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In response to an earlier workshop covering the pros and cons of quantification below the LLOQ (BLQ) the author reviews the topics discussed from the bioanalytical standpoint. Important considerations for estimating concentrations below the LLOQ include: method signal-to-noise, baseline shape and condition, close lying interference peaks (especially for protein methods), matrix effect, adsorption and stability of the analyte at low concentrations and carryover. These methodological issues are discussed as possible contributors to inaccuracy in BLQ estimations, and appropriate cautions are provided via examples. A proposed method for the evaluation of BLQ estimations utilizes extended incurred sample reanalysis analysis where BLQ samples or spiked simulated samples are analyzed with quality controls and standards in addition to those in the original study. Generally, BLQ estimations are discouraged, with the recommendation that any extrapolations should be done in close collaboration between the pharmacokinetic (PK) and bioanalytical scientists in consultation with the regulatory agency.

A refinement of protein LC–MS bioanalysis is to use predigestion immunoaffinity capture to extract the drug from matrix prior to digestion. Because of their increased sensitivity, such hybrid assays have been successfully validated and applied to a number of clinical studies; however, they can also be subject to potential interferences from antidrug antibodies, circulating ligands or other matrix components specific to patient populations and/or dosed subjects. The purpose of this paper is to describe validation experiments that measure immunocapture efficiency, digestion efficiency, matrix effect and selectivity/specificity that can be used during method optimization and validation to test the resistance of the method to these potential interferences. The designs and benefits of these experiments are discussed in this report using an actual assay case study.

This paper highlights the recommendations of a group of industry scientists in validating regulated bioanalytical LC–MS/MS methods for protein therapeutics in a 2015 AAPSJ White Paper. This group recommends that most of the same precision and accuracy validation criteria used for ligand-binding assays (LBAs) be applied to LC–MS/MS-based assays where proteins are quantified using the LC–MS/MS signal from a surrogate peptide after proteolytic digestion (PrD-LCMS methods). PrD-LCMS methods are generally more complex than small molecule LC–MS/MS assays and may often include LBA procedures, leading to the recommendation for a combination of chromatographic and LBA validation strategies and appropriate acceptance criteria. Several key aspects of this bioanalytical approach that are discussed in the White Paper are treated here in additional detail. These topics include selectivity/specificity, matrix effect, digestion efficiency, stability and critical reagent considerations.

This paper represents the consensus views of a cross-section of companies and organizations from the USA and Canada regarding the validation and application of liquid chromatography tandem mass spectrometry (LC-MS/MS) methods for bioanalysis of protein biotherapeutics in regulated studies. It was prepared under the auspices of the AAPS Bioanalytical Focus Group’s Protein LC-MS Bioanalysis Subteam and is intended to serve as a guide to drive harmonization of best practices within the bioanalytical community and provide regulators with an overview of current industry thinking on applying LC-MS/MS technology for protein bioanalysis. For simplicity, the scope was limited to the most common current approach in which the protein is indirectly quantified using LC-MS/MS measurement of one or more of its surrogate peptide(s) produced by proteolytic digestion. Within this context, we considered a range of sample preparation approaches from simple in-matrix protein denaturation and digestion to complex procedures involving affinity capture enrichment. Consideration was given to the method validation experiments normally associated with traditional LC-MS/MS and ligand-binding assays. Our collective experience, thus far, is that LC-MS/MS methods for protein bioanalysis require different development and validation considerations than those used for small molecules. The method development and validation plans need to be tailored to the particular assay format being established, taking into account a number of important factors: the intended use of the assay, the test species or study population, the characteristics of the protein biotherapeutic and its similarity to endogenous proteins, potential interferences, as well as the nature, quality, and availability of reference and internal standard materials.

Background There are more than 100 protein and peptide drugs currently approved by the US FDA and now over 100 more are currently in active development by pharmaceutical companies worldwide [1]. The quantification of protein therapeutics has traditionally relied upon ligand-binding assays (LBAs). Such assays can be very sensitive and selective if properly developed using appropriate reagents, but are nevertheless susceptible to interferences due to circulating ligands, antidrug antibodies (ADAs), cross reactions and various forms of non-specific binding. LC– MS/MS analysis has emerged as an effective quantitative tool for protein bioanalysis. Of particular interest is LC–MS/MS analysis of therapeutic proteins via quantification of unique surrogate peptides that are produced by enzymatic digestion, a technique that is being widely used [1–4]. For simplicity, we will call this type of analysis protein digestion LC–MS/MS (PrD-LC–MS). PrD-LC– MS can be used as an alternative and supplemental approach to LBAs, and this has been extensively discussed in recent years [1–4]. Such LC–MS/MS methods, where the protein biotherapeutic is digested directly in the biomatrix prior to LC–MS/MS, can provide bioanalytical data with low interference from ADAs and other circulating ligands [5]. These methods can yield more representative quantification of total drug, but they may have limited sensitivity. Where higher sensitivity has been required, analyte enrichment or affinity capture concentration steps can be added either before [6] or after [7] proteolytic digestion. These enrichment methods can improve sensitivity by eliminating background signals either from the biomatrix itself or from the digest prior to peptide LC–MS/MS. As the methodology for PrD-LC–MS matures, there will be an increased need to use these assays in a regulated environment, both for good laboratory practice (GLP) toxicology studies and for regulated sample bioanalysis in clinical trials. Neither the recent EMA guidance [8], nor the FDA draft Bioanalytical Method Validation (BMV) guidance [9] has specifically discussed the validation of PrD-LC–MS or its application to regulated bioanalysis. Several questions need to be addressed for any regulated PrD-LC–MS assay validation

