Maternal and Neonatal Exposure to Environmental Tobacco Smoke Targets Pro-Inflammatory Genes in Neonatal Arteries
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Maternal mainstream tobacco smoking is known to have adverse outcomes on fetal respiratory function; however, no data is currently available on the effects of passive exposure to tobacco smoking and environmental tobacco smoke (ETS) on fetal systemic arterial structure and function. Eight pregnant rhesus macaque monkeys were studied at the California Regional Primate Research Center breeding colony. The estimated gestational age for each dam was established by sonography performed before gestational day 40. Two inhalation chambers were used, each with an air capacity of 3.5 m3, and each housed two dams. Aged and diluted sidestream smoke was used as a surrogate for ETS. Exposure to ETS (1 mg/m3) occurred for 6 h/day, 5 days/week, beginning on gestational day 100. All dams were allowed to give birth spontaneously and then ETS exposure continued 70–80 days postnatally with the chamber containing both the mother and infant. Carotid arteries from four control (C) and four ETS-treated newborns were analyzed for mRNA by gene macroarray and for protein by Western blotting. A total of 588 cardiovascular genes were studied. Four genes were upregulated by ETS compared to C, and nine genes were downregulated (≥2-fold change). Three genes were selected for further study. Following ETS exposure, neonatal carotid arteries of non-human primates manifested evidence of inflammation with increased gene and protein expression of LFA-1 and RANTES, proteins that are recognized to be important in vascular adhesion and inflammation, and downregulation of expression for the receptor for VEGF, which has a key role in angiogenesis. Prenatal and postnatal exposure to ETS increases expression of pro-inflammatory genes and may be responsible for early arterial vascular remodeling that is predisposing to a subsequent vascular disease.
KeywordsSmoking Vascular Inflammation Genes Macroarray Monkey Neonate Angiogenesis
Tobacco smoking is a major cause of morbidity and mortality in the U.S. and an increasingly important cause of death and disability worldwide. Further, maternal mainstream tobacco smoking is known to have multiple adverse fetal outcomes, including reduced fetal respiratory function [1, 2, 3, 4, 5, 6, 7, 8, 9, 10, 11, 12]. Exposure to tobacco smoking, either mainstream or environmental tobacco smoke (ETS), is a major modifiable cardiovascular risk factor known to exert deleterious effects on fetal systemic arterial structure and function [4, 13, 14]. This is an important area of research because arterial disease, specifically atherosclerotic cardiovascular disease, is the leading cause of morbidity and mortality in adults, which develops over decades with its onset early in life. Multiple reports have now documented that early and intermediate stage atheroma occurs in children and teenagers [14, 15, 16, 17, 18, 19]. Thus, it is plausible that early injury to fetal arteries in the in utero environment can predispose to arterial disease in adulthood.
Exposure to ETS or passive smoking is increasingly appreciated to have major adverse health effects and to result in a pro-inflammatory state [20, 21]. Our previous work showed that ETS increases endothelial layer permeability, low-density lipoprotein accumulation, and stiffening in the artery wall [21, 22]. Thus, work from a number of laboratories, including our own, indicate that exposure to either mainstream tobacco smoke or ETS acutely injures the artery wall and predisposes to chronic inflammation; however, no studies have yet been conducted that examine the effects of ETS exposure of the mother and neonate on the inflammatory status of the vasculature of the neonate.
Atherosclerosis has its origins in the arterial subendothelium and is an inflammatory state characterized by arterial injury [23, 24]. The vascular pathology is characterized by inflammation involving a number of cells, including blood-borne monocytes . Monocyte recruitment is promoted by a several factors, including cellular adhesion molecules, such as vascular cell adhesion molecule-1 resulting in monocyte transmigration to the subendothelial space. In the subendothelial space, “foam cells” or lipid-filled macrophages are formed . The interaction of macrophages and lipids play a central role in the development of atherosclerosis through foam cell formation and via the induction of numerous cytokines, chemokines, such as RANTES , and growth factors, including vascular endothelial growth factor (VEGF) . In this study, we hypothesized that chronic maternal, fetal, and neonatal exposure to ETS increases molecular markers and mediators of arterial injury and inflammation in fetal arteries.
Materials and Methods
Animals and Smoke Exposure Protocols
All studies were carried out in accordance with the declaration of Helsinki and with the Guide for the Care and Use of Laboratory Animals as adopted and promulgated by the National Institutes of Health (http://oacu.od.nih.gov/regs/guide/guide.pdf). Eight pregnant Rhesus macaque monkeys were obtained from the California National Primate Research Center breeding colony. Estimated gestational age for each dam was established by sonography performed before gestational day 40. Animals were selected based on a history of successful vaginal delivery and previous infant rearing experience with estimated delivery dates separated by approximately 1 week per animal to facilitate experimental procedures.
