Development and multicenter evaluation of the N Latex CDT direct immunonephelometric assay for serum carbohydrate-deficient transferrin.
Carbohydrate-deficient transferrin (CDT)  is considered the most accurate biomarker for identifying sustained heavy alcohol consumption and for monitoring abstinence (3, 4). Transferrin, which occurs at concentrations of 2.0-3.5 g/L in serum, exhibits a degree of microheterogeneity that depends on iron saturation (~30%), amino acid sequence, and/or carbohydrate content (5-7). Amino acid sequence variation is observed in individuals with genetic variants B, C, and D (8), whereas transferrin glycoforms with variable carbohydrate content and/or branching of the maximum 2 N-linked oligosaccharide chains (N-glycans) are always present (4, 7, 9). Typically, the major serum transferrin glycoform, tetrasialotransferrin, contains 2 disialylated biantennary glycans. Other, less abundant glycoforms are pentasialo-, trisialo-, and disialotransferrins (10). Disialo- and asialotransferrin fractions increase after sustained heavy drinking (10-12). These glycoforms, together with monosialotransferrin (10), have collectively been referred to as CDT (4). A regular intake of ~50-80 g ethanol/day for a minimum of ~1-2 weeks is required to increase the serum CDT concentration in [greater than or equal to]80% of individuals (4,13). The half-life of the CDT marker is ~1-1.5 weeks, and a return to the usual glycoform pattern requires >2 weeks of abstinence (4,14, 15).
Early methods for assaying CDT used isoelectric focusing followed by immunofixation (16-18). Alternative procedures used chromatofocusing (19), HPLC (10, 14, 20), fast protein liquid chromatography (21), and capillary electrophoresis (22-24). Immunoassays include an initial chromatographic separation of CDT glycoforms from non-CDT glycoforms on disposable minicolumns (25-27). Drawbacks with this last approach are the labor involved and the fact that transferrin genetic variants may cause falsely high or falsely low results (28). We present data on the development and multicenter evaluation of the 1st direct immunoassay for CDT (N Latex CDT; Dade Behring) and on possible interference by transferrin genetic variants and congenital disorders of glycosylation (CDG) (29).
Materials and Methods
DEVELOPMENT OF A MONOCLONAL ANTIBODY
We raised monoclonal antibodies (mAbs) against CDT by means of a recombinant nonglycosylated transferrin, which was a gift from Anne B. Mason, Ph.D. (Department of Biochemistry, College of Medicine, University of Vermont, Burlington, VT) (30), in which the 2 asparagine residues at the carbohydrate-linkage sites were mutated to aspartic acid (Asn413Asp and Asn611Asp). We immunized BALB/c mice with recombinant transferrin in complete Freund adjuvant. A booster with an emulsion prepared in incomplete adjuvant was given after 4 weeks, and another booster without adjuvant was administered after 8 weeks. During the final 3 days before the fusion, we gave the mice daily intravenous boosters.
After the mice were killed, we removed the spleens and cloned the B-cells with myeloma cells. Single hybrid cells that produced antibodies specific for CDT (i.e., binding to nonglycosylated transferrin but not to typical transferrin) were cloned, and appropriate clones were expanded. After removing the cells, we concentrated the solution and purified the antibodies with Protein A Sepharose Fast Flow (GE Healthcare/Amersham Biosciences). The CDT mAb (98/84-011) with the highest specificity for nonglycosylated transferrin but no affinity for typical human transferrin was selected for assay development (see the Data Supplement that accompanies the online version of this article at http: //www.clinchem.org/content/vol53/issue6).
We diluted the selected CDT mAb to a concentration of 80 mg/L in blocking buffer (10 g/L bovine serum albumin and 0.5 mL/L Tween 20 in Tris-buffered saline (0.02 mol/L Tris, 0.5 mol/L NaCl, pH 7.5) and then added alkaline phosphatase-linked secondary antibodies (Bio-Rad Laboratories) in blocking buffer. p-Nitrotetrazolium blue and 5-bromo-4-chloro-3-indolyl phosphate (Sigma-Aldrich) were added as substrates (31). We used sera from 1 control individual and 1 alcoholic proband to compare the specificity of the CDT mAb to that of polyclonal antibodies directed against several transferrin epitopes (Dade Behring).
