Table of Contents Author Guidelines Submit a Manuscript
Journal of Analytical Methods in Chemistry
Volume 2018 (2018), Article ID 5394527, 7 pages
https://doi.org/10.1155/2018/5394527
Research Article

Solid-Phase Extraction and Large-Volume Sample Stacking-Capillary Electrophoresis for Determination of Tetracycline Residues in Milk

1Área Académica de Química, Universidad Autónoma del Estado de Hidalgo, Carretera Pachuca-Tulancingo Km. 4.5, 42076 Pachuca, Hidalgo, Mexico
2Departamento Química Analítica, Nutrición y Bromatología, Facultad de Veterinaria, Universidad de Santiago de Compostela, Pabellón 4 planta bajo, Campus Universitario s/n, 27002 Lugo, Spain

Correspondence should be addressed to Israel S. Ibarra

Received 25 August 2017; Revised 15 November 2017; Accepted 6 December 2017; Published 20 February 2018

Academic Editor: Serban C. Moldoveanu

Copyright © 2018 Gabriela Islas et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract

Solid-phase extraction in combination with large-volume sample stacking-capillary electrophoresis (SPE-LVSS-CE) was applied to measure chlortetracycline, doxycycline, oxytetracycline, and tetracycline in milk samples. Under optimal conditions, the proposed method had a linear range of 29 to 200 µg·L−1, with limits of detection ranging from 18.6 to 23.8 µg·L−1 with inter- and intraday repeatabilities < 10% (as a relative standard deviation) in all cases. The enrichment factors obtained were from 50.33 to 70.85 for all the TCs compared with a conventional capillary zone electrophoresis (CZE). This method is adequate to analyze tetracyclines below the most restrictive established maximum residue limits. The proposed method was employed in the analysis of 15 milk samples from different brands. Two of the tested samples were positive for the presence of oxytetracycline with concentrations of 95 and 126 µg·L−1. SPE-LVSS-CE is a robust, easy, and efficient strategy for online preconcentration of tetracycline residues in complex matrices.

1. Introduction

Preconcentration methods are an important tool for sample preparation because they enrich analytes in a liquid or solid sample. This improves analytical sensitivity, with the additional advantage of removing interferences [1]. Commonly employed preconcentration techniques include liquid-liquid extraction (LLE) [2], solid-phase extraction (SPE) [3], dispersive solid-phase extraction (DSPE) [4], magnetic solid-phase extraction (MSPE) [5], and quick, easy, cheap, effective, rugged, and safe (QuEChERS) [6, 7]. These techniques are termed off-line.

On the other hand, online techniques use automated systems that minimize sample manipulation. Flow techniques are commonly coupled to SPE [8, 9] using solid phases composed of molecularly imprinted polymers (MIPs) [1012], monolithic columns [13, 14], and carbonaceous materials [15, 16].

Recently, capillary electrophoresis (CE) has received considerable attention in the development of online preconcentration systems such as transient isotachophoresis (tITP) [17], dynamic pH junction [18], sweeping [19, 20], and field-amplified stacking. The main advantages of these methods compared to off-line techniques include higher efficiency, shorter analysis time, and lower reagent and sample consumption [2123]. Online preconcentration in CE is based on injection of a larger-than-normal sample volume into the capillary via hydrodynamic or electrokinetic methods [24].

Field-amplified stacking was developed for preconcentration of several analytes based on the charges of the analytes. Figure 1 shows a large-volume sample stacking (LVSS) system, which involves a series of polarity switches in CE. The first step (Figure 1(a)) is hydrodynamic injection of a large sample volume into the capillary. Subsequently (Figure 2(b)), a voltage is applied (reverse polarity) promoting concentration of the analytes and removal of the cationic and nonionic compounds contained in the sample matrix. Finally (Figures 1(c) and 1(d)), analytes are separated in normal polarity in the background electrolyte (BGE) [25, 26].

Figure 1: Schematic diagram of a preconcentration LVSS system. (a) Sample injection, (b) application of preconcentration potential (reverse polarity), (c) normal polarity, and (d) separation by capillary electrophoresis.
Figure 2: Contour and response surface plots of interactions modes for output variables (sum): (a) injection time (min)  :  reverse potential (kV); (b) injection time (min)  :  reverse polarity time (min); and (c) reverse polarity (kV)  :  reverse polarity time (min).

