- Research article
- Open Access
Association of anticardiolipin, antiphosphatidylserine, anti-β2 glycoprotein I, and antiphosphatidylcholine autoantibodies with canine immune thrombocytopenia
- Yu-Chen Chen†1,
- Lang-Ming Chi†2, 3,
- Kuan-Chih Chow†4,
- Shiow-Her Chiou1Email author,
- Yi-Hsin Fan1,
- Shu-Peng Ho5,
- Yu-Chen Hsu1,
- Yu-Chyi Hwang1,
- Meng-Xing Wu5,
- Wei-Ming Lee5, 6,
- Shiun-Long Lin5, 6,
- Chau-Loong Tsang5 and
- Frank Chiahung Mao5
© The Author(s). 2016
- Received: 4 December 2015
- Accepted: 7 June 2016
- Published: 13 June 2016
In humans, the presence of antiphospholipid antibodies (aPL) is frequently found in immune thrombocytopenia. The present study investigated whether aPL and any aPL subtypes are associated with canine thrombocytopenia, in particular, immune-mediated thrombocytopenia (immune thrombocytopenia) that usually manifests with severe thrombocytopenia.
Sera were collected from 64 outpatient dogs with thrombocytopenia (Group I, platelet count 0 – 80 × 103/uL), and 38 of which having severe thrombocytopenia (platelet count < 30 × 103/uL) were further divided into subgroups based on the presence of positive antiplatelet antibodies (aPLT) (subgroup IA, immune thrombocytopenia, n =20) or the absence of aPLT (subgroup IB, severe thrombocytopenia negative for aPLT, n =18). In addition, sera of 30 outpatient dogs without thrombocytopenia (Group II), and 80 healthy dogs (Group III) were analyzed for comparison. Indirect ELISAs were performed to compare serum levels of aPL subtypes, including anticardiolipin antibodies (aCL), antiphosphatidylserine antibodies (aPS), antiphosphatidylcholine (aPC), and anti-β2 glycoprotein I antibodies (aβ2GPI), and antiphosphatidylinositol antibodies (aPI), among different groups or subgroups of dogs. Among outpatient dogs, aCL, being highly prevalent in outpatient dogs with thrombocytopenia (63/64, 98 %), is an important risk factor for thrombocytopenia (with a high relative risk of 8.3), immune thrombocytopenia (relative risk 5.3), or severe thrombocytopenia negative for aPLT (relative risk ∞, odds ratio 19). In addition, aPS is a risk factor for immune thrombocytopenia or severe thrombocytopenia negative for aPLT (moderate relative risks around 2), whereas aPC and aβ2GPI are risk factors for immune thrombocytopenia (relative risks around 2).
Of all the aPL subtypes tested here, aCL is highly associated with canine thrombocytopenia, including immune thrombocytopenia, severe thrombocytopenia negative for aPLT, and less severe thrombocytopenia. Furthermore, aPS is moderately associated with both canine immune thrombocytopenia and severe thrombocytopenia negative for aPLT, whereas aβ2GPI, and aPC are moderately relevant to canine immune thrombocytopenia. In contrast, aPI is not significantly associated with canine immune thrombocytopenia.
- Anticardiolipin antibodies
- Antiphosphatidylserine antibodies
- Anti-β2 glycoprotein I antibodies
- Antiphosphatidylcholine antibodies
- Antiphospholipid antibodies
- Immune thrombocytopenia
- Antiplatelet antibodies
In humans, the presence of antiphospholipid antibodies (aPL) is a diagnostic criterion for the antiphospholipid syndrome (APS), which manifests with thrombosis or recurrent fetal loss in women and is often accompanied with thrombocytopenia [1, 2]. APS in the absence of other related autoimmune diseases is referred to as primary APS. Besides being present in primary APS, the aPL autoantibodies are often found in patients with other autoimmune diseases, especially systemic lupus erythematosus (SLE) and immune thrombocytopenia (immune-mediated thrombocytopenia) [1, 3]. The aPL autoantibodies in humans have been recognized as lupus anticoagulants (LA), anticardiolipin (aCL), antiphosphatidylinositol (aPI), antiphosphatidylserine (aPS), antiphosphatidic acid (aPA), antiphosphatidylglycine (aPG), antiphosphatidylcholine (aPC), and anti-β2 glycoprotein I antibodies (aβ2GPI) [4, 5]. Among them, aCL and aβ2GPI detected by ELISA, together with LA determined by screening assays, are now required as one or more of the three laboratory criteria, along with one clinical manifestation (either vascular thrombosis or recurrent abortion in women), for the diagnosis of APS in humans . Alternatively, several reports have suggested that APhL antibody ELISAs, which detect antibodies against a mixture of noncardiolipin antigens (anti-noncardiolipin phospholipids antibodies, aPhL), can be used for human APS diagnosis [6–8]. Apart from thrombosis and pregnancy morbidity, thrombocytopenia is a common manifestation in both APS (20 to 53 %)  and SLE patients (20 %) . Although thrombocytopenia had previously been proposed to serve as a preliminary classification criterion of APS in SLE patients , it was not included in the later revised APS classification criteria . On the other hand, a recent investigation of 35 thrombocytopenia patients with aPL found that half of them developed APS . The authors of that study suggested that aPL-positive thrombocytopenia patients, along with less frequent hemolytic anemia patients, should be considered as having hematologic APS .
