Printer Friendly

Clinical measurement of von Willebrand factor by fluorescence correlation spectroscopy.

The protein von Willebrand factor (vWF) (4) functions as a recruiter, tether, and activator of platelets and as the protective carrier for factor VIII. It is normally present in plasma as a distribution of multimers containing anywhere from 2 to 40 or more vWF monomers. Abnormalities in vWF activity, most often related to abnormal concentration or multimer distribution, are the incident cause of the group of coagulopathies known as von Willebrand disease (vWD) (1, 2). As a group, vWD is considered to be the most common inherited coagulation disorder. Abnormalities in vWF are also responsible for secondary bleeding conditions, such as in acquired vWD, and are associated with inherited and acquired thrombotic states, such as the procoagulant disease known as thrombotic thrombocytopenia purpura. In addition, several common conditions have been known to affect vWF distributions including coronary artery disease, pregnancy, cancer, sepsis, diabetes, autoimmune disease, and others (3-5). Despite its importance in inherited and acquired bleeding disorders, and the mounting evidence for its role in thrombotic disease, routine evaluation is hampered by the limitations of currently available laboratory tests.

Limitations in vWF Testing

The main clinical subclassification of vWF abnormalities is based on whether the deficiency is purely a quantitative one (type 1 vWD) or includes a functional component (type 2 vWD). Type 2 vWD is most often related to a decrease in the concentration of larger multimers, which have the highest ability to bind collagen and recruit and activate platelets. A third type (type 3 vWD) is characterized by complete or near-complete absence of vWF, which is fortunately rare.

The groupings above have clinical consequences that relate to therapy and prognosis. In type 1 vWD, patients may receive the vasopressin analog 1-deamino-[8-D-arginine]-vasopressin (DDAVP), which stimulates preferentially large multimer secretion from endothelial cells (6) and often provides sufficient functional capacity for adequate hemostasis. Type 2 vWD is much more likely to require the administration of vWF concentrate. Antibody-based quantification of vWF antigen (vWF:Ag) concentration does not provide information regarding the relative multimer size distribution and cannot be used independently to subclassify vWF abnormalities.


Functional tests used for classification, such as ristocetin cofactor activity (vWF:RCof) and the collagen-binding assay (vWF:CB), suffer from poor reproducibility, limited reportable ranges, and lack of standardization. The gold standard for multimer visualization, gel electrophoresis, is a cumbersome, non-quantitative, and time-consuming assay primarily available only from reference laboratories. Additional diagnostic challenges associated with current vWF laboratory testing methods have been recently reviewed (7, 8).

Fluorescence Correlation Spectroscopy

Fluorescence correlation spectroscopy (FCS) measures the absolute concentration and mobility of fluorescent species as they diffuse through a well-defined observation volume. It has not been previously applied to clinical testing in human plasma. FCS is well suited for this type of testing in that it is rapid, simple to perform, and has a low cost per test. FCS can be performed without washing steps, with volume measurements that are optically defined, and with very small amounts of testing sample and reagents.

In FCS, when on average only a few molecules are present in a given observation volume, fluctuations in the actual number follow predictable Poisson statistics [see references (9-11) for more detailed description]. Comparison of fluctuations in the fluorescence signal to the mean fluorescence signal yields the mean number of molecules in the observation volume. The typical time scale of the fluctuations corresponds to the time it takes molecules to diffuse through the observation volume, and can therefore be related to the diffusivity of the molecules, a property that is proportional to molecule size.

