DNA damage and repair are hallmarks of cellular responses to ionizing radiation. We hypothesized that monitoring the expression of DNA repair-associated genes would enhance the detection of individuals exposed to radiation versus other forms of physiological stress. We employed the human blood ex vivo radiation model to investigate the expression responses of DNA repair genes in repeated blood samples from healthy, non-smoking men and women exposed to 2 Gy of X-rays in the context of inflammation stress mimicked by the bacterial endotoxin lipopolysaccharide (LPS). Radiation exposure significantly modulated the transcript expression of 12 genes of 40 tested (2.2E-06<p<0.03), of which 8 showed no overlap between unirradiated and irradiated samples (CDKN1A, FDXR, BBC3, PCNA, GADD45a, XPC, POLH and DDB2). This panel demonstrated excellent dose response discrimination (0.5 to 8 Gy) in an independent human blood ex vivo dataset, and 100% accuracy for discriminating patients who received total body radiation. Three genes of this panel (CDKN1A, FDXR and BBC3) were also highly sensitive to LPS treatment in the absence of radiation exposure, and LPS co-treatment significantly affected their radiation responses. At the protein level, BAX and pCHK2-thr68 were elevated after radiation exposure, but the pCHK2-thr68 response was significantly decreased in the presence of LPS. Our combined panel yields an estimated 4-group accuracy of ∼90% to discriminate between radiation alone, inflammation alone, or combined exposures. Our findings suggest that DNA repair gene expression may be helpful to identify biodosimeters of exposure to radiation, especially within high-complexity exposure scenarios.
Citation: Budworth H, Snijders AM, Marchetti F, Mannion B, Bhatnagar S, Kwoh E, et al. (2012) DNA Repair and Cell Cycle Biomarkers of Radiation Exposure and Inflammation Stress in Human Blood. PLoS ONE 7(11): e48619. https://doi.org/10.1371/journal.pone.0048619
Editor: Kerstin Borgmann, University Medical Center Hamburg-Eppendorf, Germany
Received: June 11, 2012; Accepted: September 26, 2012; Published: November 7, 2012
This is an open-access article, free of all copyright, and may be freely reproduced, distributed, transmitted, modified, built upon, or otherwise used by anyone for any lawful purpose. The work is made available under the Creative Commons CC0 public domain dedication.
Funding: This work was performed under the auspices of the U.S. Department of Energy by the University of California, Lawrence Berkeley National Laboratory under DOE contract No. DE-AC02-05CH11231. This project has been funded in whole or in part by Federal funds from the Biomedical Advanced Research and Development Authority, Office of the Assistant Secretary for Preparedness and Response, Office of the Secretary, Department of Health and Human Services, under Contract No. HHSO100201000006C. The Armed Forces Radiobiology Research Institute (AFRRI) supported the involvement of WFB in this research under AFRRI work units RBB4AR and RAB4AU; views presented in this manuscript are those of the authors; no endorsement by the Department of Defense has been given or should be inferred. 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.
Biological markers of exposure to ionizing radiation (IR) in human populations are of great interest for assessing normal tissue injury in radiation oncology and for biodosimetry in nuclear incidents and accidental radiation exposures. Current approaches to radiation biodosimetry include assessments of physical effects, such as time to emesis and blood lymphocyte kinetics, and cellular determinants such as cytogenetic biodosimetry to assess radiation-induced chromosome aberrations in circulating blood lymphocytes . However, these methods are time-consuming and do not provide results fast enough to identify people who would benefit the most from medical intervention immediately after irradiation. The use of biochemical markers, such as changes in transcript or protein expression or posttranslational modifications, represents an alternative method with the potential for high-throughput, deployable methods for initial triage as well as for the estimation of exposure dose (reviewed in , ).
Recent studies have identified large-scale changes in transcript expression in irradiated blood lymphocytes shortly following IR exposures and that transcript changes can persist for days after exposure –. A 2006 literature review from our laboratory identified over 260 radiation-responsive proteins and ranked them according to their potential usefulness in human biodosimetric applications . Genes involved in cellular DNA damage response and repair functions, including DNA repair, cell cycle functions and apoptosis were identified as priority candidates for radiation biodosimetry.
DNA is a critical cellular target of IR and the ability of the cell to repair DNA damage determines its fate after exposure. Various forms of DNA damage are induced by IR, including DNA-protein cross-links, base and sugar alterations, DNA single-strand breaks (SSBs), bulky lesions (i.e. clusters of base and sugar damage) and double-strand breaks (DSBs) . The immediate response to IR-induced DNA damage is the stimulation of the DNA repair machinery and the activation of cell cycle checkpoints, followed by down-stream cellular responses such as apoptosis that removes damaged cells. The predominant repair pathway is base excision repair (BER), which is responsible for the removal of damaged bases and DNA single-strand breaks through gap-filling by DNA polymerase and ligation of DNA ends . Nucleotide excision repair (NER) is the major pathway for the repair of bulky DNA damages that cause DNA helical distortion . NER proteins are also involved in repair of oxidative damage through stimulation of BER, including XPC and XPG, indicating cross-talk between these two repair pathways –. Several NER genes are upregulated at the gene expression level by IR, including XPC and DDB2 , . IR exposure is known to modulate transcript and/or protein levels of several cell cycle regulators (CDKN1A (p21), GADD45a, Cyclin G1 (CCNG1), CHK2-thr68) and apoptosis genes (BAX and BBC3) in diverse cell and blood model systems (in vivo, in vitro and ex vivo) , , , –. However, little is known of how co-exposure to confounding factors can affect the utility of individual biomarkers for radiation biodosimetry , , .
The human blood ex vivo irradiation exposure model has been used to investigate the early radiation-induced biological responses for potential biodosimetry applications, and was recently demonstrated to accurately reflect the in vivo peripheral blood radiation response in humans . Our study utilized this model to examine: (i) the transcriptional response of 40 well known DNA repair, cell cycle control and apoptosis genes after exposure to IR; (ii) IR-induced transcript changes associated with changes in a selected set of proteins; and (iii) transcript and protein responses in the context of inflammatory stress. Lipopolysaccharide (LPS), the principal component of the outer membrane of Gram-negative bacteria , elicits strong inflammatory responses and induces oxidative stress in exposed mammalian cells . Our findings demonstrate that inflammation significantly confounds the radiation response of some DNA repair genes at a dose that is relevant for radiation biodosimetry. We identified a small panel of DNA repair transcripts and proteins whose expression changes distinguish between unirradiated and 2 Gy ex vivo irradiated human blood samples display excellent radiation dose and time dependent responses in an independent ex vivo irradiated human dataset, show robust non-overlapping responses in blood samples from human patients treated with total body irradiation, and demonstrate high accuracy for classifying blood samples receiving radiation only, inflammation stress alone, or both.
Materials and Methods
All research involving human subjects were approved by the Lawrence Berkeley National Laboratory Institutional Review Board. Peripheral blood from healthy volunteers was obtained after written informed consent and was drawn into sodium citrate (whole blood culture model) or sodium heparin (PBMC culture model) Vacutainer tubes (Becton Dickinson and Company, Franklin Lakes, NJ).
