key: cord-1006645-jpb2jxgz
authors: Briones, Andrea; Martos, Gustavo; Bedu, Magali; Choteau, Tiphaine; Josephs, Ralf D.; Wielgosz, Robert I.; Ryadnov, Maxim G.
title: An SI-traceable reference material for virus-like particles
date: 2022-04-25
journal: iScience
DOI: 10.1016/j.isci.2022.104294
sha: 1adf9b2b079195db6982dcf85e11cf64dc40ac41
doc_id: 1006645
cord_uid: jpb2jxgz

A reference material for virus-like particles traceable to the International System of Units (Système International d'Unités – the SI) is reported. The material addresses the need for developing reference standards to benchmark virus-like gene delivery systems and help harmonize measurement approaches for characterization and testing. The material is a major component of synthetic polypeptide virus-like particles produced by the state-of-the-art synthetic and analytical chemistry methods used to generate gene delivery systems. The purity profile of the material is evaluated to the highest metrological order demonstrating traceability to the SI. The material adds to the emerging toolkit of reference standards for quantitative biology.

Continuous progress in nanotechnology and synthetic biology opens up new avenues for therapeutic and diagnostic applications (Mastrobattista et al., 2006; Tan et al., 2021) . Advanced therapies emerge as particular beneficiaries, with a repertoire of biomimetic materials becoming available to access intracellular processes with a nanoscale precision (Glover et al., 2005; Mitchell et al., 2021; Zhang et al., 2018) . Virus-like particles (VLPs) constitute a major type of such materials. They meet the need for non-toxic and biologically differential activities and provide effective solutions to structural uniformity by emulating the architecture of viral capsids (Frietze et al., 2016; Matsuura, 2018; Rohovie et al., 2017; Steinmetz et al., 2020) . The physical attributes of VLPs find use in diagnostics as contrast agents for tissue imaging and internal standards for virus detection in biopsies as well as in medicines manufacturing as in-process calibrators to validate the efficacy of viral clearance in downstream processes (Chung et al., 2020; Johnson et al., 2017; Schwarz and Douglas, 2015) . Traditional uses of VLPs such as vaccine platforms respond to new opportunities with the advent of RNA vaccines, exploring platforms capable of encapsulating RNA (Ho et al., 2021; Biddlecome et al., 2019) while emerging antimicrobial VLPs address the challenges of antimicrobial resistance including the targeting of intracellular pathogens (Kepiro et al., 2020; Rey et al., 2021) .

Virus-like gene delivery systems present a rapidly evolving area of gene therapy, with the number of clinical trials steadily increasing (Ginn et al., 2018) . The steady progress in the area, compounded by the lack of approved systems for systemic use, re-emphasizes the need for suitable standards, reference materials, and methods to benchmark the performance attributes of both synthetic and virus-derived gene delivery systems, and help harmonize approaches for characterization and testing (Iglesias-Ló pez et al., 2019; Faruqui et al., 2020) . SI-traceable reference materials play a decisive role in this regard as they allow us to demonstrate reproducibility and traceability of the systems in correlation with their physicochemical and biological properties (Plant et al., 2014; Coxon et al., 2019) .

One relevant type of reference materials relies on high-purity nucleic acids (Kalman et al., 2016) . These materials are well characterized, provide an effective means to evaluate the accuracy of next-generation sequencing assays, and can support the quantification of the total nucleic acid content. However, these materials fall short of providing a quantitative insight into gene delivery systems themselves: their identity, purity, and amount. Virus serotypes can be used to evaluate the particle, genome, and infectious titres of viral vectors (Ayuso et al., 2014) but these materials are multi-component, not necessarily homogeneous and their constituents are not fully characterized, which can lead to variations in measurement results (Lock et al., 2010) .

Each virus and virus-like particle assembles from multiple copies of one or more polypeptide monomers. The monomers pack around the surface of a sphere with a cubic symmetry thereby forming a regular nanoscale cage (Perlmutter and Hagan, 2015) . Therefore, the quantification of a VLP or a virus comes down to the quantification of its monomer (Burlina et al., 2006; Rakowska et al., 2014) .