In practice, a laser focused to a diffraction-limited spot by a microscope objective combined with a confocal detection pinhole defines the observation volume for FCS (Fig. 1A). The basic instrument is relatively simple and inexpensive to build, consisting of a microscope objective, a high-sensitivity detector, and a specialized computer card to plot the autocorrelation of the fluorescence signal, G([tau]), vs the correlation delay time [tau] (Fig. 1B). This curve can be fit to a function derived from the shape of the observation volume, yielding the mean number of molecules per volume, N, and the residence time (mean time of diffusion through observation volume), [[tau].sub.d]. For the typical confocal excitation profile, one can assume a 3-dimensional gaussian observation profile such that:


where t is the correlation time, S is the structure parameter (ratio of radial to axial observation volume diameters), [[tau].sub.t] is the triplet lifetime, and [f.sub.t] corresponds to the triplet state fraction. The residence time, [[tau].sub.d], is related to the diffusion coefficient, D, by the StokesEinstein equation via the diameter of the observation volume in the x, y direction [w.sub.x,y]: [[tau].sub.d] = [w.sup.2.sub.x,y]. Thus, the concentration of fluorescent molecules and their diffusion coefficient can be determined directly from the fluctuations in emitted photons over time.

FCS for vWF Measurement

The goal of this report is to examine whether FCS can address some of the limitations of current methods for vWF assessment, looking to develop a more practical tool than multimer gel analysis for measuring vWF size distributions in bleeding and clotting disorders. In this study, we used FCS for the measurement of vWF multimers in plasma from a cohort of patients with vWF test results within reference intervals and from patients with type 1 and type 2 vWD. We analyzed how the quantity and quality of vWF substrate affects measureable parameters in the FCS assay and present an approach that allows adequate subclassification of vWD with this simple-to-implement method.



Using institutional review board-approved protocols, we identified samples for analysis from vWF:Ag, vWF: RCof, factor VIII, and multimer gel analysis data generated during routine vWD testing at Yale-New Haven Hospital and Weill Cornell Medical College. Twenty-six samples from patients who fulfilled the respective laboratory director's criteria for von Willebrand disease (12 type 1 and 14 type 2) were selected on the basis of unequivocally low values in vWF:Ag (<50%), vWF: RCof (<50%), and/or antigen-to-activity ratio (<0.5). Although current recommendations for characterization as vWD vary, these concentrations correspond to the reference values used clinically at the testing site, and values below 50% are associated with progressively increased risk of excessive bleeding relative to average healthy controls regardless of cause. Samples were also collected from 1 patient who underwent a therapeutic DDAVP trial. Ten apparently healthy patients with all vWF values within reference intervals (75% < vWF:Ag <150%, 75% < vWF: RCof <150%) and confirmed normal multimer analyses were randomly selected for comparison. Antigen and activity percentage units refer to a normalized pooled standard representing 100%, equivalent to 100 U/dL, against which reference standards used for calibration are measured (Diagnostica-Stago).


Sample collection and testing were performed by standard procedures as described in the Data Supplement, which accompanies the online version of this article at


Samples were thawed at 37[degrees]C and then incubated with tetramethyl-rhodamine-isothiocyanate (TRITC)-labeled monoclonal anti-vWF antibody directed to the D3 domain (Santa Cruz Biotechnology) at a final concentration of 20 nmol/L for 30 min at room temperature. We diluted 40 [micro]L plasma 1:1 with antibody-containing phosphate buffer at pH 7.1. This dilution ensures a near-normalization of the viscosity to that of saline (12). We placed 40 [micro]L incubated sample atop a #0 coverslip (Thermo Fisher) and analyzed it in a Confocor 2 fluorescence correlation microscope (Zeiss) at room temperature with a 40 x 1.2-NA coverslip-corrected water immersion objective (Zeiss) by standard FCS procedures (10, 13). Excitation was done with a helium-neon laser at 543 nm, 543 nm dichroic mirror, and 560-615 nm emission filter. Pinhole diameter was 78 [micro]m. Ten runs of 30 s were averaged for each sample.


We fitted correlation curves from tagged antibody at 50 nmol/L in phosphate buffer to a 1-component FCS equation with a triplet term (Eq. 1). The structure parameter and observation volume were derived from fits of tetramethylrhodamine dye at 100 nmol/L concentration. The triplet time ([[tau].sub.t] approximately 10 [micro]s) and antibody diffusion time ([[tau].sub.d], approximately 320 [micro]s) were derived from fits of TRITC-labeled antibody at 50 nmol/L. The reduced [chi square]/degrees of freedom ([chi square]/DoF) was always on the order of 1 x [10.sup.-6]. Raw FCS curves were fitted online on Confocor or offline with Origin software (OriginLabA). Triplet fractions (ft) ranged from 8% to 10%. Autocorrelation curves of samples without added fluorescent antibody showed background plasma counts < 10% of antibody fluorescence, with a high triplet fraction and an effective mean diffusion time of approximately 120 [micro]s, dim and of fast enough diffusion time to be neglected from the comparison of mean diffusion time and component ratios in FCS curves.