Tetracyclines (TCs) are broad-spectrum antibiotics frequently employed in veterinary medicine for therapeutic purposes [5, 27] or incorporated into livestock feed at subtherapeutic doses as growth promoters. However, their indiscriminate use can produce enhanced bacterial resistance, allergic reactions, liver damage, and gastrointestinal issues [28, 29].

In order to protect human health from exposure of TC residues in milk, the European Union has established a maximum residue limit (MRL) of 100 µg·kg−1 for chlortetracycline (CT), oxytetracycline (OT), and tetracycline (TC) [30]; the Food and Drug Administration (FDA) has established a MRL of 300 µg·kg−1 for the combined residues CT, OT, and TC [31]; the Codex Alimentarius recommends a limit of 200 µg·kg−1 in milk for the combined residues CT, OT, and TC [32].

In recent years, due to the concerns caused by veterinary drugs contained in food samples, there were developed a large variety of analytical methodologies for the determination of TC residues at μg·kg−1 or μg·L−1 levels in different matrices. These methods included chemiluminescence [33], microbiological assays [34], high-performance liquid chromatography (HPLC) [35, 36], or capillary electrophoresis (CE) [37].

Taking into account the MRLs and the complexity of milk, this work develops a CE method using SPE and LVSS-CE for determination of TCs in milk that was demonstrated to be rapid, simple, and efficient. Additionally, the developed method showed higher sensitivity and accuracy than those reported by conventional methods using CZE aimed at the detection and quantification of TC residues in milk.

2. Experimental

2.1. Reagents and Chemicals

All solutions were prepared by dissolving the respective analytical grade reagent in deionized water with a resistivity not less than 18.0 MΩ·cm, which was provided by a Milli-Q system (Millipore, Bedford, MA, USA). Sodium phosphate was obtained from Sigma (St. Louis, MO, USA). EDTA sodium salt, sodium hydroxide, and hydrochloric acid were obtained from J.T. Baker (Phillipsburg, NJ, USA). Methanol was obtained from Mallinckrodt Baker (Xalostoc, Mexico), and 2-propanol was obtained from Fluka (St. Gallen, Switzerland).

Single stock standards of 100 mg·L−1 were prepared in methanol. The stock solutions were stored at −4°C. Mixed standard working solutions were prepared by diluting the standard stock solution immediately before use. The BGE solution consisted of 30 mM sodium phosphate, 2 mM EDTA disodium salt, and 2% 2-propanol. The solution pH was adjusted to 12.0 with 0.1 M·NaOH.

2.2. Apparatus

Electrophoresis was performed using a Beckman Coulter P/ACE 5500 (Fullerton, CA, USA) with a photodiode array detector. Data were collected and analyzed with a Beckman P/ACE system with MDQ version 2.3 software. TC separations were performed in a fused silica capillary (41.7 cm × 75 µm ID). A pH/ion analyzer (model 450; Corning Science Products, NY, USA) was used to accurately adjust the pH of the electrolyte solution to within 0.01 pH units.

At the beginning of each working day, the capillary was activated with 1.0 M NaOH at 35°C for 15 min, followed by 0.1 M NaOH for 10 min, deionized water at 25°C for 10 min, and then electrolyte solution at 25°C for 10 min. The capillary was washed out between successive analyses using 1.0 M NaOH for 4 min, 0.1 M NaOH for 2 min, deionized water for 2 min, and electrolyte solution for 4 min. The detector wavelength (ʎ) was set at 360 nm, and the capillary was kept at 25°C. Peaks were identified by migration times and coinjection of standard solutions [5].

2.3. Sample Treatment and Analysis

A 1.0 mL milk sample was fortified with an internal standard (50 µg·L−1) in polypropylene tubes. Proteins were precipitated by adding 0.2 mL of 2% acetic acid (v/v), followed by heating for 5 min (65°C) in a water bath and centrifuging at 3200 rpm for 15 min. Once completed, the protein-free liquid phase was diluted to 10 mL with deionized water. The solution was then passed through a cartridge (Sep-Pak Vac C18 cartridges, 1 g, 6 cc, Waters) previously activated with 5 mL of methanol, followed by 5 mL of methanol and 5 mL of deionized water at a maximum flow rate of 1 mL·min−1. Analytes retained on the SPE cartridge were washed with 2.0 mL of 5.0% methanol. Retained TCs were eluted with 3.0 mL of methanol. The eluted solution was evaporated to dryness, and the residue was dissolved in 1 mL of 0.01 M NaOH containing 50 µg·L−1 picric acid as an internal standard.