We further evaluated the specificity of the CDT mAb by investigating its reaction with CDT, other transferrin glycoforms, and enzymatically modified transferrin. Transferrin lacking the terminal sialic acid residues was obtained by treating serum with neuraminidase (2.5 mU/mg transferrin; Dade Behring) in PBS (0.048 mol/L [Na.sub.2]HP04, 0.02 mol/L K[H.sub.2]PO4, 0.145 mol/L NaCl, 0.015 mol/L Na[N.sub.3], pH 7.2) for 18 h at 37 [degrees]C. We obtained transferrin lacking entire N-glycan moieties by treating transferrin with peptide-N-glycosidase F (500 mU/mg transferrin; Roche Diagnostics) for 4 h at 37 [degrees]C in PBS (0.048 mol/L [Na.sub.2]HPO4, 0.02 mol/L [KH.sub.2]PO4, 0.145 mol/L NaCl, 0.015 mol/L Na[N.sub.3], pH 7.2) containing 10 mmol/L EDTA and 1 g/L sodium dodecyl sulfate. After this incubation, proteins were separated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis. Immunodetection was performed with the CDT mAb and a polyclonal antibody against human transferrin.
CDT mAb-BASED IMMUNOASSAY
N Latex CDT is based on an mAb that specifically recognizes transferrin glycoforms that lack one or both of the complete N-glycans [i.e., disialo-, monosialo-, and asialotransferrins (the CDT glycoforms)] in combination with a simultaneous assay for total transferrin (N Antiserum to Human Transferrin; Dade Behring). Polystyrene particles coated with the CDT mAb are agglutinated by CDT-coated polystyrene particles. CDT inhibits this reaction in a dose-dependent manner, allowing nephelometric CDT quantification over 18 min on the Dade Behring BN II[TM] and BN ProSpec[R] systems. No sample pretreatment is required. Because the degree of iron saturation of transferrin influences the binding affinity of the antibody, the transferrin-bound iron is stripped with a chelating agent in the first incubation step. The simultaneous determination of total transferrin allows an automatic calculation of the amount of CDT as a percentage of total transferrin (%CDT). The measurement range is -20-640 mg/L or 0.77%-25% CDT.
We evaluated the N Latex CDT assay at 8 sites (A-H) with 2 independent reagent lots (01 and 03). The reagent lots were distributed so that each lot was used at least once on each analyzer. Imprecision was determined according to the Clinical and Laboratory Standards Institute EP5-2A guideline. The 2 reagent set controls (N CDT Control SL/1 and SL/2; Dade Behring) and 4 different human serum pools were run in duplicate in 2 runs/day, over 20 days. Dade Behring provided 2 serum pools (R1 and R2). R1 contained samples with an increased %CDT, and R2 contained samples with low and increased %CDT values. Two other serum pools ("low" and "high" %CDT pools) were produced individually by each laboratory. We used the N Latex CDT assay to analyze a proficiency panel of 29 serum samples that were provided in frozen aliquots at 6 of the sites.
We obtained informed consent and approval of the local ethics committee whenever required. To evaluate any relationship between total transferrin concentrations and %CDT values produced by N Latex CDT, we included serum samples from 113 patients with a wide range of transferrin concentrations (0.43-4.22 g/L; reference interval, 2.0-3.6 g/L) but who had typical %CDT values with the N Latex CDT method and no evidence of alcohol abuse.
We collected serum samples from 561 apparently healthy adults (255 men, ages 20-70 years; 306 women, ages 19-79 years). We included samples only from individuals who had no clinical indications or biochemical indications (as measured by y-glutamyltransferase activity and erythrocyte mean corpuscular volume) of chronic alcohol abuse and consumed no more than 2 drinks/day (<25 g ethanol /day).