The autocorrelation curves obtained from FCS analysis of patient samples incubated with fluorescently tagged anti-vWF were fitted to a 2-component FCS equation such that:

[]([tau]) = [[] x [] ([tau], [[tau]])] + [[a.sub.bound] x [G.sub.bound] ([tau], [[tau].sub.bound])]

where []([tau]) and [G.sub.bound]([tau]) are the normalized autocorrelation functions for the free- and bound-antibody components, and [] and [a.sub.bound] are their relative contributions (corresponding fraction) to the correlation function []([tau]). The relative brightness of free and bound components affects the proportionality between [] and [a.sub.bound] and therefore these represent "effective" fractions, corresponding to the proportion if the brightness was equal between subsets (also see the online Data Supplement). Although this is not expected to be the case in these experiments, this use of effective bound fractions allowed adequate discrimination, simplified the analysis, and improved the robustness of the fits considerably. The diffusion time ([]) of the free component was fixed at the measured [[tau].sub.d] of antibody alone (320 [micro]s, appropriate for the expected molecular weight of 140 kDa and an observation volume diameter [[omega].sub.x-y] of 265 nm, calculated from dye diffusion times). For individual 2-component fits, the [chi square]/ DoF was always <2 x [10.sup.-5]. We obtained the mean nonantibody diffusion time and an effective fraction of antibody bound directly from this 2-component fit. We generated normalized curves from the G (0) calculated on the raw 2-component fits for clearer visual comparison of FCS curve shapes. These normalized curves use an alternate form of Eq. 1 that omits the leading 1.


To demonstrate the effect of vWF concentration on FCS curves, we analyzed serial saline dilutions of a normal sample. The FCS curves from these dilutions show a progressive shift toward longer mean diffusion times (curves shift to the right) with higher vWF concentrations (Fig. 2A), as might be expected with increasing binding of antibody. A global two-component fit for the dilution curves, with 1 diffusion time fixed at the antibody diffusion time, describes the data well (Fig. 2A; overall fit [chi square]/DoF = 4.0 x [10.sup.-5], [R.sup.2] = 0.9995). We calculated proportional increases in the percentage of the curve represented by the longer diffusion time (Fig. 2B). We observed an excellent linear correlation between the antigen concentration of the dilution and the effective fraction of antibody bound to vWF as determined from the 2-component fits. These results indicate that a 2-component fit is able to extract an effective bound percentage from the FCS curves, and it is consistent with the interpretation that we are operating in the concentration range where antibody is not fully bound. The correlation (Fig. 2B) also demonstrates a leveling off at the highest vWF:Ag concentrations, as would be expected when available vWF antibody-binding sites approach the antibody concentration.


By contrast, differences in the mean diffusion time between type 1 and type 2 vWD patient samples were not directly proportional to antigen concentration. Fig. 3A shows a representative comparison of normalized FCS curves from a patient with a type 1 vWD pattern (normal multimer distribution, reduced vWF:Ag concentrations), a patient with a type 2 vWD pattern (reduced mean multimer size and higher vWF:Ag concentrations higher than the type 1 sample), and a healthy control. There is an expected shift toward shorter mean diffusion times in the type 2 vWD sample, which contained only the smallest vWF multimers as seen in multimer gels (Fig. 3B). Distinction of this type 2 vWD sample from a very severe type 1 vWD sample, which would also have a fast mean diffusion time, may not be readily apparent by visual inspection of the FCS curves alone. However, the 2-component fit disentangles the effects of changes in overall vWF concentration from those of the vWF distribution, now represented by the calculated relative proportion of free and bound antibody and by the effective mean diffusion time of the bound antibody component (designated by arrows in Fig. 4).

