Background
The vasculature of the brain is specialized to function as a barrier to protect the central nervous system (CNS) by restricting entry of unwanted molecules and immune cells into the brain. This so-called blood–brain barrier (BBB) is composed of highly specialized brain endothelial cells (ECs) that line the capillary wall. These specialized ECs form a tight barrier by membrane efflux pumps that drive cellular exclusion of unwanted compounds and the expression of complex tight junctions [
1‐
4], which actively limit cellular infiltration into the brain. The ECs are enclosed together with pericytes within the basement membrane onto which astrocytes firmly project their endfeet, thereby maintaining the barrier properties within the endothelium [
5]. Strikingly, several neuroinflammatory and neurodegenerative diseases such as multiple sclerosis (MS), human immunodeficiency virus-associated dementia, capillary cerebral amyloid angiopathy and stroke are associated with an impaired function of the BBB [
6‐
9]. Especially in MS, an altered BBB function leads to enhanced entry of immune cells and potentially toxic compounds into the CNS [
10‐
12]. To date, it remains largely unknown which mechanisms underlie the altered BBB in such neurological disorders. The identification of targets to restore impaired barrier function may provide novel tools for treatment.
Sphingosine 1-phosphate (S1P) binding G-protein-coupled receptors (GPCRs) are thought to be involved in the regulation of the vasculature. In general, S1P signals through five GPCRs belonging to the endothelial differentiation gene (EDG) family which entails: S1P
1 (EDG-1), S1P
2 (EDG-5), S1P
3 (EDG-3), S1P
4 (EDG-6), and S1P
5 (EDG-8). The S1P receptors are coupled to different G-proteins resulting in divergent downstream signaling pathways. For example, S1P
1 is proposed to couple to Gα
i and Gα
o whereas S1P
5 is through to interact with Gα
i, Gα
o, Gα
12, and Gα
13[
13]. Consequently, signaling of S1P through its receptors affects a broad variety of signaling processes ranging from pathways involved in cell survival, proliferation, motility to differentiation. S1P receptors are essential in proper vascular development because deficiency of for example S1P
1 results in early embryonic death due to defects in vascular maturation [
14]. Moreover, numerous S1P-driven EC responses are reported and are found to be crucial for proper development, maintenance and regulation of peripheral vascular beds. S1P-mediated effects on the function of the endothelium are attributed to modulation of S1P
1 and S1P
3. S1P receptors are currently under extensive investigation because clinical trials demonstrate significant reduction of disease severity in neurological (autoimmune) disease models by targeting these receptors [
15‐
19]. In addition, two phase III clinical trials (TRANSFORMS, FREEDOMS) concerning the S1P receptor modulator FTY720P (Gilenya®) for treatment of relapsing remitting MS deliver robust data demonstrating greatly reduced relapse rates, significant reduction in lesion activity, and lower risk of disability progression [
20,
21].
The recent availability of non-selective and selective S1P receptor agonists has led to an increasing amount of data about S1P receptor expression and their impact on cellular function in the CNS. Apparent CNS effects of S1P receptor modulators such as FTY720P and S1P itself are translated into for example reduced immune cell infiltration across the brain vasculature [
19,
22‐
24]. Recently, we demonstrated increased astrocytic S1P
1 and S1P
3 expression in active MS lesions and an anti-inflammatory effect of FTY720P (active form of FTY720) on primary human astrocyte cultures [
25]. Interestingly, although S1P
1-4 receptors are widely expressed throughout the body, S1P
5 expression is more or less restricted to the brain. It was therefore the aim of this study to investigate the involvement of S1P
5 in underlying inflammatory processes in the CNS leading to MS lesion development. We here show that S1P
5 is primarily expressed on brain ECs in human brain suggesting a key role of S1P
5 in BBB maintenance. Our functional studies show that S1P
5 is not only crucial for the maintenance of the BBB but is also a key modulator of endothelial inflammation processes. Ultimately, specific targeting of vascular S1P
5 and subsequent repair of the BBB in patients with inflammatory disorders may have therapeutic benefits.