Whole Blood ex vivo Radiation Model
Five donors (2 male, 3 female; age range, 20–50 years) provided two peripheral blood samples each, at least one month apart for measurement of transcript and protein responses. Blood collected in Vacutainer tubes was transferred in 18 ml aliquots into 50 ml conical tubes. Blood in tubes was exposed at room temperature to 0 or 2 Gy X-rays, (∼780 mGy/min; Pantak 320 kVp X-ray machine (Precision X-ray); run at 300 kV and 10 mA). Dosimetry was performed using a RadCal AccuPro dosimeter by measuring the accumulated dose over a specific time interval. After irradiation, blood samples were diluted 1∶1 with RPMI 1640 medium (Sigma-Aldrich) supplemented with 10% heat-inactivated fetal bovine serum (Invitrogen) in 50 ml centrifuge tubes, loosely capped and maintained on a 10 degree angle at 37°C in a humidified incubator with 5% CO2 for 24 hrs. LPS was added to some blood cultures immediately after irradiation (50 ng/ml LPS from Escherichia coli O111:B4) (Sigma Aldrich). After 24 hrs, buffy coats were extracted for protein and RNA purification. Plasma was collected, aliquoted and stored at −80°C.
RNA Isolation and Quantitative RT-PCR
RNA was isolated using Trizol reagent (Invitrogen) and purification was performed according to the manufacturer’s instructions. In brief, cell pellets were homogenized in Trizol reagent (1.2 ml). The lysed cells were incubated for 5 min at room temperature, followed by the addition of 0.25 ml chloroform. After mixing, the samples were centrifuged at 12,000 g for 15 min at 4°C. The aqueous phase was separated and 0.625 ml ice-cold isopropanol was used to precipitate RNA. The samples were incubated at room temperature for 10 min and total RNA was collected by centrifugation at 12,000 g for 10 min at 4°C. The RNA pellet was washed with 1 ml 70% ethanol and dissolved in 40 µl RNase-free deionized water. The RNA was quantified using a NanoDrop-2000c spectrophotometer (Thermo Scientific), and quality was monitored with the Agilent 2100 Bioanalyzer (Agilent Technologies, Santa Clara, CA). RNA integrity numbers (RIN) ranged from between 7 to 9.5 (mean, 8.3), and 260/280 absorbance ratios ranged from 1.7 to 1.95 (mean, 1.86) .
For cDNA synthesis, an aliquot of 4 µg of total RNA was reverse transcribed using the High-Capacity cDNA Reverse Transcription Kit (Applied Biosystems, Foster City, CA) according to the manufacturer's instructions. Taqman Gene Expression Assays (Applied Biosystems, Foster City, CA, USA) were used, according to manufacturer’s instructions, to detect mRNA of 40 DNA damage response genes. 13 genes were selected for further investigation (BAX, Hs00180269_m1*, BBC3, Hs00248075_m1*, FDXR, Hs01031624_m1, CDKN1A, Hs00355782_m1*, GADD45a, Hs99999173_m1, CCNG1, Hs00171112_m1*, CHK2, Hs00200485_m1*, PCNA, Hs00696862_m1, LIG1, Hs01553527_m1*, XPC, Hs01104206_m1*, DDB2, Hs03044953_m1*, POLH, Hs00982625_m1*, RAD51, Hs00153418_m1*; * indicates manufacturer’s recommended assay for this gene, if more than one assay was available). See Table S1 for a full list of all 40 genes and assay numbers. The RT-PCR reactions were performed, in individual reaction format, with the ABI 7500 Fast Real Time PCR System using Taqman Fast Universal PCR Master Mix from ABI and following manufacturer's recommendations. The results were expressed as the threshold cycle (Ct), i.e. the cycle number at which the PCR product crosses the threshold of detection. The relative quantification of the target transcripts normalized to the endogenous control ACTB (β-Actin) was determined by the comparative Ct method (ΔCt) according to the manufacturer’s protocol. The endogenous control gene GAPDH was run concurrently but was not used for normalization since LPS treatment induced changes in GAPDH transcript levels. Relative fold inductions were calculated by the ΔΔCT method . All samples were run in triplicate. A no RT qPCR control was included for all reactions to monitor for genomic DNA contamination and was negative across all reactions.
Confirmation of Radiation Responsiveness of Our 8-gene Transcript Panel in Independent Expression Datasets of ex vivo Irradiated Human Blood and Blood Samples of Human Patients Undergoing total body Irradiation
Globally normalized whole genome microarray expression profiles of whole blood irradiated ex vivo were obtained from the NCBI GEO database (GSE8917; ). In that study, human peripheral blood was obtained from five donors and irradiated ex vivo (sham, 0.5, 2, 5 and 8 Gy). RNA was isolated from samples collected at 6 and 24 hrs after exposure and transcript levels were measured using Agilent-012391 Whole Human Genome Oligo Microarray G4112A . We then mean normalized the expression levels of each of the eight genes in this dataset across doses, times, and donors, and then summed theses values across all 8 genes for each blood sample in each treatment group. For calculating dose response, we plotted the average and standard error for each dose group, normalized to the average value of the sham group for each of the two time points.
Globally normalized whole genome expression profiles of patients undergoing total body irradiation (TBI) were obtained from the NCBI GEO database (GSE20162; ). In that study, peripheral blood gene expression profiles were obtained from 18 donors undergoing TBI. Patients were exposed to a total of 3.75 Gy in one day divided into three equal fractions of 1.25 Gy with approximately 4 hrs between fractions. Blood was collected before irradiation, 4 hrs after the first fraction of 1.25 Gy and 20–24 hrs after the first fraction. Blood from 14 healthy donors was collected as control. RNA was extracted and transcript levels were measured using Agilent Whole Human Genome Microarray G4112A . For the TBI dataset, we again mean normalized the expression levels of each of our 8 genes across all samples in the database for the patients and healthy donors. For each blood samples we calculated the sum of the normalized expression of each of the 8 genes, normalized to the average of the sum expression of the healthy donors.
Peripheral Blood Mononuclear Cell (PBMC) ex vivo Radiation Model
Seven donors (6 male, 1 female; age range, 20–50 years) provided two peripheral blood samples each, at least one month apart, for protein analyses. Blood was transferred to 3 equal (∼13 ml) aliquots into 50 ml conical tubes. Blood in tubes was exposed at room temperature to 0, 2 or 6 Gy X-rays at a rate of ∼1.25 Gy/min (2 Gy) or ∼1.30 Gy/min (6 Gy) (X-ray machine (Faxitron) set at 160 kV and 6.3 mA). Dosimetry was performed using a RadCal AccuPro dosimeter by measuring the accumulated dose over a specific time interval. After irradiation, blood samples were separated over Accuspin System-Histopaque-1077 (Sigma-Aldrich) according to the manufacturer’s instructions. PBMC were washed in phosphate buffered saline (PBS) and resuspended in RPMI 1640 medium (Sigma-Aldrich) supplemented with 10% heat-inactivated fetal bovine serum (Invitrogen) and cultured in duplicate T25 flasks for each dose group. Cells were maintained on a rocking platform at 37°C in a humidified incubator with 5% CO2 for 6 and 24 hrs.