For comparison, we obtained an additional 141 samples from children and adolescents (ages 11-18 years). None of these patients exhibited any signs of liver or metabolic diseases or of alcohol consumption. To assess alcohol consumption, we used both the section in the Kiddie-Sads-Present and Lifetime Version that is related to alcohol abuse and the Alcohol Use Disorders Identification Test.
We evaluated potential interfering factors, such as transferrin saturation, iron deficiency, lipemia, transferrin genetic variants, and CDG. We obtained serum samples from healthy white individuals who carried the BC (n = 3) and CD (n = 4) transferrin variants and from 1 CDG type le patient.
We compared %CDT results obtained with the N Latex CDT assay with those obtained by turbidimetric chromatographic separation followed by immunoassay (the Axis-Shield %CDT or the Bio-Rad %CDT TIA assay) (27). We also compared the N Latex CDT assay with an HPLC candidate reference method (10) with 100 serum samples with percent disialotransferrin values within the reference interval of the HPLC method (97.5th percentile, <1.7%) and 100 samples with increased values (>2% disialotransferrin). Samples were selected to cover a wide range of percent disialotransferrin values (0.9%-22.2%).
Results are expressed as the mean (SD). Differences between samples that were saturated with iron before analysis and unaltered samples were evaluated by means of a paired t-test. Passing-Bablok regression and the Wilcoxon test were used to compare methods. The Student t-test and ANOVA were used to evaluate sex and age differences in the control population. We defined reference values as the 2.5%-97.5% interval in the distribution of values in the reference population.
EVALUATION OF THE CDT mAb
Sodium dodecyl sulfate-polyacrylamide gel electrophoresis and Western blotting analysis with the CDT mAb showed only transferrin molecules lacking one or both N-glycans in serum samples obtained from alcoholic individuals; no reaction with transferrin was obtained with control samples (Fig. 1). The CDT mAb also detected transferrin in control samples after N-glycosidase F treatment (Fig. 1), which yields transferrin molecules lacking entire N-glycans. Control serum samples incubated with neuraminidase, which depletes only terminal sialic acid residues, were not detected by the CDT mAb (Fig. 1).
Epitope mapping of the CDT mAb with overlapping peptides corresponding to the human transferrin sequence identified 4 major binding sites (data not shown): 1 site in the N-terminal domain and 3 sites in the C-terminal domain. Because peptide sequences at or near the 2 N-glycan--binding sites (Asn413 and Asn611) were not detected, we concluded that the antibody is directed against a discontinuous structural epitope. This result suggests differences in 3-dimensional structure between transferrin molecules containing 2 N-glycans and those lacking 1 or both N-glycans (i.e., the CDT glycoforms). Apparently, this structural change and the formation of the CDT-specific structural epitope(s) occur when 1 N-glycan is missing, and no major additional changes occur when the second N-glycan is also missing.
The imprecision (CV) of the N Latex CDT assay was determined for 4 serum pools at 6 laboratory sites (Table 1). The R1 pool (mean %CDT, 3.92%; range, 3.8%-4.0%) and the R2 pool (mean, 3.08%; range, 3.0%-3.2%) were provided by Dade Behring, whereas the low pools (mean %CDT, 1.95%; range, 1.8%-2.1%) and high pools (mean, 5.33%; range, 3.0%-8.7%) were produced at each site. The intraassay CVs were 1.9%-7.0% (mean, 4.3%), and total CVs were 3.4%-10.4% (mean, 6.8%; Table 1). BN 11 systems showed higher analytical imprecision (mean total CV, 8.2%) than BN ProSpec systems (mean total CV, 5.3%). Imprecision results for the reagent set controls were similar to those for the serum pools, with total CVs of 3.8%-9.7% for Dade Behring N CDT Control SL/1 (mean concentration, 55.7 mg/L) and 3.7%-5.4% for N CDT Control SL/2 (mean concentration, 163 mg/L).