Methods
Autopsy material
Brain tissue from three non-neurological controls (Table
1) was obtained at rapid autopsy and immediately frozen in liquid nitrogen or fixed in formalin (in collaboration with The Netherlands Brain Bank, coordinator Dr. Huitinga). The Netherlands Brain Bank received permission to perform autopsies for the use of tissue and for access to medical records for research purposes from the Ethical Committee of the VU University Medical Center, Amsterdam, The Netherlands. Tissue samples from control cases without neurological disease were taken from the subcortical white matter. All controls, or their next of kin, had given informed consent for autopsy and the use of their brain tissue for research purposes.
Table 1
Clinical data of non-neurological controls
Control | 89 | NA | F | 6 | NA | Old age |
Control | 89 | NA | M | 16 | NA | Dehydration |
Control | 84 | NA | F | 5 | NA | Resp. failure |
Immunohistochemistry
For immunohistochemical analysis, 5-μm cryosections were processed and stained as described previously [
26]. Briefly, sections were incubated overnight at 4 °C with primary antibodies against S1P
5 (1:200) (Santa Cruz Biotechnology, Santa Cruz, CA, USA and Imgenex, San Diego, CA, USA). Subsequently, sections were incubated with EnVision + Dual Link (DAKO, Glostrup, Denmark) according to the manufacturer’s description. Diaminobenzidine tetrachloride (DAB; DAKO, Glostrup, Denmark) was used as the chromogen. Antibodies were diluted in PBS containing 0.1% bovine serum albumin (BSA; Boehringer Mannheim, Mannheim, Germany), which also served as a negative control. For colocalization studies, sections were incubated for 30 minutes with 5% goat serum. Subsequently, sections were incubated with primary antibodies as described above and with mouse anti-CD31 (1:200; DAKO, Glostrup, Denmark). Sections were then incubated with goat anti-mouse Alexa 488 and goat anti-rabbit Alexa 594 secondary antibodies (1:400 Molecular Probes, Eugene OR, USA). Omission of primary antibodies served as a negative control. Incubation of tissue sections with isotype controls or no secondary antibody showed no immunoreactivity.
Endothelial cell culture
The human brain EC line hCMEC/D3 was kindly provided by Prof. P-O. Couraud (Institut Cochin, Université Paris Descartes, Paris, France) [
27] and grown in Endothelial Cell Basal Medium-2 supplemented with hEGF, hydrocortisone, GA-1000, FBS, VEGF, hFGF-B, R
3-IGF-1, ascorbic acid and 2.5% fetal calf serum (FCS; EGM-2, Lonza, Basel, Switzerland). Cells were cultured as described before [
28].
Lentiviral shRNA for S1P5 knockdown
Selective gene knockdown was obtained by using a vector-based short hairpin (sh) RNA technique as described before [
29]. Plasmids encoding S1P
5-specific shRNAs were obtained from Sigma (TRCN0000004752, St Louis, MO, USA). Recombinant lentiviruses were produced by co-transfecting subconfluent HEK 293 T cells with the specific expression plasmids and packaging plasmids (pMDLg/pRRE, pRSV-Rev and pMD2G) using calcium phosphate as a transfection reagent. HEK 293 T cells were cultured in DMEM supplemented with 10% FCS, 1% penicillin/streptomycin, in a 37 °C incubator with 5% CO
2. Infectious lentiviruses were collected 48 hours after transfection and stored at −80 °C. Subsequently, lentiviruses expressing S1P
5-specific shRNA were used to transduce hCMEC/D3 cells. Control cells were generated by transduction with lentivirus expressing non-targeting shRNA (SHC002, Sigma, St Louis, MO, USA). Forty-eight hours after infection of hCMEC/D3 cells with the shRNA-expressing lentiviruses, stable cell lines were selected by puromycin treatment (2 μg/ml). The expression knockdown efficiency was determined by quantitative PCR (qPCR).
Quantitative PCR
All oligonucleotides were synthesized by Ocimum Biosolutions (Ocimum Biosolutions, Ijsselstein, The Netherlands) (Table
2), RNA was isolated using the Aurum
TM Total RNA capture kit (Biorad, CA, USA) according to the manufacturer’s instructions. cDNA was synthesized with the Reverse Transcription System kit (Promega, Madison, WI, USA) following manufacturer’s guidelines as described previously [
30]. qPCR reactions were performed in an ABI7900HT sequence detection system with the SYBR Green method (Applied Biosystems, Carlsbad, CA, USA). Obtained expression levels of transcripts were normalized to GAPDH expression levels.