Proteins and peptides with a therapeutic or diagnostic value are benchmarked against relevant reference polypeptide materials with an established traceability to the International System of Units (Systè me International d'Unité s -the SI). The first and necessary step in the development of such materials is the validation of their purity with traceability established to the SI as a measure of their physicochemical properties (Josephs et al., 2019) . These materials must contain a known mass fraction of the major component, which for VLPs is a reference monomer material. As per regulatory directives for advanced therapy medicinal products (e.g., 2009/120/EC), such as gene therapy products, a reference material should be relevant and specific to products and substances it is used to benchmark, while its physicochemical properties shall be characterized and documented. Therefore, a candidate for a reference material for VLPs must be synthetically accessible and able to predictably assemble into VLPs, encapsulate, and transfer nucleic acids into human cells and be devoid of the unwanted effects of replication-competent viruses. Here, we report such a material, with its purity established with traceability to the SI.

The material under study, which meets the outlined requirements for a candidate reference material, is based on the triskelion component of synthetic peptide capsids designed as virus-like icosahedra reported elsewhere (De Santis et al., 2017) . This triskelion is synthetically accessible, predictably assembles into VLPs, which encapsulate and transfer genes into human cells and are devoid of the adverse effects typical of viruses (De Santis et al., 2017) . The triskelion supports a C 3 rotational symmetry in the assembly of the capsids and is cationic. Therefore, it is referred to as C 3 + (Figure 1 ). Figure 1. Virus-like particle material and its major component: C 3 -triskelion peptide (A) A molecular model of the C 3 -triskelion peptide (blue) in combination with its assembly partner peptide (red) (PDB entry 4DMD rendered by Macromodel Schrö dinger). Each subunit of the triskelion corresponds to the altitude of an equilateral triangle. The peptide adopts a 3-fold symmetry (C 3 ) matching that of triangular faces in an icosahedron, assembling into a capsid. (B) A molecular model of T = 4 icosahedron assembled from the C 3 -triskelions. For clarity, only one 5-fold axis is shown in color.

(C) A molecular model of one arm of the triskelion (blue), its corresponding sequence, and the chemical structure (box). In the sequence, lysine residues are highlighted in blue, leucines and isoleucines are in orange. iScience Article

The C 3 + peptide was chemically synthesized, purified by ultra-performance liquid chromatography (UPLC), and lyophilized to give rise to the C 3 + material. The purity of the purified peptide estimated by LC-UV from the relative peak area response was above 98%. The purity of the peptide was then assessed against primary reference calibrants (amino acids and peptides with certified purity traceable to the SI with associated uncertainty) through an uninterrupted chain of calibrations including the associated uncertainty evaluations to establish the traceability of the mass fraction value.

The reference measurement procedure used to characterize the material has been validated for a range of peptide and protein analytes Little et al., 2017; Stoppacher et al., 2013; Burkitt et al., 2008) . The purity assignment by the mass balance approach is achieved by employing a combination of analytical techniques to quantify the mass fraction content of all impurities present and estimate the mass fraction of the main peptide component . Thus, the purity value calculated was cross-validated with two orthogonal methods based on amino acid analysis (AAA) and quantitative nuclear magnetic resonance (qNMR).

Mass balance approach to assign the purity of the material Metrological traceability and measurement of uncertainty are prerequisites for ensuring that substances comply with international quality control regulations. In clinical chemistry, drug development, and diagnostics, purity is understood as a mass fraction of a major component that is present in the material of interest. The mass fraction for each of the impurities in the material is determined and the summation of these subtracted from the upper limit of 100% (1000 mg/g).

In this study, we utilized the mass balance method developed at the Bureau International des Poids et Mesures (BIPM) to assign the purity of the major (peptide) component in the C 3 + material Josephs et al., 2018) . Under this approach, the material of interest is assessed and quantified in terms of the following:

-related impurities (w RS )

These are modified forms of the peptide component in the material, which can arise from side reactions during chemical synthesis, deletions, or insertions in the amino acid sequence or from the compromised stability of the final product. These are assessed by liquid chromatography-mass spectrometry (LC-MS).

-water (w W )

An SI-traceable Karl Fisher (KF) coulometric titration method with associated water standards is a principal method to determine water content in the material. The results obtained by KF are cross-validated using microanalysis (% C, H, N content).

-residual organic solvent (total volatile organic compounds) (w OS )

Residual organic solvents can be determined by direct injection of a peptide solution into a gas chromatography-mass spectrometer (GC-MS) or by 1 H qNMR.