Cell Lysates for Protein Analyses by Enzyme-linked Immunosorbent Assays (ELISA)
Buffy coats were collected from whole blood cultures and treated with a 1∶3 mixture of warm (37°C) RBC Lysis buffer (5 Prime) for two steps and then washed once with cold phosphate buffered saline. The obtained cell pellets or PBS-washed PBMC pellets, from the PBMC culture model, were then lysed with Pierce M-PER Mammalian Protein Extraction Reagent and 1X Halt protease/phosphatase inhibitors (Thermo Scientific). Extracts were collected, aliquoted and stored at −80°C. Protein concentrations were measured using Pierce BCA Protein Assay Reagent (Thermo Scientific). Amounts of protein in lysate or plasma were quantified using ELISA kits; human BAX ELISA kit (Assay Designs), human phosphorylated CHK2-thr68 ELISA kit (Cell Signalling). The biological effectiveness of LPS was confirmed by measuring secretion of IL-6 and TNF-α in plasma by ELISA following manufacturer’s recommended protocol (R&D Systems). ELISAs were performed following manufacturer’s instructions. BAX ELISAs were performed using 0.1 or 1 µg protein cell lysate per well for irradiated and non-irradiated samples, respectively. pCHK2-thr68 ELISAs were performed using 25 µg of protein cell lysate for all samples. IL-6 and TNF-α ELISAs were performed using undiluted or 1∶100-fold dilution of plasma for non-LPS and LPS-co-treated samples, respectively. All ELISA absorbance readings were read with reference to the standard curve, except for pCHK2-thr68 that had no standard curve and used average difference data between control and test samples as readout (Figure S1). The majority of absorbance readings were within a 0.1–0.7 range (Table S2). All samples were run in duplicate. ELISA plates were read using TECAN Infinite M200 plate reader and analyzed using the TECAN Magellan software. Raw ELISA data was loge transformed and mean-zero standardized to obtain a standard normal distribution. We performed inferential tests of hypothesis via independent 2 sample t-tests for each dose-time experimental group for each biomarker.
We investigated the classification characteristics of our panel of transcript and protein biomarkers for assigning individual samples into their correct exposure/treatment group: no treatment (N), radiation exposure only (R), LPS treatment only (L), and samples exposed to both radiation and LPS (RL). Classification was performed using marker expression values for n = 40 observations per marker, based on the replicate pair of observations per subject and 4 classes (40 = 2×5×4). A 4-class problem was considered for which the true class labels of observations were N, R, L, and RL. Marker order was determined via filtering by considering all possible pairs of classes, and for each pair ranking all 9 markers by their Gini index  for pairwise class discrimination; this involved 6 possible pairwise comparisons (6 = 4(3)/2). The Gini index, G, is a measure of class impurity among objects assigned to a given node in a decision tree . For a given tree node, , where pk is the proportion of node members in class k, and K is the number of classes. Gini has range 0≤G≤1, and is equal to zero when there is class purity in the node, and equal to unity when K→∞ and all pk tend to zero. The first gene selected was therefore the best discriminating marker for the N and R classes, followed by the best discriminating marker for the N and L class pairs. Any markers that were the best for multiple pairs of classes were selected in the order of their first appearance among ranks. After filtering to identify marker order based on discrimination, k-nearest neighbor (KNN) classification analysis was performed with K = 5, so the KNN model was called 5NN. An odd value for K was chosen to prevent ties in the predicted class membership of nearest neighbors. Classification accuracy based on ten 10-fold cross-validation for predicting the correct true class label was performed using sets of the 1, 2,…, 9 ordered markers. Linear discriminant analysis and PCA were not performed because covariance (correlation) is undefined for one marker. Diagnostic screening was also determined for the 9-marker set to determine sensitivity, specificity, positive predictive value (PV+), and negative predictive value (PV−). Sensitivity is equal to the proportion of observations in a given class with the correct class prediction, whereas specificity is the proportion of observations not in a given class whose predicted membership is not in the given class. On the other hand, PV+ reflects the proportion of observations predicted to be in a given class that are truly in the class, while PV− is defined as the proportion of observations that are not predicted to be in a given class which are not in the given class.
Radiation Response of DNA Repair Genes
The radiation response of 40 genes associated with various aspects of DNA damage response (Table S1) was surveyed. Twelve genes (Figure 1) were significantly modulated in transcript response 24 hrs after ex vivo exposure to 2 Gy X-rays, relative to sham-irradiated samples (individual t-test 2.2E-06<p<0.03; Figure S2). Most of these genes (11 of 12) showed increased expression after exposure (Figure 1), ranging from 2.3-fold for LIG1 to 17-fold for FDXR. RAD51, a key component of homologous recombination repair, was the only gene in this set that showed significant down regulation after exposure (2.5-fold). Expression responses for sham and irradiated samples showed little inter-individual variation and reproducible responses within donors sampled twice at approximately one month apart. These findings indicate that transcript responses of this panel of 12 DNA repair genes are robust biomarkers of radiation exposure in peripheral blood cells. Among these 12 genes, we found no overlap between sham and irradiated samples for 8 biomarkers (BBC3, FDXR, CDKN1A, GADD45a, PCNA, XPC, DDB2 and POLH; individual T-test 2.24E-06<p<7.45E-04), and found only slight overlaps for the other 4 biomarkers (BAX, CCNG1, LIG1 and RAD51; individual t-test 7.64E-04<p<2.57E-02) (Figure S2). CHK2 is included as an example of a gene that does not respond to radiation (Figure 1; p = 0.5). Our findings predict that when blood samples prior to exposure are not available, our panel of eight DNA repair markers can distinguish between 2 Gy irradiated and unirradiated individuals with 100% accuracy 24 hrs after a 2 Gy exposure.
Relative transcript level responses using human blood from 5 healthy human donors measured by quantitative RT-PCR analysis 24 hrs after 2 Gy exposure with respect to sham (0 Gy) transcript levels. Expression of the sham (0 Gy) and 2 Gy transcript responses were calculated relative to the average expression of ACTB (β-Actin). The delta Ct for β-Actin between sham and 2 Gy irradiated samples was <0.3 for all but one sample, which was excluded from this analysis. The fold-change for each gene between sham and irradiated samples was calculated using the delta-delta Ct method. Similar results were obtained when normalized using GAPDH expression as endogenous control (data not shown).