This paper was developed with the support of the International Consortium for Innovation and Quality in Pharmaceutical Development (IQ). IQ is a not-for-profit organization of pharmaceutical and biotechnology companies with a mission of advancing science-based and scientifically driven standards and regulations for pharmaceutical and biotechnology products worldwide. Within the IQ, various working groups (WG) have been formed, where the microsampling WG is committed to providing a scientific forum for the advancement of both wet and dry microsampling techniques within the pharmaceutical industry. This first output from the microsampling WG is to summarize and reflect on the current knowledge and opinions on DBS sampling, to stimulate discussion, and to encourage future creative applications of DBS sampling. Dried blood spot (DBS) sampling has established itself as an innovative sampling technique where wet blood is spotted onto absorbent paper or other paper materials and allowed to dry (1–4). DBS offers several potential benefits inherent to the technique, namely a low blood volume, simplified blood sample collection (5), and convenient sample storage and transfer. In certain applications, DBS sampling has been shown to stabilize certain analytes or metabolites without the addition of chemical modifiers (6–9). DBS has been routinely applied for decades in neonatal screening for phenylketonuria and other congenital metabolic disorders (10). The utility of DBS sampling has also been demonstrated for therapeutic drug monitoring (11) and for epidemiological studies (e.g., HIV and HBV detection/monitoring) (12) due to the practical advantages along with simplified sample collection and handling procedures. Finally, DBS can also be used for quantitative biomarker (PD) assessment from blood, where appropriate. However, the technique is relatively new to the pharmaceutical industry and to government regulators overseeing new drug applications. Nevertheless, over the past 5 to 7 years, the technique has been extensively evaluated for quantifying drug exposure in nonclinical and/or clinical studies in various stages of drug discovery and development. The ease to collect, transfer, store, and process small volumes of blood samples has generated considerable interest in providing utility in volume-limited situations (e.g., small rodent, human pediatric studies) for toxicokinetic (TK), pharmacokinetic (PK), or pharmacodynamic (PD) sampling. Discovery and nonclinical studies Rodent animal models are typically employed in these studies. The reduced blood volumes required for DBS can enable serial bleeding and, consequently, elimination of satellite animal groups and reduction of compound use. The ability to eliminate the satellite animal groups enables the assessment of exposure and toxic effects within the same animal. Studies involving expensive animal models (i.e., transgenic mice, knock-out mice, humanized mice, etc.) further highlight a persuasive scientific and economic case for DBS sampling since a complete pharmacokinetic profile can be obtained from a single study animal without the need for extra rodents merely for generating exposure data. These are perfectly in line with the principles of the 3Rs: reduction, refinement, and replacement of humane animal research (13–15). With greater emphasis from the regulatory authorities to study new drugs for infants, neonates, and pediatric populations, the requirement to conduct associated nonclinical juvenile rodent toxicity studies serves as an ideal scenario where the advantage of low blood volume in DBS sampling is undeniable. Although the advantages of DBS heavily favor rodent studies, it can also be used to refine non-rodent studies.

The detection of tetracyclines in HPLC by sensitized Europium phosphorescence has been reinvestigated using a dedicated LC detector with time-resolved luminescence capability. A micellar Eu3+ post column reagent was developed which contained 1% Triton X-100 and 200uM tri-n-octyl phosphine oxide buffered at pH 10.5. This reagent provided optimized time-resolved detection and was found to be compatible with a several mobile phases used in reversed phase chromatography of tetracyclines. The sensitivity and quantitative linearity of the technique was determined using standard fluorometric and time-resolved modes of detection with both grating and filter emission monochromation. Peak areas were linear with concentration from 2 ug on column to the limit of detection. Subnanogram limits of detection were obtained for both tetracycline and oxytetracycline. The relative sensitivity of the technique for compounds tested was oxytetracycline=tetracycline > doxycycline > chlortetracycline > minocycline. The h...