Samples treated by SPE were introduced by hydrodynamic injection at 5 psi for 180 s (around 98% of capillary capacity). The capillary was then set in BGE vials, and a potential of 12 kV was applied for 120 s (reverse polarity) to preconcentrate TCs at the inlet, while water and other ions were removed from the capillary. Finally, polarity was returned to normal (14 kV), and CE separation was carried out.

3. Results and Discussion

3.1. LVSS Optimization

Development of an LVSS preconcentration technique for capillary electrophoresis requires optimization of control variables. Optimization involves selection of factors that influence the analytical signal and enrichment factor. Box–Behnken design (BBD) was selected for optimization because it allows evaluation of control factors using an adjusted surface response.

The experimental design matrix describes the combination of factors in each experiment and allows simultaneous evaluation of several variables. Optimization of the system with BBD involves four steps: (i) identifying the output variable to optimize, (ii) identifying and selecting factors and levels that affect the LVSS system, (iii) data analysis and fitting of the surface response model, and (iv) confirmation under the optimal conditions obtained.

For LVSS, the output variable selected is the sum of the enrichment factors of the four TCs. The variables optimized in the procedure were the injection time (min) in the hydrodynamic mode using a pressure of 5 psi, applied potential (kV), and time (min) of reverse polarity. Injection time was varied between 2.0 and 3.0 min to evaluate the time required to fill the capillary. The reverse potential was evaluated between 8.0 and 12 kV. These values were selected to ensure sufficient stacking time to remove the sample matrix from the capillary without losing analytes. Additionally, time during preconcentration (2.0–3.0 min) must be sufficient to increase analyte enrichment.

Table 1 shows the design matrix produced and the output variable in function of the sum of each enrichment factor obtained in each condition. All experiments were performed using 1 mL of a standard solution of TCs at a concentration of 1.0 mg·L−1. Enrichment factors were estimated as the area ratio of the signals obtained with and without application of online LVSS.

Table 1: Optimal conditions determined with Box–Behnken design.

Results were analyzed using MINITAB® version 17 software. Data were adjusted to the quadratic model according to the analysis of variance (ANOVA). The coefficient of determination (r2) for the adjustment was 0.785, and the equation for the surface response waswhere Y1 is the sum of the enrichment factor, X1 is the injection time (min), X2 is the inversion electric current (kV), and X3 is the applied time in the inversion electric current (min). The critical variables during LVSS are the reverse potential and applied time (). The lack-of-fit test is designed to determine if the proposed model is adequate for the observed data. The test is performed by comparing the variability of residuals from observations at replicate settings of the factors. Since the value for lack of fit in the ANOVA table (0.744) is greater than 0.05, the model is adequate for the observed data at the 95.0% confidence level.

Based on the response surfaces (Figure 2), a clear interaction between the variables is observed, which is commonly observed for preconcentration systems employing LVSS-CE. Optimal conditions determined by BBD were X1: injection time (3.0 min), X2: reverse potential (12 kV), and X3: preconcentration time (2.0 min).

The proposed methodology (LVSS-CE) was applied for the determination of TCs in commercial milk samples using a modification of the method proposed by Islas et al. [4]. However, different electrophoretic mobilities were obtained for the internal standard, which can be attributed to the ionic strength of the sample. Ionic strength significantly increases the electrophoretic mobility of analytes, thereby affecting LVSS preconcentration and causing loss of analyte if care is not taken when applying the negative polarity [38].

For these reasons and given the complexity of the sample, one of the most important steps in LVSS-CE analysis is sample cleanup. However, this may be difficult for analysis of antibiotics. For these reasons, an extraction and cleanup step was used previous to preconcentration and analysis by LVSS-CE. SPE was used for extraction and cleanup of TCs in milk samples. This technique decreases ionic strength effects, making samples suitable for analysis by LVSS-CE. For sample pretreatment, following protein removal from the milk sample, the liquid phase is diluted to 10.0 mL with deionized water and then passed through an activated C18 SPE cartridge. Analytes retained on the SPE cartridge were washed with 2.0 mL of 5.0% methanol. Retained TCs were eluted with 3.0 mL of methanol. The eluted solution was evaporated to dryness and redissolved in 1.0 mL of 0.01 M NaOH containing 50 µg·L−1 picric acid [39].