Two inhalation chambers were used, each with an air capacity of 3.5 m3, and each housed two dams. Aged and diluted sidestream smoke was used as a surrogate control for ETS. Standardized 1R4F research cigarettes were smoked simultaneously with a single puff volume of 35 ml per cigarette and a duration of 2 s, once per min. ETS was generated by a smoke exposure system (Teague Enterprises, Davis, CA) using IR4F conditioned cigarettes from the Tobacco and Health Research Institute of the University of Kentucky. Sidestream smoke from the smoldering end of each cigarette was collected into a conditioning chamber where it was aged over a period of approximately 2 to 3 min while being diluted with filtered air and then further diluted as it passed into the exposure chambers to produce total suspended particulate concentrations of 1.0 mg/m3, 4–5 ppm carbon monoxide and 200–300 μg/m3 nicotine. This level of exposure is highly reminiscent of ETS concentrations found in homes or the workplace where smoking is permitted. The exposure chambers were stainless steel and glass Hinners type and 4.2 m3 in size. Each chamber has an air capacity of 3.5 m3. Airflow through the system was set for 15 changes per hour.
Exposure to ETS (1 mg/m3) occurred for 6 h/day, 5 days/week, beginning on gestational day 100. All dams were allowed to give birth spontaneously (five male and three female infants born), and then ETS or sidestream control exposure continued for 70–80 days postnatally for the four experimental and four control animals, respectively with the chamber containing both the mother and infant. Infants were then sacrificed (mean age, 72 days) and bilateral carotid arteries dissected and cleansed of adventitial fat. Carotid arteries from four control and four ETS-treated newborns (mean weight of animals at sacrifice, 0.84 kg) were then analyzed for mRNA by gene macroarray and for protein by Western blotting. Tissues were flash-frozen and stored at −80°C until assayed.
All procedures were performed under RNAse-free conditions. RNA was isolated from the carotid artery samples from the neonatal monkeys using Tri Reagent (Molecular Research Center, Inc., Cincinnati, OH) following tissue disruption with a mortar and pestle and subsequent use of a tissue hand-held glass homogenizer (Kontes). Total RNA was extracted using chloroform or 1-Bromo-3-Chloropropane (BCP) Phase Separation Reagent (Molecular Research). Each carotid (25–33 mg tissue) yielded approximately 2.0–3.3 mg of total RNA. Following extraction, RNA was treated with DNAse using Clontech DNAse-1 per the manufacturer’s instructions (MessageClean DNAse-1; GenHunter Corporation, Nashville, TN). Total RNA from the control and ETS-exposed aortas were used to prepare two radioactive probes for array hybridization.
Probe Preparation and Array Hybridization
The Atlas Human Cardiovascular cDNA Expression Array Kit and reagents (Clontech, Palo Alto, CA) were used for these studies. The array contains duplicate copies of 588 cardiovascular genes and multiple control and housekeeping genes (http://www.clontech.com). The cardiovascular genes consist of six major categories as follows: (1) cell cycle regulators/intermediate filament markers, (2) apoptosis/oncogenes/tumor suppressors, (3) DNA damage/repair and cell development, (4) cell adhesion/mobility and angiogenesis, (5) cell–cell interactions, and (6) growth factors/cytokines.
The 33P-labeled cDNA probes were synthesized by reverse transcription of total RNA from filtered air (control) and environmental tobacco smoke-exposed monkey carotids using a gene-specific primer mix (1 μl, 0.2 μM of each primer) and annealed to 2.13 μg of total RNA. The mixture was heated for 2 min at 70°C in a thermal cycler (Perkin Elmer, Waltham, MA), then incubated for 2 min at 50°C. First strand cDNA synthesis was initiated by mixing the annealed primer with the RNA and master mix [containing 4 μl of 5X reaction buffer (250 mM Tris–HCl, pH 8.3, 375 mM KCl, 15 mM MgCl2), 2 μl of dNTP mix (0.5 mM of each dGTP, dCTP, and dTTP), 5 μl of [α-33P]dATP (3,000 Ci/mmol), (10 mCi/ml; NEN, Boston, MA.), 1 μl DTT (100 mM), and 2 μl of MMLV reverse transcriptase (50 U/μl)]. The reaction was incubated in a thermal cycler (Perkin Elmer) at 50°C for 25 min and stopped by addition of 1 μl termination mix [0.1 M EDTA (pH 8.0), 1 mg/ml glycogen]. The labeled cDNA probe was purified from unincorporated 33P-labeled nucleotides by gel filtration chromatography using a 1-ml NucleoSpin extraction spin column (Clontech) per the manufacturer’s instructions. The purified-labeled cDNA probes (approximately 1X106 cpm for control and ETS-exposed monkey carotid) were utilized for macroarray hybridization.