[FIGURE 1 OMITTED]
REFERENCE INTERVAL FOR %CDT VALUES
We studied the distribution of N Latex CDT values with 561 serum samples from healthy nonalcoholic individuals. Transferrin concentrations were 1.7-4.4 g/L (2.5th percentile, 2.0 g/L; 97.5th percentile, 3.8 g/L). The overall mean %CDT value was 1.76% (0.26%), and the range was 1.01%-2.85%. The %CDT results for men [1.78% (0.27%)] and women [1.77 (0.25%)] were not significantly different (P = 0.538), and no significant age-related differences were found (data not shown). We proposed an upper reference limit of 2.35% (97.5th percentile) for %CDT values obtained with the N Latex CDT assay. The 141 serum samples collected from children and adolescents showed similar results, with a median %CDT of 1.91% and 2.5th and 97.5th percentiles of 1.45% and 2.40%, respectively. On the basis of these results, we proposed the same upper reference limit (2.35%, 97.5th percentile) for %CDT obtained with the N Latex CDT assay (Table 2).
For the 113 serum samples with a wide range of transferrin values, we found no marked effect of transferrin concentration on N Latex CDT results within the reference interval (2.0-3.6 g/L). At abnormally low concentrations, however, we noted increased %CDT values for some samples. A %CDT value >2.35% was observed in 8 of 10 samples with transferrin concentrations of <1.1 g/L. Of the 113 samples, 25 serum samples with a median transferrin concentration of 1.0 g/L (23 of the samples <1.5 g/L) had CDT values below the measurement range of the method (<20 mg/L). %CDT values could not be calculated for these samples.
Because the N Latex CDT assay requires iron depletion of serum transferrin before analysis, we investigated the efficiency of the iron-chelating capacity. In patients with pronounced iron overload (transferrin saturation >70%) but without signs of alcohol abuse, all %CDT values were within the reference range (data not shown).
An abstinent student had a markedly increased %CDT value of 8.2% according to the Axis-Shield photometric method. Measurement with the N Latex CDT method on the BN ProSpec system yielded a typical %CDT value of 2.1%. An HPLC analysis of this sample revealed a CD phenotype, which was confirmed by genotyping. For a sample from an individual presenting with a B2C phenotype, a typical %CDT value of 2.2% with the Axis-Shield method was obtained, whereas the N Latex CDT assay produced an increased %CDT value of 2.9%.
The %CDT values obtained with the Axis-Shield CDT assay for an individual who had been abstinent for >1 year (2.8%-3.0%) did not show a return from increased values to typical values; however, N Latex CDT revealed a typical value of 1.7%. This patient had a highly increased trisialotransferrin fraction, which led to falsely increased results in the Axis-Shield assay. The trisialo glycoform normally accounts for <5% of the total transferrin. In our experience, an increased trisialo fraction occurs more often in Europeans than CD genetic variants (28).
A 3-year-old boy with a type le CDG syndrome had an abnormally high %CDT value (17.1%) with the N Latex CDT method and a 27.4% value with the Axis-Shield assay.
Two of 8 lipemic samples (serum triglycerides >3.5 mmol/L) showed 15% and 35% relative increases in CDT in the low-normal CDT range after the samples were cleared by high-speed centrifugation. Two other lipemic samples showed relative decreases of 15% and 20% after centrifugation, and 4 other samples remained within 3% of the original value. Highly lipemic samples can cause problems, and we recommend avoiding such samples.
%CDT values obtained with N Latex CDT were correlated with those obtained with the Bio-Rad %CDT TIA (n = 132; y = 0.838x + 0.354; [r.sup.2] = 0.862; [S.sub.y x] = 0.58). Passing-Bablok regression analysis revealed the N Latex CDT results to be generally lower in the low %CDT range than with the Bio-Rad %CDT TIA (see the Figure in the online Data Supplement).