S1P1
| 5′-TGCGGGAAGGGAGTATGTTT-3′ | 5′-CGATGGCGAGGAGACTGAAC-3′ |
S1P2
| 5′-TCTCTACGCCAAGCATTATGTGC-3′ | 5′-TGGCCAACAGGATGATGGA-3′ |
S1P3
| 5′-TGCAGCTTCATCGTCTTGGAG-3′ | 5′-GCCAATGAAAAAGTACATGCGG-3′ |
S1P5
| 5′-CCTTGGTGGCATGTTGGG-3′ | 5′-GGGTTCAGAAGTGAGTTGGG-3′ |
GLUT | 5′-GCCCCTGTGAAGATTGAGAG-3′ | 5′-CCCGAAGCAGCCAATCC-3′ |
BCRP | 5′-AGATGGGTTTCCAAGCGTTCAT-3′ | 5′-CCAGTCCCAGTACGACTGTGACA-3′ |
PGP | 5′-GTCCCAGGAGCCCATCCT-3′ | 5′-CCCGGCTGTTGTCTCCATA-3′ |
VE-cadherin | 5′-TGACGTGAACGACAACTGGC-3′ | 5′-GACGCATTGAACAACCGATG-3′ |
Claudin-5 | 5′-GCCCCTGTGAAGATTGAGAG-3′ | 5′-CCCGAAGCAGCCAATCC-3′ |
TNF-α | 5′-CCAAGCCCTGGTATGAGCC-3′ | 5′-GCCGATTGATCTCAGCGC-3′ |
IL-1β | 5′-GCTGATGGCCCTAAACAGATG-3′ | 5′- GCAGAGGTCCAGGTCCTGG-3′ |
IL-8 | 5′-TGAGAGTGGACCACACTGCG-3′ | 5′-TCTCCACAACCCTCTGCACC-3′ |
MCP-1 | 5′-ATCTCAGTGCAGAGGCTCGC-3′ | 5′-GCACAGATCTCCTTGGCCAC-3′ |
VCAM | 5′-TGAAGGATGCGGGAGTATATGA-3 | ′5′-TTAAGGAGGATGCAAAATAGAGCA-3 |
ICAM | 5′-TAGCAGCCGCAGTCATAATGGG-3′ | ′5′-AGGCGTGGCTTGTGTGTTCG-3 |
Western blot
Cell homogenates were prepared by replacing the culture medium with sodium dodecyl sulfate (SDS) sample buffer containing 5% ß-mercaptoethanol and subsequent heating at 95 °C for 5 minutes. Samples were separated by SDS-PAGE and blotted onto nitrocellulose membranes. Membranes were blocked with Odyssey block buffer and incubated with an antibody against S1P5 (Santa Cruz Biotechnology, Santa Cruz, CA, USA). Binding was visualized using the Odyssey® Infrared Imaging System after application of IgG labeled with Infrared dye (IRdye) 800 (Rockland Immunochemicals, Gilbertsville, PA, USA). For quantification, S1P5
.protein levels were corrected for tubulin using a specific anti-tubulin antibody (Cedarlane, Canada). The basal expression of p65 in S1P5 knockdown and control cells was assessed with a rabbit anti-p65 antibody (Cell Signaling Technology, Danvers, MA, USA) followed by secondary donkey anti-rabbit 800 (IRDye). Protein expression was normalized to beta-actin (Santa Cruz Biotechnology, Santa Cruz, CA, USA) detected with donkey anti-goat 680 (IRDye).