The probes were prepared for hybridization by adding 10X denaturing solution (1 M NaOH, 10 mM EDTA) to the entire pool of labeled probe and incubated at 68°C for 20 min. Cot-1 DNA and 2X neutralizing solution (1 M NaH2PO4, pH 7.0) was added to the denatured probe and incubated at 68°C for 10 min. The labeled probe solution was mixed together with preheated ExpressHyb hybridization solution. Each of the two duplicate Atlas Human Cardiovascular Array membranes were pre-wet with de-ionized H2O and prehybridized for 30 min at 68°C. Under continuous agitation, the array membranes were hybridized overnight at 68°C, washed three times with 2X SSC, 1% sodium dodecyl sulfate (SDS) at 68°C, washed twice with 0.1X SSC, 0.5% SDS for 30 min at 68°C, and then washed for 5 min with 2X SSC at room temperature (RT).
Signal Detection and Image Analysis
The washed membranes were sealed in plastic wrap and exposed directly to a storage phosphor screen (Molecular Dynamics, Sunnyvale, CA) for 8 days. The screen was scanned using Storm 840 in storage phosphor mode. Signal intensity was quantified using an ImageQuant software for identification of differentially expressed genes. In ImageQuant, grid objects were created and used for simultaneous quantitation of all duplicate spots on each array. Grids of seven columns by 14 rows were used to analyze the six main gene groupings on the macroarrays. Separate grids were created for housekeeping gene spots and for determining background (unspotted, unhybridized areas of the membrane), which was subtracted from volume densitometry values for the grid cells. Twenty-three kilo Daltons highly basic protein and 60S ribosomal protein L13A (aka RPL 13A) housekeeping gene values were used for normalization based on the equality of signal strength between both arrays. This normalization scheme was further validated by the equality in normalized expression of many of the common genes on both arrays.
Real-Time RT-PCR-Based Confirmation of Differential Gene Expression
To further confirm differential mRNA expression of the genes identified to be regulated by ETS in the macroarray analysis, we performed real-time polymerase chain reaction (PCR) utilizing two additional ETS-exposed and control monkey aortas. Thus, for these experiments, a total of six aortas were studied for ETS-exposed and control neonatal monkeys, respectively. The aortas were from the same experimental animal cohort as described earlier in the “Materials and Methods” section. Briefly, total RNA from the ETS and control aortas was treated with DNAse (MessageClean DNAse-I; GenHunter) and cDNA generated by reverse transcriptase (RT)-PCR. A mixture of oligo (dT) oligodeoxynucleotide primers (T12–18) and random hexamer primers were used for these studies following the protocol for SuperScript RNAse H-Reverse Transcriptase (GibcoBRL, Rockville, MD). Real-time detection of PCR was performed using the GeneAmp 5700 Sequence Detection System (Applied Biosystems, Foster City, CA) according to the manufacturer’s instructions. The same gene-specific primers used for semiquantitative PCR analysis were used for real-time PCR detection of the genes of interest. Equal amounts of duplicate or triplicate sample cDNA were amplified with the SYBR Green I Master Mix (Applied Biosystems). The thermal cycling parameters were thermal activation for 10 min at 95°C followed by 40 cycles of PCR (melting for 15 s at 95°C and annealing extension for 1 min at 60°C). A standard curve was constructed using a template dilution series (1:10, 1:20, 1:40, 1:80, and 1:160) of total RNA from monkey aorta. A “no template” negative control was included with each PCR. Amplification efficiency for each of the genes of interest was then validated and normalized against glyceraldehyde-3-phosphate dehydrogenase (GAPDH). In order to compare the relative expression of the various genes, data was expressed as the normalized densitometry ratio of ETS to control aortas.
