The pulmonary microvasculature plays a critical role in endotoxin-induced acute lung injury. However, the relevant signaling remain unclear. Specifically the role of endothelial Ca2+ in the induction of endotoxin-mediated responses in lung microvessels remains undefined. Toward elucidating this, we used the isolated blood-perfused rat lung preparation. We loaded microvessels with the Ca2+ indicator, Fura 2 AM and then determined Ca2+ responses to infusions of lipopolysaccharide (LPS) into the microvessels. LPS induced a more than two-fold increase in the amplitude of cytosolic Ca2+ oscillations. Inhibiting inositol 1,4,5 trisphosphate receptors on endoplasmic reticulum (ER) Ca2+ stores with Xestospongin C (XeC), blocked the LPS-induced increase in the Ca2+ oscillation amplitude. However, XeC did not affect entry of external Ca2+ via plasma membrane Ca2+ channels in lung microvascular endothelial cells. This suggested that LPS augmented the oscillations via release of Ca2+ from ER stores. In addition, XeC also blocked LPS-mediated activation and nuclear translocation of nuclear factor-kappa B in lung microvessels. Further, inhibiting ER Ca2+ release blunted increases in intercellular adhesion molecule-1 expression and retention of naïve leukocytes in LPS-treated microvessels. Taken together, the data suggest that LPS-mediated Ca2+ release from ER stores underlies nuclear factor-kappa B activation and downstream inflammatory signaling in lung microvessels. Thus, we show for the first time a role for inositol 1,4,5 trisphosphate-mediated ER Ca2+ release in the induction of LPS responses in pulmonary microvascular endothelium. Mechanisms that blunt this signaling may mitigate endotoxin-induced morbidity.
Citation: Kandasamy K, Bezavada L, Escue RB, Parthasarathi K (2013) Lipopolysaccharide Induces Endoplasmic Store Ca2+-Dependent Inflammatory Responses in Lung Microvessels. PLoS ONE 8(5): e63465. https://doi.org/10.1371/journal.pone.0063465
Editor: Salvatore V. Pizzo, Duke University Medical Center, United States of America
Received: January 12, 2013; Accepted: April 3, 2013; Published: May 10, 2013
Copyright: © 2013 Kandasamy et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This study was funded by the National Heart, Lung, and Blood Institute, National Institutes of Health, grant number HL75503. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Sepsis is characterized by rapid retention of leukocytes in lung microvessels. Vascular administration of endotoxin (lipopolysaccharide; LPS), a model of sepsis, reveals a major role for the endothelium in this process. Using real-time fluorescence imaging, we recently reported that targeted infusion of LPS into lung capillaries and venules increased endothelial intercellular adhesion molecule-1 (ICAM-1) expression and augmented retention of LPS-untreated naïve leukocytes . Thus, endothelial mechanisms by themselves may be critical in initiating LPS-induced pathophysiological responses. However, signaling that underlies LPS-induced ICAM-1 expression in lung microvessels remains unclear.
In endothelial cells, LPS acting via toll-like receptor 4 (TLR4) initiates transcriptional upregulation of proinflammatory and adhesion molecules , . Our previous findings showed that the magnitude of the LPS-induced increase in ICAM-1 expression in microvessels was proportional to the duration post-LPS treatment, suggesting transcriptional regulation of ICAM-1. LPS-mediated induction of adhesion molecules in endothelial cells involves activation of nuclear factor-kappa B (NF-κB) –. Ca2+, in tandem with calmodulin, can activate NF-κB and downstream gene transcription in multiple cell types –. Recent evidence suggests that in lung endothelial cell monolayers, increase in cytosolic Ca2+ underlies LPS-induced inflammatory responses . However, in pulmonary microvessel segments, it remains unknown whether Ca2+ plays a role in the induction of LPS-mediated responses.
In lung microvessels, cytosolic Ca2+ plays a role in the induction of proinflammatory responses elicited by both receptor-mediated and -independent agonists –. Receptor-mediated agonists induce release of Ca2+ from endoplasmic reticulum (ER) Ca2+ stores, via the second messenger inositol 1,4,5-trisphosphate (IP3) , , . In contrast, receptor-independent agonists initiate entry of external Ca2+ via plasma membrane Ca2+ channels . Release of Ca2+ from ER stores is associated with modulations in the amplitude and frequency of cytosolic Ca2+ oscillations –, which in turn can regulate nuclear transcription factors , –. However, in lung microvessels, both the characteristic of the LPS-induced Ca2+ response and its role in initiating downstream signaling remain undefined.
Toward this, we determined endothelial cytosolic Ca2+ responses to infusions of LPS into lung microvessels using the isolated blood-perfused rat lung model. We then established the role of Ca2+ in the induction of downstream responses. Our data revealed that LPS initiates release of Ca2+ from ER stores, which then mediates the increase in endothelial ICAM-1 expression and microvascular leukocyte retention.
Materials and Methods
Animal use and studies were approved by the Institutional Animal Care and Use Committee of the University of Tennessee Health Science Center. Animals were housed and maintained by our Lab Animal Care Unit accredited by the Association for Assessment and Accreditation of Laboratory Animal Care. Animals were given access to feed and water ad libitum, and placed on a 12 h light-dark cycle. Surgery was only done on animals that were anesthetized and confirmed to be under a surgical plane of anesthesia.
Adult male Sprague-Dawley rats weighing 250–350 g were anesthetized by intraperitoneal injection of Ketamine/Xylazine and exanguinated by cardiac puncture. The chest wall was opened and the pulmonary artery and left atrium were cannulated. Subsequently, the lungs and heart were excised en bloc and placed on a microscope stage. The lungs were constantly inflated at an airway pressure of 5 cmH2O and continuously pump-perfused at 14 ml/min with autologous blood warmed to 37°C. The pulmonary artery and left atrial pressures were maintained at 10 and 3 cmH2O, respectively. The lung surface was kept moist with saline throughout the experiment.