%CDT values obtained with the N Latex CDT assay were also correlated with percent disialotransferrin values obtained by HPLC in an analysis of 100 serum samples with typical values and 100 samples with increased percent disialotransferrin values (range, 0.9%22.2%; Fig. 2; n = 200; y = 0.700x + 0.970; [r.sup.2] = 0.978; [S.sub.y x] = 0.49). We used ROC curve analysis and the 97.5th percentile for percent disialotransferrin as determined with the HPLC method as a reference, along with these 200 samples to calculate the agreement of N Latex CDT results with reference method results. With the upper reference limit of 2.35% for %CDT obtained with N Latex CDT as a cutoff point, 97% of the results that showed increased %CDT in the HPLC analysis were increased in N Latex CDT, and 94% of the results that were below the cutoff point according to the HPLC method were also below the cutoff point in the N Latex CDT assay (Table 3).
The important component of N Latex CDT is the mAb, which specifically recognizes the transferrin glycoforms that lack one or both entire N-glycans (corresponding to asialo-, monosialo- and disialotransferrins) (4). Disialo- and asialotransferrins are associated with sustained heavy drinking, whereas monosialotransferrin is correlated with the amount of trisialotransferrin (28). Monosialotransferrin probably represents no obstacle to %CDT testing with N Latex CDT because it is usually present in very low concentrations (10). Trisialotransferrin has caused some confusion in CDT testing (7, 28, 32), because this glycoform is always present at higher concentrations and was (26,33)--and still is (34)--included in the CDT fraction of some methods. Immunoblotting analysis, however, has demonstrated that the CDT mAb does not detect trisialotransferrin in the N Latex CDT assay.
[FIGURE 2 OMITTED]
Another advantage of N Latex CDT over the indirect column-based immunoassays is that the CDT mAb is not influenced by transferrin genetic variants. Genetic variants, which are rare in white individuals but more common in other populations (8,35), may cause falsely low and high CDT values with the column-based immunoassays (28). For example, trisialotransferrin D in samples from individuals with C and D genetic variants will coelute with disialotransferrin C and thereby cause overestimation of CDT. Use of the N Latex CDT assay may therefore decrease the need for confirmatory CDT testing by HPLC or capillary electrophoresis (36). Additional studies are needed to confirm that other transferrin genetic variants and samples with divergent N-glycan structures, such as those occurring in the CDG subtypes, do not interfere with the N Latex CDT assay (22, 37, 38).
Besides variations in amino acid sequence and carbohydrate content, the degree of transferrin microheterogeneity also depends on the number of bound iron molecules (7). Under physiological conditions, serum transferrin is ~30% saturated with iron. Four transferrin glycoforms can be distinguished with respect to iron content: apotransferrin, N-terminal and C-terminal monoferric transferrins, and diferric transferrin. To exclude analytical interference due to variation in iron saturation, many CDT methods completely saturate the transferrin in the sample with iron before analysis. The degree of iron saturation also influences the binding affinity of the CDT mAb in the N Latex CDT assay, but this assay uses a chelating agent to completely deplete the iron from transferrin before analysis. The reproducibility results indicate that iron depletion is complete and stable during the immunonephelometric analysis.
The %CDT results obtained with the N Latex CDT assay correlated well with those of a column-based %CDT immunoassay (27) and with the percent disialotransferrin values obtained with an HPLC candidate reference method (10); however, because these methods measure different transferrin glycoforms as CDT, the values obtained with the different methods are not interchangeable. This fact highlights the need for standardization of CDT measurements.
Grant/funding support: The N Latex CDT assay and control materials used for the Multicenter evaluation, as described in Materials and Methods, were provided by Dade Behring. Financial disclosures: The authors had complete independence in the interpretation of data and writing of the report.
Received December 11, 2006; accepted March 8, 2007. Previously published online at DOI: 10.1373/clinchem.2006.084459
(1.) Wallace P, Cutler S, Haines A. Randomised controlled trial of general practitioner intervention in patients with excessive alcohol consumption. BMJ 1988;297:663-8.
(2.) Conigrave KM, Saunders JB, Whitfield JB. Diagnostic tests for alcohol consumption. Alcohol Alcohol 1995;30:13-26.
(3.) Helander A. Biological markers in alcoholism [Review]. J Neural Transm Suppl 2003;15-32.