Validation of the Dose and Time Response Characteristics of Our 8-gene Transcript Panel in Independent Human ex vivo and in vivo Datasets
We tested the dose response characteristics of our 8-gene panel (BBC3, FDXR, CDKN1A, PCNA, XPC, GADD45a, DDB2 and POLH) using an independent public dataset containing microarray transcript expression data collected at 6 and 24 hrs after ex vivo exposures (sham, 0.5, 2, 5 and 8 Gy) in human blood from 5 independent donors. This analysis confirmed our primary finding of no overlap in transcript responses for any of the 8 genes between sham and irradiated samples at 24 hrs after 2 Gy exposures (Figure S3). We then investigated the dose and time response characteristics of our panel using the sum expression values of the 8 genes for each donor (Figure 2A). The average expression of our panel among the donor group was increased above sham for all dose groups tested at 6 hrs (p<5.5E-05) and 24 hrs (p<2.32E-04). The average sum expression at 6 hrs was consistently higher compared to 24 hrs for all doses tested (5.9E-04<p<0.02). Furthermore, the samples irradiated with 2 Gy were significantly different from those irradiated with 0.5 Gy (p<6.09E-03), 5 Gy (p<8.47E-03) or 8 Gy (p<1.65E-04) at 6 and 24 hrs, demonstrating the significant dose response characteristics of our panel.
The robustness of our panel of 8 non-overlapping radiation biomarkers was confirmed using two published expression array data sets: (A) ex vivo irradiated (0, 0.5, 2, 5, 8 Gy) human blood samples obtained from five independent donors 6 and 24 hrs after radiation exposure (GSE8917; ) and (B) human in vivo irradiated blood samples obtained from patients undergoing total body irradiation (GSE20162; ). A. Shown is the average of the summed expression for the samples in each exposure group (+/− standard error) normalized to the average expression of the 0 Gy samples for each time-point. B. Shown is the plot of the summed expression of the 8-gene panel of each blood sample in the in vivo study, normalized to the average of the healthy donor samples.
We then tested whether our 8-gene panel could distinguish human patients receiving total body irradiation (TBI) from pre-irradiation patients and healthy controls. We obtained a public dataset containing microarray transcript expression data of blood collected from 14 independent healthy donors and from 18 patients who provided blood samples before TBI treatment, at 4 hrs after the first of three fractions of 1.25 Gy and at 20–24 hrs after the first fraction. We calculated the sum expression value for blood sample for each patient and control subject to investigate their variation across experimental groups. As shown in Figure 2B, there was no overlap in expression between TBI treated blood samples and pre-TBI and control group values. The average expression of the 8-gene panel after TBI treatment was increased above the levels of healthy control group and pre-TBI blood levels for both timepoints tested, at 4 hrs after first fraction (1.25 Gy; p<1.34E-11) and at 20–24 hrs after the first fraction (3.75 Gy; p<1.45E-11).
In a separate analysis of human in vivo radiation response, we compared our 8-gene panel against a 25-gene signature developed by Meadows et al  to distinguish healthy individuals and pre-irradiation patients from the irradiated patients. In their study, peripheral blood was obtained from TBI patients before irradiation and 6 hrs after 1.5–2.0 Gy. Peripheral blood was also obtained from a population of healthy control individuals. Interestingly, 5 of our eight biomarkers were present in their signature (XPC, PCNA, CDKN1A, DDB2 and BBC3). These comparisons against two independent groups of blood samples from irradiated human patients provide compelling in vivo corroborative support for the utility of our 8-gene panel for radiation biodosimetry in blood cells.
LPS Modulation of Transcript and Protein Expression in Irradiated Whole Blood Cultures
We investigated the specificity of the radiation response of our biomarkers in the ex vivo blood radiation model in the context of inflammatory stress simulated by LPS. We confirmed that LPS treatment (50 ng/ml) induced an inflammatory response in white blood cells by measuring the secretion of IL-6 and TNF-α into plasma of all donors tested, (Figure S4). LPS treatment showed no significant changes in baseline transcript expression in 5 biomarkers (fold-change <1.5; GADD45a, PCNA, XPC, DDB2, POLH) (Figure 3). Significant changes were observed in 3 biomarkers (Figure 3): >8-fold (±1.1) increase in CDKN1A and reduced expression in BBC3 and FDXR (2.9-fold (±0.08) and 1.5-fold (±0.1), respectively).
Transcript level responses measured by quantitative RT-PCR analysis 24 hrs after LPS treatment of whole blood of two apoptosis, three cell cycle and three DNA repair genes with respect to transcript levels in untreated blood cultures. CDKN1A was strongly upregulated (∼8.2-fold) by LPS treatment alone in the absence of radiation exposure with little variation among donors. BBC3 and FDXR expression was downregulated (∼3-fold and ∼1.5-fold, respectively) by LPS treatment. LPS treatment did not modulate expression levels of GADD45a, PCNA, XPC, DDB2 and POLH (<1.5-fold change in expression compared to untreated samples). ACTB was used to normalize gene expression in samples in which the delta Ct of LPS treated vs untreated was less than 0.3 (donor 1.1, 3, 4.1, 5 and 5.1). GAPDH was not used to normalize since its levels varied depending on the presence of LPS (the average Ct difference between GAPDH in LPS treated and untreated samples was 0.54).
We then investigated the effect of LPS treatment on radiation response of the 8 genes in our panel, using blood cultures exposed to 2 Gy X-rays and co-treated with LPS (50 ng/ml). The strongest effect of LPS on the radiation responses was seen for CDKN1A, BBC3 and FDXR (Figure 4; fold-change difference >1.4-fold and p<0.03). LPS modified the radiation response of CDKN1A by an additional 1.4-fold increase over the effects of radiation on CDKN1A expression alone (p = 0.03; Figure 4A). BBC3 and FDXR expression, on the other hand, were repressed 1.6-fold (2.7-fold upregulated after radiation vs. 1.7-fold after radiation in the presence of LPS; p = 0.03) and 1.7-fold (17-fold upregulated after radiation vs. 10-fold after radiation in the presence of LPS; p = 1.2E-04) after radiation and subsequent culture in the presence of LPS in comparison to the effects of radiation alone (Figure 4B and C). The radiation responses of the remaining five biomarkers were not significantly altered by LPS treatment (Figure 5; <1.4-fold change or p>0.03).
Transcript level responses measured by quantitative RT-PCR analysis 24 hrs after exposure to 2 Gy, LPS treatment, and combined LPS and 2 Gy of whole blood of CDKN1A (A), BBC3 (B), and FDXR (C) genes with respect to transcript levels in un-treated blood cultures. A. A radiation exposure of 2 Gy in the absence of LPS (left panel) or LPS treatment alone (middle panel) induced CDKN1A to approximately the same level at 24 hrs: 7.3 vs 8.2-fold, respectively (T-Test p = 0.47). LPS treatment in the presence of a 2 Gy radiation exposure induced CDKN1A expression ∼10.2-fold (right panel), which is a 1.4-fold increase compared to 2 Gy alone (T-test p = 0.03). B. In the absence of LPS, radiation induced BBC3 ∼2.7-fold (left panel). LPS treatment alone (middle panel) suppresses BBC3 ∼2.9-fold. LPS treatment in the presence of a 2 Gy radiation exposure induced BBC3 expression ∼1.7-fold (right panel), a ∼1.6-fold decrease in BBC3 expression when compared to 2 Gy alone (T-test p = 0.03). C. In the absence of LPS, radiation induced FDXR ∼17-fold (left panel). LPS treatment alone (middle panel) suppressed FDXR ∼1.5-fold. LPS treatment in the presence of a 2 Gy radiation exposure induced FDXR expression ∼10-fold (right panel), a ∼1.7-fold decrease in FDXR expression when compared to 2 Gy alone (T-test p = 1.2E-04).
