII and the key transcription factors of hedgehog signaling Gli1/2 in BMECs, which largely depended on the action of α-hemolysin. Strikingly, the hedgehog signaling agonist SAG presented powerful protection of the BBB integrity and the mice survival from meningitic E. coli challenge. Together, these findings reveal a novel pathogenic mechanism in meningitic E. coli-caused BBB disruption from the perspective of intercellular communication between astrocytes and vascular endothelium within BBB, and highlight the critical roles of hedgehog signaling in preventing the CNS dysfunction caused by bacterial infection.

Fig. 10
figure10

Schematic presentation of the TGFβ1-mediated intercellular communication for maintaining the normal BBB function as well as the disturbance by meningitic E. coli for the BBB disruption. Without infection, astrocytes-derived TGFβ1 physiologically triggered the TGFβ1-TGFBRII-Smad2/3-Gli1/2-ZO-1 axis in BMECs to maintain the normal BBB function (left panel). Upon meningitic E. coli infection, bacterial virulence determinant α-hemolysin effectively helped to disturb this functional cross-talking between astrocytes and BMECs by attenuating both TGFβ1 receptor TGFBRII as well as the hedgehog signaling transcription factors Gli1/2 in BMECs, thus led to the BBB dysfunction

Availability of data and materials

All data generated or analyzed during this study are included in this published article and its additional information files.

Abbreviations

CNS:

Central nervous system

E. coli :

Escherichia coli

BBB:

Blood–brain barrier

BMECs:

Brain microvascular endothelial cells

hBMECs:

Human brain microvascular endothelial cells

TEER:

Trans-endothelial electrical resistance

TGFβ1:

Transforming growth factor-β1

Hly:

Hemolysin

RTX:

Repeats-in-toxin

UPEC:

Uropathogenic E. coli

DAPI:

4′,6-diamidino-2-phenylindole

ECIS:

Electric cell-substrate impedance sensing

CDS:

Coding sequence

ChIP:

Chromatin immunoprecipitation

TAIL-PCR:

Thermal asymmetric interlaced PCR

PKA:

Protein kinase A

EGTA:

Ethyleneglycolbis(2-aminoethylether)-N,N,N′,N′-tetraaceticacid

References

  1. 1.

    McGill F, Heyderman RS, Panagiotou S, Tunkel AR, Solomon T. Acute bacterial meningitis in adults. Lancet. 2016;388(10063):3036–47.

    PubMed  Article  PubMed Central  Google Scholar 

  2. 2.

    Agrawal S, Nadel S. Acute bacterial meningitis in infants and children: epidemiology and management. Paediatr Drugs. 2011;13(6):385–400.

    PubMed  Article  PubMed Central  Google Scholar 

  3. 3.

    Kim KS. Acute bacterial meningitis in infants and children. Lancet Infect Dis. 2010;10(1):32–42.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  4. 4.

    Janowski A, Newland J. Of the Phrensy: an update on the epidemiology and pathogenesis of bacterial meningitis in the pediatric population. F1000Res. 2017;6:86.

    Article  CAS  Google Scholar 

  5. 5.

    Kim KS. Pathogenesis of bacterial meningitis: from bacteraemia to neuronal injury. Nat Rev Neurosci. 2003;4(5):376–85.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  6. 6.

    Keaney J, Campbell M. The dynamic blood–brain barrier. FEBS J. 2015;282(21):4067–79.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  7. 7.

    Correale J, Villa A. Cellular elements of the blood–brain barrier. Neurochem Res. 2009;34(12):2067–77.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  8. 8.

    Saunders NR, Ek CJ, Habgood MD, Dziegielewska KM. Barriers in the brain: a renaissance? Trends Neurosci. 2008;31(6):279–86.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  9. 9.

    Dejana E, Tournier-Lasserve E, Weinstein BM. The control of vascular integrity by endothelial cell junctions: molecular basis and pathological implications. Dev Cell. 2009;16(2):209–21.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  10. 10.

    Edwards VL, Wang LC, Dawson V, Stein DC, Song W. Neisseria gonorrhoeae breaches the apical junction of polarized epithelial cells for transmigration by activating EGFR. Cell Microbiol. 2013;15(6):1042–57.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  11. 11.

    Igarashi Y, Utsumi H, Chiba H, Yamada-Sasamori Y, Tobioka H, Kamimura Y, et al. Glial cell line-derived neurotrophic factor induces barrier function of endothelial cells forming the blood–brain barrier. Biochem Bioph Res Co. 1999;261(1):108–12.

    CAS  Article  Google Scholar 

  12. 12.

    Zacharek A, Chen J, Cui X, Li A, Li Y, Roberts C, et al. Angiopoietin1/Tie2 and VEGF/Flk1 induced by MSC treatment amplifies angiogenesis and vascular stabilization after stroke. J Cerebr Blood F Met. 2007;27(10):1684–91.

    CAS  Article  Google Scholar 

  13. 13.

