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Conceived and designed the experiments: KLK GHM. Performed the experiments: AM RS KLK GHM. Analyzed the data: JG BD WCW BHC KLK GHM. Wrote the paper: KLK GHM. Data acquisition: AM RS SEW MJZ PAL AAL CLD RRR JB KLK GHM.
Mycobacterium tuberculosis (Mtb) infection may cause overt disease or remain latent. Interferon gamma release assays (IGRAs) detect Mtb infection, both latent infection and infection manifesting as overt disease, by measuring whole-blood interferon gamma (IFN-γ) responses to Mtb antigens such as early secreted antigenic target-6 (ESAT-6), culture filtrate protein 10 (CFP-10), and TB7.7. Due to a lack of adequate diagnostic standards for confirming latent Mtb infection, IGRA sensitivity for detecting Mtb infection has been estimated using patients with culture-confirmed tuberculosis (CCTB) for whom recovery of Mtb confirms the infection. In this study, cytokines in addition to IFN-γ were assessed for potential to provide robust measures of Mtb infection.
Cytokine responses to ESAT-6, CFP-10, TB7.7, or combinations of these Mtb antigens, for patients with CCTB were compared with responses for subjects at low risk for Mtb infection (controls). Three different multiplexed immunoassays were used to measure concentrations of 9 to 20 different cytokines. Responses were calculated by subtracting background cytokine concentrations from cytokine concentrations in plasma from blood stimulated with Mtb antigens.
Two assays demonstrated that ESAT-6, CFP-10, ESAT-6+CFP-10, and ESAT-6+CFP-10+TB7.7 stimulated the release of significantly greater amounts of IFN-γ, IL-2, IL-8, MCP-1 and MIP-1β for CCTB patients than for controls. Responses to combination antigens were, or tended to be, greater than responses to individual antigens. A third assay, using whole blood stimulation with ESAT-6+CFP-10+TB7.7, revealed significantly greater IFN-γ, IL-2, IL-6, IL-8, IP-10, MCP-1, MIP-1β, and TNF-α responses among patients compared with controls. One CCTB patient with a falsely negative IFN-γ response had elevated responses with other cytokines.
Multiple cytokines are released when whole blood from patients with CCTB is stimulated with Mtb antigens. Measurement of multiple cytokine responses may improve diagnostic sensitivity for Mtb infection compared with assessment of IFN-γ alone.
Tuberculosis remains a public health threat and is a leading cause of death worldwide, with an estimated 1.7 million deaths annually . Approximately one third of the world's population are infected with the causative bacterium, Mycobacterium tuberculosis (Mtb), and at risk for developing tuberculosis disease. Without intervention, approximately five to ten percent of those latently infected will develop overt disease and the potential to transmit Mtb to others .
Measurement of the IFN-γ response to Mtb antigens has proven useful in detecting Mtb infection, both latent infection and infection manifesting as overt disease –. These assays, referred to as IFN-γ release assays (IGRAs), use enzyme-linked immunosorbent assays (ELISAs) to measure differences in the concentration of IFN-γ, or enzyme-linked immunospot assays (ELISpots) to measure differences in the number of cells that produce IFN-γ, after incubation of whole blood or peripheral blood mononuclear cells (PBMCs) with Mtb antigens. Initially, IGRAs assessed response to tuberculin purified protein derivative (PPD) or culture filtrate of Mtb , . Eventually, proteins that are present in Mtb but absent from bacillus Calmette-Guérin (BCG) vaccine strains and most nontuberculous mycobacteria were found to improve IGRA specificity –. Early-secreted antigenic target-6 (ESAT-6), culture filtrate protein 10 (CFP-10), and TB7.7 (also called Rv2654) can induce IFN-γ release, and manufactured peptides representing these Mtb proteins are used in various combinations as antigenic stimuli in commercially available IGRAs designed to detect Mtb infection , , . While estimates of IGRA specificity for Mtb infection are generally high, estimates of IGRA sensitivity vary widely and in most situations are less than ideal. Estimates of IGRA sensitivity range from 70 to 90% based on pooled data from published reviews involving predominantly adults with Mtb infection that was confirmed by culture, i.e., adults with culture-confirmed tuberculosis (CCTB) , . Studies in high TB-endemic countries have shown lower IGRA sensitivity than studies in low TB-endemic countries . Suboptimal IGRA sensitivity may result from a reduction in IFN-γ release in patients with active or advanced tuberculosis and the fact that fewer antigenic epitopes are presented by specific Mtb antigens compared with PPD. A lack of accurate diagnostic standards hampers attempts to estimate test sensitivity for latent Mtb infection. There is no gold diagnostic standard with which to confirm the presence of latent Mtb infection. However, recovery of Mtb by culture in a patient with symptoms compatible with tuberculosis is adequate confirmation for Mtb infection, and has been used in most studies to estimate IGRA sensitivity , . Other cytokines used in combination or as alternatives to IFN-γ may improve sensitivity for detecting Mtb infection. Use of antigens in combination (e.g., ESAT-6, CFP-10, & TB7.7 combined) may also increase analytic and clinical sensitivity by increasing the number of epitopes available to stimulate lymphocytes, thus increasing the amount of cytokine released.