The 26 samples with vWF abnormalities also tested by FCS are described in Table 1. There is significant overlap between type 1 vWD and type 2 vWD patient samples for vWF:Ag and vWF:RCof results, making individual tests insufficient for an accurate classification. The effective percentage of slowly diffusing antibody and the mean diffusion time of this bound component was calculated from 2-component fits of the FCS curve. As shown in Fig. 4, specimens from healthy controls, type 1 vWD patients, and type 2 vWD patients cluster into 3 separate groups when plotted for these 2 parameters. As physiologically expected, type 1 vWD patients show an effective bound fraction (percentage bound) that is lower than that of controls, but with a mean diffusion of the bound component (bound [tau]) that is in the normal range. Type 2 vWD patients show an effective bound fraction that is in the range of type 1 vWD patients (as they have largely over lapping total antigen concentrations; see Table 1), but with a reduced mean diffusion of the bound component, reflective of the lack of large multimers that defines most type 2 vWD cases. Finally, 3 samples with clinically established relatively mild acquired type 2 deficiency, but with vWF:Ag concentrations higher than 50%, appropriately demonstrated a high bound antibody percentage but with a small mean multimer size (Fig. 4). The overall results provide a rational basis for disease classification by FCS analysis.


Additional experiments were performed with samples from a type 1 vWD patient taken at baseline, 1 h, and 4 h after administration of DDAVP, a compound that stimulates endothelial cell release of ultra-large multimers, which are subsequently cleaved in the circulation to achieve the steady-state distributions observed. There are corresponding changes noted with FCS with slower diffusion at 1 h and partial return to baseline at 4 h (Fig. 5A). Two-component fits (Fig. 5B) yielded a pattern of DDAVP response consistent at 1 h with an increase in the quantity (effective percentage bound) and mean size (mean bound diffusion time) of the multimer distribution. When compared to 1 h, the 4-hour sample shows a decrease in the mean size with only a small decrease in total antigen. The antigen assays are consistent with this result (Table 1). The cofactor activity assays are also generally consistent with this result, but are difficult to interpret because activity is affected by the antigen concentration in such a way that multimer size is not easily inferred. The gel multimer analysis is also not easily quantifiable for this DDAVP response (Fig. 5C).



Current functional tests for vWF include the ristocetin cofactor activity assay and the collagen-binding assay. The vWF:RCof assay measures the ability of patient-derived vWF to agglutinate formalin-fixed healthy donor platelets. The vWF:CB assay measures the ability of patient vWF to bind collagen affixed to reaction wells. Both tests have been designed to be sensitive to the distribution of vWF multimers, but they suffer from important limitations (14). The vWF:RCof assay has limited sensitivity and poor reproducibility. Furthermore, there is disagreement about the optimal threshold for disease classification. Repeated runs of vWF: RCof are needed for adequate precision, and a relatively high lower end of the reportable range observed with some vWF:RCof assays can render it useless in patients with moderate antigen deficiencies (< 20%), as exemplified by several samples listed in Table 1. The utility of the other functional assay, vWF: CB, is limited by the lack of adequate reagent standardization and variability in the types of collagen used. The lack of a reference standard for this test makes extensive internal validations necessary. Additionally, data are lacking on the reliability of both the vWF:RCof and vWF:CB assays in detecting clinically relevant increases in large vWF multimers.

The only method in current clinical use to directly visualize vWF multimers remains gel electrophoresis, which suffers from high technical complexity and a time-consuming nature (15). The use of gel electrophoresis for vWF multimers is generally restricted to reference laboratories, most often for the second-stage evaluation of vWD. A typical setup requires overnight electrophoretic runs of denatured protein in 1%-2% agarose gel. Detection is often completed through radio-immunoblotting, creating additional difficulties associated with the use of radiation-containing reagents in the clinical laboratory. Variability in results from gel to gel is another confounding factor inherent to this technique, particularly when attempting to use these results to quantify multimer distributions. Whereas minor stimuli may cause rapid, significant changes to the circulating concentrations of vWF protein (and to multimer distributions for which repeated measurements could aid in diagnosis and risk assessment), the challenges associated with vWF gel electrophoresis procedures make the technique impractical for use in this manner.