3.2. Analytical Parameters

Under optimal conditions, analytical parameters of the LVSS-CE method were evaluated at concentrations of 0–200 µg·L−1 for each TC. Each standard was prepared and analyzed in triplicate using the proposed methodology. Peak areas were measured, and calibration curves were constructed from the peak area ratios (analyte  :  internal standard). Calibration curves showed a linear dependence on TC concentration. Calibration regression parameters are shown in Table 2. LODs were calculated for a signal-to-noise ratio of 3.29 according to IUPAC recommendations [40].

Table 2: Regression parameters of calibration: absorbance (mUA) versus TC concentration (µg·L−1).

The accuracy and precision of the method proposed was measured in terms of intra- and interday repeatabilities for migration times and peak areas. Results were determined as the relative standard deviation (%RSD) obtained in the analysis of TCs at two concentrations (75 and 150 µg·L−1). Based on these results and using the most restrictive MRLs established by EU regulations, the LVSS is adequate for analysis of TCs in milk samples.

3.3. Application

The proposed SPE-LVSS-CE method was applied for the determination of TCs in 15 commercial milk samples from different brands. Three replicate determinations of each analyte in the selected samples were performed. Two samples were determined to be positive for the presence of OT with concentrations of 95 and 126 µg·L−1, respectively, which was identified by their migration times. In order to confirm the presence of the analyte, a standard addition was made to the sample extract. An increase in the peak area confirmed the presence of the antibiotic residue. Samples with TC concentrations outside the linear response range were diluted tenfold with deionized water. Confirmation using mass spectrometry is also required. The electropherograms obtained are shown in Figure 3.

Figure 3: Electropherograms. (a) Standard sample of 10 mg·L−1 TCs and 50 mg·L−1 IS by CE; (b) standard sample of 1 mg·L−1 TCs and 5 mg·L−1 IS by LVSS-CE; (c) blank milk sample by SPE-LVSS-CE; and (d) real milk sample by SPE-LVSS-CE.

4. Conclusions

The proposed SPE-LVSS-CE technique provided sensitive, rapid, simple, and efficient online preconcentration of TC residues in complex matrices such as milk. This methodology only required 1.0 mL of milk, whereas traditional methods require about 100.0 mL to reach the MRLs established by international regulations.

Additionally, this technique provides good sensitivity and accuracy compared to CZE and has a much higher stacking efficiency for the four analytes with LODs of 18.60–23.83 µg·L−1. The developed method allowed achieve enrichment factors from 50.33 to 70.85 compared to conventional injection mode. The SPE-LVSS-CE method achieves appropriate LODs for identification and quantification of TCs according to MRLs established by the EU, FDA, and Codex Alimentarius. The developed method was applied to preconcentrate, identify, and quantify TCs in real milk samples with satisfactory outcomes.

Conflicts of Interest

The authors declare that they have no conflicts of interest.

Acknowledgments

The authors wish to thank Programa para el Desarrollo Profesional Docente, para el Tipo Superior (PRODEP) for the approved project in the incorporation of new PTC-Profesores de Tiempo Completo; Consejo Nacional de Ciencia y Tecnología (CONACyT) (Project INFR-2014-227999 and Retention Grant no. 251112) and Xunta de Galicia and Fondo Europeo de Desarrollo Regional (FEDER) (Project GRC 2014/004), for financial support.