Numerous cytokines have been implicated in the pathogenesis and control of Mtb infection –. Measurement of multiple proinflammatory and anti-inflammatory cytokines, chemokines, and growth factors associated with Mtb infection (collectively referred to as cytokines for simplicity) may facilitate its detection.
The objectives of this study were: 1) to assess the responses of multiple cytokines to individual and combinations of Mtb antigens, 2) to compare the diagnostic potential of other cytokines with IFN-γ for detecting Mtb infection, and 3) to determine if measurement of multiple cytokines can improve detection accuracy. To increase the likelihood of identifying diagnostically important alternative cytokines, we studied subjects categorized with a high degree of confidence into those with Mtb infection (i.e., patients with CCTB) and those without infection (low-risk control subjects), and used three different multiplexed assays that examined different panels of cytokines.
We previously described comparisons of tuberculin skin test (TST) and QuantiFERON®-TB Gold test (QFT-G, Cellestis Ltd., Victoria, Australia) results among patients with suspected tuberculosis  and among low-risk Navy recruits . People were excluded if they were known to have received >7 days of therapy for tuberculosis or latent Mtb infection. During these studies, most subjects provided blood for evaluation of additional cytokines and antigens after providing written informed consent as approved by Human Subjects Protection Review Boards at all participating institutions: the Centers for Disease Control and Prevention (CDC) Institutional Review Board (IRB), the Boston University Medical Center IRB, the Colorado Multiple Institutional Review Board for Denver Public Health Department, the University of North Texas Health Science Center at Fort Worth and Texas College of Osteopathic Medicine IRB for the Protection of Human Subjects, the National Naval Medical Center IRB, the University of Medicine and Dentistry of New Jersey IRB, the San Diego State University IRB, and the University of California, San Francisco Committee on Human Research. Subjects consented to provide at least 5 mL of blood for the parent study, but could provide up to 30 mL of blood (to allow evaluation of other tests) if possible without additional venipuncture. When the volume of blood was adequate, one-mL aliquots of heparinized blood were incubated simultaneously with saline (Nil), phytohemagglutinin A (mitogen), and cocktails of overlapping peptides representing Mtb antigens, including ESAT-6, CFP-10, TB7.7, and combinations of these antigens (ESAT-6+CFP-10 or ESAT-6+CFP-10+TB7.7), for 16 to 24 hours at 37°C within 12 hours of collection. The peptides simulating ESAT-6 and CFP-10 were identical to those used in QFT-G and the QuantiFERON-TB Gold In-Tube test (QFT-GIT); the peptide representing TB7.7 was identical to that used in QFT-GIT; the peptide cocktails were provided by Cellestis Ltd., Victoria, Australia. After incubation, the plasma supernatants were transferred to micro-tubes in 96-well format, and frozen at −80°C.