Endothelial Cell Culture
Primary rat lung microvascular endothelial cells (RLMVEC) were purchased from VEC Tech (Rochester, NY) and cultured in medium 199 supplemented with growth factors. RLMVEC were used in passage numbers 3–5.
LPS from E. coli (serotype 0111:B4), nuclear stain Hoechst-33342, Ficoll gradient Histopaque-10771, and rhodamine 6G (R6G) were from Sigma Aldrich (St. Louis, MO). Inhibitors Xestospongin C (XeC) and 2,5-Di-(t-butyl)-1,4-hydroquinone (t-BHQ) were from Calbiochem/EMD Millipore (Billerica, MA). KappaB-kinase NEMO-binding domain (IKK-NBD) peptide and 1-oleoyl;-2-acetyl-sn-glycerol (OAG) were from Enzo Life Sciences (Farmingdale, NY). Alexa-Fluor 488-conjugated goat anti-mouse secondary Ab and Alexa-Fluor 488-conjugated goat anti-rabbit secondary Ab were from Invitrogen/Life Technologies (Grand Island, NY). Mouse monoclonal anti-ICAM-1 antibody and anti-NF-κB p65 TRITC-conjugated Ab were from Santa Cruz Biotechnology (Santa Cruz, CA). Anti-phosphoSer536 NF-κB p65 antibody was from Cell Signaling (Danvers, MA). The Ca2+ indicator Fura2-AM was from Invitrogen. All other chemicals were from Sigma.
Agents and leukocytes were infused into microvessels in a calcium rich HEPES-buffered Ringer’s solution (HBS; 150 mM Na+, 5 mM K+, 1 mM Ca2+, 1 mM Mg2+, 10 mM glucose, 20 mM HEPES) with 4% dextran (40 kDa) and 1% fetal bovine serum. Ca2+-free HBS was prepared as similar to HBS, but without adding Ca2+. Prior to infusion into microvessels, 4% dextran and 0.05 mM EGTA were added to Ca2+-free HBS. Both HBS and Ca2+-free HBS were adjusted to a final pH of 7.4.
A portion of the autologous blood was set aside for leukocyte isolation as described previously . In brief, leukocytes were isolated using a Ficoll gradient, washed with phosphate-buffered saline, counted with a hemocytometer, and labeled with R6G (2 µM). The final concentration was adjusted to 100000 leukocytes/ml in HBS.
Real-time Fluorescence Microscopy
The isolated blood-perfused rat lung was positioned on a custom-made stage. A PE10 (BD Biosciences, Sparks, MD) microcatheter was introduced through the left atrial cannula and blood cell-free conditions were established in microvessels by flushing with HBS in a small portion of the lung. We infused either HBS or LPS (100 µg/ml) for 30 min into microvessels, and then washed off luminal LPS with infusion of HBS for 60 min.
Subsequently, R6G-labeled leukocytes were infused by microcathether into the LPS-treated microvessels and their transit through the vessel was imaged in real-time using a fluorescence microscope (BX61WI, Olympus America, Center Valley, PA) fitted with the appropriate interference filters (excitation 545 nm and emission >560 nm). At the end of leukocyte infusion, we flushed the vessels with HBS. We then captured images of several microvessels within the LPS-treated region.
Post-experiment, we analyzed the fluorescence images with Metamorph (Molecular devices, Sunnyvale, CA) and quantified the number of leukocytes retained in microvessels separately for all treatment groups.
In situ Immunofluorescence of ICAM-1, Phospho p65 and NF-kB by Confocal Microscopy
Expression of ICAM-1, phosphorylation of NF-κB p65 subunit, and nuclear translocation of NF-κB p65 subunit were determined by in situ immunofluorescence as previously reported , . In brief, following LPS (100 µg/ml) infusion for 30 min and subsequent HBS wash for 60 min, we fixed the microvessels with 3.7% paraformaldehyde. However for establishing phosphorylation of NF-κB p65 subunit, the microvessels were fixed immediately following 30 min of LPS infusion. For ICAM-1 and phosphorylation of NF-κB p65 determinations, we infused the primary Ab (10 µg/ml) for 30 min, followed by a brief HBS wash, and then a fluorophore-tagged secondary Ab (10 µg/ml) for 30 min. For NF-κB translocation determination, we infused the TRITC-tagged primary Ab for 30 min. After the antibody infusions, we washed off excess Ab with HBS and imaged microvessels with a confocal laser scanning imaging system (LSM-710; Zeiss, Thornwood, NY). In experiments to determine phosphorylation of NF-κB p65 and NF-κB p65 nuclear translocation, we infused the nuclear marker Hoechst-33342 (10 µg/ml).
To determine the role of IP3-mediated ER Ca2+ release, we pretreated microvessels for 10 min before LPS infusion with XeC (25 µM) or t-BHQ (10 µM) with Ca2+ free HBS. To inhibit NF-κB, we infused IKK-NBD peptide (100 µM) that selectively inhibits NF-κB activation, for 30 min before and during LPS infusion.
Cytosolic Ca2+ Determinations in Microvessels
To determine endothelial cytosolic Ca2+, we loaded microvessels with the cell-permeable ratiometric Ca2+ indicator Fura2-AM (10 µM) for 30 min. We then obtained images of the microvessels with our fluorescence microscope by exciting sequentially at 340 and 380 nm, and collecting the fluorescence emission at 515 nm. Images were obtained at 10 s intervals. The fluorescence emissions from both 340 and 380 excitations were quantified at a single region along a vessel wall. Changes in Ca2+ were indicated as changes in the ratio of the fluorescence emissions at 340 and 380 nm (F340/F380).