Until now, canine aPL-related studies have been limited. In 2005, the presence of aCL was detected in 33 of 63 diseased dogs by setting a cut-off value based on the sera of 134 healthy dogs, and four APS-like diseased dogs, including one dog with recurrent abortion and severe thrombocytopenia, were found to have high levels of aCL . Interestingly, 22 Bernese Mountain dogs, a breed which has been shown to have a prolonged phospholipid-dependent coagulation time, presented with significantly higher levels of aCL than the controls (healthy dogs of other breeds) . Nonetheless, a recent study did not correlate aPL with thrombosis or immune-mediated hemolytic anemia in dogs . The involvement of aPL with thrombocytopenia, a clinical manifestation frequently occurred in APS patients, remains to be clarified in dogs.
We initiated the investigation on dogs with thrombocytopenia, in particular, immune thrombocytopenia that usually manifests with significantly lower platelet counts than thrombocytopenia of other origins . The objective of this study was to explore whether any subtypes of aPL are associated with thrombocytopenia or immune thrombocytopenia in pet dogs. Indirect ELISAs were performed to measure and compare the levels and prevalence of aPhL, aβ2GPI, aCL, aPI, aPC, and aPS IgG antibodies in outpatient dogs with or without thrombocytopenia and in healthy dogs.
Normal platelet reference range of dogs is 200 – 500 × 103/uL . However, dogs with a platelet count of less than 80 × 103/uL are more likely to have clinical complications . In our study, serum samples were divided into three groups. Group I consisted of 64 outpatient dogs with thrombocytopenia (platelet count 0 – 80 × 103/uL). Group II consisted of 30 outpatient dogs without thrombocytopenia (platelet count 250 – 500 × 103/uL). To avoid any interference from other APS-related manifestations, dogs with thrombosis, pregnancy morbidity, and hemolytic anemia were not included in Group I and Group II outpatient dogs. As a control, Group III consisted of 80 healthy dogs. Group I has an average age of 5.2 years and a female to male ratio of 1.1. Group II has an average age of 5.9 years and a female to male ratio of 1.2. Group III has an average age of 2.8 and a female to male ratio of 0.7. Basic information (including breed) of three groups of dogs and clinical manifestations of outpatient dogs (Group I and Group II) are listed in the Additional file 1.
In dogs, immune thrombocytopenia often manifests with significantly lower platelet counts than other forms of thrombocytopenia . Therefore, a diagnosis of presumptive immune thrombocytopenia is usually made if a dog’s platelet count falls below certain cut-off values . For example, O’Marra et al.  have categorized thrombocytopenic dogs with platelet counts of less than 30 × 103/μL and without any other underlying disease as having presumptive primary immune thrombocytopenia. Furthermore, a recent study by Iraqi et al.  has verified the pathological role of antiplatelet antibodies (aPLT) in the development of immune thrombocytopenia. In the present study, we selected 38 outpatient dogs with severe thrombocytopenia (platelet count < 30 × 103/μL) from Group I and examined their sera for the presence of aPLT. Positive threshold for aPLT (1.5 ng/mL) was determined as 99th percentile of healthy dogs (in the Group III). Group I dogs were further divided into three subgroups. Severe thrombocytopenic dogs with positive aPLT were designated as Group IA (categorized as having immune thrombocytopenia) (n = 20), which included outpatient dogs with primary immune thrombocytopenia and those with immune thrombocytopenia secondary to other diseases. Severe thrombocytopenic dogs negative for aPLT were designated as Group IB (n = 18). On the other hand, less severe thrombocytopenic dogs with platelet count between 30 – 80 × 103/μL were designated as Group IC (n = 26). The average level of aPLT in Group IA was 3.8 ng/mL (ranging from 1.9 to 15.3 ng/mL). The results of aPLT measurement in Group IA, Group IB, and healthy control are shown in the Additional file 2.