-non-volatiles (w NV ), with the potential contributions from inorganic impurities and non-volatile organics.

Ion chromatography (IC) is used to quantify these impurities in ionic forms including trifluoroacetate (TFA), other anions such as formate, nitrate, oxalate, chloride, acetate, phosphate, and sulfate and cations such as ammonium, magnesium, calcium, potassium, and sodium. The measurements are performed following calibration using relevant anion or cation reference materials and typically in combination with other approaches. For example, to measure the fraction of TFA as a by-product of chemical synthesis, one can apply an orthogonal approach by cross-correlating the data with that obtained by 19 F-NMR, microanalysis (% N, C, H content), or TGA for the total content of non-volatile inorganic impurities.

iScience 25, 104294, May 20, 2022 3 iScience Article

The identification and mass fraction assignments of impurities for the C 3 + material was performed using such an approach, with each method calibrated with standards of certified purity, ensuring that the results are traceable to the SI.

The assigned mass fraction values for all impurity types are presented in Equation 1, which allows to quantify the mass fraction of the peptide (w P ) in mg g À1 .

and w NV as mass fractions in mg g À1 of related structural impurities, water, organic solvents, and non-volatiles, respectively.

In addition, the combined standard uncertainty of peptide purity is calculated by a quadratic combination of the standard uncertainties of each impurity assignment.

In the cases where there is no statistically significant difference between the blank control and sample, the assigned value is zero with an associated uncertainty corresponding to the limit of detection of the method.

The mass fraction of non-volatile impurities in the C 3 + material such as TFA was determined by IC and 19 F-qNMR. For IC measurements, oxytocin was used as a peptide reference control, while external instrument calibrations were performed with appropriate reference materials (see STAR Methods) . The results were obtained for two series of measurements performed on different days.

IC revealed TFA as a significant component in the C 3 + material, with lower signals (<0.1% of that for TFA) observed for acetate, formate, chloride, nitrate, and sulfate ions ( Figure S1A ). The TFA mass fraction value determined by IC was 253 G 16 mg g À1 . This value agreed with the TFA mass fraction determined by 19 F qNMR (267.0 G 2.2 mg g À1 ). The NMR signal used for TFA quantification was the singlet at À76.6 ppm, along with its four asymmetric satellite peaks due to the 19 F coupling to 13 C present either in the a (large J coupling) or b position (small J coupling) of the TFA molecule ( Figure S1B ). IC results also revealed small amounts of cations (mainly Na + , K + , and Ca 2+ ) corresponding to 2.01 G 0.18 mg g À1 .

Signals at chemical shift regions characteristic of residual solvents were searched for in the 1 H NMR spectra as well. Only some trace levels of ethanol and dimethyl sulfoxide could be ascertained (not shown).

Water content was measured by Karl Fischer titration (KFT), which indicated the mass fraction of water (w W ) in the material to be 62.3 G 15 mg/g (k = 2) ( Figure S2 ). Table 1 shows mass fraction assignments and associated expanded uncertainties for each of the contributing impurities and the pure peptide in the material.

After subtracting impurity contributions from the upper limit of 100% or 1000 mg g À1 , the peptide component mass fraction in the material was 669 G 15 mg g À1 . The mass fractions of elemental carbon, hydrogen, and nitrogen determined by elemental analysis were compared to the expected mass fraction values as determined from the mass balance approach. 

The purity values for the peptide component by AAA-IDMS were calculated from mass fractions of leucine and isoleucine residues. The two amino acid residues are the constituent amino acids of the C 3 + material, which are stable under the conditions of complete hydrolysis and yield excellent recovery rates for quantification. This is supported by the results of key comparison studies , under the Consultative Committee for Amount of Substance (CCQM). Importantly, for both amino acid residues calibrator, amino acid materials with assigned SI-traceable purity values are available, which allowed for accurate and traceable quantification of the material. The values for leucine were slightly higher (657 G 14 mg/ g) than those for isoleucine (614 G 56 mg/g), averaging the final purity value to 636 G 45 mg/g (Figure 2A ).

Given the variations between the two residues, different contributions of uncertainty sources to the final purity value were assessed ( Figure 2B ). For leucine the major uncertainty source was the intermediate precision, u(IntPre), which accounts for variability in the efficacy of hydrolysis and the signal integrations of mass spectra for injection replicates. Other minor uncertainty contributors are from weighing and the purity of the amino acid standards used in the analysis, u(IDMS) ( Figure 2B ).