F340/F380 oscillation amplitude in lung microvessels were determined as reported previously . In brief, temporal changes in F340/F380 for venules and capillaries were plotted separately. Then, the oscillation amplitude was quantified for three consecutive oscillations and the mean was taken as the amplitude of Ca2+ oscillation. The results were confirmed by a blinded analysis.
To quantify baseline F340/F380 in a vessel, the value at a single region on the vessel wall was determined for 15 consecutive images, and then the mean F340/F380 quantified.
Cytosolic Ca2+ Determinations in RLMVECs
RLMVECs were loaded with Fura2-AM for 40 min and washed with cell culture media. The cells were then imaged using parameters described above for microvessels. Images of cells were obtained from several distinct regions within a culture dish. After obtaining a series of images at baseline, either LPS (1 µg/ml) or OAG (100 µM) was added to the media and the imaging continued. To determine the role of IP3 receptor inhibition, RLMVECs were pretreated with XeC (10 µM) for 20 min before agonist treatment.
To quantify F340/F380 in RLMVEC, an outline was drawn around cells in the image field and the F340/F380 calculated. For each RLMVEC, F340/F380 was calculated from three consecutive images and the mean taken as the F340/F380 for that cell. For each culture dish, a minimum of three cells per region and greater than three regions per dish were analyzed.
LPS Increased the Magnitude of Cytosolic-Ca2+ Oscillation in Lung Microvessels
Fluorescence images of lung microvessels, loaded with the cytosolic Ca2+ indicator Fura2-AM (Figure 1A, B) were captured at 10 s interval and the corresponding F340/F380 fluorescence ratio images (Figure 1C) were derived in real-time for the entire duration of an experiment. At baseline, mean F340/F380 in venules was slightly higher than that in capillaries (2.8±1.6%; range 0 to 9%; n = 6 lungs). Temporal changes in single vessel F340/F380 quantified from the images indicated that infusion of LPS into microvessels, induced a rapid increase in the amplitude of Ca2+ oscillations (Figure 1D). XeC infusion into microvessels, prior to LPS infusion, blunted the LPS-induced response (Figure 1D). As XeC blocks IP3 receptors on the ER, the inhibition suggested that LPS induced an IP3-mediated Ca2+ release from the ER. LPS induced a more than 2-fold increase in oscillation amplitude in both venules and capillaries (Figure 1E, F). XeC was effective in inhibiting the response in both microvessel segments (Figure 1E, F).
A–C Pseudocolor images show fluorescence emission in response to exciting Fura2-AM loaded microvessels at 340 nm (A) and 380 nm (B). The corresponding 340/380 fluorescence ratio was quantified on a pixel-by-pixel basis and displayed as a pseudocolored image (C). Scale bar = 20 µm. D. Tracings show temporal changes in F340/F380 in response to LPS infusions (100 µg/ml) into control (black tracing) and XeC-pretreated (gray tracing) lung microvessels. E, F Bar graphs show composite increase in the LPS-induced F340/F380 oscillation amplitude above baseline values for venules (E) and capillaries (F). Mean±SE. n = 4 vessels from 3 lungs per group. *-p<0.05 compared to XeC and XeC+LPS treatment groups.
To establish that XeC did not block entry of external Ca2+ via plasma membrane Ca2+ channels, we determined Ca2+ responses in RLMVEC. Fura2-AM loaded RLMVEC were treated with the OAG, a cell-permeable diacylglycerol analog, which induces entry of external Ca2+ through transient receptor potential canonical (TRPC) 6 on the plasma membrane , . OAG increased F340/F380 above baseline levels in RLMVEC (Figure 2A–F). Pretreating RLMVECs with XeC, did not affect the OAG-induced increase in cytosolic Ca2+ (Figure 2G). In contrast, as observed in microvessels, XeC blunted the LPS-induced increase in cytosolic Ca2+ increases in RLMVEC (Figure 2G). Thus, external Ca2+ entry via plasma membrane Ca2+ channels remained unaffected by XeC.
A–F Images show fluorescence emission intensity in response to exciting Fura2-AM loaded RLMVEC at 340 nm (A, D) and 380 nm (B, E) The corresponding 340/380 fluorescence ratio was quantified on a pixel-by-pixel basis and displayed as pseudocolored images (C, F). The images were obtained at baseline (A–C) and after OAG (100 µM) treatment (D-F). Scale bar = 20 µm. G. Bar graph shows increase in F340/F380 above baseline in RLMVEC treated with LPS (1 µg/ml) or OAG (100 µM), with and without XeC (10 µM) pretreatment (20 min). Mean±SE. n = 2−3 separate experiments and >50 RLMVECs per treatment group. *-p<0.05 compared to XeC+LPS treatment group.
ER Ca2+ Release Mediated LPS-induced ICAM-1 Expression in Lung Microvessels
We previously established that LPS increased ICAM-1 expression in pulmonary capillaries and venules . Here we defined the role of cytosolic Ca2+ in this response. In situ immunofluorescence images of ICAM-1 indicated that as compared to HBS, LPS infusion into microvessels increased venular and capillary ICAM-1 expression (Figure 3A,B). To define whether ER Ca2+ played a role in this response, we determined ICAM-1 expression in the presence of inhibitors of ER store Ca2+ release. In microvessels pretreated with XeC, the LPS-induced increase in ICAM-1 expression was lower (Figure 3C). In addition, pretreating microvessels with t-BHQ, which inhibits the Ca2+-ATPase pumps on ER , also limited the LPS-induced ICAM-1 expression (Figure 3D). XeC- and t-BHQ-dependent inhibition was evident in both venules and capillary microvessel segments (Figure 3F, G). Taken together, the data suggest a role for ER Ca2+ in the induction of LPS-induced ICAM-1 response in lung microvessels.