(4.) Stibler H. Carbohydrate-deficient transferrin in serum: a new marker of potentially harmful alcohol consumption reviewed [Review]. Clin Chem 1991;37:2029-37.
(5.) van Eijk HG, van Noort WL, Kroos MJ, van der Heul C. Analysis of the iron-binding sites of transferrin by isoelectric focussing. J Clin Chem Clin Biochem 1978;16:557-60.
(6.) de Jong G, van Dijk JP, van Eijk HG. The biology of transferrin [Review]. Clin Chim Acta 1990;190:1-46.
(7.) Arndt T. Carbohydrate-deficient transferrin as a marker of chronic alcohol abuse: a critical review of preanalysis, analysis, and interpretation [Review]. Clin Chem 2001;47:13-27.
(8.) Kamboh MI, Ferrell RE. Human transferrin polymorphism [Review]. Hum Hered 1987;37:65-81.
(9.) Fu D, van Halbeek H. N-glycosylation site mapping of human serotransferrin by serial lectin affinity chromatography, fast atom bombardment-mass spectrometry, and 1H nuclear magnetic resonance spectroscopy. Anal Biochem 1992;206:53-63.
(10.) Helander A, Husa A, Jeppsson J0. Improved HPLC method for carbohydrate-deficient transferrin in serum. Clin Chem 2003;49: 1881-90.
(11.) Landberg E, Pahlsson P, Lundblad A, Arnetorp A, Jeppsson J-0. Carbohydrate composition of serum transferrin isoforms from patients with high alcohol consumption. Biochem Biophys Res Commun 1995;210:267-74.
(12.) Flahaut C, Michalski JC, Danel T, Humbert MH, Klein A. The effects of ethanol on the glycosylation of human transferrin. Glycobiology 2003;13:191-8.
(13.) Schellenberg F, Schwan R, Mennetrey L, Loiseaux MN, Pages JC, Reynaud M. Dose-effect relation between daily ethanol intake in the range 0-70 grams and %CDT value: validation of a cut-off value. Alcohol Alcohol 2005;40:531-4.
(14.) Jeppsson J0, Kristensson H, Fimiani C. Carbohydrate-deficient transferrin quantified by HPLC to determine heavy consumption of alcohol. Clin Chem 1993;39:2115-20.
(15.) Helander A, Carlsson S. Carbohydrate-deficient transferrin and gamma-glutamyl transferase levels during disulfiram therapy. Alcohol Clin Exp Res 1996;20:1202-5.
(16.) Schellenberg F, Weill J. Serum desialotransferrin in the detection of alcohol abuse. Definition of a Tf index. Drug Alcohol Depend 1987;19:181-91.
(17.) Bean P, Peter JB. Allelic D variants of transferrin in evaluation of alcohol abuse: differential diagnosis by isoelectric focusing-immunoblotting-laser densitometry. Clin Chem 1994;40:2078-83.
(18.) Stibler H, Blennow G, Kristiansson B, Lindehammer H, Hagberg B. Carbohydrate-deficient glycoprotein syndrome: clinical expression in adults with a new metabolic disease. J Neurol Neurosurg Psychiatry 1994;57:552-6.
(19.) Storey EL, Mack U, Powell LW, Halliday JW. Use of chromatofocusing to detect a transferrin variant in serum of alcoholic subjects. Clin Chem 1985;31:1543-5.
(20.) Helander A, Bergstrom JP. Determination of carbohydrate-deficient transferrin in human serum using the Bio-Rad %CDT by HPLC test. Clin Chim Acta 2006;371:187-90.
(21.) Sillanaukee P, Lof K, Harlin A, Martensson 0, Brandt R, Seppa K. Comparison of different methods for detecting carbohydrate-deficient transferrin. Alcohol Clin Exp Res 1994;18:1150-5.
(22.) Oda RP, Prasad R, Stout RL, Coffin D, Patton WP, Kraft DL, et al. Capillary electrophoresis-based separation of transferrin sialoforms in patients with carbohydrate-deficient glycoprotein syndrome. Electrophoresis 1997;18:1819-26.