In accordance with the AAA-IDMS data, analyses by 1 H qNMR returned the value of 639 G 16 mg g À1-(k = 2) for the mass fraction of the peptide in the material. The calculated value and uncertainty were based on the resonance signals of the lysine ε-CH 2 and leucine and isoleucine methyl protons. Proton assignments in the peptide were performed using homonuclear correlation spectroscopy (COSY), total correlation spectroscopy (TOCSY), and by comparing chemical shifts obtained to those of free amino acids in solution. Spectral regions for lysine ε-CH 2 protons (labeled D) and for leucine and isoleucine -CH 3 protons (labeled B and C) were integrated for comparison and to display relative proton stoichiometry (Table 3 and Figure 3 ). The peptide was measured against an internal standard.

Proton-proton correlations in COSY and TOCSY experiments are indicated in brackets ( Figure 3A ). BTMSB-F 4 was used as the internal standard and was chosen to perform 1 H and 19 F qNMR measurements on the same samples (Westwood et al., 2019) . The mass fraction of the peptide was calculated based on lysine ε-methylene and leucine and isoleucine methyl 1 H NMR signals, while the TFA mass fraction was calculated based on the trifluomethyl 19 F NMR signal.

The purity mass fraction values of 636 G 45 mg g À1 by AAA-IDMS and 639 G 16 mg/g by 1 H qNMR were averaged to a total peptide mass fraction of 638 G 24 mg g À1 . Related structure impurities were investigated by LC-hrMS in order to rule out the presence of major peptide components other than C 3 + peptide. Despite numerous efforts to separate chromatographically C 3 + peptide from minor co-eluting species of iScience Article similar mass (G5%), only one impurity could be clearly differentiated from in-source or adduct ions (Figure S3 ). This impurity of mass 7918.31 Da was attributed to a modified C 3 + peptide that lacked 3 Lys residues and its mass fraction was estimated to be 18 mg g À1 with an asymmetric expanded uncertainty of +21 mg g À1 and -18 mg g À1 . In the absence of an appropriate standard, this value remained indicative only and was not used to correct the calculated total peptide mass fraction.

Taking into consideration the expanded uncertainty values for different measurements, it can be concluded that the total peptide mass fraction value calculated by the mass balance approach agreed with the combined value calculated through orthogonal methods based on isotope dilution amino acid analysis and 1 H qNMR ( Figure 3C ).

The field of VLPs is burgeoning with many systems available commercially. The applications range from research tool kits to therapeutics approved for clinic or undergoing clinical trials. VLPs developed as vaccines against different viruses, from hepatitis B virus to SARS-CoV-2, have been licensed and commercialized (Van Bö mmel and Berg, 2021; Knoll and Wonodi, 2020), with at least over 100 vaccines available against influenza alone (Quan et al., 2016) . Similarly, in gene therapy, virus-derived and VLP-based therapeutics continue to dominate clinical trials (Ginn et al., 2018) . However, the growing number of commercial systems demands comparability assessments from early stages, i.e., R&D, to manufacturing. The need is further echoed by existing and emerging requirements regulatory policies set up for vendors to demonstrate the traceability of their products. Given that VLPs vary in composition, there remain difficulties in the comparability of their physicochemical properties against the highest point of reference, i.e., SI-traceable reference materials, which is lacking. Therefore, the first SI reference materials should be developed to benchmark the physicochemical properties of VLPs to help address variabilities in their composition.