Expression of β2GPI antigen for aβ2GPI antibodies detection
The presence of aβ2GPI antibodies has been listed as one of the laboratory criteria for the diagnosis of APS . For the detection of aβ2GPI antibodies in dogs, we cloned human β2GPI cDNA from HeLa cells and expressed the recombinant β2GPI (rβ2GPI). The rβ2GPI protein was purified by metal chelation chromatography. The purified rβ2GPI protein was analyzed by SDS-PAGE and Western blot, and the identity of rβ2GPI was verified by mass spectrometry (Additional file 3).
Dog IgG and human aPhL IgG standard curves
As a comparison, reference human aPhL IgG standards (200, 100, 50, 25, 12.5, and 6.25 μg/mL) available in a human APhL IgG ELISA kit were used. A standard ELISA curve was generated by using linear regression, with an R squared value of 0.9961 (Fig. 1b).
Comparing serum levels of aPL subtypes in different groups of dogs
By using an indirect ELISA, a mixture of non-cardiolipin phospholipids (PhL) consisting of PS, phosphatidic acid (PA), and β2GPI, available from an APhL IgG HRP ELISA kit, were incubated sequentially with diluted (1:50) canine sera and with HRP conjugated-rabbit anti-dog IgG antibodies to measure aPhL in canine sera. Similarly, using rβ2GPI, CL, PI, PC, and PS as the coated antigens, we added canine sera (1:50) and HRP conjugated-rabbit anti-dog IgG antibodies to measure aβ2GPI, aCL, aPI, aPC, and aPS in canine sera by indirect ELISAs.
Average IgG levels of antiphospholipid antibodies (aPL) among different groups of dogs
98th/99thpercentile cut-off GPL
(n = 20)
(n = 18)
(n = 26)
(n = 30)
(n = 80)
GPLb (95 % CI)c
GPL (95 % CI)
GPL (95 % CI)
GPL (95 % CI)
GPL (95 % CI)
95.9 (79.3 – 112.5)
116.7 (99.4 – 134.0)
130.9 (105.2 – 156.6)
66.8 (56.5 – 77.0)
7.4 (5.8 – 9.1)
65.7 (50.6 – 80.7)
40.8 (30.2 – 51.4)
64.9 (44.6 – 85.2)
40.4 (29.0 – 51.8)
6.1 (4.0 – 8.3)
38.8 (28.8 – 48.8)
49.6 (34.3 – 65.0)
58.9 (43.8 – 73.9)
18.3 (11.9 – 24.8)
0.8 (0.2 – 1.3)
18.5 (12.6 – 24.3)
24.4 (19.2 – 29.7)
17.1 (10.8 – 23.4)
15.6 (11.4 – 19.8)
4.2 (2.4 – 5.9)
21.0 (14.5 – 27.4)
17.4 (12.7 – 22.1)
17.5 (12.6 – 22.3)
11.8 (8.4 – 15.2)
3.2 (2 – 4.4)
16.8 (11.0 – 22.5)
18.0 (12.9 – 23.0)
13.5 (8.4 – 18.6)
11.2 (6.3 – 16.2)
0.8 (0.2 – 1.4)
Because the average age of Group III healthy dogs was lower than the average ages of the outpatient dogs (Group I and Group II) (Additional file 1), we investigated whether age affected the level of antiphospholipid antibodies in healthy dogs. Group III (healthy dogs) were divided into older and younger subgroups. The average ELISA OD readings for aPhL, aβ2GPI, aCL, aPI, aPC, and aPS obtained from older and younger subgroups were not significantly different (Additional file 4). In addition, considering that the female to male ratio in Group III healthy dogs was lower than the ratios among the outpatient dogs (Group I and Group II), we divided Group III into female and male subgroups to explore whether gender was a factor for the antiphospholipid antibodies in healthy dogs. The average ELISA OD readings for aPhL, aβ2GPI, aCL, aPI, aPC, and aPS were comparable in the female and male subgroups (Additional file 4). The fact that levels of aPhL, aβ2GPI, aCL, aPI, aPC, and aPS were comparable between older and younger subgroups, and between female and male subgroups among healthy dogs excludes the need for setting any age- or gender-specific positive thresholds.