A–E Confocal images show immunofluorescence of ICAM-1 in lung microvessels following treatments as indicated. Treatment durations were as outlined in Methods. v-venule, c-capillary. Scale bar = 20 µm. F, G Bar graphs show ICAM-1 immunofluorescence intensity quantified along the vessel wall over the length of single microvessels for both venules (F) and capillaries (G). Mean±SE. n - number of vessels analyzed per group from a minimum of 2 lungs per group, except for XeC+LPS (3 lungs) and NBD (1 lung) groups. *-p<0.05 compared to HBS, XeC+LPS and NBD+LPS groups. BHQ = t-BHQ, NBD = IKK-NBD.
As NF-κB is known to play a role in the induction of LPS-induced responses, we blocked NF-κB activation with the peptide inhibitor, IKK-NBD. Infusion of IKK-NBD into microvessels prior to and during LPS infusion, blunted the LPS-induced increase in ICAM-1 expression (Figure 3E). The inhibition was evident in both venular and capillary microvessel segments (Figure 3F, G).
LPS-induced Leukocyte Retention in Lung Microvessels was Dependent on ER Ca2+ Release
Since LPS increased leukocyte retention in lung microvessel segments as reported previously , we determined whether this response was mediated by ER Ca2+ release. Fluorescence images reveal that retention of R6G-labeled naïve leukocytes in LPS-treated microvessels was higher than in HBS-treated leukocytes (Figure 4A, B). To define the role of ER Ca2+ in leukocyte retention, we first infused XeC into microvessels. Then, we infused LPS into these microvessels followed by infusion of R6G-labeled leukocytes. As evident from the fluorescence images, XeC completely blocked the increase in LPS-induced leukocyte retention (Figure 4C). This inhibition was significant in both capillaries and venules (Figure 4E, F). These data suggest that LPS-induced leukocyte retention in lung microvessels was dependent on ER Ca2+ release. In addition, blocking NF-κB activation by infusing IKK-NBD peptide into microvessels prior to LPS infusion, also blunted leukocyte retention (Figure 4D–F).
A–D Fluorescence images show retention of R6G-labeled leukocytes in lung microvessels following treatments, as indicated. Treatment durations and agent concentrations were as outlined in Methods. Scale bar = 20 µm. E, F Bar graphs show number of retained leukocytes per image frame in venules (E) and capillaries (F) following the indicated treatments. Mean±SE. n - number of images analyzed per group (3 lungs per group). *-p<0.05 compared to HBS, XeC+LPS and NBD+LPS groups. NBD = IKK-NBD.
ER Ca2+ Release Mediated LPS-induced NF-κB Activation in Lung Microvessels
To establish whether LPS activates NF-κB in an ER Ca2+-dependent manner, we determined phosphorylation of the p65 subunit of NF-κB in lung microvessels by in situ immunofluorescence. Confocal immunofluorescence images revealed that LPS increased p65 phosphorylation (Figure 5 A, B). The images also indicated that pretreating microvessels with XeC blunted the LPS-induced p65 phosphorylation (Figure 5C). The XeC-dependent inhibition was evident in both venules and capillaries (Figure 5D, E). Together, the data suggest that LPS-induced ER Ca2+ release mediated the phosphorylation of NF-κB p65 subunit in lung microvessels.
A–C Confocal immunofluorescence images show phosphorylation of the NF-κB p65 subunit in lung microvessels (green) and fluorescence of the nuclear marker Hoechst-33342 (blue) for the indicated treatments. Treatment durations and agent concentrations were as outlined in Methods. Scale bar = 20 µm. D, E Bar graphs show NF-κB p65 phosphorylation levels along the vessel wall over the length of single microvessels for both venules (D) and capillaries (E). Mean±SE. n - number of vessels analyzed per group. Each treatment repeated in 3 lungs each. *-p<0.05 compared to HBS and XeC+LPS groups.
Since the p65 subunit of NF-κB translocates to the nucleus upon activation , , we determined LPS-induced nuclear localization of NF-κB p65 by in situ immunofluorescence imaging. As evident from the confocal images, overlap between the NF-κB immunofluorescence and nuclear fluorescence was greater in LPS-treated microvessels compared to HBS-treated vessels (Figure 6A, B). Pretreating microvessels with XeC blunted the LPS-induced translocation, indicating that NF-κB activation and its translocation to the nuclear region were dependent on ER Ca2+ release (Figure 6C). In addition, the translocation was also lower in microvessels pretreated with the IKK-NBD peptide (Figure 6D).
Confocal images show immunofluorescence of NF-κB p65 subunit in lung microvessels (red, left column), fluorescence of the nuclear marker Hoechst-33342 (blue, column 2) and merge (column 3) for the indicated treatments. Pink color in the merged images indicates colocalization of NF-κB immunofluorescence and nuclear marker fluorescence. Treatment durations were as outlined in Methods. Nuclear localization of NF-κB immunofluorescence in the region marked by the rectangles (column 3 images) is shown magnified on far right column. Again, pink color indicates localization of NF-κB immunofluorescence (red) and nuclear marker fluorescence (blue). Treatment groups repeated in 3 lungs, except for NBD treatment group (n = 1). Note the higher colocalization in LPS-treated microvessels (B), compared to HBS-treated (A), and XeC- (C) and NBD-pretreated microvessels. NBD = IKK-NBD.