Among the key drivers to develop synthetic VLPs for intracellular delivery, one is to overcome the inherent drawbacks of viruses including limited loading capacities and insertional mutagenesis. Designs from the bottom up allow better predictability for relating structure with activity and increasing the complexity of next generation designs to be endowed with specialist functions. Emulating the virus architecture appears to be an obvious route for designing VLP systems as it allows us to capitalize on the advantageous properties of viruses such as morphological uniformity and modularity. Top-down designs of virus-derived systems are equally valuable as they build upon bio-functional optimizations of the virus architecture. However, irrespective of apparent differences between bottom-up and top-down designs, quantification and traceability are the ultimate quality attributes of all gene delivery systems. SI-traceable reference materials iScience Article provide an optimal solution in this regard and help meet emerging requirements for commercial vendors to demonstrate traceability for their products and technologies. As a rule of thumb, the purity of such reference materials must be demonstrated to the highest metrological order. In this report, we described the characterization of a synthetic reference material demonstrating its traceability to the SI. The material was produced by the state-of-the-art synthetic and analytical approaches used by the developers and manufacturers of commercial systems, thus ensuring compatibility with their processes and final products. Impurities of the material reported are typical of synthetic materials and hence the obtained impurity profile can be used to benchmark those of commercial systems. Impurities were quantified and subtracted from the total sample mass to obtain the content of the major component, i.e. the C 3 + peptide. The mass fraction of the total peptide content was 669 G 15 mg g À1 based on the mass balance approach, which was cross-validated using an orthogonal approach consisting in the combination of qNMR and isotope dilution amino acid analysis that resulted in a confirmatory value of 638 G 24 mg g À1 . The reported reference material can be used for the characterization and validation of native and synthetic virus-like particles as well as other peptide-and protein-based drug delivery systems. The applicability of the material is multifold. For example, it can be used to confirm the purity of a commercial VLP, or virus-derived products as required by the manufacturer or a regulatory body or can help quantify the encapsulation efficacy of a designed gene delivery system. Often, recombinantly prepared VLPs contain nucleic acids, either via nonspecific encapsulation of host nucleic acids or via designed encapsulation. The challenge here is that the average amount of nucleic acids per VLP remains uncertain. With its proven ability to encapsulate nucleic acids upon assembly into a VLP (De Santis et al., 2017) , the reported material can be adapted to establish the ratio of loaded versus empty VLP particles and probe the stoichiometry between protein and gene constituents. All such validations can be performed in different sample matrices, in vitro and in cell extracts, thus providing an SI-traceable evaluation route for the amount of a desired material in target media. The material, the first of the type to the best of our knowledge, adds to the emerging toolkit of reference standards for quantitative biology.

The study introduced an SI-traceable reference material for virus-like particles as gene delivery systems. It can also be used for related applications which require the quantification of an exogenous material in a given biological matrix. Biomaterials developed for immunoengineering and engineering biology are exemplar areas of material dissemination. Practical considerations for benchmarking experimental gene delivery systems or other systems, e.g. vaccines, are not discussed in the study. The study also does not address the promise of the material for correlative imaging applications, e.g., the monitoring of transfection in live cells, the measurement and trafficking of VLPs in vivo, or the quantification of nucleic acid content per VLP, which would require orthogonal measurements, e.g., PCR, and complementary reference materials, i.e., nucleic acids. These types of analysis merit a series of follow-up investigations focusing on the development of appropriate extraction and measurement protocols and associated uncertainty evaluations.

Detailed methods are provided in the online version of this paper and include the following: 

We acknowledge funding from the UK's Industrial Strategy Challenge Fund and thank Prof Paul Brewer for the critical assessment of the work. Table 3 ) and are integrated to display the relative proton stoichiometry.

(C) Comparison of results of the mass balance method and AAA & qNMR. Where, the value obtained for the C 3 + peptide in the mass balance method was of 669 G 15 mg/g (k = 2) and the averaged value obtained for the measurements with the AAA & qNMR was 638 G 24 mg/g (k = 2). Error bars are expanded uncertainties (k = 2).

Ultrapure water (18.2 MU$cm-1 ) was produced using a Milli-Q system from Millipore (Molsheim, France). The C 3 + peptide was purchased from CEM (North Carolina, USA). Isotopically labelled amino acids L-2Ile-13 C 6 and L-Leu-13 C 6 -15 N and naturally occurring L-Ile and L-Leu were characterised in-house for purity after the purchase as per the key resources iScience Article Data and code availability d All data supporting the measurements carried on the C 3 + peptide can be found within the manuscript and the supplemental information or can be shared by the lead contact upon request.

d The paper does not report an original code. All software and pipelines used in the study are listed and referenced in the key resources table.

d Any additional information required to reanalyze the data reported in this paper is available from the lead contact upon request