Frequencies of aPL subtypes based on the 98th or 99th percentile cut-off values and relative risks for thrombocytopenia
Frequency of antiphospholipid antibodies among different groups of dogs based on the 98th percentile cut-off
n = 64/20/18/26
n = 30
n = 80
relative risk (odds ratio)d, e
relative risk (odds ratio)
76 ***/(1287)***/(1162)***/73 ***
7.0 ***/22 ***/22 ***/12 ***
8.3 ***/5.3 */(19)**/(27)***
74 ***/67 ***/(819) ***/(1174) ***
2.8 ***/4.8 ***/10 ***/4.1 ***
1.4*/2.3 */2.5 */1.5
3.5 ***/9.0 ***/10 ***/5.2 ***
1.6**/2.6 */3.2 */1.8
5.7 ***/15 ***/19 ***/9.2 ***
Frequency of antiphospholipid antibodies among different groups of dogs based on the 99th percentile cut-off
n = 64/20/18/26
n = 30
n = 80
relative risk (odds ratio)d, e
relative risk (odds ratio)
76 ***/(1287)***/(1162)***/73 ***
30 ***/24 ***/12 ***/12 ***
8.3 ***/5.3 */(19)**/(27)***
74 ***/67 ***/(819)***/(1174)***
2.2 ***/5.3 ***/7.1 ***/3.8 ***
3.2 ***/7.8 ***/8.7 ***/4.8 ***
1.4*/2.9 */2.7 */1.3
4.5 ***/16 ***/15 ***/6.2 ***
Among outpatient dogs, the positive frequency of aCL (98th or 99th percentile cut-off) was significantly higher in Group I (98 %) and subgroup IA (95 %), IB (100 %), and IC (100 %) than in outpatient dogs without thrombocytopenia (Group II) (Tables 2 and 3). The relative risks of aCL positive outpatient dogs (vs. aCL negative outpatient dogs) for having thrombocytopenia (Group I), immune thrombocytopenia with aPLT (subgroup IA), severe thrombocytopenia without aPLT (IB), and less severe thrombocytopenia (IC) were 8.3, 5.3, ∞ (odds ratio 19) and ∞ (odds ratio 27), respectively. In addition to aCL, significantly higher positive frequencies of aβ2GPI (85 %), aPC (65 % or 60 %), and aPS (80 %) were observed in Group IA than those observed in Group II, with relative risks around 2 (1.9 – 2.9). In comparison with Group II, the positive frequency of aPS (83 % or 78 %) was significantly higher in Group IB, with a relative risk of 3.2 or 2.7 (Tables 2 and 3).
In this study, we used indirect ELISAs to measure and compare serum IgG levels of aPL subtypes (aPhL, aβ2GPI, aCL, aPI, aPC, and aPS) in dogs with or without thrombocytopenia and in healthy dogs. Using a secondary antibody to amplify signal, indirect ELISA is more sensitive than direct ELISA . In addition, indirect ELISA allows us to use one common conjugated secondary antibody to measure different aPL subtypes.
At this point, reference dog sera are not available nor have cut-off values been established for canine aPL subtypes other than aCL. In an earlier report, Papini et al.  estimated canine aCL levels based on an equation obtained from measuring human reference sera and determined the cut-off value as mean plus 2 SD. In our study, we measured levels of aPL subtypes based on a standard curve established for dog IgG calibration (Fig. 1a), which appeared comparable to that generated by using reference human aPhL IgG standards (Fig. 1b). In humans, ELISA cut-off values for aCL have been diversely determined as mean plus 2 SD (around 98th percentile) or 3 SD or 5 SD, or at the 95th or 99th percentiles [21–26]. In our present study, we assessed and compared the association of aPL subtypes with thrombocytopenia based on the 98th percentile (mean of healthy dogs plus 2 SD) and 99th percentile (mean plus 2.33 SD) cut-off values. Based on these cut-off values, canine sera determined as aPhL positive could compete with human reference serum (available in the APhL IgG HRP ELISA kit) for PhL (non-cardiolipin phospholipids) binding (Additional file 5), indicating that our ELISA is reliable.