Stored plasma samples from a convenient number of patients (N=21) with CCTB and from a similar number of subjects (N=24) at low risk for Mtb infection (controls) were selected (as depicted in Figures 1A–B) for evaluation. Funding limitations determined the number of samples assayed. Stored plasma samples from subjects with HIV infection or indeterminate QFT-G results were not included; otherwise, plasma was selected by convenience sampling from lists of patients with CCTB and subjects at low risk of Mtb infection without other bias. Clinical and epidemiologic data were collected as part of the parent study. Patients with symptoms or signs of active tuberculosis were considered to have CCTB if Mtb was recovered from one or more clinical specimens by culture. Subjects were eligible to be controls and presumed to be uninfected if they denied contact with persons with tuberculosis, were not born (or had not lived >1 month) in a country with an estimated TB prevalence higher than 20 per 100,000 population based on reported nativity and estimates of TB prevalence for 1990 , and had not resided, worked or volunteered >1 month at a homeless shelter, prison, drug rehabilitation unit, hospital, or nursing home.
For this study, stored plasma was thawed, aliquoted, and assayed immediately or aliquots were refrozen and thawed once for additional assays. When possible, plasma from the same subject was tested with more than one multiplexed immunoassay. However, this was rare because of limitations in the amount of available plasma and in the allowed number of freeze-thaw cycles.
IFN-γ concentrations were measured by a commercial ELISA using methods and reagents as previously described for the QFT-G . The concentrations of IFN-γ reported in international units/mL (IU/mL) were converted to pg/mL by multiplying by 40 pg/IU . When the optical density for a plasma sample was higher than that of the highest standard, which was common following mitogen stimulation, the value was extrapolated.
An in-house multiplexed microsphere-based immunoassay (MMIA), also called suspension array, was modified to measure the concentrations of 10 different cytokines. An 8-plex assay that was developed and validated using Luminex technology (Luminex Corp., Austin, TX) for IFN-γ, TNF-α, IL-2, IL-4, IL-6, IL-8, IL-10 and IL-12 (p70) , was modified to include VEGF (BioSource/Invitrogen, Carlsbad, CA) and IL-1β (R&D Systems, Minneapolis, MN). The resulting 10-plex cytokine immunoassay was validated by testing for both cross-reactivity of reagents and recovery of spiked multiplexed cytokine standards, as described previously , . The assay proceeded as described previously . Briefly, the multiplexed immunoassay was performed by combining all 10 cytokine standards at a concentration of 5000 pg/mL each in phosphate-buffered saline, pH 7.4–0.5% bovine serum albumin −0.02% sodium azide (PBN) and serially diluting the mixture three-fold to obtain concentrations in the range of 5000 to 2.29 pg/mL for the standard curves. Pooled normal human plasma (pretested to ensure undetectable cytokine levels) was added so that the volume of plasma in the standards was equal to the final volume of plasma in each sample. Subject samples were diluted 15 in PBN. The assay proceeded with the sequential addition of a mixture of spectrally distinct fluorescent microspheres (Luminex Corp., Austin, TX), each coupled with a capture antibody for one of the 10 analytes, similarly mixed biotinylated detection antibodies, and finally the reporter, streptavidin phycoerythrin, in a series of incubation steps and washes similar to ELISA methodology. A minimum of one hundred microspheres per cytokine was acquired on a compact flow cytometer (Luminex 100) and the median fluorescent intensity (MFI) of the phycoerythrin conjugate for each microsphere set in each well was reported. Blank values (from wells with all reagents except cytokine or sample) were subtracted from all readings and the concentrations of unknowns were calculated from the standard curves derived with a weighted 5-parameter logistic (5PL) curve-fitting model (Bio-Plex Manager 3.0 and 4.1.1). Values that fell below the lowest range for the standard curve were recorded as 0 pg/mL and upper values were set at 25,000 pg/mL. The precision of the in-house 10-plex assays for this study averaged 7.8% (intra-assay variability, range 5–12% for all cytokines, n=10). The average lowest range for each cytokine standard was: IL-2 (2.4 pg/mL), IL-4 (2.5 pg/mL), IL-6 (2.7 pg/mL), IL-8 (2.3 pg/mL), IL-10 (2.2 pg/mL), IL-12 (2.4 pg/mL), TNF-α (2.3 pg/mL), IFN-γ (1.9 pg/mL), IL-1β (2.3 pg/mL) and VEGF (7.3 pg/mL) (n=10, except for VEGF, n=8; average CV=0.43).