An LC series 1200 instrument (Agilent, Waldbronn, Germany) consisting of a model G1379B degasser, G1312B binary pump SL, G1367C autosampler SL, and G1316B column thermostat SL was employed for LC-hrMS/MS analysis. The LC was coupled online to an LTQ-Orbitrap XL high-resolution tandem mass spectrometer (Thermo Electron, Bremen, Germany) fitted with a heated electrospray ionization (HESI) source. For AAA by IDMS, a microwave hydrolysis system (CEM, Saclay, France) and a rotational vacuum concentrator connected to a freeze-dryer system (Christ, Germany) were used to hydrolyse and concentrate samples, respectively. An Exion LC coupled online to a QTRAP 6500+ mass spectrometer (AB Sciex, Les Ulis, France) fitted to an electrospray ionisation (ESI) source was used for the detection of amino acids. A 930 compact IC flex and 863 compact autosampler (Metrohm AG, Switzerland) and a Metrohm Titrando 851 coupled to a Metrohm 874 Oven sample processor were used for IC and KF titration, respectively. Elemental analysis was performed using a Vario Micro Cube Elemental Analyser (Elementar, Lyon, France), whereas NMR measurements were performed on an ECS-400 MHz NMR instrument equipped with a direct type (Royal) automatic tuning probe (JEOL, Tokyo, Japan).

Chromatographic separations were performed using a Jupiter column, 250 mm 3 4.6 mm, 5mm, 300 Å (Phenomenex, Le Pecq, France). After optimisation, the following conditions were used for all subsequent LC-hrMS/MS experiments with C 3 + peptide solutions: flow rate at 1 mL/min, the column thermostat temperature at 38 C, the autosampler rack temperature at 5 C, and the injection volume at 10 mL. Eluent A was water containing 0.1% formic acid (v/v) and eluent B was AcN containing 0.1% formic acid (v/v). The LC gradient programme used was as follows: 10% eluent B (5 min hold), gradient to 30% eluent B in 55.1 min, gradient to 90% B in 10 s (5 min hold), back to 30% B in 10 s, and gradient back to 10% B in 10 min, and hold for 10 min (total method duration 82 min).

The LTQ-Orbitrap-XL MS instrument was operated in a positive ionisation mode. The spray voltage was set at +4 kV. The flow rate sheath gas was 90 a.u. and the flow rate of the auxiliary gas was 5 a.u. Capillary temperature was 370 C and the tube lens was set at 105 V. The full scan detection mode at 30000 resolution and dependent MS/MS (HCD activation) scans at 15000 resolution targeting the most intense ions were used across the chromatographic elution.

An internal standard (IS) was prepared in ultrapure water containing the 13 C isotopically labelled amino acids. Similarly, a standard mixture prepared in ultrapure water contained the unlabelled amino acid reference materials of known purity. The IS was added to the standard mixture and to the C 3+ peptide solution to prepare the calibration blend and the sample blend, respectively. The calibration blend was prepared so that it contained the same amount of unlabelled and labelled amino acids as expected in the sample blend after acid hydrolysis (exact matching). Furthermore, the amount of IS was adjusted so as to produce the same signal intensity as the unlabelled amino acids in the mass spectrometer during LC-MS/MS analysis. The blends were prepared in glass microvials and volumetric additions were controlled gravimetrically.

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After optimization, the following conditions were used for all LC-MS/MS experiments for AAA: flow rate at 1 mL/min, the column thermostat temperature at 25 C, the autosampler rack temperature at 5 C, and the injection volume at 10 mL. The eluent A consisted of AcN/water (35v/65v) and eluent B was water/AcN (35v/65v) with 1% formic acid. The LC gradient program was as follows: 60% eluent B (1 min hold), gradient to 100% eluent B in 31 min (3 min hold)

The instrument was operated in a positive mode (ESI+). The ion spray voltage was set at +5.5 kV with ion source temperature at 500 C. Ion source gas and curtain gas were set up at 50 and 25, respectively. The instrument was optimized by direct infusion of single LC standards of Ile, Leu, Phe, Pro and Val until protonation was observed for all. Ions were detected and monitored by Multiple Reaction Monitoring (MRM) approach. Parameters for each amino acid and their internal standards are listed in Table S2 . Data acquisition and processing was performed using Analyst software version 1.7.1 (SCIEX). Amino acid concentrations were calculated comparing original amino acid ( 12 C-AA) peak area to isotope labelled internal standards ( 13 C-AA) ratio from sample and calibrant blends as per Equation 3:) W x and W z are AA mass fraction in the sample solution (mg/g) and mass fraction of the standard AA solution added to the calibrant blend (mg/g). The terms m z , m yc , m y and m x indicate the mass of standard AA solution added to the calibrant blend (g), the mass of labelled AA solution added to the calibration blend (g), the mass of labelled AA solution to the sample blend (g) and the mass of sample solution added to the sample blend (g). R 0 B is the analyte/IS ratio measured in the sample blend and R 0 Bc is the analyte/IS ratio measured in the calibration blend.