We show here for the first time that infusion of LPS into lung microvessels, induced release of Ca2+ from ER stores and attendant increase in the amplitude of cytosolic Ca2+ oscillations. In addition, our data also reveal that store Ca2+ release mediated the nuclear translocation of NF-κB. Thus, the current findings clearly attribute a major role for Ca2+ release from endothelial ER stores in the induction of LPS-induced inflammatory responses in lung microvessels.
LPS infusion into microvessels induced both the phosphorylation and nuclear translocation of the p65 subunit of NF-κB. However, pretreating microvessels with XeC limited both the phosphorylation and translocation, suggesting that Ca2+ release from ER stores mediated these responses. Further, the cell-permeable IKK-NBD peptide also blocked the translocation. IKK-NBD blocks association of the NF-κB essential modifier with the IKK complex and thus, NF-κB activation . Together the data suggest that LPS-mediated released of ER Ca2+ caused activation of NF-κB, leading to its nuclear translocation. While LPS-mediated NF-κB activation is well established , , , a role for store Ca2+ in this process is less defined. In addition, while store Ca2+ release has been indicated to mediate LPS responses in inflammatory cells , , , such a role remains unknown in endothelial cells. Our studies provide the first indication that release of Ca2+ from ER stores may play a role in LPS-induced NF-κB activation. Calmodulin, a calcium sensor that is activated upon binding Ca2+, may be an intermediary in the Ca2+-dependent NF-κB activation , , , . Whether calmodulin mediates the responses in pulmonary vasculature remains to be established. Since, even small increases in Ca2+ are reported to elicit NF-κB-dependent responses , , , it is possible that the present responses observed in the pulmonary microvessels may be sufficient to initiate activation of NF-κB and attendant downstream signaling.
Studies on LPS-induced responses, implicate influx of external Ca2+ via TRPC-permeable channels as the primary mechanism underlying cytosolic Ca2+ increase and downstream signaling , –. However, in this study the increase in Ca2+ oscillations were mediated by store Ca2+ release, as evinced by the inhibition of the LPS-induced response by the ER IP3 receptor blocker, XeC. This interpretation is supported by the finding that in RLMVEC, XeC did not inhibit cytosolic Ca2+ increases by OAG. As OAG induces entry of external Ca2+ via TRPC6 channels , , it is evident that XeC pretreatment had no direct effect on plasma membrane Ca2+ channels. In addition, using fluorescent probes that report store Ca2+ levels it has been shown previously that XeC inhibits store Ca2+ release, but not entry of external Ca2+ in lung microvessels . Taken together, our data clearly suggests that in lung microvessels the primary mechanism of endothelial Ca2+ increase by LPS is via IP3-dependent release of ER store Ca2+.
Previous studies in lung microvessels suggest that receptor-mediated agonists initiate IP3-dependent release of store Ca2+ . Since, the LPS-induced responses are also receptor-mediated, it follows that in lung microvessels LPS is likely to initiate Ca2+ release from ER stores. This possibility is supported by the observation that inhibiting ER Ca2+-ATPase pumps also blocked the LPS-induced ICAM-1 release. The difference in Ca2+ responses observed in this study from that recently reported in lung endothelial cells  may be attributed to signaling differences between micro- and macro-vascular endothelial cells. It is well established that agonist-induced responses and the underlying signaling are different in macro- vs micro-vascular endothelium . Our findings determined via focal infusions of LPS reveal signaling specific to microvessels and thus, the microvascular endothelium. These interpretations are further supported by the inhibition of LPS-induced Ca2+ increase in primary RLMVEC by blocking ER store Ca2+ release. Thus in pulmonary microvessels, we interpret that LPS signals via release of Ca2+ from ER stores.
The effect of LPS on lung microvessels was to increase the amplitude of cytosolic Ca2+ oscillations. Modulations in frequency and amplitude of cytosolic Ca2+ oscillations underlie several Ca2+-dependent signaling pathways in various cell types , , , –, –. In lung microvessels, an increase in the amplitude of cytosolic Ca2+ oscillation augmented reactive oxygen species production and P-selectin expression . Further, changes in Ca2+ oscillations activate transcriptional events, possibly via the action of calcium/calmodulin kinases –. These reports support our finding that increases in the amplitude of endothelial cytosolic Ca2+ oscillations induced by LPS lead to NF-κB translocation to the nucleus and an increase in ICAM-1 expression.
In the present study, ICAM-1 expression was elevated at 90 minutes post-LPS infusion. However, we reported that ICAM-1 expression was detectable in both venules and capillaries as early as 30 minutes after initiating LPS infusion . In contrast, in umbilical vein and pulmonary artery endothelial cells, induction of ICAM-1 expression by inflammatory stimuli, including LPS, thrombin, tumor necrosis factor-α, and interleukin-1β, occurs several hours after stimulus application –. This difference suggests that transcription of ICAM-1 is rapid in microvessels. LPS and other proinflammatory stimuli induce transcription in two stages; a first stage occurring within 30 minutes involves induction of immediate-early response genes, and a second stage occurring between 1 and 4 hours leads to the induction of primary and secondary response genes , –. In LPS-treated cells, these two stages parallel the two waves of NF-κB recruitment to the nucleus . As ICAM-1 expression was evident in lung microvessels after only 30 min of LPS treatment, it is likely ICAM-1 induction is part of the early response. It has been posited that factors involved in transcriptional regulation are primarily upregulated during the rapid first stage . Interestingly, antibody ligation of ICAM-1 in endothelial cells, a procedure that mimics leukocyte adhesion , itself initiates transcription of an early response gene, c-Fos  and the transcription factor complex, activator protein 1 . Moreover, we showed that leukocyte retention in lung microvessels parallels the increase in endothelial ICAM-1 expression, suggesting a role for ICAM-1 in the transcription process . Taking these together, we speculate that in lung microvessels LPS initiates rapid induction of ICAM-1 and concomitant increase in leukocyte adhesion to endothelium. Leukocyte adhesion then leads to further rapid transcription in the endothelium. Thus, the rapid increase in ICAM-1 expression may facilitate fast microvascular responses to an inflammatory insult. However, additional studies are required to elucidate this possibility in lung microvessels.