Our analyses of protein expression confirm that phosphorylated CHK2 protein is a radiation responsive biomarker , and demonstrate that the transcript levels of CHK2 were unaffected by radiation only, LPS only, and co-exposure to both agents. Phosphorylated CHK2-thr68 protein levels showed a modest ∼1.6 (±0.1; p = 2.9E-05) fold increase in the whole blood ex vivo culture model at 24 hours post 2 Gy irradiation compared to sham (Figure 6). However, in the presence of LPS, this protein response was completely suppressed and indistinguishable from sham-irradiated samples without LPS co-treatment (p>0.4) (Figure 6). This is compelling evidence that pCHK2-thr68 may not be a suitable biomarker of radiation exposure when in the context of inflammatory stress. Interestingly, we found that by including pCHK2-thr68 as a member of the panel of biomarkers improved the discrimination of radiation-exposed individuals with inflammatory stress from those exposed to radiation alone. We arrived at this conclusion by comparing the relative protein radiation responses in our PBMC model compared to our data from the whole blood culture model. We measured pCHK2-thr68 as well as BAX protein levels in PBMCs of healthy donors at 6 and 24 hours after ex vivo exposure to 2 or 6 Gy X-rays. BAX was included in this study as a surrogate indicator for the role of apoptosis in these models (Figure S5A). As expected, the pCHK2-thr68 responses were stronger at the earlier timepoint, while the BAX responses were stronger at later time (Figure S5B). Both BAX and pCHK2-thr68 proteins showed significant increases at 6 and 24 hrs after both 2 and 6 Gy exposures (p<0.05) (Figure S5C). Due to the substantial variability in radiation response in the PBMC model system both among donors and between repeated blood draws of the same donor, we used the protein response data from the whole blood model in our further analyses.
Transcript level responses measured by quantitative RT-PCR analysis 24 hrs after exposure to 2 Gy, LPS treatment, and combined LPS and 2 Gy of whole blood of GADD45a, PCNA, XPC, POLH and DDB2 genes with respect to transcript levels in un-treated blood cultures. Transcript levels of none of these five genes were significantly modulated 24 hrs after 2 Gy exposure in the presence of LPS compared to 2 Gy alone (fold-change <1.4-fold or p>0.03). Interestingly, the radiation response of all five genes was slightly suppressed by LPS treatment suggesting that LPS had a small effect on the 2 Gy response of these genes.
Protein levels of phosphorylated CHK2-thr68 in protein lysate from cultured whole blood in the presence or absence of LPS (50 ng/ml) were measured by ELISA. Absorbance values were normalized with respect to the average pCHK2-thr68 level in unirradiated donors. In the absence of LPS, radiation induced CHK2-thr68 levels ∼1.6-fold (±0.1) relative to sham irradiated samples, whereas in the presence of LPS, CHK2-thr68 levels were indistinguishable from sham irradiated samples (p>0.4).
Multi-group Classification of Blood Samples by their Radiation and Inflammation Status
We tested our combined nine-gene panel of eight transcript and one protein biomarkers in our ex vivo blood model to test its ability to discriminate among four exposure/treatment groups: radiation exposure only (R), inflammatory stress only (L), combined exposures with both radiation and LPS (RL), and samples with no radiation exposure or LPS treatment (N) (Figure 7). Marker filtering with the Gini index (see methods) resulted in the following marker order: PCNA, CDKN1A, pCHK2-thr68, BBC3, FDXR, DDB2, XPC, POLH and GADD45a. Figure 8 illustrates the cumulative 4-class accuracy for the sets of 1, 2,…,9 markers based on their order of selection during filtering. The overall accuracy for the single best marker, PCNA, was 0.65, and the accuracy of 0.88 was attained when 5 markers were used, after which the overall accuracy leveled off. Table 1 lists the results of diagnostic screening analysis for the 9-marker set. The majority of sensitivity calculations approached 0.9 or greater. Specificity was in the 0.8–0.9 range. The positive predictive value (PV+) was unity (1.00) for the NL class, 0.96 for the L class, and below 0.8 for the R and RL classes, whereas the negative predictive value (PV−) ranged from 0.81–0.91. This analysis has identified a subpanel of 5 biomarkers that correctly assign individual blood samples to one of the four different experimental conditions with an overall classification accuracy of ∼ 90%.
In comparison to untreated sham samples, inflammation in the absence of radiation exposure upregulates CDKN1A (red) and downregulates FDXR and BBC3 (green). Samples exposed to 2 Gy radiation only exhibit increased expression of all nine biomarkers, whereas subjects exposed to 2 Gy plus inflammation stress show modified induction of CDKN1A, FDXR and BBC3 and abrogation of the phosphorylation of CHK2 protein. The arrows in the radiation and inflammation combined treatment group indicate the direction of expression relative to the radiation alone group.
Our findings showcase the advantage of using blood cells and the expression of genes associated with the DNA repair for human radiation biodosimetry, and furthermore that these genes have the ability to discriminate between radiation dose and inflammation stress. In a survey of 40 DNA repair genes in the human peripheral blood cells ex vivo radiation model (Table S1), twelve genes showed more than two fold changes in transcript levels at 24 hours after 2 Gy exposures. These included the cell cycle regulators (CDKN1A, GADD45a, PCNA and CCNG1), apoptosis regulators (BAX, BBC3 and FDXR) and genes involved in specific DNA repair functions (XPC, DDB2, LIGI, POLH and RAD51). We compared the responses to radiation and inflammation stress to develop a panel of 8 genes that we validated using publicly available expression datasets for (1) an independent group of donors in a blood ex vivo model, and (2) a second independent group of patients who provided blood samples before and after whole body radiation (, , , Figure 2A). Our findings support the strength of using DNA repair related genes to detect radiation exposure in the context of inflammation stress, which may become helpful for discriminating between worried-well, those exposed to medically significant doses of ionizing radiation and those experiencing inflammation stress (Table 1). By including protein expression markers we developed a 9-gene panel (8 transcripts and one protein marker) that correctly discriminated irradiated from unirradiated blood samples independent of the presence or absence of inflammation stress (Figure 7), with a ∼90% 4-group classification accuracy (Figure 8).
Classification accuracy based on ten 10-fold cross-validation as a function of the number of markers considered, based on order determined during filtering with the Gini index. The four classes used in this analysis are: radiation only (R), inflammation stress only (L), combined exposures involving both radiation and LPS (RL), and samples with no radiation exposure and no LPS treatment (N). Marker order is: PCNA, CDKN1A, pCHK2-thr68, BBC3, FDXR, DDB2, XPC, POLH, and GADD45a. Maximum classification accuracy was 0.88 for the top 5-marker set.