Protein was prepared from monkey carotid sections from filtered air (control) and ETS-exposed monkeys using Tri Reagent (Molecular Research Center, Inc., Cincinnati, OH) or NE-PER Nuclear and Cytoplasmic Extraction Reagents (Pierce, Rockford, IL), and mammalian Protease Inhibitor Cocktail (Sigma, Saint Louis, MO) per the manufacturer’s protocol. Protein quantity was assayed by detergent-compatible DC protein assay (BioRad, Hercules, CA). Ready gels for SDS-PAGE electrophoresis (BioRad) were used with the appropriate gel concentration for the size of the protein of interest (loading ~44 mg of protein per lane). Kaleidoscope molecular weight markers (BioRad) were loaded in one or two lanes of the gels for size markers. The gels were electrophoresed at 60 V for 15–30 min, followed by 60–90 min at 120 V depending on the speed of migration. After electrophoresis, electroblotting proceeded for 1 h at 100 V on ice.
The blot was blocked in 10% w/v non-fat dry milk Tris-Buffered Saline Tween-20 (TBST) solution overnight at 4°C. The nitrocellulose membrane was washed three times with TBS, 0.05% Tween. The primary antibody was diluted in TBST to concentrations previously determined or according to manufacturer’s recommendations and incubated for ~1 h at RT. The secondary antibody was diluted in TBST and incubated for ~1 h at RT. The nitrocellulose was washed two times with TBST. Electrochemiluminescence (ECL) Detection Reagents (Amersham Pharmacia Biotech, Buckinghamshire, England) horseradish peroxidase (HRP)-based detection was used. Blots were wrapped in saran and exposed to autoradiograph film (Kodak Biomax, Rochester, NY). Densitometry was performed on a Kodak 1D gel imaging system. Some blots were stripped with Restore Western Blot Stripping Buffer (Pierce) and re-probed with mouse anti-actin or a different primary antibody than that stripped, followed by a secondary antibody and ECL detection as described. Details of the antibodies used and protein products of the genes studied (see “Results”) are as follows:RANTES (8 kDa protein)—primary antibody goat polyclonal anti-RANTES (Santa Cruz Biotech, Santa Cruz, CA; 1:1000 dilution) and secondary antibody bovine anti-goat IgG HRP (Santa Cruz Biotech; 1:10,000–1:30,000 dilution); VEGFR2 [flk-1] (130 kDa protein)—primary antibody rabbit polyclonal anti-neuropilin-1 (Oncogene Research Products, La Jolla, CA; 1:100–1:200 dilution) and secondary antibody goat anti-rabbit IgG HRP (BioRad; 1:15,000 dilution), as well as primary antibody goat polyclonal anti-neuropilin-2 (Santa Cruz Biotech; 1:100 dilution) and secondary antibody bovine anti-goat Ig G HRP (Santa Cruz Biotech; 1:10,000–1:30,000 dilution); LFA-1 [integrin alpha L] (180 kDa protein)—primary antibody goal polyclonal anti-LFA1 (Santa Cruz Biotech; 1:100 dilution) and secondary antibody bovine anti-goat IgG HRP (Santa Cruz Biotech; 1:10,000–1:30,000 dilution); actin control (41 kDa protein)—primary antibody mouse monoclonal anti-actin (Sigma; 1:1,000 dilution) and secondary antibody goat anti-mouse IgG HRP (BioRad; 1:15,000 dilution).
Densitometry values were obtained for each array cDNA from ETS-treated and control samples, and quantification of spots on arrays from ETS-treated and control (sidestream air) aortas was performed. In order to allow the array products to be quantified comparatively, arrays were also spotted with two housekeeping genes. This permitted the spot densitometry values of the ETS-treated and control array signals to be normalized to the housekeeping signals and to calculate normalized densitometry ratios. Background signal was subtracted from the control and ETS spots prior to analysis. Normalized ratio data from the arrays were then evaluated for differential expression (i.e., greater or less than a 2-fold difference in expression in the ETS-treated versus the control samples). All arrays were spotted in duplicate. Four aortas each were used for the ETS-treated and the control arrays.
Quantification of PCR products was performed in a similar fashion. PCR amplifications were conducted with GAPDH in order to permit normalization of signals to GAPDH and to account for any minor variations in DNA loading in the PCR product signals. Normalized ratio data from PCR reactions were then evaluated for differential expression (i.e., greater or less than a 2-fold difference in expression in the ETS-treated versus the control samples). All PCR reactions were performed in duplicate. Six aortas each were used for the ETS-treated and the control PCRs. Normalized data from arrays and PCR were expressed as relative fold change in expression for ETS compared to control-treated aortas.