Immunocytochemistry
Transduced (mock and S1P5) hCMEC/D3 cells were plated in collagen coated μ-slide 8 well slides (Ibidi, Martinsried, Germany) and cultured as described before. Upon confluence, cells were cultured in Endothelial Cell Basal Medium-2 containing 2,5% human serum and 5 ng/ml basic fibroblast growth factor (bFGF) overnight and fixed in 4% formaldehyde (Sigma, St Louis, MO, USA) in PBS (Gibco) in the presence of 0.5% Triton (Sigma, St Louis, MO, USA). Cells were washed and blocked with PBS containing 0.1% BSA (Sigma, St Louis, MO, USA) and 5% normal goat serum (NGS). Subsequently, cells were incubated with mouse anti-VE-cadherin primary antibody (1:500: Becton & Dickinson, San Jose, CA, USA) in PBS containing 0.1% BSA and 5% NGS overnight. Cells were washed and incubated with goat anti-mouse Alexa 488 secondary antibody (1:400: Molecular Probes, Eugene OR, USA). After washing the cells with PBS, rhodamine phalloidin (1:300) (Molecular Probes, Eugene OR, USA) was used for F-actin staining and Hoechst (1:1000 Molecular Probes, Eugene OR, USA) for nuclear staining.
Electrical cell-substrate impedance sensing
Transendothelial electric resistance in confluent monolayers of hCMEC/D3 cells was measured using an electrical cell-substrate impedance sensing (ECIS) model ZTheta (Applied BioPhysics, NY, USA) and 8W10E + arrays. In short, 300 μl cell suspension (1,0 × 10
5 cells) was added to in each well in Endothelial Cell Basal Medium-2 supplemented with 2,5% human serum and 5 ηg/ml bFGF. Cells were seeded in medium containing dimethyl sulfoxide (DMSO; 1 μM serving as vehicle control), FTY720P (1 μM), or a S1P
5 selective agonist (1 μM compound 18, a kind gift from Professor Stephen Hanessian, Université de Montreal, Montreal, Canada) [
31]. Prior to seeding the collagen-coated ECIS arrays were equilibrated with growth medium and Rb values were calculated using ECIS software version 1.2.55.0 PC.
Permeability of the brain endothelial layer
Permeability of human brain EC monolayers was analyzed as described previously [
28]. hCMEC/D3 and hCMEC/D3 S1P
5 knockdown cells were seeded at confluence onto collagen-coated Costar Transwell filter (pore-size 0.4 μm; Corning Incorporated, Corning, NY, USA) in growth medium containing 2.5% FCS and grown for 4 days. Paracellular permeability to FITC-dextran (150 kDa, 500 μg/ml in culture medium; Sigma, St Louis, MO, USA-Aldrich) in the apical to basolateral direction was assayed at various time points. Samples were collected from the acceptor chambers for measurement of fluorescence intensity using a FLUOstar Galaxy microplate reader (BMG Labtechnologies, Offenburg, Germany), excitation 485 nm and emission 520 nm.
Monocyte migration
Human blood monocytes were isolated from buffy coats of healthy donors (Sanquin, Blood Bank, Amsterdam, NL) by Ficoll gradient and CD14-positive beads [
32]. Control and S1P
5 knockdown hCMEC/D3 cells were seeded at confluence onto collagen-coated Costar Transwell filters (pore-size 5 μm; Corning Incorporated, Corning, NY, USA) in growth medium containing 2.5% FCS and were grown for 4 days. ECs were exposed to DMSO (1 μM) as a vehicle control, FTY720P (1 μM) or S1P
5 agonist (1 μM) agonist for 16 hours and washed prior to addition of monocytes [
31]. Hereafter, 100 μl 1.6 × 10
6/ml primary human monocytes suspended in Endothelial cell Growth medium-2 containing 2,5% FCS were added to the upper compartment for 8 hours at 37°C, 5% CO
2 in air. Next, the suspension in the lower compartment containing transmigrated monocytes was harvested and quantified using anti-CD14 beads (Flow-count fluorospheres, BeckmanCoulter, Inc., Brea, CA, USA) and subsequent FACScan flow cytometer (Becton & Dickinson, San Jose, CA, USA) analyses.
Monocyte adhesion assay
Monocyte adhesion to confluent monolayers of control and S1P5 knockdown hCMEC/D3 cells was analyzed by using primary human monocytes isolated as described before. Human monocytes were fluorescently labeled with 0.5 μM calcein-Am (Molecular Probes, Eugene OR, USA) and suspended in RPMI + 0.5% BSA + 25 mM Hepes to a final concentration of 1 × 10
6 cells [
33]. A standard curve of human monocytes was made with 0, 12.5, 25, 50, and 100% of this cell suspension. ECs were washed and monocytes were added and incubated for 5, 15, 30, and 60 minutes in a 37 °C incubator with 5% CO
2. Non-adherent cells were removed and adherent cells were lysed with 0.1 M NaOH. Fluorescence intensity was measured (FLUOstar Galaxy, BMG Labtechnologies, Offenburg, Germany; excitation 480 nm, emission 520 nm) and the number of adhered monocytes was calculated using the standard [
33].