Although it has found widespread use within the biophysics community since its first implementation almost 40 years ago, FCS has not been widely used for clinically relevant diagnostics. One factor affecting the application of FCS to immunoassay-type clinical analysis is that >6-fold changes in molecular weight are typically required for shifts in mean diffusion time to be reliably detected. However, given that functional characteristics of vWF depend on the relative size of multimers present, and that the multimers achieve such large sizes, FCS is particularlywell suited for vWF measurement. Additional discussion on multimeric protein analysis via FCS is presented in the online Data Supplement.

In the present report, experimental FCS measurements of vWF in patients with type 1 and type 2 vWD followed in perfect agreement with the qualitative results from multimer gel analysis. Even if the measured bound fraction and bound mean diffusion times are only surrogate markers of the actual multimer size distribution, in contrast to labor-intensive gel electrophoresis, the FCS method was able to obtain clinically useful data with only 30-min antibody incubation and 5-min analysis time. The cost per test was minimal, and execution of the analysis was straightforward and quick. Also, the end points were easily comparable numerical results.

As in traditional gel multimer analysis, distinction of certain type 2 vWD subtypes (such as type 2B and type 2M), would require testing in addition to multimer analysis for accurate clinical classification. The overall utility of multimer analysis, however, would still be augmented by a simpler and faster method that provides the most relevant information, i.e., the effective mean multimer size and overall amount of antigen present. The quantitative nature, short analysis time, and potential for very low cost per test in FCS would make it possible to obtain these parameters on virtually every sample for which antigen and activity are being measured, as well as potentially obviate the need for slow, laborious, nonquantitative multimer gel testing, which requires subjective interpretation.



The DDAVP trial demonstrates how FCS with 2-component fits can help characterize the response to therapy. Mechanisms of type 1 vWD vary and include decreased synthesis, increased clearance, and/or increased breakdown of vWF. In addition to providing therapeutic prognosis, 4-h DDAVP trials can sometimes help elucidate the underlying defect (e.g., the rapid clearance of type 1 Vincenza). Theoretically, multimer distribution changes in response to DDAVP are affected bythe specific vWF abnormality, i.e., secretion, multimerization, cleavage, etc. Thus, there exists an opportunity to gain additional insight into the mechanisms responsible for vWF deficiencies during a DDAVP trial by looking at multimer distribution time-courses. The current limitations of multimer gels, such as lack of reliable quantitative data and the other aforementioned difficulties, make this investigation currently impractical. Whether FCS is indeed capable of yielding complementary information relevant to the mechanism responsible for vWF deficiency in individual patients should be explored further, as it could have direct implications in the therapeutic approach. Because of its ability to produce numerical results sensitive to changes in large multimers, FCS analysis may similarly be useful in assessing thrombotic risk and/or extent of abnormalities in conditions known to be associated with hypercoagulability.


The findings presented in this report show that FCS can be used to measure parameters that reflect vWF distributions in patient samples and, through these measurements, can produce clinically meaningful results. To our knowledge, it represents the first medical diagnostic application of this biophysical technique directly on human plasma. Fluctuation-based immunoassays could find a role in the routine evaluation of vWF, in both vWD diagnosis and the assessment of therapeutic response. Implementation in clinical use will require further characterization of its analytical capabilities. We also believe that establishing FCS as a clinically relevant technique would create opportunities for expansion of this simple-to-implement approach to address a variety of shortcomings in current clinical laboratory techniques.

Authors' Disclosures or Potential Conflicts of Interest: Upon manuscript submission, all authors completed the author disclosure form. Disclosures and/or potential conflicts of interest:

Employment or Leadership: None declared. Consultant or Advisory Role: None declared. Stock Ownership: None declared. Honoraria: None declared.