References

  1. L. Pillonel, J. O. Bosset, and R. Tabacchi, “Rapid preconcentration and enrichment techniques for the analysis of food volatile. A review,” LWT-Food Science and Technology, vol. 35, no. 1, pp. 1–14, 2002. View at Publisher · View at Google Scholar · View at Scopus
  2. C. Wang, L. Qu, X. Liu et al., “Determination of a metabolite of nifursol in foodstuffs of animal origin by liquid–liquid extraction and liquid chromatography with tandem mass spectrometry,” Journal of Separation Science, vol. 40, no. 3, pp. 671–676, 2017. View at Publisher · View at Google Scholar · View at Scopus
  3. R. Gogoi, D. C. Roy, and S. Sinha, “Determination of chlortetracycline residues in swine tissues using high performance liquid chromatography,” Pharma Innovation Journal, vol. 6, pp. 34–36, 2017. View at Google Scholar
  4. G. Islas, J. A. Rodríguez, M. E. Páez-Hernández, S. Corona-Avendaño, A. Rojas-Hernández, and E. Barrado, “Dispersive solid phase extraction based on butylamide silica for determination of sulfamethoxazole in milk samples by capillary electrophoresis,” Journal of Liquid Chromatography & Related Technologies, vol. 39, no. 14, pp. 658–665, 2016. View at Publisher · View at Google Scholar · View at Scopus
  5. I. S. Ibarra, J. A. Rodriguez, J. M. Miranda, M. Vega, and E. Barrado, “Magnetic solid phase extraction based on phenyl silica adsorbent for the determination of tetracyclines in milk samples by capillary electrophoresis,” Journal of Chromatography A, vol. 1218, no. 16, pp. 2196–2202, 2011. View at Publisher · View at Google Scholar · View at Scopus
  6. C. Guo, M. Wang, H. Xiao et al., “Development of a modified QuEChERS method for the determination of veterinary antibiotics in swine manure by liquid chromatography tandem mass spectrometry,” Journal of Chromatography B, vol. 1027, pp. 110–118, 2016. View at Publisher · View at Google Scholar · View at Scopus
  7. W. H. Tsai, T. C. Huang, J. J. Huang, Y. H. Hsue, and H. Y. Chuang, “Dispersive solid-phase microextraction method for sample extraction in the analysis of four tetracyclines in water and milk samples by high-performance liquid chromatography with diode-array detection,” Journal of Chromatography A, vol. 1216, no. 12, pp. 2263–2269, 2009. View at Publisher · View at Google Scholar · View at Scopus
  8. W. Liu, Z. Zhang, and Z. Liu, “Determination of β-lactam antibiotics in milk using micro-flow chemiluminescence system with on-line solid phase extraction,” Analytica Chimica Acta, vol. 592, no. 2, pp. 187–192, 2007. View at Publisher · View at Google Scholar · View at Scopus
  9. M. F. El-Shahat, N. Burham, and S. M. A. Azeem, “Flow injection analysis–solid phase extraction (FIA–SPE) method for preconcentration and determination of trace amounts of penicillins using methylene blue grafted polyurethane foam,” Journal of Hazardous Materials, vol. 177, no. 1–3, pp. 1054–1060, 2010. View at Publisher · View at Google Scholar · View at Scopus
  10. E. Caro, R. M. Marcé, P. A. G. Cormack, D. C. Sherrington, and F. Borrull, “Synthesis and application of an oxytetracycline imprinted polymer for the solid-phase extraction of tetracycline antibiotics,” Analytica Chimica Acta, vol. 552, no. 1-2, pp. 81–86, 2005. View at Publisher · View at Google Scholar · View at Scopus
  11. T. Jing, X. D. Gao, P. Wang et al., “Determination of trace tetracycline antibiotics in foodstuffs by liquid chromatography-tandem mass spectrometry coupled with selective molecular-imprinted solid-phase extraction,” Analytical and Bioanalytical Chemistry, vol. 393, no. 8, pp. 2009–2018, 2009. View at Publisher · View at Google Scholar · View at Scopus
  12. F. Tan, D. Sun, J. Gao et al., “Preparation of molecularly imprinted polymer nanoparticles for selective removal of fluoroquinolone antibiotics in aqueous solution,” Journal of Hazardous Materials, vol. 244-245, pp. 750–757, 2013. View at Publisher · View at Google Scholar · View at Scopus
  13. Y. K. Lv, C. L. Jia, J. Q. Zhang, P. Li, and H. W. Sun, “Preparation and evaluation of a novel molecularly imprinted hybrid composite monolithic column for on-line solid-phase extraction coupled with HPLC to detect trace fluoroquinolone residues in milk,” Analytical Methods, vol. 5, no. 7, pp. 1848–1855, 2013. View at Publisher · View at Google Scholar · View at Scopus