A commercial quantitative immuno-microarray (Microarray, Quantibody Human Cytokine Array 1, RayBiotech, Inc., Norcross, GA) was used to measure the concentrations of 20 cytokines in plasma samples; specifically, IFN-γ, IL-1α, IL-1β, IL-2, IL-4, IL-5, IL-6, IL-8, IL-10, IL-12, IL-13, GM-CSF, GRO, MCP-1, MIP-1α, MIP-1β, MMP-9, RANTES, TNF-α, and VEGF were measured. The manufacturer's procedure was followed and the results were analyzed with the RayBiotech Q Analyzer program. Samples and standards were diluted in the Sample Diluent provided with each kit. The standard curves for each cytokine varied in range from a low of 5–400 pg/mL for IL-13 to 370–30,000 pg/mL for MMP-9. The procedure was similar to that used for the in-house MMIA and ELISA, with the detection antibodies labeled with Alexa 555 that was measured with an Axon Gene Pix 4200 A laser scanner (Molecular Devices, Silicon Valley, CA) at a wavelength of 555 and settings of 450, 550 and 650 pmt. Standard curves were analyzed by regression based on linear and logarithmic transformations of the data. The results of any one assay were based on the same pmt readings and data transformation for all cytokines if the correlation coefficient was ≥0.90 for the standard curve. Data not meeting this latter criterion were excluded.
A custom commercial MMIA (Bio-Plex Cytokine Assay, Bio-Rad Laboratories, Hercules, CA) was used to measure 9 cytokines: IFN-γ, IL-2, IL-6, IL-8, IL-12, IP-10, MCP-1, MIP-1β, and TNF-α. This assay was used to examine responses to the combination antigen, ESAT-6+CFP-10+TB7.7, and included samples from additional patients with CCTB and controls. The manufacturer's instructions for performing and interpreting the assay were followed and were similar to those used for the in-house MMIA. Samples and standards were diluted with Human Serum Sample Diluent and Human Serum Standard Diluent, respectively. The ranges of the standard curves varied for each cytokine. When cytokine concentrations were higher than the upper range of the standard curves (i.e. for MCP-1 and MIP-1β), the values were reported as the upper range multiplied by the dilution factor.
Statistical analyses were conducted with SPSS statistical software (Ver. 15.0, SPSS Inc., Chicago, Ill). The Mann-Whitney U test (also known as the Wilcoxon rank-sum test) was used to compare age of patients with CCTB versus low-risk control subjects. The Chi-squared test or, when an expected frequency was five or less, Fisher's Exact test was used to compare proportions for other subject characteristics. Each cytokine response was determined by subtracting the background cytokine concentration in plasma from blood incubated with saline (Nil) from the cytokine concentration in plasma from blood stimulated with mitogen or Mtb antigens. Sensitivity was calculated by dividing the number of patients with CCTB and positive results by the number tested; specificity was calculated by dividing the number of low-risk control subjects with negative results by the number of controls tested. The Mann-Whitney U test was used to compare background cytokine concentrations (and cytokine responses) of patients with CCTB with the background concentrations (or responses) of control subjects. The Wilcoxon signed-rank test was used to compare cytokine responses to different antigens among patients with CCTB. P values <0.05 were considered significant. Dot-plots were prepared with Analyse-it for Microsoft Excel v2.20 (Analyse-it Software, Ltd., Leeds, United Kingdom). Histograms were prepared by Microsoft Office Excel 2007.
Characteristics of the 21 patients with CCTB and the 24 low-risk control subjects selected for this study are summarized in Table 1. Significant differences in age, sex, ethnicity, prevalence of tuberculosis in the country of birth, and BCG vaccination status existed between the two populations. TST induration ranged from 0 to 33 mm (mean=18, median=19) among CCTB patients, and was 0 for all control subjects. Because of limitations in the amount of available plasma and in the number of allowed freeze-thaw cycles, none of the plasma specimens were tested in all three multiplexed immunoassays; five patient and 5 control plasmas were analyzed in two different multiplexed assays. These limitations and failure of portions of an assay to meet quality control criteria occasionally caused data to be missing for an antigen or cytokine for a few samples. Characteristics of the 21 CCTB patients tested by the commercial ELISA did not differ significantly from characteristics of the 6 patients tested by in-house MMIA, the 6 patients tested by microarray, or the 12 patients tested by commercial MMIA. Plasmas from a similar number of CCTB patients and control subjects were tested with each assay.