Western blot experiments were performed in triplicate or greater, and data expressed as mean +/− standard error of the mean (SEM) for net densitometry values for the four control and the four ETS-treated aortas. Means +/− SEM and mean fold change in protein expression in the ETS-treated and control protein products was then calculated. Statistical significance was at the p < 0.05 level.
For the array, PCR, and Western assays, the calculated fold-change differences between the ETS-treated and control samples were based on the mean values of the four subjects in each of the control and study groups.
Up- and Downregulated Aortic Genes by Macroarray Analysis
Summary of differential gene expression by ETS utilizing the atlas human cardiovascular cDNA expression array
Array coordinate (block, row, column)
Gene name (Gene Functional Classification Category)
T cell-specific rantes protein precursor; sis delta; small inducible cytokine A5 (growth factor, cytokine and chemokines)
Adipocyte fatty acid-binding protein 4 (trafficking and targeting proteins)
Lumican precursor (extracellular matrix proteins)
Leukocyte adhesion glycoprotein LFA-1 alpha subunit precursor; leukocyte function-associated molecule 1 alpha chain; CD11A antigen; integrin alpha L (cell–cell adhesion receptors)
Vascular endothelial cell growth factor 165 receptor [VEGF-R2] (growth factor and chemokine receptors)
Caveolin 3 (GTP/GDP Exchangers and GTPase activity modulators)
GAP junction alpha-1 protein (cell–cell adhesion receptors and other membrane channels and transporters)
Integrin alpha 8 (cell–cell adhesion receptors)
Procollagen 1 alpha 2 subunit precursor (extracellular matrix proteins)
Profilin 1 (cytoskeleton and motility proteins)
Tissue inhibitor of metalloproteinase 1 precursor [TIMP-1] (extracellular matrix proteins and protease inhibitors)
N-acetylglucosamine-6-sulfatase precursor; glucosamine-6-sulfatase (complex carbohydrate metabolism)
Natriuretic peptide precursor B (hormones)
Three genes of interest were identified for further study based on the level of expression and/or their physiological/functional significance in the vasculature as follows: (1) T cell-specific rantes protein (RANTES) precursor, (2) leukocyte adhesion glycoprotein (LFA-1; CD11a/CD18) alpha subunit, and (3) vascular endothelial cell growth factor receptor (VEGFR2; FLk1). RANTES and LFA-1 were upregulated by ETS relative to filtered air control with expression levels that were 19.7 and 8.5 greater than the control, respectively. VEGFR2 was downregulated (2.8-fold less) by ETS exposure relative to the control (Table 1).
Differential Expression of Genes of Interest
We performed RT-PCR to confirm differential expression for the genes of interest. The expression ratios for ETS were 12.2-fold greater than the control for LFA-1 and 1.7-fold less than the control for VEGFR2. Despite repeated attempts, however, we were unable to verify the differential expression for RANTES by real-time PCR despite there being a clear increase in gene expression for this gene by macroarray and in protein expression by Western blotting following ETS exposure (see below).
Comparison of gene macrochip array, real-time PCR, and Western blot protein expression for the three genes of interest in this study
Fold change in expression for ETS vs filtered air control
This study shows that inhalation of ETS by the mother alters neonatal gene and protein expression in systemic arteries. How ETS has these effects on fetal arteries is not clear. The injury to fetal arteries could occur in a number of ways, including reduced placental blood flow, activation of platelets and leukocytes, and vascular wall inflammation.
Two genes were upregulated by ETS and are of particular interest in this study: (1) RANTES (regulated on activation of normal T cell expressed and secreted) and (2) LFA-1 (a β2 integrin leukocyte function antigen, also known as CD11a/CD18). These genes are pro-inflammatory. RANTES is a small inducible cytokine that functions as a chemoattractant and an activating cytokine for monocyte cell recruitment to atherosclerotic plaque , a chemokine for inflammatory cells  and mediator of inflammation [29, 30, 31]. It is also implicated in atherosclerotic lesion formation as it is a macrophage inflammatory protein  and is secreted by vascular endothelial cells . RANTES is strongly induced in response to cellular insult. LFA-1 is a surface glycoprotein and cell adhesion molecule that plays a key role in cell trafficking and cell-to-cell contact, including leukocyte/monocyte adhesion to the endothelium, one of the early events in atherogenesis and has a role in vascular injury, as reviewed by Galkina and Ley . LFA-1 also has an important role in the pathophysiology of inflammation and immunity [34, 35]. Thus, the coordinated upregulation by ETS of expression for plasma membrane glycoproteins involved in leukocyte adhesion, such as LFA-1, and chemoattractants, such as RANTES, provide a molecular mechanism for ETS-mediated vascular injury in neonatal arteries.