A simple, rapid and sensitive LC-MS/MS bioanalytical method has been developed to simultaneously quantify Camptosar (CPT-11) and its active metabolite, SN-38, in mouse plasma and tissues. A single step protein precipitation with acetonitrile in 96-well plates was used for sample preparation. Camptothecin (CPT) was used as the internal standard. Fast separation of SN-38, CPT-11 and CPT was carried out isocratically on a C18, 2 mm x 50 mm, 5 microm HPLC column with a mobile phase containing acetonitrile and 20 mM ammonium acetate (pH 3.5) and a 2.5 min chromatographic run time. The API 4000 MS/MS system was operated in positive ionization multiple reaction monitoring mode, and the transitions for SN-38, CPT-11 and CPT were 393.4 --> 349.3, 587.6 --> 167.2 and 349.3 --> 305.3, respectively. The SN-38 and CPT-11 concentrations in samples were calculated from a standard curve of peak area ratios of the analyte to that of the internal standard using a 1/chi2 weighted linear regression. The quantitation limit of 0.5 ng/mL was achieved by using a low sample volume (100 microL) of plasma or tissue homogenates. The assay was linear over the concentration range of 0.5-500 ng/mL with acceptable precision and accuracy. The method was used for the quantification of CPT-11 and SN-38 in plasma and tissues to support a preclinical pharmacokinetics and tissue distribution study of CPT-11 in mice.

An LC-MS/MS method was developed to quantify an antisense oligonucleotide against Raf-1 expression (rafAON) in monkey and mouse plasma and in mouse tissue homogenates from animals dosed with a liposome-entrapped rafAON easy-to-use formulation (LErafAON-ETU) intended for use as an antineoplastic agent. RafAON was extracted from mouse and monkey plasma using solid-phase extraction. Tissues were homogenized and sample cleanup was achieved by protein precipitation. RafAON and the internal standard (IS) were separated on a Hamilton PRP-1 column and quantified by tandem mass spectrometry using an electrospray source in negative ion mode. The total run time was 4.0 min. The peak areas of two rafAON transitions were summed and plotted against the peak area of an IS transition to generate the standard curve. In monkey plasma the linear range was 50-10,000 ng/mL, and in mouse plasma it was 25-5000 ng/mL. The lower limit of quantification was 500 ng/mL (10 microg/g tissue) in heart, kidney, liver, lung and spleen homogenates, and the standard curve was linear up to 10,000 ng/mL. Accuracy, precision and stability were evaluated and found to be acceptable in all three matrices. The assay was used to support pharmacokinetics and tissue distribution studies of LErafAON-ETU in mice and monkeys.

Levulinic acid (LA), a competitive inhibitor of δ-aminolevulinic acid (ALA) dehydratase (EC 4.2.1.24), has been used extensively in the study of ALA formation during greening. When [1-14C]LA is administered to etiolated barley (Hordeum vulgare L. var. Larker) shoots in darkness, 14CO2 is evolved. This process is accelerated when such tissues are incubated with 2 millimolar ALA or placed under continuous illumination. Label from the C-1 of LA becomes incorporated into organic acids, amino acids, sugars, lipids, and proteins during a 4-hour incubation in darkness or in the light. This metabolism is discussed in relation to the use of LA as a tool in the study of chlorophyll synthesis in higher plants.

A pool of chlorophyllide b has been detected in greening cucumber cotyledons. This pool exhibited the same spectrofluorometric properties as that of Chl b in diethyl ether at 298 and 77 K (Rebeiz, C.A., Belanger, F.C., Freyssinet, G. and Saab, D.G. (1980) Biochim. Biophys. Acta 590, 234–247) but had the chromatographic mobility and solubility of a monocarboxylic phorbin. The presence of a free carboxylic group and of a formyl group in this putative chlorophyllide b pool was demonstrated by methylation with diazomethane and by its conversion into chlorophyllide b oxime upon treatment with hydroxylamine. The concentration of this chlorophyllide b pool in greening tissues was in the same range as those of the protochlorophyllide and chlorophyllide a pools. Less than 15% of the chlorophyllide b pool could have arisen from chlorophyllase activity in vitro, as confirmed by the extent of hydrolysis of 14 C-labeled Chl b added to the tissue just before extraction.