The DNA repair-associated genes we surveyed are regulated by TP53 signaling . The TP53 tumor suppressor protein is central to cell signaling networks following cellular stressors, including DNA damage such as that caused by ionizing radiation. TP53 modulates the main DNA repair processes in eukaryotic cells (base excision repair (BER), nucleotide excision repair (NER), non-homologous end-joining (NHEJ) and homologous recombination (HR) along with direct roles in induction of DNA damage-induced cell cycle arrest and apoptosis. TP53 is activated after DNA damage through phosphorylation to function as a transcriptional regulator inducing expression of a number of downstream target genes that directly control cellular outcomes . Activators of TP53 include CHK2, a serine/threonine kinase that, upon activation directly by ATM phosphorylation (e.g., threonine-68) or indirectly by other protein kinases (e.g., DNA-PKcs), acts as both a downstream signal transducer of DNA damage and an effector for DNA repair, checkpoint control and apoptosis . In our study we did not observe changes in transcript expression of CHK2 following irradiation, consistent with the role of CHK2 as an upstream mediator of TP53 rather than a downstream target, however, an increase in phosphorylated CHK2 protein was observed. Phosphorylation of TP53 at serine-20 by CHK2 prevents MDM2-mediated TP53 degradation. This enhancement of TP53 stability allows for the continuance of downstream DNA damage response pathways including apoptosis, of which BAX is an effector . CHK2, a direct substrate of ATM, is an earlier DNA damage response protein than BAX. Hirao et al.  observed by Western blot that CHK2 levels in both sham- and 5 Gy irradiated wild-type mouse thymocytes precede BAX up until 6 h post-irradiation, which is consistent with our protein ELISA results post-irradiation.
Our radiation-response results in the ex vivo blood model are consistent with previous human studies , , , –,  with the exception of RAD51, which showed a decrease in expression in our study . A recent study in mice of radiation effects on gene expression showed significant increases in expression of CDKN1A, BBC3 and GADD45a at 24 hrs after 2 Gy whole body irradiation . However, in that study DDB2 was downregulated and no significant changes were observed for FDXR or XPC, which is inconsistent with our results and those of others in humans irradiated ex vivo . Expression of GADD45a, LIG1 and XPC were decreased at 24 hours after 6 Gy IR in mice, whereas we observed increased expression at 24 hrs after 2 Gy in our ex vivo human blood culture model consistent with published human ex vivo and in vivo literature , , . Also, our use of a 2 Gy exposure (rather than 6 Gy used in a prior mouse study ) is more relevant for radiation biodosimetry because individuals having a radiation exposure dosage of less than 2 Gy require no immediate treatment as opposed to those having a dosage higher than 2 Gy. The inherent differences between murine and human assays emphasize the importance of using human model systems to validate biomarkers for human radiation biodosimetry. Our study investigates the blood of unrelated people and we confirm our findings in a separate independent group of unrelated people, suggesting that interindividual variation in the transcript response is not a major factor for the genes in our panel.
Understanding the effects of confounding factors, such as inflammation stress, on radiation-responsive biomarkers is important for assessing their utility in radiation biodosimetry in practical human exposure scenarios , , . Of the 8 radiation-responsive genes in our study, only three (CDKN1A, FDXR and BBC3) were confounded by LPS-induced inflammation stress. CDKN1A is a canonical marker of DNA damage response and has been proposed as a biomarker of radiation exposure , . While cigarette smoking did not confound the radiation response of CDKN1A , our study shows that inflammatory stress induced CDKN1A transcript levels in the absence of radiation exposure. Our finding seriously undermines the promise of CDKN1A as a predictive tool for radiation exposure in individuals suffering simultaneous inflammatory stress. Studies in the murine central nervous system also identified CDKN1A as an inflammatory response gene  and LPS exposure upregulated CDKN1A transcripts in mice . LPS-induced and the radiation-induced CDKN1A responses were indistinguishable in our human blood model, while in the mouse the upregulation of CDKN1A at 24 hours after LPS injection did not mask the ability to detect a radiation response . This difference in murine vs human responses might be attributed to the differences in LPS dosage (50 ng/ml in our study vs. 0.3 mg/kg which equals 7.2 µg per mouse), LPS bioavailability and species differences in response.
We have made the new observation that LPS co-treatment confounds the transcript response of FDXR and BBC3, also compromising their utility as radiation biodosimeters. The pro-apoptotic gene, BBC3, is responsible for induction of apoptosis pathways following DNA damage. Whole blood cultured in the presence of LPS repressed the expression of BBC3 ∼2.5-fold. Co-treatment with LPS and radiation diminished BBC3 transcripts compared to either LPS alone or radiation alone. Consistent with our finding, LPS suppressed apoptosis in human blood monocytes , but some studies found opposite responses . The transcription of BBC3 is regulated by a complex combination of pro-apoptotic and pro-survival mechanisms , suggesting that LPS may suppress BBC3 transcription in blood cultures through activation of pro-survival signals. In contrast to our findings, Tucker and colleagues observed a marginal confounding effect of LPS treatment on the radiation response of BBC3 in mice , again emphasizing the importance of validating biomarker panels in a human model.
The increases in protein levels of phosphorylated CHK2 after radiation-alone exposures were fully suppressed in the presence of LPS, also undermining it as a useful protein biomarker for radiation response in the context of inflammation stress. CHK2 protein is phosphorylated in response to DNA damage which activates the protein , . While we demonstrate that LPS co-treatment fully abrogates this radiation-induced CHK2 phosphorylation process, the underlying mechanisms for this confounding effect remain unclear.
The LPS-modified CDKN1A, FDXR and BBC3 transcript levels were remarkably uniform among donors, even though the secretions of IL-6 and TNF-α two genes well-known to be induced by LPS, were more variable (Figure S4). The levels of LPS-induced IL-6 and TNF-α were highly correlated (R2 = 0.8; Figure S6). Among 4 of the donors, IL-6 and TNF-α levels in the first blood draw were nearly identical to those in the second blood draw, 1 month later. These findings point to the hypothesis that the induction of inflammatory response genes IL-6 and TNF-α depend on genetic background, while the inductions of CDKN1A and BBC3 are more ‘switch-like’. This would predict that other confounding stimuli might also affect CDKN1A and BBC3 expression.
Our research has identified a small panel of DNA repair-related biomarkers that distinguish among human blood samples from four radiation exposure scenarios: no radiation exposure, 2 Gy radiation exposure only, inflammation stress without radiation exposure, and combined 2 Gy exposure plus inflammation stress. Independent validation for dose and time response and with in vivo total body irradiated samples further supports the utility of these biomarkers for clinical applications, accident scenarios and other situations involving potential radiation exposure. Future studies will be needed to evaluate our panel for effects of gender, age, and inter-individual variations, to examine the influence of differential radiation cytotoxicities of the white cell subtypes on expression biodosimetry , and to investigate the radiation specificity of our panel using other inflammation, chemical, and physical stressors that are relevant for human radiation biodosimetry applications in various hypothetical exposure scenarios.
Standard curves for ELISAs. BAX, IL-6 and TNF-α representative standard curves are shown. pCHK2-thr68 did not use a standard curve.