Two independent 1000 mg/g C 3 + peptide solutions were prepared and diluted ten times in mobile phase and analyzed by ion chromatography on two different days. Standard solutions were prepared from concentrated sodium trifluoroacetate (Na + TFA À ) (>99%) supplied by Sigma Aldrich Chemicals. TFA and anions content were determined using ion chromatography system composed of 930 compact IC flex and 863 compact autosampler (Metrohm AG, Switzerland) coupled with suppressed conductivity detection performed with 0.05 M sulfuric acid regenerated suppressor module. Metrosep A Supp 5, 250 3 4.0 mm analytical anions exchange (Metrohm AG, Switzerland) with sodium carbonate/bicarbonate (3.2 mM/1mM) eluent flowing at 0.7 mL/min was used at 30 C.

KF titration was performed using a Titrando 851 titrator instrument (Metrohm, Herisau, Switzerland), coupled to a Metrohm 874 oven sample processor and operated by the Tiamo (version 2.3) software. The C 3 + peptide samples (between 2 and 6 mg) were placed in the oven and the released water was transferred to the titrator cell via a stream of dried, high purity nitrogen carrier gas. The coulometric determinations were carried out with the KF titration reagents HYDRANALä Coulomat CG-K and Coulomat AG-Oven (VWR, Fontenay-sous-Bois, France). Water content was calculated after correction of water determined in blank samples. A lactose standard 5% (Merck, France) was used as a control sample and the SI traceability of the results was established through calibration with NIST SRM 2890 standard (NIST, MD, USA).

iScience 25, 104294, May 20, 2022 iScience Article

A temperature gradient experiment was run to define the optimal oven temperature for the sample. The release of water was observed up to 180 C and the sample completely degraded at 200 C. The Karl Fisher titrator was then prepared by purging with dried carrier gas to remove any water traces. After the determination of the blank value, the samples were analyzed using the optimized method ( Figure S2 ). A minimum sample intake of 2.3 mg was used for each analysis. The average mass fraction of water was 62.3 G 7.4 mg/g (k = 2).

The elemental analysis was performed using a Vario Micro elemental analyser (Elementar Analysensysteme GmbH, Langenselbold, Germany). The analyser was calibrated using standard samples of acetanilid (Merck, France) ranging from 1 to 10 mg. Subsequently, four C 3 + samples were mixed with magnesium oxide (Merck, France) in small tin crucibles, sealed and placed into the furnace for high-temperature oxygen combustion, followed by gas chromatography and thermal conductivity detection.

The peptide material and the internal standard (IS) 2,3,5,6-tetrafluoro-1,4-bis(trimethylsilyl)-benzene (BTMSB-F 4 , NMIJ Certified Reference Material 4602a) were accurately weighed in an ultra-micro balance XP2U (Mettler Toledo), co-dissolved in deuterated methanol, transferred to an NMR tube and analysed first by 1 H qNMR and then by 19 F qNMR. Four replicate spectra were acquired for each of the two prepared sample mixtures. The determined 90 pulse widths were 6.2 and 14.4 ms for 1 H and 19 F, respectively. The longest T1 relaxation times were 2.17 and 2.8 s corresponding to the internal standards in 1 H and 19 F NMR, respectively. The repetition time was set to 15 3 T1 and the number of scans was 128. The transmitter offsets were set at the midpoint between the quantification and internal standard signals and 13 C decoupling and spinning were not used. Post-acquisition data processing was performed using MestReNova software version 14 (Mestrelab Research).The purity value was calculated using Equation 4 and its uncertainty corresponded to the square root of the sum of the squared uncertainties associated to each of the intervening factors in the equation (Westwood et al., 2019) . (Equation 4) where IStd, NStd, MStd, mStd and wStd are the signal area, number of protons or fluorines, molecular weight, weighed mass and mass fraction of the IS, respectively. The terms Ix, Nx, Mx, mx and wx indicate the signal area, number of protons or fluorines, molecular weight, weighed mass and mass fraction of the analyte, respectively.