As shown in Table 2 for measurements by commercial ELISA, highly significant differences in IFN-γ responses to ESAT-6, CFP-10, TB7.7, ESAT-6+CFP-10, and ESAT-6+CFP-10+TB7.7 were observed for CCTB patients compared with controls (p for each comparison <0.001). While the difference in the median IFN-γ response to TB7.7 for patients compared with controls was small (3 vs. 0 pg/mL), the difference was statistically significant (p<0.001). As shown in Table 3 for CCTB patients, the difference in IFN-γ response to ESAT-6+CFP-10 versus ESAT-6+CFP-10+TB7.7 was not significant (p=0.327), but responses to the combination antigens were significantly greater than the responses to the individual antigens (p ranged from ≤0.001 to 0.007). When a cutoff of 14 pg/mL (equivalent to the 0.35 IU/ml cutoff approved by the FDA for the QFT-G and QuantiFERON-TB Gold In-Tube test) was used to separate positive and negative responses to ESAT-6+CFP-10+TB7.7, nineteen (95%) of 20 CCTB patients were classified as positive and 23 (100%) of 23 controls were classified as negative (one patient and one control did not have ELISA results for plasma stimulated with ESAT-6+CFP-10+TB7.7). None of the Mtb antigens, including ESAT-6+CFP-10+TB7.7, induced a measureable IFN-γ response for one patient with CCTB.
Cytokine responses measured by in-house MMIA are shown in Table 4. Comparisons of responses to ESAT-6 show significantly greater responses for CCTB patients compared with controls for IFN-γ (94 vs. 0 pg/mL, p=0.006), IL-2 (116 vs. 0 pg/mL, p<0.001), and IL-8 (207 vs. 23 pg/mL, p=0.003). Similarly, significant differences in these cytokine responses, as well as IL-6 responses, were found following stimulation with CFP-10, ESAT-6+CFP-10, and ESAT-6+CFP-10+TB7.7. In contrast to findings with ELISA, no difference in IFN-γ response to TB7.7 was observed between patients and controls with the in-house MMIA (p=0.094), which had a much smaller sample size (N=16 vs. N=45). Similarly, no differences in responses to TB7.7 were observed between patients and controls with other cytokines included in the in-house MMIA. IL-1β, IL-4, IL-10, and TNF-α responses to antigen stimulation were generally very low. Several control subjects had detectable IL-12 responses but responses to mitogen were low. The background values for VEGF were higher for CCTB patients compared with controls. As shown in Table 5, responses for CCTB patients to combination antigens tended to be greater (lower p values) than for individual antigens for IFN-γ, IL-2, IL-6, and IL-8.
As shown in Tables 6 and and7,7, microarray analysis for 20 cytokines confirmed that IFN-γ, IL-2, IL-8, and variably IL-6 responses to Mtb antigens were significantly greater for patients with CCTB than for controls. In addition, MCP-1 and MIP-1β responses to the Mtb antigens tested were significantly higher for patients than controls, and MIP-1α responses were significantly greater for the antigen combinations. No consistent trend in differences between individual and combinations of Mtb antigens was evident for patients with this method (Table 8).
Additional samples were analyzed to confirm findings from the previous two assays. For this analysis a custom commercial MMIA was chosen and a chemokine not yet tested, IP-10, was included. As shown in Table 9, IFN-γ, IL-2, IL-6, IL-8, IP-10, MCP-1, MIP-1β and TNF-α responses were significantly greater for CCTB patients compared with controls after whole blood was stimulated with ESAT-6+CFP-10+TB7.7. In addition, background IP-10, MCP-1, and MIP-1β concentrations in plasma from unstimulated blood (Nil) from patients were significantly greater than from controls. IL-12 responses were low and not significant. Another observation was that the IL-2 Mitogen response was significantly greater for controls versus patients, which was also suggested by the results shown in Table 4, but was not significant.