The effect of light on the levels of activity of six enzymes which are light-modulated in higher plants was examined in the photosynthetic procaryot Anacystis nidulans. Ribulose-5-phosphate kinase (EC 2.7.1.19) was found to be light-activated in vivo and dithiothreitol-activated in vitro while glucose-6-phosphate dehydrogenase (EC 1.1.1.49) was light-inactivated and dithiothreitol-inactivated. The enzymes fructose-1,6-diphosphate phosphatase (EC 3.1.3.11), sedoheptulose-1,7-diphosphate phosphatase, NAD- and NADP-linked glyceraldehyde-3-phosphate dehydrogenase (EC 1.2.1.12; EC 1.2.1.13) were not affected by light treatment of the intact algae, but sedoheptulose-diphosphate phosphatase and the glyceraldehyde-3-phosphate dehydrogenases were dithiothreitol-activated in crude extracts. Light apparently controls the activity of the reductive and oxidative pentose phosphate pathway in this photosynthetic procaryot as in higher plants, through a process which probably involves reductive modulation of enzyme activity.

The conversion of divinyl protochlorophyllide a (DV Pchlide a) (E443 F625), where E and F refer to fluorescence excitation and emission maxima respectively in ether at 77 K, into chlorophyllide a (Chlide a) (E459 F675) is reported. This reaction was demonstrated by first inducing etiolated cucumber cotyledons to accumulate DV Pchlide a (E443 F625) devoid of monovinyl (MV) contamination by a series of light/dark treatments. The accumulated DV Pchlide a (E443 F625) was then converted into Chlide a (E459 F675) by a 2.5-ms light pulse (L). The Chlide a (E459 F675) thus generated exhibited spectrofluorometric properties which differed from those of MV Chlide a (E447 F674) at 77 K and at room temperature before and after demetallation. The techniques described in this work permit the preparation of Chlide a (E459 F675) devoid of MV Chlide a contamination, for further chemical structural identification of this novel chlorophyll (Chl) precursor.

By subjecting etiolated cucumber cotyledons to three successive light/ dark treatments, the cotyledonary tissue was induced to accumulate divinyl (DV) protochlorophyllide (Pchlide). The DV Pchlide-enriched etiochloroplasts were isolated and the DV Pchlide was converted into DV chlorophyllide a (Chlide a) by irradiating the plastids with a 2.5 ms pulse of actinic white light. After a few minutes of incubation in the dark, most of the newly formed DV Chlidea was converted into monovinyl (MV) Chlide a in vitro. When etiolated cucumber cotykedons were induced to accumulate [14C]DV Pchlide and the latter was photoconverted into [14C]DV Chlide a by a 2.5 ms actinic light treatment, the [14C]DV Chlide a was converted into [14C]MV Chlide a, during a post-illumination 5-min-dark incubation period.

The in vivo oxidation of the C(4) and C(5) of 5-aminolevulinic acid (ALA) to CO(2) has been studied in etiolated barley (Hordeum vulgare L. var. Larker) leaves in darkness. The rate of (14)CO(2) evolution from leaves fed [4-(14)C]ALA is strongly inhibited by aminooxyacetate, anaerobiosis, and malonate. The rate of (14)CO(2) evolution from leaves fed [5-(14)C]ALA is also inhibited by these treatments but to a lesser extent. These results suggest that (a) one step in ALA catabolism is a transamination reaction and (b) the C(4) is oxidized to CO(2) via the tricarboxylic acid cycle to a greater extent than is the C(5).

The capacity of a particulate pea (Pisum sativum L.) leaf chloroplast system for light-modulation of enzyme activity is diminished by brief exposure to sodium sulfite and, when intact seedlings are exposed to atmosphric SO

When [2,4- 14 C]porphobilinogen (PBG) or [2 (aminomethyl),5- 14 C]PBG is administered to etiolated barley ( Hordeum vulgare L. var. Larker) leaves in darkness, label becomes incorporated into CO 2 , organic and amino acids, sugars, lipids, and proteins during a 4-hour incubation. Less than 1% of the label, however, is incorporated into porphyrins. The rate of 14 CO 2 evolution from leaves fed [2,4- 14 C]PBG is strongly inhibited by anaerobiosis but is unaffected by aminooxyacetic acid, while the rate of 14 CO 2 evolution from [2(aminomethyl),5- 14 C]PBG is strongly inhibited by aminooxyacetic acid but is not affected by anaerobiosis. These results suggest that: (a) exogenous PBG is taken up and metabolized by etiolated barley leaves; (b) PBG is not metabolized exclusively to porphyrins but can be converted to a variety of intermediary metabolites; (c) this metabolism involves reactions which are partially dependent upon O 2 and pyridoxal phosphate.

Light inactivation of glucose-6-phosphate dehydrogenase within the pea (Pisum sativum L.) leaf chloroplast has a narrow pH optimum between 7.2 and 7.4 and is NADP-sensitive. The pH optimum for dark activation is slightly lower. Inactivation apparently results in a simple decrease in maximal velocity of the chloroplastic and cytoplasmic forms of the enzyme with no concomitant change in pH optimum or K(m) (glucose 6-phosphate).