We mainly investigated aPL subtypes on clinically relevant thrombocytopenic outpatient dogs (Group I) that have much lower platelet count (0 – 80 × 103/uL) than Group II (250 – 500 × 103/uL). This approach reduces the chance of overlapping grouping. We further divided thrombocytopenic dogs into three subgroups to explore the relevance of aPL subtypes to the severity of the disease (Group IA/Group IB vs. Group IC) and to the presence or absence of aPLT (Group IA vs. Group IB). Frequencies of aPC, and aPS appeared higher in severe thrombocytopenic dogs (Group IA and Group IB) than in less severe thrombocytopenic dogs (Group IC) whereas frequencies of aCL and aβ2GPI were higher within thrombocytopenic outpatient dogs than in those without thrombocytopenia (Tables 2 and 3). In contrast, aPhL frequencies are comparably high among outpatient dogs (Tables 2 and 3). Interestingly, such tendencies (regarding aCL, aβ2GPI, aPC, aPS, aPhL) were also observed when we compared frequencies of aPL subtypes in mild thrombocytopenic dogs (platelet count 81 – 199 × 103/uL) with those in Group I (platelet count 0 – 80 × 103/uL) thrombocytopenic dogs or those in Group II (platelet count 250 – 500 × 103/uL) (Additional file 6, Tables 2 and 3). These results suggest that aCL and aβ2GPI could have potential to be markers for thrombocytopenia among outpatients dogs and the presence of aPC and aPS may help to reflect the severity of thrombocytopenia.
Among all tested aPL subtypes, aCL poses the highest relative risk in outpatient dogs for having thrombocytopenia (8.3), immune thrombocytopenia with aPLT (5.3), severe thrombocytopenia without aPLT (∞, odds ratio 19), or less severe thrombocytopenia (∞, odds ratio 27) (Tables 2 and 3). This result indicates an important role of aCL in canine thrombocytopenia, including immune thrombocytopenia and particularly in severe thrombocytopenia without aPLT and in less severe thrombocytopenia. Furthermore, based on higher relative risks, outpatient dogs present with aβ2GPI (relative risk 2.9 or 1.9) and aPC (relative risk 2.3 or 2.0) are around two fold more likely to have immune thrombocytopenia (with aPLT) and those with aPS are two to three fold more likely to have immune thrombocytopenia (relative risks 2.6 or 2.9) or severe thrombocytopenia without aPLT (3.2 or 2.7) (Tables 2 and 3). In the future, it would be interesting to explore whether aCL, aβ2GPI, aPC, and aPS poses differential risks under the presence or absence of aPLT in less severe thrombocytopenia or even mild thrombocytopenia. It is worth noting that our supplement data indicate that the levels of all the aPL subtypes examined here were not significantly different between older and younger subgroups of normal healthy dogs (Additional file 4). This observation is in agreement with that reported by Budd et al.  for human aCL.
Although the average IgG levels of aPhL were significantly higher (P < 0.001) in outpatient dogs with thrombocytopenia or immune thrombocytopenia than in those without (Fig. 2), the fact that prevalences of positive aPhL in thrombocytopenia or immune thrombocytopenic outpatient dogs and in outpatient dogs with other diseases were comparably high indicates that the presence of aPhL may thus not be applicable as a diagnostic criterion for canine thrombocytopenia, immune thrombocytopenia, or APS-related disorders. Interestingly, aPhL, recognizing a mixture of non-cardiolipin antigens, which are comprised of PS, PA, and β2GPI, have been reported to be specifically detected in human patients with antiphospholipid syndrome (APS) and not in other disorders [6–8]. There could be disparities between human and canine APS regarding the specificity of aPL subtypes or clinical manifestations. For example, the results of our study indicate that aPhL, preferentially detected in human APS patients, may not be specific for APS-related disorders in dogs. In particular, canine aPA that was not examined individually in our present study (as opposed to two other aPhL subtypes, aPS and aβ2GPI) deserves future investigation. In addition, a recent study has shown that thrombosis, which is known to be associated with aPL and is listed as one marked manifestation for the diagnosis of APS in humans [2, 27], may not be correlated well with aPL in dogs . Overall, here in our study we observed a high prevalence of aPL (adding up all aPL subtypes) in outpatient dogs with thrombocytopenia (98 %, Group I), immune thrombocytopenia with positive aPLT (100 %, Group IA), severe thrombocytopenia without aPLT (100 %, Group IB). Interestingly, in the recently held 14th International Antiphospholipid Congress, experts in the field discussed whether to include thrombocytopenia and several other non-criteria clinical manifestations of APS as APS classification criteria . Based on data presented in related medical literature and considering that aPL related thrombocytopenia increases the risk of thrombosis, Abreu et al.  categorize thrombocytopenia as “recommended to be included as part of APS criteria revision” although the quality of data is low. In the future, it is imperative to carry out extensive investigations to clarify whether thrombocytopenia can be listed as one clinical manifestation of human APS or canine APS-related disorders. Follow-up surveys are needed to compare the incidence of thrombocytopenia, pregnancy morbidity, hemolytic anemia, and thrombosis among dogs with positive antiphospholipid antibodies.