Flow cytometric analysis
Control and S1P
5 knockdown hCMEC/D3 cells were detached from 24-well culture plates, washed and incubated with monoclonal mouse anti-intercellular adhesion molecule-1(ICAM-1) (Rek-1, 5 μg/ml, a kind gift from the Department of Tumour Immunology, University Medical Center St. Radboud, Nijmegen, The Netherlands) or mouse anti-vascular cell adhesion molecule-1(VCAM-1; AbD Serotec, UK) for 30 minutes at 4 °C [
34]. Binding was detected using goat anti-mouse Alexa 488 (Molecular Probes, Eugene, OR). Omission of primary antibodies served as negative control. To investigate the role of Nuclear factor kappa-light-chain-enhancer of activated B cells (NFκB) in the enhanced inflammatory status of S1P
5 knockdown cells, the cells were treated for 16 hours with 4 μM NFκB inhibitor Bay 11–7085 (Sigma, MO, USA) or vehicle control. Fluorescence intensity was measured using a FACS Calibur flow cytometer (Becton & Dickinson, San Jose, CA, USA). The mean fluorescence intensity was used as a measure for the expression of ICAM-1 and VCAM-1.
Statistical analysis
Data are presented as ± SEM and were analyzed statistically by means of single-column t-test. Statistical significance was defined as *P <0.05, **P <0.002, and ***P <0.001.
Discussion
Our present study demonstrates the constitutive expression of the S1P receptor S1P5 by brain ECs, constituting the BBB in human brain and its involvement in both integrity and regulation of the inflammatory status of the brain endothelium. We have delineated a role for S1P5 in the induction of specific BBB properties such as low paracellular permeability and the expression of key brain endothelial proteins such as tight junction and specific ATP binding cassette and glucose transporter molecules. We have assessed the potential therapeutic improvements upon pharmacological modulation of S1P5 receptor activity in gaining barrier function. Moreover, the lack of S1P5 provoked a proinflammatory status of brain endothelium as shown by enhanced transendothelial migration of monocytes and increased production of proinflammatory molecules and adhesion molecules for leukocytes, a process which was mediated by NF-κB activation.
Within our findings, we showed the non-selective S1P receptor agonist FTY720P and a selective S1P
5 agonist both improve brain endothelial function through the increase of the paracellular resistance in the immortalized human brain EC line, hCMEC/D3. This cell line reflects the key features of primary brain ECs such as high TEER, expression of tight junctions and transporter molecules. Our results are in line with previous reports on the endothelial barrier enhancing effect of FTY720P on pulmonary ECs, human microvascular ECs, and human umbilical vein ECs [
22,
36‐
38]. However, we are the first to show that selective activation of S1P
5 induces a significant increase in paracellular resistance of brain ECs. Moreover, in concordance with ECs exposed to FTY720P, brain endothelium exposed to a selective S1P
5 agonistic compound prevented the transendothelial passage of monocytes in a similar fashion [
31]. Enhanced endothelial barrier integrity is probably the result of the enhanced expression of tight junction and adherent junction proteins and their localization at the cell–cell contacts, as was shown in this study. To date, there is emerging evidence that S1P
1 and S1P
3 play an important role in the maintenance of endothelial function. For instance, it has been described that the assembly of junction proteins to the cell–cell junctions is dependent on S1P
1 and S1P
3-induced signaling pathways, involving the small GTP-ases Rac and Rho [
39]. Strikingly, in our S1P
5-deficient brain ECs a significant reduction of S1P
1 and S1P
3 was detected, indicating that S1P
5 is involved in the expression of these receptors. Given the importance of S1P
1 and S1P
3 in the maintenance of vascular function, the reduced barrier function of the brain endothelium due to the lack of S1P
5 may also be in part caused by the lack of S1P
1 and S1P
3. Together, our findings point to an important function of S1P
5 in the regulation of the barrier phenotype of brain ECs.
