Quantification of 9-Carboxy-11-nor-Δ9-tetrahydrocannabinol in Urine Using Brominated 9-Carboxy-11-nor-Δ9-tetrahydrocannabinol as the Internal Standard and High-Performance Liquid Chromatography with Electrochemical Detection

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  • BIOMEDICAL CHROMATOGRAPHY, VOL. 10, 161-166 (1996)

    Quantification of 9-Carboxy-ll-nor-A- tetrahydrocannabinol in Urine Using Brominated 9- Carboxy - 11 -nor=A= tetrahydrocannabinol as the Internal Standard and High-Performance Liquid Chromatography with Electrochemical Detection

    Daniel H. Fisher* and Marc I. Broudy Department of Medical Laboratory Science, 206 Mugar Building, Northeastern University, Boston. MA 021 15. USA

    L. Megan Fisher Department of Biology, 414 Mugar Building, Northeastern University, Boston, MA 02115. USA

    A method was developed for quantitating 9-carboxy-ll-nor-A-tetrahydrocannabinol in human urine as part of the process for validating an automated enzyme immunoassay for marijuana metabolites. Sample cleanup was accomplished using a mixed-mode solid-phase extraction. 9-Carboxy-ll-nor-A-tetrahydrocannabinol and the internal standard, brominated 9-carboxy-ll-nor-A9-tetrahydrocannabinol, were quantified using high-perform- ance liquid chromatography with electrochemical detection (+0.85 V). The linear range for this method is 0.0124.20 pglmL. No interference was seen for 22 drugs and metabolites. The pooled relative standard deviation is 4.1% (n=27) for the quality control samples. This method was compared to gas chromatography with mass spectrometry by linear regression analysis. The slope of the line is 1.00*0.05 (standard error), the intercept is approximately zero, the coefficient of determination is 0.994, and the standard error of the estimate is 0.006 pglmL.

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    INTRODUCTION

    Our goal was to develop a high-performance liquid chromatographic (HPLC) method for determining 9-car- ~ x y - 1 1 -nor-A9-tetrahydrocannabinol (THC-COOH) con- centrations in human urine. This was part of the process of adapting immunoassay reagents to an automated chemistry analyser. The following constraints had to be met: (1) the urine volume must not exceed 2 mL so that duplicates of expensive immunoassay urine standards could be analysed (2) the limit of quantification for THC-COOH must be approximately 10ng/mL of human urine in order to quantify the lowest expected concentrations in the urine samples; (3) the procedure must be amenable to batch analysis because of the large number of urine samples to be analysed; (4) the method must be practical and cost effective.

    Gas chromatography with mass spectrometry (GC/MS) is an excellent method for analysis of THC-COOH (Bronner and Xuy, 1992; Dixit and Dixit, 1991; Jenkins et al., 1995; Joern, 1992; Lisi et al., 1993; Liu et al., 1994; Moody et af. 1992 a, b; Wu et al., 1993, but was not selected for this application because the cost of sample analysis using MS is relatively high compared to other forms of quantitation. THC-COOH has also been quantified by high-performance liquid chromatography With electrochemical detection ( H P L a C D ) or gas chromatography with electron capture detection (GCECD). HPLCECD is a less time consuming method than GCECD because derivatization is required in

    *Author to whom correspondence should be addressed at: Center for Bioandytical Research, University of Kansas, Lawrence, KS 66047, USA.

    order to improve the signal and reduce chromatographic tailing (Maseda et a!.. 1986; Rosenfield et al., 1986, 1989). No derivatization is required prior to HPLCECD because an acidic pH is used to suppress ionization and the signal is generated by oxidation of the phenol moiety of THC- COOH.

    A significant limitation associated with previously reported HPLCECD or GCECD methods is the lack of an ideal internal standard. A variety of compounds have been used as internal standards. For example, p,p-DDT (Maseda et af., 1986), tetracosanoate (Rosenfeld ef af., 1986, 1989). cannabinol (Bourquin and Brenneisen, 1987), 4dodecylre- sorcinol (Thompson and Cone, 1987), 1 l-hydr~xy-A-tetrahydrocannabinol (Craft et al.. 1989). and n-octyl-p-hydroxybenzoate (Nakahara and Cook, 1988; Nakahara et al., 1989). These internal standards are not ideal (Nakamura et al. 1990) because they either do not have the Same basic ring structure as THC-COOH, or they are present in marijuana.

    The best internal standard for HPLC/ECD quantification would be a chemical derivative of THC-COOH that does not modify the carboxyl moiety or phenol moiety and results in a final structure identical to a compound present in marijuana. Retaining the acidic and lipophilic properties of THC-COOH would allow the use of a mixed-mode solid- phase extraction (SPF) column. The mixed-mode SPE employed here was designed to extract THC-COOH based on hydrophobic, polar and anionic interactions, and this type of SPE provides enhanced sample clean-up when compared to liquid-liquid extraction or reversed-phase SPE (Pocci er af., 1992).

    We report here the synthesis of brominated THC-COOH for use as an internal standard and validation of a HPLC/

    Received 14 November 1995 Accepted 22 February 19%

  • I62 D. H. FISHER ETAL.