Of all the aPL subtypes tested here, aCL is highly associated with canine thrombocytopenia, including immune thrombocytopenia, and particularly severe thrombocytopenia negative for aPLT and less severe thrombocytopenia. Furthermore, aPS is moderately associated with both canine immune thrombocytopenia and severe thrombocytopenia negative for aPLT, whereas aβ2GPI, and aPC are moderately relevant to canine immune thrombocytopenia. In contrast, aPI is not significantly associated with canine immune thrombocytopenia.
Canine blood and platelet count
EDTA-anticoagulated blood samples (for platelet count) or sera were taken from outpatient dogs admitted to the Veterinary Medical Teaching Hospital, National Chung Hsing University (Taichung, Taiwan, ROC) or from healthy dogs (based on physical examination and/or platelet count) whose owners had volunteered to bring their dogs in for a checkup. Platelet counts were measured using a KX-21 N Hematology Analyzer (Sysmex, Kobe, Japan). Owner consents were obtained before collecting blood from dogs. Sera were stored at -20 °C.
Detection of canine aPLT by indirect ELISAs
For the detection of aPLT in serum samples, an indirect ELISA was carried out according to the manual of the canine PA-IgG/M/A ELISA kit (Novatein Biosciences, Woburn, MA, USA). Positive threshold for aPLT was determined as mean plus 2.33 SD (99th percentile cut-off value) of healthy dogs (Group III of this study). Detailed method was described in the supporting information (Additional file 2).
β2GPI expression and identification
Methods for the cDNA cloning, recombinant protein expression and identification of human β2GPI were described in the supporting information (Additional file 3).
ELISA for dog IgG calibration
Fifty μL per well of 50 ng/mL rabbit anti-dog IgG-F(ab)2 fragment antibodies (Bethyl Laboratories, Montgomery, TX, USA) in ELISA coating buffer (15 mM NaCO3, 35 mM NaHCO3 at pH 9.6) were added into a 96-well plate and incubated overnight at 4 °C. The next day, each well was fixed with 100 μL of methanol for 10 min and washed twice with phosphate-buffered saline (PBS). The plate was air-dried. Each well was incubated with 100 μL of blocking buffer for 60 min. After removing the blocking buffer, 100 μL of serial 2-fold dilutions (in PBS) of dog IgG (Sigma, St. Louis, MO, USA) were added into each well and incubated for 30 min at 37 °C. After washing three times (15 min for each wash) with 200 μL of PBS, 100 μL of horseradish peroxidase (HRP)-conjugated rabbit anti-dog IgG Fc fragment specific antibodies (Jackson ImmunoResearch, West Grove, PA, USA) (1:10000 in blocking buffer, PBS containing 3 % normal rabbit serum) were added to each well and incubated for 30 min at 37 °C. After three washes, 100 μL of 3,3’,5,5’-tetramethylbenzidine (TMB) solution was added and incubated for 30 min in the dark. Finally, 100 μL of 1 M H2SO4 was added to stop the reaction. The optical density (OD) was measured at 450 nm by using a μquant ELISA reader (BioTek, Winooski, VT, USA). Each of the concentrations above were repeated in triplicate to establish a standard ELISA curve.