We reported that LPS-induced ICAM-1 expression in venules was higher than that in capillaries . Data from the present study and other reports on endothelial cells indicate that induction of ICAM-1 expression is mediated by Ca2+ , . Thus, it is possible that differences in Ca2+ signaling underlie differences in ICAM-1 expression in venules and capillaries. While the increase in the amplitude of Ca2+ oscillation was similar in both microvascular segments, the baseline Ca2+ was lower for capillaries compared to venules. Since, heterogeneity in baseline Ca2+ can lead to differences in the induction of Ca2+-dependent signaling , it is likely that differences in venular versus capillary Ca2+ at baseline contributed to their dissimilar ICAM-1 expression. Whether small differences in Ca2+ can significantly modulate endothelial responses and the specifics of the signaling mechanisms require further consideration.
Our findings show that LPS induces IP3-dependent ER Ca2+ release and downstream responses in lung microvessels. Inhibiting IP3 receptors with XeC blocked induction of ICAM-1 and leukocyte retention, suggesting that blunting ER Ca2+ release may limit inflammatory responses in lung microvessels. In addition, reports indicate that inhibiting IP3-dependent store Ca2+ release also blunts LPS-induced cytokine production in macrophages , , . Leukocyte retention in lung microvessels followed by their subsequent migration into the airspace, and cytokine production by activated macrophages are major characteristics of LPS-induced lung inflammation and injury. Mitigating these LPS-induced responses attenuates injury and improves survival –. Thus, limiting release of Ca2+ from ER stores by blocking IP3 receptors may be effective in blunting LPS-induced inflammation and injury, and thus, facilitate survival.
Thus, our data obtained using real-time fluorescence imaging reveal a new signaling pathway for LPS-induced responses in pulmonary microvessels that involves IP3-mediated Ca2+ release leading to increase in cytosolic Ca2+ oscillations, activation followed by nuclear translocation of NF-κB, an increase in ICAM-1 expression and attendant leukocyte retention. These findings may lead to development of novel intervention strategies for endotoxin-induced lung injury.
The authors thank Dr. Anjaparavanda P. Naren (Department of Physiology, University of Tennessee Health Science Center) for his helpful comments on the manuscript.
Conceived and designed the experiments: KK KP. Performed the experiments: KK LB RBE KP. Analyzed the data: KK LB RBE KP. Contributed reagents/materials/analysis tools: KK LB RBE KP. Wrote the paper: KK KP.
- 1. Kandasamy K, Sahu G, Parthasarathi K (2012) Real-time imaging reveals endothelium-mediated leukocyte retention in LPS-treated lung microvessels. Microvasc Res 83: 323–331.
- 2. Dauphinee SM, Karsan A (2006) Lipopolysaccharide signaling in endothelial cells. Lab Invest 86: 9–22.
- 3. Lu Z, Li Y, Jin J, Zhang X, Lopes-Virella MF, et al. (2012) Toll-like receptor 4 activation in microvascular endothelial cells triggers a robust inflammatory response and cross talk with mononuclear cells via interleukin-6. Arterioscler Thromb Vasc Biol 32: 1696–1706.
- 4. Maloney E, Sweet IR, Hockenbery DM, Pham M, Rizzo NO, et al. (2009) Activation of NF-kappaB by palmitate in endothelial cells: a key role for NADPH oxidase-derived superoxide in response to TLR4 activation. Arterioscler Thromb Vasc Biol 29: 1370–1375.
- 5. Guo F, Zhou Z, Dou Y, Tang J, Gao C, et al. (2012) GEF-H1/RhoA signalling pathway mediates lipopolysaccharide-induced intercellular adhesion molecular-1 expression in endothelial cells via activation of p38 and NF-kappaB. Cytokine 57: 417–428.
- 6. Tauseef M, Knezevic N, Chava KR, Smith M, Sukriti S, et al. (2012) TLR4 activation of TRPC6-dependent calcium signaling mediates endotoxin-induced lung vascular permeability and inflammation. J Exp Med 209: 1953–1968.
- 7. Lai D, Wan M, Wu J, Preston-Hurlburt P, Kushwaha R, et al. (2009) Induction of TLR4-target genes entails calcium/calmodulin-dependent regulation of chromatin remodeling. Proc Natl Acad Sci U S A 106: 1169–1174.
- 8. Wurster AL, Precht P, Pazin MJ (2011) NF-kappaB and BRG1 bind a distal regulatory element in the IL-3/GM-CSF locus. Mol Immunol 48: 2178–2188.
- 9. Hu Q, Natarajan V, Ziegelstein RC (2002) Phospholipase D regulates calcium oscillation frequency and nuclear factor-kappaB activity in histamine- stimulated human endothelial cells. Biochem Biophys Res Commun 292: 325–332.
- 10. Parthasarathi K, Ichimura H, Quadri S, Issekutz A, Bhattacharya J (2002) Mitochondrial reactive oxygen species regulate spatial profile of proinflammatory responses in lung venular capillaries. J Immunol 169: 7078–7086.
- 11. Ichimura H, Parthasarathi K, Quadri S, Issekutz AC, Bhattacharya J (2003) Mechano-oxidative coupling by mitochondria induces proinflammatory responses in lung venular capillaries. J Clin Invest 111: 691–699.