    Fu J, Li L, Huo D, Zhi S, Yang R, Yang B, et al. Astrocyte-derived TGFbeta1 facilitates blood–brain barrier function via non-canonical Hedgehog signaling in brain microvascular endothelial cells. Brain Sci. 2021;11(1):77.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  14. 14.

    Welch RA. The Escherichia coli hemolysin. EcoSal Plus. 2005;1:2.

    Article  CAS  Google Scholar 

  15. 15.

    Spitz O, Erenburg IN, Beer T, Kanonenberg K, Holland IB, Schmitt L. Type I secretion systems-One mechanism for all? Microbiol Spectr. 2019;7(2):PSIB–0003.

    CAS  Article  Google Scholar 

  16. 16.

    Thomas S, Holland IB, Schmitt L. The Type 1 secretion pathway-the hemolysin system and beyond. Biochim Biophys Acta. 2014;1843(8):1629–41.

    CAS  PubMed  Article  Google Scholar 

  17. 17.

    Nagamatsu K, Hannan TJ, Guest RL, Kostakioti M, Hadjifrangiskou M, Binkley J, et al. Dysregulation of Escherichia coli alpha-hemolysin expression alters the course of acute and persistent urinary tract infection. Proc Natl Acad Sci U S A. 2015;112(8):E871-80.

    PubMed  Article  CAS  Google Scholar 

  18. 18.

    Dhakal BK, Mulvey MA. The UPEC pore-forming toxin alpha-hemolysin triggers proteolysis of host proteins to disrupt cell adhesion, inflammatory, and survival pathways. Cell Host Microbe. 2012;11(1):58–69.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  19. 19.

    Surewaard BGJ, Thanabalasuriar A, Zeng Z, Tkaczyk C, Cohen TS, Bardoel BW, et al. alpha-Toxin induces platelet aggregation and liver injury during Staphylococcus aureus sepsis. Cell Host Microbe. 2018;24(2):271–84. e3.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  20. 20.

    Chen C, Nguyen BN, Mitchell G, Margolis SR, Ma D, Portnoy DA. The listeriolysin O PEST-like sequence co-opts AP-2-mediated endocytosis to prevent plasma membrane damage during Listeria infection. Cell Host Microbe. 2018;23(6):786–95. e5.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  21. 21.

    Yang R, Liu W, Miao L, Yang X, Fu J, Dou B, et al. Induction of VEGFA and Snail-1 by meningitic Escherichia coli mediates disruption of the blood–brain barrier. Oncotarget. 2016;7(39):63839–55.

    PubMed  PubMed Central  Article  Google Scholar 

  22. 22.

    Szulcek R, Bogaard HJ, van Nieuw Amerongen GP. Electric cell-substrate impedance sensing for the quantification of endothelial proliferation, barrier function, and motility. JoVE-J Vis Exp. 2014(85):51300.

  23. 23.

    Jiang Y, Chen B, Duan C, Sun B, Yang J, Yang S. Multigene editing in the Escherichia coli genome via the CRISPR-Cas9 system. Appl Environ Microbiol. 2015;81(7):2506–14.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  24. 24.

    Wang X, Maruvada R, Morris AJ, Liu JO, Wolfgang MJ, Baek DJ, et al. Sphingosine 1-Phosphate activation of EGFR as a novel target for meningitic Escherichia coli penetration of the blood–brain barrier. PLoS Pathog. 2016;12(10):e1005926.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  25. 25.

    Zheng Y, Wang H, Huang L, Zhang T, Zong B, Ren X, et al. Effect of O antigen ligase gene mutation on oxidative stress resistance and pathogenicity of NMEC strain RS218. Microb Pathog. 2019;136:103656.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  26. 26.

    Liu YG, Chen Y. High-efficiency thermal asymmetric interlaced PCR for amplification of unknown flanking sequences. Biotechniques. 2007;43(5):649–50. 52, 54 passim.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  27. 27.

    Jia X, Lin X, Chen J. Linear and exponential TAIL-PCR: a method for efficient and quick amplification of flanking sequences adjacent to Tn5 transposon insertion sites. AMB Express. 2017;7(1):195.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  28. 28.

    Stanek O, Masin J, Osicka R, Jurnecka D, Osickova A, Sebo P. Rapid purification of endotoxin-free RTX toxins. Toxins (Basel). 2019;11(6):336.

    CAS  Article  Google Scholar 

  29. 29.

    Yang RC, Qu XY, Xiao SY, Li L, Xu BJ, Fu JY, et al. Meningitic Escherichia coli-induced upregulation of PDGF-B and ICAM-1 aggravates blood–brain barrier disruption and neuroinflammatory response. J Neuroinflamm. 2019;16(1):101.

    Article  Google Scholar 

  30. 30.

    Linhartova I, Bumba L, Masin J, Basler M, Osicka R, Kamanova J, et al. RTX proteins: a highly diverse family secreted by a common mechanism. FEMS Microbiol Rev. 2010;34(6):1076–112.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  31. 31.

    Ghosh A, Greenberg ME. Calcium signaling in neurons: molecular mechanisms and cellular consequences. Science. 1995;268(5208):239–47.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  32. 32.