  14. M. Seifrtová, A. Pena, C. M. Lino, and P. Solich, “Determination of fluoroquinolone antibiotics in hospital and municipal wastewaters in Coimbra by liquid chromatography with a monolithic column and fluorescence detection,” Analytical and Bioanalytical Chemistry, vol. 391, no. 3, pp. 799–805, 2008. View at Publisher · View at Google Scholar · View at Scopus
  15. H. Niu, Y. Cai, Y. Shi et al., “Evaluation of carbon nanotubes as a solid-phase extraction adsorbent for the extraction of cephalosporins antibiotics, sulfonamides and phenolic compounds from aqueous solution,” Analytica Chimica Acta, vol. 594, no. 1, pp. 81–92, 2007. View at Publisher · View at Google Scholar · View at Scopus
  16. S. Álvarez-Torrellas, R. S. Ribeiro, H. T. Gomes, G. Ovejero, and J. García, “Removal of antibiotic compounds by adsorption using glycerol-based carbon materials,” Chemical Engineering Journal, vol. 296, pp. 277–288, 2016. View at Publisher · View at Google Scholar · View at Scopus
  17. X. Wang and Y. Chen, “Determination of aromatic amines in food products and composite food packaging bags by capillary electrophoresis coupled with transient isotachophoretic stacking,” Journal of Chromatography A, vol. 1216, no. 43, pp. 7324–7328, 2009. View at Publisher · View at Google Scholar · View at Scopus
  18. L. Wang, D. MacDonald, X. Huang, and D. D. Y. Chen, “Capture efficiency of dynamic pH junction focusing in capillary electrophoresis,” Electrophoresis, vol. 37, no. 9, pp. 1143–1150, 2016. View at Publisher · View at Google Scholar · View at Scopus
  19. R. Fang, G. Chen, L. Yi et al., “Determination of eight triazine herbicide residues in cereal and vegetable by micellar electrokinetic capillary chromatography with on-line sweeping,” Food Chemistry, vol. 145, pp. 41–48, 2014. View at Publisher · View at Google Scholar · View at Scopus
  20. A. Šlampová, Z. Malá, P. Gebauer, and P. Boček, “Recent progress of sample stacking in capillary electrophoresis (2014–2016),” Electrophoresis, vol. 38, no. 1, pp. 20–32, 2017. View at Publisher · View at Google Scholar · View at Scopus
  21. C. Kukusamude, S. Srijaranai, M. Kato, and J. P. Quirino, “Cloud point sample clean-up and capillary zone electrophoresis with field enhanced sample injection and micelle to solvent stacking for the analysis of herbicides in milk,” Journal of Chromatography A, vol. 1351, pp. 110–114, 2014. View at Publisher · View at Google Scholar · View at Scopus
  22. L. Y. Thang, H. H. See, and J. P. Quirino, “Field-enhanced sample injection-micelle to solvent stacking in non aqueous capillary electrophoresis,” Talanta, vol. 161, pp. 165–169, 2016. View at Publisher · View at Google Scholar · View at Scopus
  23. L. Liu, Q. Wan, X. Xu, S. Duan, and C. Yang, “Combination of micelle collapse and field-amplified sample stacking in capillary electrophoresis for determination of trimethoprim and sulfamethoxazole in animal-originated foodstuffs,” Food Chemistry, vol. 219, pp. 7–12, 2017. View at Publisher · View at Google Scholar · View at Scopus
  24. F. Kitagawa and K. Otsuka, “Recent applications of on-line sample preconcentration techniques in capillary electrophoresis,” Journal of Chromatography A, vol. 1335, pp. 43–60, 2014. View at Publisher · View at Google Scholar · View at Scopus
  25. N. Wang, M. Su, S. Liang, and H. Sun, “Sensitive residue analysis of quinolones and sulfonamides in aquatic product by capillary zone electrophoresis using large-volume sample stacking with polarity switching combined with accelerated solvent extraction,” Food Analytical Methods, vol. 9, no. 4, pp. 1020–1028, 2016. View at Publisher · View at Google Scholar · View at Scopus
  26. A. V. Herrera-Herrera, L. M. Ravelo-Pérez, J. Hernández-Borges, M. M. Afonso, J. A. Palenzuela, and M. A. Rodríguez-Delgado, “Oxidized multi-walled carbon nanotubes for the dispersive solid-phase extraction of quinolone antibiotics from water samples using capillary electrophoresis and large volume sample stacking with polarity switching,” Journal of Chromatography A, vol. 1218, no. 31, pp. 5352–5361, 2011. View at Publisher · View at Google Scholar · View at Scopus