- 12. Kiefmann R, Islam MN, Lindert J, Parthasarathi K, Bhattacharya J (2009) Paracrine purinergic signaling determines lung endothelial nitric oxide production. Am J Physiol Lung Cell Mol Physiol 296: L901–910.
- 13. Berridge MJ (1993) Inositol trisphosphate and calcium signalling. Nature 361: 315–325.
- 14. Scharbrodt W, Abdallah Y, Kasseckert SA, Gligorievski D, Piper HM, et al. (2009) Cytosolic Ca2+ oscillations in human cerebrovascular endothelial cells after subarachnoid hemorrhage. J Cereb Blood Flow Metab 29: 57–65.
- 15. Johnson JD, Misler S (2002) Nicotinic acid-adenine dinucleotide phosphate-sensitive calcium stores initiate insulin signaling in human beta cells. Proc Natl Acad Sci U S A 99: 14566–14571.
- 16. Valdes JA, Hidalgo J, Galaz JL, Puentes N, Silva M, et al. (2007) NF-kappaB activation by depolarization of skeletal muscle cells depends on ryanodine and IP3 receptor-mediated calcium signals. Am J Physiol Cell Physiol 292: C1960–1970.
- 17. Parthasarathi K, Ichimura H, Monma E, Lindert J, Quadri S, et al. (2006) Connexin 43 mediates spread of Ca2+-dependent proinflammatory responses in lung capillaries. J Clin Invest 116: 2193–2200.
- 18. Inoue R, Jensen LJ, Jian Z, Shi J, Hai L, et al. (2009) Synergistic activation of vascular TRPC6 channel by receptor and mechanical stimulation via phospholipase C/diacylglycerol and phospholipase A2/omega-hydroxylase/20-HETE pathways. Circ Res 104: 1399–1409.
- 19. Zhou X, Yang W, Li J (2006) Ca2+- and protein kinase C-dependent signaling pathway for nuclear factor-kappaB activation, inducible nitric-oxide synthase expression, and tumor necrosis factor-alpha production in lipopolysaccharide-stimulated rat peritoneal macrophages. J Biol Chem 281: 31337–31347.
- 20. Otterson MF, Nie L, Schmidt JL, Link BJ, Jovanovic N, et al. (2012) EUK-207 protects human intestinal microvascular endothelial cells (HIMEC) against irradiation-induced apoptosis through the Bcl2 pathway. Life Sci 91: 771–782.
- 21. May MJ, D’Acquisto F, Madge LA, Glockner J, Pober JS, et al. (2000) Selective inhibition of NF-kappaB activation by a peptide that blocks the interaction of NEMO with the IkappaB kinase complex. Science 289: 1550–1554.
- 22. Hughes K, Edin S, Antonsson A, Grundstrom T (2001) Calmodulin-dependent kinase II mediates T cell receptor/CD3- and phorbol ester-induced activation of IkappaB kinase. J Biol Chem 276: 36008–36013.
- 23. Aul R, Armstrong J, Duvoix A, Lomas D, Hayes B, et al. (2012) Inhaled LPS challenges in smokers: a study of pulmonary and systemic effects. Br J Clin Pharmacol 74: 1023–1032.
- 24. Bader MF, Taupenot L, Ulrich G, Aunis D, Ciesielski-Treska J (1994) Bacterial endotoxin induces [Ca2+]i transients and changes the organization of actin in microglia. Glia 11: 336–344.
- 25. Lowry MA, Goldberg JI, Belosevic M (1999) Treatment of the macrophage-like P388D.1 cells with bacterial lipopolysaccharide and interferon-gamma causes long-term alterations in calcium metabolism. Dev Comp Immunol 23: 253–261.
- 26. Antonsson A, Hughes K, Edin S, Grundstrom T (2003) Regulation of c-Rel nuclear localization by binding of Ca2+/calmodulin. Mol Cell Biol 23: 1418–1427.
- 27. Meffert MK, Chang JM, Wiltgen BJ, Fanselow MS, Baltimore D (2003) NF-kappa B functions in synaptic signaling and behavior. Nat Neurosci 6: 1072–1078.
- 28. Beck A, Penner R, Fleig A (2008) Lipopolysaccharide-induced down-regulation of Ca2+ release-activated Ca2+ currents (I CRAC) but not Ca2+-activated TRPM4-like currents (I CAN) in cultured mouse microglial cells. J Physiol 586: 427–439.
- 29. Wehrhahn J, Kraft R, Harteneck C, Hauschildt S (2010) Transient receptor potential melastatin 2 is required for lipopolysaccharide-induced cytokine production in human monocytes. J Immunol 184: 2386–2393.
- 30. Yamashiro K, Sasano T, Tojo K, Namekata I, Kurokawa J, et al. (2010) Role of transient receptor potential vanilloid 2 in LPS-induced cytokine production in macrophages. Biochem Biophys Res Commun 398: 284–289.
- 31. Stevens T (2011) Functional and molecular heterogeneity of pulmonary endothelial cells. Proc Am Thorac Soc 8: 453–457.
- 32. Schumann MA, Gardner P, Raffin TA (1993) Recombinant human tumor necrosis factor alpha induces calcium oscillation and calcium-activated chloride current in human neutrophils. The role of calcium/calmodulin-dependent protein kinase. J Biol Chem 268: 2134–2140.
- 33. Adachi T, Nakashima S, Saji S, Nakamura T, Nozawa Y (1997) Possible involvement of pertussis toxin-sensitive G protein in hepatocyte growth factor-induced signal transduction in cultured rat hepatocytes: pertussis toxin treatment inhibits activation of phospholipid signaling, calcium oscillation, and mitogen-activated protein kinase. Hepatology 26: 295–300.