Dot-plots (Figures 2A–H) and histograms (Figures 3A–B) showing patterns of cytokine responses represented in Table 9, illustrate the dramatic cytokine activity that occurs when whole blood from CCTB patients are stimulated with ESAT-6+CFP-10+TB7.7. The split y-axis at 2000 pg/mL highlights the tremendous IP-10, MCP-1, and MIP-1β responses seen for the majority of patients. Sensitivity and specificity were 100% with IL-2, IL-6, IP-10, and MIP-1β, based on cutoffs equal to the mean responses to ESAT-6+CFP-10+TB7.7 plus three standard deviations for control subjects. With IFN-γ measured by the custom commercial MMIA, similar calculations demonstrated a specificity of 100% with a sensitivity of 91.6%. One CCTB patient classified as negative based on the IFN-γ response was considered positive based on the responses of IL-2, IL-6, IL-8, IP-10, or MIP-1β. This subject was also classified as negative based on the IFN-γ response to ESAT-6+CFP-10+TB7.7 as well as other Mtb antigens measured by commercial ELISA.
The sensitivity of FDA approved IGRAs is less than ideal, and typically no better than the sensitivity of the TST , . This pilot study was designed to investigate the use of other cytokines as markers of Mtb infection and to evaluate the potential impact of their use on detection sensitivity. Cytokine responses to individual Mtb antigens and antigen combinations were compared.
Each of three multiplexed assays demonstrated that in addition to IFN-γ, multiple cytokines are released in response to Mtb antigens with significantly greater responses among patients with CCTB than among control subjects. The in-house MMIA and microarray demonstrated that IFN-γ, IL-2, IL-6, and IL-8 responses to the combination antigen ESAT-6+CFP-10+TB7.7 were greater among patients than among controls. In addition, the microarray data demonstrated significantly greater MCP-1, MIP-1α, and MIP -1β responses among patients. The custom commercial MMIA confirmed that multiple cytokines were released in response to Mtb antigens, and that IFN-γ, IL-2, IL-6, IL-8, IP-10, MCP-1, MIP-1β, and TNF-α responses to ESAT-6+CFP-10+TB7.7 were significantly greater for patients than for controls. Four of these cytokines appear to be excellent candidates as diagnostic markers of Mtb infection; sensitivity and specificity were 100% with IL-2, IL-6, IP-10, and MIP-1β. In contrast, IFN-γ sensitivity with the custom commercial MMIA was 91.6% and specificity was 100%.
One CCTB patient failed to demonstrate an IFN-γ response with any of the Mtb antigens using multiple test formats including QFT-G. The subject had a robust IFN-γ response to mitogen, no other evidence of immune dysfunction, nor any unusual IFN-γ measurements to suggest laboratory errors. In stark contrast to the lack of IFN-γ response, this subject's IL-2, IL-6, IL-8, IP-10, and MIP-1β responses to ESAT-6+CFP-10+TB7.7 were greater than corresponding mean responses plus three standard deviations for controls. This observation demonstrates that the use of other cytokines in addition to IFN-γ or as alternatives to IFN-γ can improve sensitivity for detecting Mtb infection.
Plausible reasons for false-negative IGRA results include: 1) measurement errors , 2) host-mediated inhibition of IFN-γ release , 3) drug or disease induced immune suppression , , 4) genetic defects in IFN-γ production , , and 5) Major Histocompatibility Complex (MHC) determined restriction in the ability to recognize presented epitopes . The potential for improving diagnostic sensitivity by assessing responses of multiple cytokines has been suggested previously . By assessing both IP-10 response and IFN-γ response, Ruhwald et al. noted an increase in detection rate to 90% (i.e., detection by either cytokine) from 83% and 81%, respectively, for IP-10 or IFN-γ alone. Individual cytokines have been found to be down-regulated in some patients with tuberculosis, suggesting that assessment of multiple cytokines may reduce the possibility of a negative response with any single analyte .