    ECD method using brominated THC-COOH for internal standard quantification of THC-COOH in human urine.

    dimethyldichlorosilane in toluene for 30 rnin (Knapp, 1979). The surface was then rinsed with toluene followed by methanol. The glassware was allowed to dry at room temperature.

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    EXPERIMENTAL

    Chemicals. Chloracetic acid (99%) and triethylamine (99%) were obtained from Aldrich (Milwaukee, WI, USA). HPLC grade water, methanol, acetonitrile and tetrahydrofuran were supplied by Fisher Scientific (Pittsburgh, PA, USA). High purity helium (99%) was prepared by Medical Technical Gases (Medford, MA, USA). All other chemicals were reagent grade. d-9-Carboxy-l l -nor-A9- tetrahydrocannabinol was purchased from Alltech-Applied Science Labs, State College, PA, USA.

    HPLC system. The HPLC system consisted of a SP8800 ternary pump (Spectra-Physics. San Jose, CA, USA), a 7125 injector with a 200pL sample loop (Rheodyne, Cotati, CA, USA), a Bio- analytical Systems column (3.2 x 100 mm) packed with octadecyldimethylsilyl 3 pm silica gel (BAS, West Lafayette, IN, USA), a BAS LC4A amperometric detector, a BAS LC-44 thin- layer cell housed in a BAS CC-5 cabinet, and an Eldex CH-150 column heater (San Carlos, CA, USA), Chromatograms were recorded with a Spectra-Physics SP4270 integrator.

    Mobile phases. Mobile phase A was prepared by adding 100 mL of a 0.5 M, pH 3.0 monochloroacetic acid buffer and 1.4 mL of triethylamine to a 1 L volumetric flask. The flask was filled to the mark with a solution of 30% H,O:70% CH,OH (v/v). Mobile phase B was prepared by adding 100 mL of a 0.5 M, pH 3.0 monochloroacetic acid buffer and 1.4 mL of triethylamine to a 1 L volumetric flask. The flask was then filled to the mark with a solution of 5 % H,O:15% THF8O% CH30H (v/v/v). The mobile phases were filtered using an all-glass filtration apparatus and a Gelman Nylaflo membrane (0.20 pm x 45 mm, Fisher Scientific). Mobile phase A was stored in a tightly capped bottle in the refrigerator. Mobile phase B was partitioned equally into three storage bottles, tightly capped and stored in the refrigerator. Both mobile phases were prepared weekly.

    Chromatographic conditions. A two-foot long coil of stainless steel tubing connecting the pump to the injector, the injector and the analytical column were maintained at 40C in the column heater. The tubing connecting the analytical column to the detector was insulated with glass wool. A BAS L C 4 A amperometric detector was connected electrically in accordance with manu- facturers directions to a BAS LC-44 thin-layer cell with a dual glassy-carbon electrode housed in a BAS CC-5 cabinet. The dual glassy-carbon electrode was polished weekly in accordance with manufacturers directions. The LC4A amperomehc detector was set to +0.85 V relative to a Ag/AgCI reference electrode. The mobile phases were degassed for 10 rnin with helium before use and continuously thereafter. The mobile phase flow was set at 1.0 mllmin. The initial mobile phase composition was 90% A: 10% B. The SP8800 was programmed to linearly decrease the concentration of A to 70% in the first 15 rnin and then to 40% A in the next 15 min where the mobile phase composition was held for 5 min. At the end of each day, the column was washed with 40% H,O:60% CH,OH (v/v). the cell was washed with water and methanol and the reference electrode was stored in 3 M NaCI. The mobile phase reservoirs were tightly capped and stored overnight in the refrigerator.

    Silanization. Borosilicate glassware was silanized by allowing the surface to remain in contact with a 5% (v/v) solution of

    Standards. The following solutions were prepared in freshly voided drug-free urine preserved with 0.05% (w/v) sodium azide. The 2.0 pg/mL working solution was prepared by adding a 200 pL aliquot of a 100 pg/mL stock solution of d-9-carboxy- 1 1 -nor-A9-tetrahydrocannabinol to a silanized 10-mL volumetric flask and filling to the mark with urine. Six standards were prepared in 16 x 125 mm borosilicate test tubes before each use by diluting the2.0 Fg/mL working solution 1 5 , l:lO, 1:20, 1:40. 1:80 and 1 : 160 with an aliquot of urine such that the final total volume of each standard was 2.0 mL.

    Internal standard. The internal standard was synthesized by brominating THC-COOH in carbon tetrachloride. A 0.58 mmoV mL stock solution of Br, in CCI, was prepared before each synthesis by adding 150 p L of neat Br, to 5.0 mL of CCI, in an amber vial. A 1.16 pmoVmL solution of Br, in CCI, was then prepared by adding 10.0 p L of the 0.58 mmoVmL stock solution to 5.0 mL of CCl, in an amber vial. A 100 p L aliquot of a 100 pg/mL (0.29 pmoVmL) solution of THC-COOH was added to a 1.5 mL silanized amber vial and the methanol was removed by evapora- tion under a gentle stream of nitrogen at ambient temperature. A 100 p L aliquot of the 1.16 FmoVmL solution of Br, in CCI, was added to t