An indirect ELISA for human IgG aPhL standards
Using APhL IgG calibrators (provided in the kit) containing quantified reference human aPhL IgG, an indirect ELISA was performed according to the manual of the APhL IgG HRP ELISA kit (Louisville APL Diagnostics, Doraville, GA, USA). Briefly, each of the 96 wells was incubated for 30 min with 100 μL of pre-diluted reference human sera. After three washes, HRP conjugated anti-human IgG antibodies provided in the kit was added into each well and incubated for 30 min. Substrate solution was added and incubated for 30 min in the dark. Finally, 100 μL of stop solution was added to stop the reaction. The optical density (OD) was measured at 450 nm by using a μquant ELISA reader (BioTek).
Detection of canine aPhL, aCL, aPI, aPC, aPS, and aβ2GPI IgG by indirect ELISAs
The coated phospholipid antigens in an APhL IgG HRP ELISA kit (Louisville APL Diagnostics) were used as antigens to detect aPhL in canine sera. For aCL, aPI, aPC, and aPS detections, 30 μL (50 μg/mL in ethanol) of cardiolipin (CL), phosphatidylinositol (PI), phosphatidylcholine (PC), and PS (Sigma) were coated onto each of the 96 wells by evaporation. For the detection of aβ2GPI IgG antibodies, 50 μL of rβ2GPI (1 μg/mL in ELISA coating buffer) were added into each of the 96 wells. The plate was coated and fixed with methanol. The following procedures were the same as described above for the dog IgG sandwich ELISA, except that 100 μL of diluted canine serum (1:50 in blocking buffer) were added instead of adding serial 2-fold dilutions of dog IgG.
Sequence accession number
The sequence of human β2GPI cDNA isolated in this study was deposited in GenBank under accession number HM212425.
Chi-square (χ2) analysis, two-sided Fisher’s exact test (for small expected frequencies), and t-test were employed, and relative risks or odds ratios were calculated to correlate aPhL, aβ2GPI, aCL, aPI, aPC, and aPS IgG antibodies with thrombocytopenia or immune thrombocytopenia by using Prism statistical software (version 6.0, GraphPad Software, La Jolla, CA).
aCL, anticardiolipin antibodies; aPA, antiphosphatidic acid; aPC, antiphosphatidylcholine; aPG, antiphosphatidylglycine; aPhL, anti-noncardiolipin phospholipids antibodies; aPI, antiphosphatidylinositol antibodies; aPL, antiphospholipid antibodies; aPLT, antiplatelet antibodies; aPS, antiphosphatidylserine antibodies; APS, antiphospholipid syndrome; aβ2GPI, anti-β2 glycoprotein I antibodies; LA, lupus anticoagulants; rβ2GPI, recombinant β2GPI; SLE, systemic lupus erythematosus
This study was supported by the Ministry of Education, Taiwan, R.O.C., under the Aiming for the Top University (ATU) plan and by the Animal Disease Diagnostic Center, National Chung Hsing University, Taiwan, R.O.C. (grants 102D116, 103DA116, and 104DA116). We thank Dr. Linjing Kong for her assistance in data collection.
Funding is mentioned in the Acknowledgements. The funding sources have no role in the design of the study and collection, analysis, and interpretation of data and in writing the manuscript.
Availability of data and materials
All the data supporting our findings can be found in the manuscript. In addition, we have uploaded 6 additional files containing basic information of three groups of dogs, antiplatelet antibodies measurement, β2GPI expression and identification, antiphospholipid antibodies in subgroups of healthy dogs, competition of canine aPhL with reference human aPhL, and frequencies of aPL subtypes in all thrombocytopenic dogs.
SHC conceived and designed the study. YCC, LMC, KCC, YHF, WML, SLL, YC Hsu, MXW, and CLT collected the data. SHC, KCC, LMC, YCC, YC Hsu, YC Hwang, SPH, and FCM performed the analyses. SHC, LMC, YCC, and KCC drafted the manuscript. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
Consent for publication
Ethics approval and consent to participate
Blood samples were collected in accordance with the Guidebook for the Care and Use of Laboratory Animals of the Council of Agriculture, Executive Yuan, Taiwan. The protocol of this study was approved by the Institutional Animal Care and Use Committee, National Chung Hsing University (IACUC of NCHU), Taiwan. The IACUC approval number of this study is 10357.
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