The amount of cytokine in unstimulated plasma from patients with CCTB was generally not significantly different from the amount in unstimulated plasma from control subjects. However, background levels of IP-10, MCP-1, and MIP-1β measured with the custom MMIA were statistically higher for patients than for controls. This observation has also been made for IP-10 and MCP-3 previously , . The specificity and sensitivity of this observation for Mtb infection should be further investigated. If these cytokines are consistently elevated without antigen stimulation in Mtb infected persons, as opposed to those with other infections, they could serve as the basis for a more rapid test for Mtb infection. If antigen stimulation is not required, detection of elevated cytokine levels in the urine may be of diagnostic value .
IP-10 has been targeted as a potential diagnostic marker for tuberculosis in other studies –, , , –. In conjunction with our results, these studies provide clear evidence that IP-10 is produced in nanogram amounts when fresh blood samples from most sensitized persons are stimulated with mycobacterial antigens. Azzurri et al. noted an association between unstimulated IP-10 plasma levels and disease activity, as well as response to treatment . In a pilot study, Syed Ahamed Kabeer et al. found that tuberculosis treatment was associated with a significant decrease in IP-10 response to certain peptides representing ESAT-6 and CFP-10 . Other promising indicators of Mtb infection include antigen-induced MCP-2, MCP-3, and IL-1RA responses , , , .
The antigen or combination of antigens used to stimulate blood can have a dramatic impact on the magnitude of the cytokine response observed. Among sensitized persons, the number of epitopes in an antigen and Major Histocompatibility Complex (MHC) restrictions determines the number of T-lymphocyte clones that will be stimulated by the antigen, and in turn, affects the amount of IFN-γ released upon stimulation , . For example, among CCTB patients, IFN-γ responses measured by ELISA to ESAT-6+CFP-10 or ESAT-6+CFP-10+TB7.7 were greater than the response to any of the individual antigens alone. However, the IFN-γ response to ESAT-6+CFP-10+TB7.7 was not significantly greater than the response to ESAT-6+CFP-10. This trend toward higher response to the combination antigens continued for other cytokines measured with the in-house MMIA. For this reason, and because ESAT-6+CFP-10+TB7.7 is used in the QuantiFERON®-TB Gold In-Tube test, only responses to ESAT-6+CFP-10+TB7.7 were measured with the custom commercial MMIA.
Cytokine levels vary considerably from individual to individual, so the range of values observed with the multiplexed assays was rather large. Despite these large variations and the relatively small sample sizes, significant differences between CCTB patients and controls were observed, and measurements of IL-2, IL-6, IP-10, and MIP-1β responses allowed complete separation of the two groups. The dot plots and histograms (Figures 2 and and3)3) illustrate the multiple sizeable cytokine responses and the pattern seen among patients. For IP-10 and MIP-1β, the magnitude of the responses to Mtb antigens was so large compared to background cytokine levels that subtraction of the background had little effect on the calculated responses. This has two implications. First, the complexity and cost of testing may be reduced by screening only Mtb-antigen stimulated plasma for characteristically high cytokine concentrations. If increased concentrations of IP-10 or MIP-1β are found in the Mtb-antigen stimulated plasma, a more sensitive and complex assay could be performed that would take into account the background cytokine concentrations. Second, significant cytokine responses may be detectable with shorter incubation times, thus allowing for more rapid assessments.
Differences are often seen in the magnitude of cytokine concentrations measured with different ELISAs or different multiplexed immunoassay systems . These differences are primarily due to varying antibody affinities for the assay targets, as well as differences in the platforms employed. We used three multiplexed immunoassay systems that assessed some of the same cytokines with presumably different capture and detection antibodies. In all three systems, differences in IL-2, IL-6, IL-8, and IFN-γ responses between CCTB patients and controls were significant. In two systems, differences in MCP-1 and MIP-1β responses were significant. TNF-α responses were significantly greater among patients versus controls using the in-house MMIA and commercial MMIA, but not when using the microarray. However, TNF-α concentrations were generally low and highly variable, which may explain why the differences in TNF-α response were not significant for all three assays.