Transcript level radiation responses of twelve DNA repair-related biomarkers. Relative expression of the sham (0 Gy) and 2 Gy transcript responses were calculated relative to the mean expression of ACTB (β-Actin). Each symbol represents mean of 3 replicate relative expression levels for the designated DNA repair genes from a blood collection of a single donor. Data are plotted for 5 donors, each donating two blood samples. The delta Ct for β-Actin between sham and 2 Gy irradiated samples was <0.3 for all but one sample, which was excluded from this analysis. A two-sided T-test was performed on the distribution of expression levels between sham and irradiated samples (p-values are shown in the lower right of each box-plot).
Transcript level radiation responses of eight DNA repair-related biomarkers in an independent dataset. Normalized expression intensities of the sham (0 Gy) and 2 Gy transcript responses are shown. Each symbol represents expression levels for the designated DNA repair gene from a blood collection of a single donor. Data are plotted for 5 donors. A two-sided T-test was performed on the distribution of expression levels between sham and irradiated samples (p-values are shown in the lower right of each box-plot).
Increased plasma protein levels of IL-6 and TNF-α in LPS-treated human blood in 24-hour culture. Levels of IL-6 (A) and TNF-α (B) were measured by ELISA in human whole blood culture after LPS treatment (50 ng/ml) for 24 hrs. Blood cultures, from five unique donors, each sampled twice (second samples from each donor indicated by x.1), were assessed for IL-6 and TNF-α protein levels in plasma at 24 hrs by ELISA. Concentrations of protein (mg/ml) in each sample and treatment group are listed in the tables below the figures. In the absence of LPS-induced inflammatory stress, there is little detectable protein for either IL-6 or TNF-α. The presence of LPS induces up to a 7000-fold increase in protein levels for IL-6 (donor 4) and a 3000-fold increase in TNF-α (donor 4). Responses varied across donors but were consistent between the two different protein markers of inflammatory stress for each donor (donor 3 and donor 4 showed the greatest induction of both proteins).
Radiation-induced increased protein levels of BAX and phosphorylated CHK2-thr68 in human ex vivo quiescent PBMC. A. BAX and pCHK2-thr68 responses by ELISA after 0, 2 or 6 Gy at 6 and 24 hrs in independent replicate culture flasks from the same blood sample of two donors produce minimal technical variability (R2 = 0.95 for pCHK2-thr68; R2 = 0.92 for BAX). B. Levels of BAX and pCHK2-thr68 were measured by ELISA in unstimulated PBMC after 0, 2, or 6 Gy ionizing radiation. PBMC cultures from six or five unique donors were assessed for BAX and pCHK2-thr68 protein levels at 6 hrs and 24 hrs by ELISA. Data were normalized with respect to sham for each timepoint. Repeat draws from the same donor ∼ 1 month after the first blood draw are indicated with a “.1” after the donor identifier. C. T-test results (t-statistics and p-values in parentheses) identify significant mean differences in BAX and pCHK2-thr68 ELISA data for the 0- vs. 2 Gy and 0- vs. 6 Gy groups at 6 hrs and 24 hrs after irradiation.
Correlation between IL-6 and TNF-α responses in LPS treated whole blood cultures. Secretion of IL-6 and TNF-α were measured by ELISA for 5 donors. Each donor is represented with a different color. All donors were sampled twice at least one month apart. Note that the TNF-α and IL-6 secretory response after LPS treatment is variable among donors, but highly correlated between the replicate blood draws for each donor with the exception of the donor represented in red.
Target genes selected from DNA damage response pathways for transcript analysis.
Conceived and designed the experiments: HB AMS FM SXW WFB MC LP AJW. Performed the experiments: HB AMS BM SB EK YT. Analyzed the data: HB AMS FM BM SB YT LP AJW. Contributed reagents/materials/analysis tools: YT LP. Wrote the paper: HB AMS AJW.
- 1. Fenech M (2011) Current status, new frontiers and challenges in radiation biodosimetry using cytogenetic, transcriptomic and proteomic technologies. Radiation Measurements 46: 737–741.
- 2. Pinto MM, Santos NF, Amaral A (2010) Current status of biodosimetry based on standard cytogenetic methods. Radiat Environ Biophys 49: 567–581.
- 3. Falt S, Holmberg K, Lambert B, Wennborg A (2003) Long-term global gene expression patterns in irradiated human lymphocytes. Carcinogenesis 24: 1837–1845.
- 4. Amundson SA, Do KT, Shahab S, Bittner M, Meltzer P, et al. (2000) Identification of potential mRNA biomarkers in peripheral blood lymphocytes for human exposure to ionizing radiation. Radiat Res 154: 342–346.
- 5. Turtoi A, Sharan RN, Srivastava A, Schneeweiss FH (2010) Proteomic and genomic modulations induced by gamma-irradiation of human blood lymphocytes. Int J Radiat Biol 86: 888–904.
- 6. Kabacik S, Mackay A, Tamber N, Manning G, Finnon P, et al. (2011) Gene expression following ionising radiation: identification of biomarkers for dose estimation and prediction of individual response. Int J Radiat Biol 87: 115–129.
- 7. Amundson SA, Grace MB, McLeland CB, Epperly MW, Yeager A, et al. (2004) Human in vivo radiation-induced biomarkers: gene expression changes in radiotherapy patients. Cancer Res 64: 6368–6371.
- 8. Kang CM, Park KP, Song JE, Jeoung DI, Cho CK, et al. (2003) Possible biomarkers for ionizing radiation exposure in human peripheral blood lymphocytes. Radiat Res 159: 312–319.
- 9. Dressman HK, Muramoto GG, Chao NJ, Meadows S, Marshall D, et al. (2007) Gene expression signatures that predict radiation exposure in mice and humans. PLoS Med 4: e106.
- 10. Paul S, Amundson SA (2008) Development of gene expression signatures for practical radiation biodosimetry. Int J Radiat Oncol Biol Phys 71: 1236–1244.
- 11. Daino K, Ichimura S, Nenoi M (2002) Early induction of CDKN1A (p21) and GADD45 mRNA by a low dose of ionizing radiation is due to their dose-dependent post-transcriptional regulation. Radiat Res 157: 478–482.
- 12. Paul S, Barker CA, Turner HC, McLane A, Wolden SL, et al. (2011) Prediction of in vivo radiation dose status in radiotherapy patients using ex vivo and in vivo gene expression signatures. Radiat res 175: 257–265.
- 13. Marchetti F, Coleman MA, Jones IM, Wyrobek AJ (2006) Candidate protein biodosimeters of human exposure to ionizing radiation. Int J Radiat Biol 82: 605–639.
- 14. Breen AP, Murphy JA (1995) Reactions of oxyl radicals with DNA. Free Radic Biol Med 18: 1033–1077.
- 15. Inoue M, Shen GP, Chaudhry MA, Galick H, Blaisdell JO, et al. (2004) Expression of the oxidative base excision repair enzymes is not induced in TK6 human lymphoblastoid cells after low doses of ionizing radiation. Radiat Res 161: 409–417.