(23.) Prasad R, Stout RL, Coffin D, Smith J. Analysis of carbohydrate deficient transferrin by capillary zone electrophoresis. Electrophoresis 1997;18:1814-8.
(24.) Bortolotti F, De Paoli G, Tagliaro F. Carbohydrate-deficient transferrin (CDT) as a marker of alcohol abuse: a critical review of the literature 2001-2005. J Chromatogr B Analyt Technol Biomed Life Sci 2006;841:96-109.
(25.) Stibler H, Borg S, Joustra M. A modified method for the assay of carbohydrate-deficient transferrin (CDT) in serum. Alcohol Alcohol Suppl 1991;1:451-4.
(26.) Helander A. Absolute or relative measurement of carbohydrate-deficient transferrin in serum? Experiences with three immunological assays. Clin Chem 1999;45:131-5.
(27.) Helander A, Fors M, Zakrisson B. Study of Axis-Shield new %CDT immunoassay for quantification of carbohydrate-deficient transferrin (CDT) in serum. Alcohol Alcohol 2001;36:406-12.
(28.) Helander A, Eriksson G, Stibler H, Jeppsson JO. Interference of transferrin isoform types with carbohydrate-deficient transferrin quantification in the identification of alcohol abuse. Clin Chem 2001;47:1225-33.
(29.) Jaeken J. Komrower Lecture: congenital disorders of glycosylation (CDG): it's all in it [Review]! J Inherit Metab Dis 2003;26:99-118.
(30.) Mason AB, Miller MK, Funk WD, Banfield DK, Savage KJ, Oliver RW, et al. Expression of glycosylated and nonglycosylated human transferrin in mammalian cells: characterization of the recombinant proteins with comparison to three commercially available transferrins. Biochemistry 1993;32:5472-9.
(31.) Blake MS, Johnston KH, Russell-Jones GJ, Gotschlich EC. A rapid, sensitive method for detection of alkaline phosphatase-conjugated anti-antibody on Western blots. Anal Biochem 1984;136: 175-9.
(32.) Lipkowski M, Dibbelt L, Seyfarth M. Is there an analytical or diagnostic advantage from including trisialo transferrin into the fraction of carbohydrate-deficient transferrin? Lessons from a comparison of two commercial turbidimetric immunoassays with the carbohydrate-deficient transferrin determination by high-performance liquid chromatography. Clin Biochem 2000;33:63541.
(33.) Wuyts B, Delanghe JR, Kasvosve I, Wauters A, Neels H, Janssens J. Determination of carbohydrate-deficient transferrin using capillary zone electrophoresis. Clin Chem 2001;47:247-55.
(34.) Alden A, Ohlson S, Pahlsson P, Ryden I. HPLC analysis of carbohydrate deficient transferrin isoforms isolated by the Axis-Shield %CDT method. Clin Chim Acta 2005;356:143-6.
(35.) Kasvosve I, Delanghe JR, Gomo ZA, Gangaidzo IT, Khumalo H, Wuyts B, et al. Transferrin polymorphism influences iron status in blacks. Clin Chem 2000;46:1535-9.
(36.) Helander A, Wielders JP, Te Stroet R, Bergstrom JP. Comparison of HPLC and capillary electrophoresis for confirmatory testing of the alcohol misuse marker carbohydrate-deficient transferrin. Clin Chem 2005;51:1528-31.
(37.) Helander A, Bergstrom J, Freeze HH. Testing for congenital disorders of glycosylation by HPLC measurement of serum transferrin glycoforms. Clin Chem 2004;50:954-8.
(38.) Carchon HA, Chevigne R, Falmagne JB, Jaeken J. Diagnosis of congenital disorders of glycosylation by capillary zone electrophoresis of serum transferrin. Clin Chem 2004;50:101-11.
 Nonstandard abbreviations: CDT, carbohydrate-deficient transferrin; CDC, congenital disorders of glycosylation; mAb, monoclonal antibody; %CDT, CDT as a percentage of total transferrin.