    Osterlund T, Kogerman P. Hedgehog signalling: how to get from Smo to Ci and Gli. Trends Cell Biol. 2006;16(4):176–80.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  33. 33.

    Satchell KJ. Structure and function of MARTX toxins and other large repetitive RTX proteins. Annu Rev Microbiol. 2011;65:71–90.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  34. 34.

    Bumba L, Masin J, Macek P, Wald T, Motlova L, Bibova I, et al. Calcium-driven folding of RTX domain beta-rolls ratchets translocation of RTX proteins through type I secretion ducts. Molecular cell. 2016;62(1):47–62.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  35. 35.

    Benz R. Channel formation by RTX-toxins of pathogenic bacteria: Basis of their biological activity. Biochim Biophys Acta. 2016;1858(3):526–37.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  36. 36.

    Vazquez RF, Mate SM, Bakas LS, Munoz-Garay C, Herlax VS. Relationship between intracellular calcium and morphologic changes in rabbit erythrocytes: Effects of the acylated and unacylated forms of E. coli alpha-hemolysin. Biochim Biophys Acta. 2016;1858(8):1944–53.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  37. 37.

    Liu A. Proteostasis in the Hedgehog signaling pathway. Semin Cell Dev Biol. 2019;93:153–63.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  38. 38.

    Montagnani V, Stecca B. Role of protein kinases in Hedgehog pathway control and implications for cancer therapy. Cancers (Basel). 2019;11(4):449.

    CAS  Article  Google Scholar 

  39. 39.

    Jia J. Phosphorylation regulation of Hedgehog signaling. Vitam Horm. 2012;88:253–72.

    CAS  PubMed  Article  Google Scholar 

  40. 40.

    Riobo NA, Lu K, Ai X, Haines GM, Emerson CP Jr. Phosphoinositide 3-kinase and Akt are essential for Sonic Hedgehog signaling. Proc Natl Acad Sci USA. 2006;103(12):4505–10.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  41. 41.

    Tran ND, Correale J, Schreiber SS, Fisher M. Transforming growth factor-beta mediates astrocyte-specific regulation of brain endothelial anticoagulant factors. Stroke. 1999;30(8):1671–8.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  42. 42.

    Singh VB, Singh MV, Gorantla S, Poluektova LY, Maggirwar SB. Smoothened agonist reduces human immunodeficiency virus type-1-induced blood–brain barrier breakdown in humanized mice. Sci Rep. 2016;6:26876.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  43. 43.

    Singh VB, Singh MV, Piekna-Przybylska D, Gorantla S, Poluektova LY, Maggirwar SB. Sonic Hedgehog mimetic prevents leukocyte infiltration into the CNS during acute HIV infection. Sci Rep. 2017;7(1):9578.

    PubMed  PubMed Central  Article  Google Scholar 

  44. 44.

    Alvarez JI, Dodelet-Devillers A, Kebir H, Ifergan I, Fabre PJ, Terouz S, et al. The Hedgehog pathway promotes blood–brain barrier integrity and CNS immune quiescence. Science. 2011;334(6063):1727–31.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

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Acknowledgements

We would like to thank Prof. Kwang Sik Kim at Johns Hopkins University School of Medicine for kindly providing hBMECs cells.

Funding

This research was funded by The National Natural Science Foundation of China, Grant number 31772736; China Agriculture Research System of MOF and MARA, Grant number CARS-35; The National Key R&D Program of China, Grant number 2016YFD0500406; The Outstanding youth project of Natural Science Foundation in Hubei Province, Grant number 2018CFA070; The Fundamental Research Funds for the Central Universities, Grant number 2662018PY032.

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Conceptualization, JF and XW; Data curation, JF; Formal analysis, JF; Funding acquisition, HC and XW; Investigation, JF; Methodology, LL, BY, and XY; Project administration, MD and CT; Software, RY; Validation, JF, DH, and BX; Visualization, DH; Writing—original draft, JF; Writing—review & editing, XW. All authors read and approved the final manuscript.

Corresponding author

Correspondence to Xiangru Wang.

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The current study was carried out in accordance with the guidelines established by the China Regulations for the Administration of Affairs Concerning Experimental Animals (1988) and Regulations for the Administration of Affairs Concerning Experimental Animals in Hubei Province (2005). All procedures and handling techniques were approved by The Scientific Ethic Committee of Huazhong Agricultural University (Animal Welfare Assurance No. HZAUMO-2019-021).

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Fu, J., Li, L., Huo, D. et al. Meningitic Escherichia coli α-hemolysin aggravates blood–brain barrier disruption via targeting TGFβ1-triggered hedgehog signaling. Mol Brain 14, 116 (2021). https://0-doi-org.brum.beds.ac.uk/10.1186/s13041-021-00826-2

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Keywords

  • Escherichia coli
  • α-Hemolysin
  • Blood–brain barrier
  • Intercellular communication
  • TGFβ1
  • Hedgehog signaling