- 16. Batty DP, Wood RD (2000) Damage recognition in nucleotide excision repair of DNA. Gene 241: 193–204.
- 17. Bessho T (1999) Nucleotide excision repair 3′ endonuclease XPG stimulates the activity of base excision repairenzyme thymine glycol DNA glycosylase. Nucleic Acids Res 27: 979–983.
- 18. Klungland A, Hoss M, Gunz D, Constantinou A, Clarkson SG, et al. (1999) Base excision repair of oxidative DNA damage activated by XPG protein. Mol Cell 3: 33–42.
- 19. Shimizu Y, Uchimura Y, Dohmae N, Saitoh H, Hanaoka F, et al.. (2010) Stimulation of DNA Glycosylase Activities by XPC Protein Complex: Roles of Protein-Protein Interactions. J Nucleic Acids 2010.
- 20. Shimizu Y, Iwai S, Hanaoka F, Sugasawa K (2003) Xeroderma pigmentosum group C protein interacts physically and functionally with thymine DNA glycosylase. EMBO J 22: 164–173.
- 21. D’Errico M, Parlanti E, Teson M, de Jesus BM, Degan P, et al. (2006) New functions of XPC in the protection of human skin cells from oxidative damage. EMBO J 25: 4305–4315.
- 22. Zschenker O, Borgmann K, Streichert T, Meier I, Wrona A, et al. (2006) Lymphoblastoid cell lines differing in p53 status show clear differences in basal gene expression with minor changes after irradiation. Radiother Oncol 80: 236–249.
- 23. Mayer C, Popanda O, Greve B, Fritz E, Illig T, et al. (2011) A radiation-induced gene expression signature as a tool to predict acute radiotherapy-induced adverse side effects. Cancer Lett 302: 20–28.
- 24. Amundson SA, Do KT, Fornace AJ Jr (1999) Induction of stress genes by low doses of gamma rays. Radiat Res 152: 225–231.
- 25. Brengues M, Paap B, Bittner M, Amundson S, Seligmann B, et al. (2010) Biodosimetry on small blood volume using gene expression assay. Health Phys 98: 179–185.
- 26. Tichy A, Zaskodova D, Rezacova M, Vavrova J, Vokurkova D, et al. (2007) Gamma-radiation-induced ATM-dependent signalling in human T-lymphocyte leukemic cells, MOLT-4. Acta biochimica Polonica 54: 281–287.
- 27. Wang S, Guo M, Ouyang H, Li X, Cordon-Cardo C, et al. (2000) The catalytic subunit of DNA-dependent protein kinase selectively regulates p53-dependent apoptosis but not cell-cycle arrest. Proceedings of the National Academy of Sciences of the United States of America 97: 1584–1588.
- 28. Zhang Y, Lim CU, Zhou J, Liber HH (2007) The effects of NBS1 knockdown by small interfering RNA on the ionizing radiation-induced apoptosis in human lymphoblastoid cells with different p53 status. Toxicology letters 171: 50–59.
- 29. Paul S, Amundson SA (2011) Gene expression signatures of radiation exposure in peripheral white blood cells of smokers and non-smokers. Int J Radiat Biol 87: 791–801.
- 30. Tucker JD, Grever WE, Joiner MC, Konski AA, Thomas RA, et al. (2012) Gene expression-based detection of radiation exposure in mice after treatment with granulocyte colony-stimulating factor and lipopolysaccharide. Radiat res 177: 209–219.
- 31. Guha M, Mackman N (2001) LPS induction of gene expression in human monocytes. Cell Signal 13: 85–94.
- 32. Lavnikova N, Laskin DL (1995) Unique patterns of regulation of nitric oxide production in fibroblasts. J Leukoc Biol 58: 451–458.
- 33. Schroeder A, Mueller O, Stocker S, Salowsky R, Leiber M, et al. (2006) The RIN: an RNA integrity number for assigning integrity values to RNA measurements. BMC Mol Biol 7: 3.
- 34. Quinlan JR (1986) Induction of decision trees. Machine Learning 1: 81–106.
- 35. Meadows SK, Dressman HK, Muramoto GG, Himburg H, Salter A, et al. (2008) Gene expression signatures of radiation response are specific, durable and accurate in mice and humans. PloS one 3: e1912.
- 36. Ahn JY, Schwarz JK, Piwnica-Worms H, Canman CE (2000) Threonine 68 phosphorylation by ataxia telangiectasia mutated is required for efficient activation of Chk2 in response to ionizing radiation. Cancer Res 60: 5934–5936.
- 37. Amundson SA, Patterson A, Do KT, Fornace AJ Jr (2002) A nucleotide excision repair master-switch: p53 regulated coordinate induction of global genomic repair genes. Cancer biology & therapy 1: 145–149.
- 38. Zhang XP, Liu F, Wang W (2011) Two-phase dynamics of p53 in the DNA damage response. Proceedings of the National Academy of Sciences of the United States of America 108: 8990–8995.
- 39. Antoni L, Sodha N, Collins I, Garrett MD (2007) CHK2 kinase: cancer susceptibility and cancer therapy - two sides of the same coin? Nature reviews Cancer 7: 925–936.
- 40. Zhivotovsky B, Kroemer G (2004) Apoptosis and genomic instability. Nature reviews Molecular cell biology 5: 752–762.
- 41. Hirao A, Kong YY, Matsuoka S, Wakeham A, Ruland J, et al. (2000) DNA damage-induced activation of p53 by the checkpoint kinase Chk2. Science 287: 1824–1827.
- 42. Li MJ, Wang WW, Chen SW, Shen Q, Min R (2011) Radiation dose effect of DNA repair-related gene expression in mouse white blood cells. Medical science monitor : international medical journal of experimental and clinical research 17: BR290–297.
- 43. Russell JS, Brady K, Burgan WE, Cerra MA, Oswald KA, et al. (2003) Gleevec-mediated inhibition of Rad51 expression and enhancement of tumor cell radiosensitivity. Cancer Res 63: 7377–7383.
- 44. Ring RH, Valo Z, Gao C, Barish ME, Singer-Sam J (2003) The Cdkn1a gene (p21Waf1/Cip1) is an inflammatory response gene in the mouse central nervous system. Neurosci Lett 350: 73–76.
- 45. Eslick J, Scatizzi JC, Albee L, Bickel E, Bradley K, et al. (2004) IL-4 and IL-10 inhibition of spontaneous monocyte apoptosis is associated with Flip upregulation. Inflammation 28: 139–145.
- 46. Han J, Flemington C, Houghton AB, Gu Z, Zambetti GP, et al. (2001) Expression of bbc3, a pro-apoptotic BH3-only gene, is regulated by diverse cell death and survival signals. Proceedings of the National Academy of Sciences of the United States of America 98: 11318–11323.
- 47. Riecke A, Rufa CG, Cordes M, Hartmann J, Meineke V, et al. (2012) Gene expression comparisons performed for biodosimetry purposes on in vitro peripheral blood cellular subsets and irradiated individuals. Radiat res 178: 234–243.