  27. M. E. Hume and C. J. Donskey, “Effect of vancomycin, tylosin, and chlortetracycline on vancomycin-resistant Enterococcus faecium colonization of broiler chickens during grow-out,” Foodborne Pathogens and Disease, vol. 14, no. 4, pp. 231–237, 2017. View at Publisher · View at Google Scholar · View at Scopus
  28. J. Cornejo, E. Pokrant, D. Araya et al., “Residue depletion of oxytetracycline (OTC) and 4-epi-oxytetracycline (4-epi-OTC) in broiler chicken’s claws, by liquid chromatography tandem mass spectrometry (LC-MS/MS),” Food Additives & Contaminants: Part A, vol. 34, no. 4, pp. 469–476, 2017. View at Publisher · View at Google Scholar · View at Scopus
  29. F. Granados-Chinchilla and C. Rodríguez, “Tetracyclines in food and feeding stuffs: from regulation to analytical methods, bacterial resistance, and environmental and health implications,” Journal of Analytical Methods in Chemistry, vol. 2017, Article ID 1315497, 24 pages, 2017. View at Publisher · View at Google Scholar · View at Scopus
  30. “Commission Regulation (EC) No 508/1999 of 4 March 1999 amending Annexes I to IV to Council Regulation (EEC) No 2377/90 laying down a community procedure for the establishment of maximum residue limits of veterinary medical products in foodstuffs of animal origin,” Official Journal of the European Community, vol. L60, pp. 16–52, 1999.
  31. US Code of Federal Regulations, Food and Drugs, Chapter I; Food and Drugs Administration, Department of Health and Human Services, Subchapter E; Animal Drugs, Feed, and Related Products, Part 556; Tolerances for residues of New Animal Drugs, vol. 6, US Government Printing Office, Washington, DC, USA, 1998, http://www.fda.govElectronic Code of Federal Regulations (e-CFR).
  32. Codex Alimentarius, Maximum residue limits (MRLs) and risk management recommendations (RMRs) for residues of veterinary drugs in foods, CAC/MRL 2-2017, Codex Alimentarius Commission, 2017.
  33. C. Long, B. Deng, S. Sun, and S. Meng, “Simultaneous determination of chlortetracycline, ampicillin and sarafloxacin in milk using capillary electrophoresis with electrochemiluminescence detection,” Food Additives & Contaminants: Part A, vol. 34, no. 1, pp. 1–8, 2016. View at Publisher · View at Google Scholar · View at Scopus
  34. M. Tumini, O. G. Nagel, and R. L. Althaus, “Microbiological bioassay using Bacillus pumilus to detect tetracycline in milk,” International Dairy Journal, vol. 82, no. 2, pp. 248–255, 2015. View at Publisher · View at Google Scholar · View at Scopus
  35. E. Patyra and K. Kwiatek, “Development and validation of multi-residue analysis for tetracycline antibiotics in feed by high performance liquid chromatography coupled to mass spectrometry,” Food Additives & Contaminants: Part A, vol. 34, no. 9, pp. 1553–1561, 2016. View at Publisher · View at Google Scholar
  36. D. Wei, S. Wu, and Y. Zhu, “Magnetic solid phase extraction based on graphene oxide/nanoscale zero-valent iron for the determination of tetracyclines in water and milk by using HPLC-MS/MS,” RSC Advances, vol. 7, no. 70, pp. 44578–44586, 2017. View at Publisher · View at Google Scholar
  37. C. Zhou, J. Deng, G. Shi, and T. Zhou, “β-cyclodextrin-ionic liquid polymer based dynamically coating for simultaneous determination of tetracyclines by capillary electrophoresis,” Electrophoresis, vol. 38, no. 7, pp. 1060–1067, 2017. View at Publisher · View at Google Scholar · View at Scopus
  38. J. A. Hunt and D. G. Dalgleish, “Heat stability of oil-in-water emulsions containing milk proteins: Effect of ionic strength and pH,” Journal of Food Science, vol. 60, no. 5, pp. 1120–1123, 1995. View at Publisher · View at Google Scholar · View at Scopus
  39. J. A. Rodriguez, J. Espinosa, K. Aguilar-Arteaga, I. S. Ibarra, and J. M. Miranda, “Determination of tetracyclines in milk samples by magnetic solid phase extraction flow injection analysis,” Microchimica Acta, vol. 171, no. 3-4, pp. 407–413, 2010. View at Publisher · View at Google Scholar · View at Scopus
  40. K. Danzer and L. A. Currie, “Guidelines for calibration in analytical chemistry. Part I. Fundamentals and single component calibration (IUPAC Recommendations 1998),” Pure and Applied Chemistry, vol. 70, no. 4, pp. 993–1014, 1998. View at Publisher · View at Google Scholar