JORIS R. DELANGHE,  * ANDERS HELANDER,  JOS P.M. WIELDERS,  J. MAURITS PEKELHARING,  HEINZ J. ROTH  FRANCOIS SCHELLENBERG,  CATHERINE BORN,  ERAY YAGMUR,  WOLFGANG GENTZER,  and HARALD ALTHAUS 
 Department of Clinical Chemistry, Ghent University Hospital, Ghent, Belgium.
 Alcohol Laboratory, Karolinska Institute and Karolinska University Hospital, Stockholm, Sweden.
 Department of Clinical Chemistry, Meander Medical Center, Amersfoort, The Netherlands.
 Reinier de Graaf Groep, Diagnostic Center SSDZ, Delft, The Netherlands.
 Limbach Laboratories, Heidelberg, Germany.
 Laboratory of Clinical Chemistry, Hopital Trousseau, Centre Hospitalier Regional Universitaire, Tours, Tours, France.
 Institut Regional pour la Sante, La Riche, France.
 Central Laboratory, University Hospital, Rheinisch Westfalische Technische Hochschule, Aachen, Germany.
 Research Laboratories, Dade Behring Marburg GmbH, Marburg, Germany.
* Address correspondence to this author at: Department of Clinical Chemistry, De Pintelaan 185, B-9000 Ghent, Belgium. Fax 32-9-240-4985; e-mail email@example.com.
Table 1. Multicenter analytical performance of the N Latex CDT assay. Imprecision (CV), % Sample Within-run Total Mean %CDT Site A: BNII (a) R1 (b) 5.0 8.3 4.0 R2 (b) 5.8 8.6 3.1 Low pool (c) 6.5 8.4 1.8 High pool (c) 5.8 8.1 5.8 Site C: BN ProSpec R1 1.9 4.9 3.9 R2 3.2 6.4 3.0 Low pool 2.9 6.0 2.1 High pool 2.5 5.5 4.8 Site F: BN ProSpec R1 2.9 4.7 3.8 R2 5.2 7.3 3.0 Low pool 3.3 6.4 1.9 High pool 2.8 5.3 4.7 Imprecision (CV), % Sample Within-run Total Mean %CDT Site B: BN R1 (b) 2.6 3.8 4.0 R2 (b) 3.8 4.9 3.1 Low pool (c) 3.7 5.3 1.9 High pool (c) 2.7 3.4 8.7 Site D: BN II R1 5.7 8.7 3.8 R2 7.0 10.4 3.1 Low pool 6.2 9.1 2.0 High pool 5.2 7.3 3.0 Site H: BN II R1 4.3 6.8 4.0 R2 5.2 8.7 3.2 Low pool 4.8 8.6 2.0 High pool 4.3 5.3 5.0 (a) The study sites used either the BN II or the BN ProSpec system (Dade Behring). (b) R1 and R2 were serum sample pools provided by Dade Behring. (c) The low and high pools were individual serum pools produced at each study site. Table 2. Distribution of %CDT values produced by the N Latex CDT assay for serum samples collected from healthy individuals at 2 study sites. (a) %CDT 2.5th Group n percentile Median Total 561 1.29 1.76 Men 255 1.27 1.77 Women 306 1.37 1.76 97.5th 99th Group percentile percentile Total 2.35 2.47 Men 2.36 2.47 Women 2.35 2.44 (a) The samples were collected in The Netherlands and France. Table 3. Sensitivity and specificity for the N Latex CDT assay calculated at different %CDT thresholds. %CDT threshold Specificity, % (a) Sensitivity, % (a) 2.2 90 99 2.3 93 96 2.4 97 94 2.5 97 93 2.6 97 86 (a) The percent disialotransferrin results obtained with the HPLC method (10) were used as a reference (threshold, 1.7%).
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|Title Annotation:||Automation and Analytical Techniques|
|Author:||Delanghe, Joris R.; Helander, Anders; Wielders, Jos P.M.; Pekelharing, J. Maurits; Roth, Heinz J.; S|
|Date:||Jun 1, 2007|
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