- 34. Chin ER (2005) Role of Ca2+/calmodulin-dependent kinases in skeletal muscle plasticity. J Appl Physiol 99: 414–423.
- 35. Wildner O, Lipkow T, Knop J (1992) Increased expression of ICAM-1, E-selectin, and VCAM-1 by cultured human endothelial cells upon exposure to haptens. Exp Dermatol 1: 191–198.
- 36. Rahman A, Anwar KN, Malik AB (2000) Protein kinase C-zeta mediates TNF-alpha-induced ICAM-1 gene transcription in endothelial cells. Am J Physiol Cell Physiol 279: C906–914.
- 37. Berendji-Grun D, Kolb-Bachofen V, Kroncke KD (2001) Nitric oxide inhibits endothelial IL-1[beta]-induced ICAM-1 gene expression at the transcriptional level decreasing Sp1 and AP-1 activity. Mol Med 7: 748–754.
- 38. Rahman A, True AL, Anwar KN, Ye RD, Voyno-Yasenetskaya TA, et al. (2002) Galpha(q) and Gbetagamma regulate PAR-1 signaling of thrombin-induced NF-kappaB activation and ICAM-1 transcription in endothelial cells. Circ Res 91: 398–405.
- 39. Kojima S, Hayashi S, Shimokado K, Suzuki Y, Shimada J, et al. (2000) Transcriptional activation of urokinase by the Kruppel-like factor Zf9/COPEB activates latent TGF-beta1 in vascular endothelial cells. Blood 95: 1309–1316.
- 40. Segura BJ, Zhang W, Xiao L, Logsdon CD, Mulholland MW (2005) Sphingosine-1-phosphate induces early response gene expression in C6 glioma cells. Brain Res Mol Brain Res 133: 325–328.
- 41. Ramirez-Carrozzi VR, Nazarian AA, Li CC, Gore SL, Sridharan R, et al. (2006) Selective and antagonistic functions of SWI/SNF and Mi-2beta nucleosome remodeling complexes during an inflammatory response. Genes Dev 20: 282–296.
- 42. Tullai JW, Schaffer ME, Mullenbrock S, Sholder G, Kasif S, et al. (2007) Immediate-early and delayed primary response genes are distinct in function and genomic architecture. J Biol Chem 282: 23981–23995.
- 43. Kayama H, Ramirez-Carrozzi VR, Yamamoto M, Mizutani T, Kuwata H, et al. (2008) Class-specific regulation of pro-inflammatory genes by MyD88 pathways and IkappaBzeta. J Biol Chem 283: 12468–12477.
- 44. Saccani S, Pantano S, Natoli G (2001) Two waves of nuclear factor kappaB recruitment to target promoters. J Exp Med 193: 1351–1359.
- 45. Wang Q, Yerukhimovich M, Gaarde WA, Popoff IJ, Doerschuk CM (2005) MKK3 and -6-dependent activation of p38alpha MAP kinase is required for cytoskeletal changes in pulmonary microvascular endothelial cells induced by ICAM-1 ligation. Am J Physiol Lung Cell Mol Physiol 288: L359–369.
- 46. Thompson PW, Randi AM, Ridley AJ (2002) Intercellular adhesion molecule (ICAM)-1, but not ICAM-2, activates RhoA and stimulates c-fos and rhoA transcription in endothelial cells. J Immunol 169: 1007–1013.
- 47. Lawson C, Ainsworth M, Yacoub M, Rose M (1999) Ligation of ICAM-1 on endothelial cells leads to expression of VCAM-1 via a nuclear factor-kappaB-independent mechanism. J Immunol 162: 2990–2996.
- 48. Thor D, Zhang R, Anderson L, Bose DD, Dube GP, et al. (2012) Effects of 17 beta-estradiol on lipopolysacharride-induced intracellular adhesion molecule-1 mRNA expression and Ca(2)+ homeostasis alteration in human endothelial cells. Vascul Pharmacol 53: 230–238.
- 49. Hoffmann A, Kann O, Ohlemeyer C, Hanisch UK, Kettenmann H (2003) Elevation of basal intracellular calcium as a central element in the activation of brain macrophages (microglia): suppression of receptor-evoked calcium signaling and control of release function. J Neurosci 23: 4410–4419.
- 50. Xie YC, Schafer R, Barnett JB (1997) Inhibitory effect of 3,4-dichloro-propionaniline on cytokine production by macrophages is associated with LPS-mediated signal transduction. J Leukoc Biol 61: 745–752.
- 51. Shinji H, Akagawa KS, Tsuji M, Maeda M, Yamada R, et al. (1997) Lipopolysaccharide-induced biphasic inositol 1,4,5-trisphosphate response and tyrosine phosphorylation of 140-kilodalton protein in mouse peritoneal macrophages. J Immunol 158: 1370–1376.
- 52. Karpurapu M, Wang X, Deng J, Park H, Xiao L, et al. (2011) Functional PU.1 in macrophages has a pivotal role in NF-kappaB activation and neutrophilic lung inflammation during endotoxemia. Blood 118: 5255–5266.
- 53. Islam MN, Das SR, Emin MT, Wei M, Sun L, et al. (2012) Mitochondrial transfer from bone-marrow-derived stromal cells to pulmonary alveoli protects against acute lung injury. Nat Med 18: 759–765.
- 54. Song Y, Dou H, Gong W, Liu X, Yu Z, et al. (2013) Bis-N-norgliovictin, a small-molecule compound from marine fungus, inhibits LPS-induced inflammation in macrophages and improves survival in sepsis. Eur J Pharmacol 705: 49–60.