Besides improving barrier function, the current report shows that targeting of S1P
5 is important for maintenance of the immunoquiescent state of brain ECs. First, our results reveal a prominent role for S1P
5 in maintaining low expression levels of leukocyte adhesion molecules, including VCAM-1 and ICAM-1, and several important proinflammatory cytokines and chemokines, such as TNF-α and MCP-1. In addition, S1P
5 activation limits monocyte adhesion to and migration over the brain endothelial barrier, which is an initial step in the formation of new MS lesions. Therefore, our findings are of potential interest for future treatment of neuroinflammatory disorders that are marked by a cellular migration across the vessel wall. Modulation of the S1P receptors through FTY720P was shown to be protective in various experimental animal models with neuroinflammation in the brain [
19,
40,
41]. Moreover, in other vascular disorders, such as atherosclerosis, FTY720P exerts protective effects by dampening ongoing inflammatory processes in the vascular smooth muscle cells. In the validated experimental animal model for MS, experimental allergic encephalomyelitis FTY720P was either given as a prophylactic, therapeutic or as a rescue agent. In these animals, FTY720P treatment resulted in a delayed onset of disease and reduced disease severity through the induction of lymphopenia. Besides its general immunosuppressive effect, FTY720P treatment also reduced the expression of vascular adhesion molecules and cytokines in the spinal cord of treated animals [
19]. Moreover, in models of brain ischemia FTY720P was able to reduce infarct size and could, in transient focal cerebral ischemia, positively regulate neurological deficits. Observed beneficial effects were associated with a reduction in activated neutrophil and microglia/macrophage cell numbers and, in line with our results, also with reduced numbers of ICAM-1 positive blood vessels [
41]. However, these studies did not investigate the role of endothelial S1P signaling, which may play a crucial role in the early onset of disease [
40]. Several
in vitro studies support the notion that S1P signaling is relevant in ECs because it was shown that S1P or/and FTY720P limit leukocyte adhesion and transmigration into the vessel wall in the early atherosclerosis pathology. In addition, S1P
1 modulation resulted in reduced endothelial production of TNF-α-induced production of proinflammatory chemokines [
42‐
44]. Given that both S1P and FTY720P are general modulators of all S1P receptors, it remains unclear which specific receptor is involved in these processes. More specifically, it is unclear what the role of the brain-specific S1P
5 receptor is in these processes. Our study clearly shows that S1P
5 receptors might play a crucial role in barrier formation and immunoquiescence. Although this study utilized a selective S1P
5 receptor agonist, it is important to identify new more potent and more selective S1P
5 tools to fully elucidate the mechanism by which S1P
5 might exert these effects.
We are also the first to show that NF-κB underlies the anti-inflammatory activity of endothelial S1P
5. To date, no data exist on the downstream signaling pathways in ECs upon activation of S1P
5. It has been shown that incubation of mouse aortas from type 1 non-obese diabetic mice with S1P reduces VCAM expression and monocyte adhesion to the endothelium. The authors also show that S1P
1 is the receptor that mediates this anti-inflammatory response to S1P, which is related to the inhibition of NFkB translocation to the nucleus. In accordance with these findings, our results suggest an anti-inflammatory role for S1P
5 in brain ECs. Furthermore, in Chinese Hamster Ovary-K1 cells it was demonstrated that S1P
5 expression results in inhibition of extracellular signal-regulated kinase (ERK) activity [
45]. Since ERK activity is a potent regulator of NFκB-dependent inflammatory responses, this pathway may be responsible for the observed increase in NF-κB driven of ICAM-1 and VCAM expression in S1P
5 knockdown brain ECs.
Competing interests
The authors declare that they have no competing interests.
Authors’ contributions
RvD carried out the experiments, analyzed the data and drafted the manuscript. MALP carried out the NFκB analyses. GK performed the transmigration studies. KL, BvhH and SvdP did the culture work and participated in the qPCR analyses. DG provided the shRNA construct. JvH and PvdV were responsible for the human brain tissues and immunohistochemical analyses. EvdK and ER participated in design and coordination, provided useful advice and reviewed the manuscript. AR and HEdV participated in the design and coordination, and wrote and reviewed the manuscript. All authors read and approved the final manuscript.