Research Funding: R. Torres, partial salary support from the National Center for Research Resources (NCRR), a component of the NIH, NIH Roadmap for Medical Research, and partial salary support from the National Heart, Lung, and Blood Institute (NHLBI) of the NIH; M.J. Levene, partial salary support and Clinical and Translational Science Awards grant UL1 RR024139 from NCRR and partial salary support and grant R21 HL094796 from NHLBI. Expert Testimony: None declared.

Role of Sponsor: The funding organizations played no role in the design of study, choice of enrolled patients, review and interpretation of data, or preparation or approval of manuscript.

Acknowledgments: The authors thank Dr. David Andrews from University of Miami Miller School of Medicine for helping perform multimeric gel analysis and providing the gel scans presented here. We also thank Dr. Brian R. Smith for participating in the development of the research concept.

Author Contributions: All authors confirmed they have contributed to the intellectual content of this paper and have met the following 3 requirements: (a) significant contributions to the conception and design, acquisition of data, or analysis and interpretation of data; (b) drafting or revising the article for intellectual content; and (c) final approval of the published article.


(1.) Sadler J, Budde U, Elckenboom J, Favaloro E, Hill F, Holmberg L, et al. Update on the pathophysiology and classification of von Willebrand disease: a report of the subcommittee on von Willebrand factor. J Thromb Haemost 2006;4: 2103-14.

(2.) Torres R, Fedoriw Y. Laboratory testing for von Willebrand disease: toward a mechanism-based classification. Clin Lab Med 2009;29: 193-228.

(3.) Ono T, Mimuro J, Madoiwa S, Soejima K, Kashiwakura Y, Ishiwata A, et al. Severe secondary deficiency of von Willebrand factor cleaving protease (ADAMTS13) in patients with sepsisinduced disseminated intravascular coagulation: its correlation to development of renal failure. Blood 2006;107: 528-34.

(4.) Chion CKNK, Doggen CJM, Crawley JTB, Lane DA, Rosendaal FR. ADAMTS13 and von Willebrand factor and the risk of myocardial infarction in men. Blood 2007;109: 1998-2000.

(5.) Nguyen TC, Carcillo JA. Understanding the role of von Willebrand factor and its cleaving protease ADAM TS13 in the pathophysiology of critical illness. Pediatr Crit Care Med 2007;8: 187-9.

(6.) Ruggeri Z, Mannucci P, Lombardi R, Federici A, Zimmerman T. Multimeric composition of factor VIII/von Willebrand factor following administration of DDAVP: implications for pathophysiology and therapy of von Willebrand's disease subtypes. Blood 1982;59: 1272-8.

(7.) Chandler WL, Peerschke EIB, Castellone DD, Meijer P. Von Willebrand factor assay proficiency testing: the North American Specialized Coagulation Laboratory Association experience. Am J Clin Pathol 2011;135: 862-9.

(8.) Marques MB, Fritsma GA. Von Willebrand disease laboratory diagnosis: the saga continues. Am J Clin Pathol 2011;135: 818-20.

(9.) Magde D, Elson E, Webb WW. Thermodynamic fluctuations in a reacting system: measurement by fluorescence correlation spectroscopy. Phys Rev Lett 1972;29:705-8.

(10.) Magde D, Elson EL, Webb WW. Fluorescence correlation spectroscopy. 2. Experimental realization. Biopolymers 1974;13: 29-61.

(11.) Elson E, Magde D. Fluorescence correlation spectroscopy. I. Conceptual basis and theory. Biopolymers 1974;13:1-27.

(12.) Janzen J, Elliott TG, Carter CJ, Brooks DE. Detection of red cell aggregation by low shear rate viscometry in whole blood with elevated plasma viscosity. Biorheology 2000;37: 225-37.

(13.) Applications manual LSM 510--Confocor 2: fluorescence correlation spectroscopy. Carl Zeiss Advanced Imaging Microscopy; 2001. http://www. pdf (Accessed April 2012)

(14.) Favaloro EJ. An update on the von Willebrand factor collagen binding assay: 21 years of age and beyond adolescence but not yet a mature adult. Semin Thromb Hemost 2007;33: 727-44.