These experiments also demonstrated a downregulation of gene expression for vascular endothelial growth factor receptor (VEGFR) by ETS exposure. VEGF is derived from vascular smooth muscle cells and fibroblasts, acts on endothelium, and is a key regulator of physiological and pathological angiogenesis (tumor angiogenesis). VEGF is found in human coronary vessels where it participates in atherosclerosis and plaque growth and angiogenesis [36, 37]. VEGF also participates in revascularization in response to injury and is mitogenic for vascular endothelial cells [38, 39]. Two VEGFR genes are known, the VEGFR-1 (flt-1) and VEGFR-2 (KDR/flk-1), which are genes that encode VEGF-specific tyrosine kinase. In this study, downregulation of VEGFR2 gene expression by ETS was not accompanied by substantial downregulation of protein expression (~ 7% downregulation), suggesting gene regulation by ETS at the translational level. Translation is the target of multiple regulatory proteins. Translational repression of mRNA is consistent with reduced or absent translation known as translational silencing. There are examples of translational silencing of a complex of inflammatory RNAs that share similar co-regulatory factors. One example is the interferon-gamma-activated translational inhibitor (GATI) complex known to be involved in translational silencing. Inflammatory genes are known to be a target of this pathway. Although no prior negative translational regulation had been previously described for VEGF, this gene has recently been reported to be a target of the GATI pathway . Since the endothelial cell-specific VEGF and its cellular receptors Flt-1 and Flk-1 have been implicated in the formation of the embryonic vasculature, this mechanism of translational silencing by ETS of an angiogenesis gene may be of potential importance in local angiogenic responses and in regulating translational inhibition of angionesis.
This study has limitations. A major question posed is whether arterial injury that occurs in the pre- and postnatal period has long-term adverse outcomes. There is some precedence for this in asthma where rodent studies have shown that perinatal exposure to tobacco smoke early in life increased airway responsiveness later ; however, our studies were not designed to address these long-term questions. An additional limitation relates to the lack of success in amplifying the RANTES gene for real-time PCR confirmation of the macroarray findings. Further attempts were limited by lack of availability of additional tissue; however, we are confident of our findings given concomitant upregulation of gene expression by macroarray and protein expression by Western blotting for this gene. Atherosclerosis lesion development was not directly studied because the animals were not hyperlipidemic or cholesterol-fed, and they were of a very young age (70–80 days). In addition, biomarkers of exposure were not analyzed because the primary focus of the study was the molecular changes in the carotid arteries; however, a recent publication by a co-author of the present study  utilized a similar system to demonstrate biomarkers of ETS exposure are present; following 1 year of postnatal exposure, non-human primates’ aortas were found to have increased vascular oxidative stress (protein carbonyls and SOD) and mitochondrial dysfunction/damage (cytochrome oxidase, mitochondrial DNA) that were coupled to reductions in mitochondrial antioxidant capacity and copy number in vascular tissue compared to filtered air-exposed controls. Furthermore, basic histologic analysis suggested early atherosclerotic changes in smoke exposed aortas. These findings may be of significance in explaining the potential for increased atherosclerotic disease susceptibility in adulthood following early life smoke exposure because inflammation and mitochondrial damage and dysfunction in response to tobacco smoke exposure are features of early atherosclerosis.
In conclusion, our study demonstrates that prenatal and postnatal maternal exposure to environmental tobacco smoke increases neonatal arterial expression of genes that are pro-inflammatory and induce or contribute to vascular injury while reducing the arterial expression of a gene for angiogenesis. These observations have not been previously reported and provide a molecular explanation for early deleterious effects of ETS on the vasculature that relates to at least two vascular physiologic processes: activation of a pro-inflammatory gene cascade and inhibition of vascular repair to injury via inhibition of angiogenic genetic control. Further studies are needed to determine if the arterial injury and activation observed in neonatal vessels in response to ETS exposure will translate into increased susceptibility to vascular disease later in life.
The authors would like to acknowledge the assistance of the Center for Health and the Environment and the technical assistance of Kristine Lewis at the University of California, Davis in the performance of these studies. This work was also made possible by the Frances Lazda endowment in Women’s Cardiovascular Medicine to AV. JR was supported by an NIH R01 (HL55667) and the Richard A. and Nora Eccles Harrison endowed chair in Diabetes Research. These studies were also supported by grants from the National Institutes of Health (ES00628, ES011634, ES05707 and P51 RR00169).
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