Limitations of this study stem from the examination of small subsets of subjects with each of the different multiplexed immunoassays. However, even with small numbers of subjects significant differences in cytokine responses were demonstrated between CCTB patients and controls. While differences in demographic and clinical characteristics for the patient and control populations were observed (listed in Table 1), it is unlikely that these explain the differences in cytokine responses seen. Subtracting the background cytokine concentration (in the Nil plasma) from the concentration in the antigen stimulated plasma adjusts for demographic and clinical factors that may contribute to nonspecific release of cytokines. The observed differences in unstimulated concentrations for some cytokines (including IFN-γ) is likely due to elevated background levels of cytokine associated with acute or chronic illness, including tuberculosis. Another limitation is the lack of adequate diagnostic standards to confirm all forms of Mtb infection, including the most common, which is latent infection. We addressed this limitation by comparing responses among patients with confirmed Mtb infection (i.e., among patients with tuberculosis confirmed by recovery of Mtb by culture) and control subjects at low-risk of Mtb exposure who were presumed to be uninfected. Clearly, immunologic differences exist between latent Mtb infection and infection manifesting as active disease, but specific immunologic differences have been difficult to demonstrate , . Larger epidemiologically based studies will be required to identify and confirm these differences. Multiplexed assays, which can be readily automated for high-throughput, can facilitate these larger studies.
MMIAs, which are also referred to as suspension arrays, are gaining wide acceptance as tools for research and diagnostic assays , . These assays are performed in 2 to 4 hours, similar to the time required to perform ELISAs. However, in addition to measuring more than one analyte per test, MMIAs require smaller sample volumes (4 µL in this study), less amounts of reagent and operator time, and cost less than multiple ELISAs. These three dimensional assays have a detection range 1–2 logs broader than ELISAs, so fewer sample dilutions are necessary. Already a simpler, less expensive instrument is available that is not dependent on the fluidics system of a flow cytometer (MAGPIX®, Luminex Corporation). This and similar systems are more compact and portable and show potential for use in developing regions of the world where both reduction in assay cost and time delay between diagnosis and treatment are important. As multiplexed assays that show potential for detection of Mtb infection are optimized, they can be incorporated onto other platforms that are fully automated or designed for point-of-care diagnostics.
In conclusion, multiple cytokines are released when whole blood samples from patients with CCTB are stimulated with specific Mtb antigens. Compared with measurement of IFN-γ alone, multiplexed assays can improve diagnostic sensitivity for Mtb infection by assessing multiple cytokine responses simultaneously, using smaller sample volumes and reducing the cost of testing compared to ELISAs and other methods. The use of combinations of specific Mtb antigens may also increase diagnostic sensitivity by increasing the magnitude of cytokine responses as compared to individual antigens. Larger studies are needed to confirm the clinical utility of multiplexed assays that examine the cytokines identified in this study as potential diagnostic markers of Mtb infection and to examine the possibility of differentiating infection with disease from latent infection.
The authors would like to express their gratitude to the volunteers who participated in the parent studies and gave consent for their blood to be stored for further research and analysis; to Patrick K. Moonan and Arlene L. Hankinson for assistance in designing the parent study and recruiting subjects; to Tarek Elbeik, Richard Stephens, Wei Lu, Sean R. Toney, and David Temporado for laboratory assistance; and to Laura Daniels for administrative assistance.
The views expressed in this article are those of the authors and do not necessarily reflect the official policy or position of the CDC, Department of the Navy, Department of Defense, nor the U.S. Government.
Competing Interests: The authors have read the journal's policy and recognize the following potential conflicts: Cellestis Ltd. provided antigens and kits that were used to measure interferon gamma by the commercial ELISA. This does not alter the authors' adherence to all the PLoS ONE policies on sharing data and materials. None of the authors have conflicts of interest.
Funding: This study had no specific support or funding. Plasma samples were from a larger IRB approved project supported by CDC, the Department of the Navy, and Cellestis Limited. Cellestis Limited provided antigens and kits that were used to measure interferon gamma by the commercial ELISA. CDC, the Department of the Navy, and Cellestis, Ltd. reviewed the study design, data collection methods, and analysis plans prior to approval and funding. CDC and the Department of the Navy cleared the manuscript for publication according to established guidelines.