(15.) Smejkal GB, Shainoff JR, Kotte-Marchant KM. Rapid high-resolution electrophoresis of multimeric von Willebrand factor with a thermopiloted gel apparatus. Electrophoresis 2003;24: 582-7.

Richard Torres, [1,2] Jonathan R. Genzen, [3] and Michael J. Levene [1] *

[1] Department of Biomedical Engineering and [2] Department of Laboratory Medicine, Yale University and Yale School of Medicine, New Haven, CT; [3] Department of Pathology and Laboratory Medicine, Weill Cornell Medical College, New York Presbyterian Hospital, New York, NY.

* Address correspondence to this author at: P.O. Box 208260, New Haven, CT 06520. E-mail:

Received November 26, 2011; accepted March 5, 2012.

Previously published online at DOI: 10.1373/clinchem.2011.179200

[4] Nonstandard abbreviations: vWF, von Willebrand factor; vWD, von Wille brand disease; DDAVP, 1-deamino-[8-D-arginine]-vasopressin; vWF:Ag, vWF antigen; vWF:RCof, ristocetin cofactor activity; vWF:CB, collagen-binding assay; FCS, fluorescence correlation spectroscopy; TRITC, tetramethyl-rhodamine isothiocyanate.
Table 1. Characteristics of vWD samples subsequently tested by FCS.

Sample Antigen, RCoF, Factor Multimer analysis Type
 % % VIII,

1 44 44 43 All multimers present Type 1
 in decreased amounts

2 43 28 38 All multimers present Type 1
 in decreased amounts

3 43 40 53 All multimers present Type 1
 in decreased amounts

4 45 42 73 All multimers present Type 1
 in decreased amounts

5 39 <20 42 All multimers present Type 1/
 in decreased amounts 2M

6 13 <20 13 All multimers present Type 1
 in decreased amounts

7 43 40 63 All multimers present Type 1
 in decreased amounts

8 15 <20 48 All multimers present Type 1
 in decreased amounts

9 48 48 69 All multimers present Type 1
 in decreased amounts

10 37 26 26 All multimers present Type 1
 in decreased amounts

11 38 42 78 All multimers present Type 1
 in decreased amounts

12 32 25 37 All multimers present Type 1
 in decreased amounts

13 68 <20 14 No large or Severe
 intermediate type 2A

14 31 <20 39 Absence of large Type 2A

15 19 <20 39 Absence of large Type 2A

16 50 <20 41 Absence of large Acquired
 multimers type 2

17 21 <20 31 Absence of large Type 2A

18 17 <20 31 Absence of largest Type 2A

19 41 <20 103 Absence of largest Mild
 multimers type 2A

20 77 35 65 Absence of large Acquired
 multimers Type 2

21 38 18 29 Absence of large Type 2A

22 51 28 72 Absence of large Acquired
 multimers type 2?

23 31 <20 39 Absence of large Type 2A

24 100 39 74 Absence of large Type 2

25 146 62 132 Absence of large Acquired
 multimers type 2

26 188 121 112 Absence of largest Mild
 multimers acquired
 type 2
COPYRIGHT 2012 American Association for Clinical Chemistry, Inc.
No portion of this article can be reproduced without the express written permission from the copyright holder.
Copyright 2012 Gale, Cengage Learning. All rights reserved.

Article Details
Printer friendly Cite/link Email Feedback
Title Annotation:Hemostasis and Thrombosis
Author:Torres, Richard; Genzen, Jonathan R.; Levene, Michael J.
Publication:Clinical Chemistry
Article Type:Report
Geographic Code:1USA
Date:Jun 1, 2012
Previous Article:Correction.
Next Article:Rapid diagnosis of aneuploidy by high-resolution melting analysis of segmental duplications.

Terms of use | Privacy policy | Copyright © 2022 Farlex, Inc. | Feedback | For webmasters |